Asepsis

Asepsis Training for Veterinary Staff

Asepsis

X min read

Owners

Learn essential asepsis training for veterinary staff to prevent infections and ensure safe animal care in clinics and hospitals.

Sustainable Vet Group

Updated on

August 13, 2026

This article is for informational purposes only and is not a substitute for professional veterinary advice. Every case is unique, so always consult your veterinarian for guidance specific to your pet.

This content is intended for veterinary professionals for educational purposes. It does not replace clinical judgment or tailored advice. Always rely on your training, expertise, and the specific context of your patients.

Asepsis training in veterinary practice is not a one-time orientation event. It is a continuous program with defined curriculum, structured competency assessment, and scheduled refresher cycles.

The distinction matters because the evidence is clear: knowledge of correct aseptic technique does not reliably translate into consistent intraoperative behavior without external monitoring and feedback. Training that addresses only knowledge without building the behavioral and cultural components of correct asepsis produces limited improvement.

What this covers: The design, content, delivery, and assessment components of an effective asepsis training program for veterinary surgical staff.Who needs training: All personnel involved in surgical procedures, including surgeons, veterinary nurses, scrub technicians, circulating nurses, and ancillary staff who clean and prepare the OR.Evidence base: AJVR (2025) documented a 46.3% aseptic protocol breach rate during scrubbing, gowning, and gloving in veterinary students, with no association between breach rate and prior experience. This data indicates that experience alone does not maintain aseptic performance without structured reinforcement.Training goal: Not just knowledge of correct technique but consistent performance of correct technique under real surgical conditions, including the ability to recognize and name breaks in the sterile field.

Key takeaways

Knowledge is necessary but not sufficient: Studies consistently show that personnel who can describe correct aseptic technique still make technique errors in practice. Competency assessment must include observed performance, not just written tests.
No association exists between experience level and breach rate: AJVR 2025 found no significant difference in protocol breach rates based on prior scrub experience. Experienced staff need refresher programs as much as new staff.
The cultural component of training is as important as the technical component: Training must address the expectation that breaks will be named and corrected immediately, without hierarchy or blame.
Competency assessment should be periodic, not only at orientation: A one-time assessed training at hiring does not maintain performance over months and years of practice.
Different staff roles require different training emphasis: Surgeons, scrub technicians, circulating nurses, and OR cleaners share a common asepsis foundation but have role-specific responsibilities that training should address separately.
SSI surveillance data should feed back into training: If post-operative infection rates rise, training is one of the first corrective levers to pull.

Training curriculum: what to cover

Core content for all surgical personnel

1. Foundations of surgical asepsis

Definition and scope: sterility vs. asepsis vs. medical asepsis
The surgical site infection pathway: how bacteria enter, colonize, and cause SSI
Wound class and SSI risk stratification (clean, clean-contaminated, contaminated, dirty)
The five domains of surgical asepsis: patient prep, instrument sterilization, team preparation, OR environment, intraoperative technique

2. Hand hygiene and surgical hand antisepsis

Correct traditional scrub technique: sequence, surfaces, duration
Alcohol-based surgical hand rub (ABHR): correct application and contact time
Common failures: insufficient duration, missed surfaces, incorrect drying technique
When to re-scrub vs. when ABHR suffices between cases

3. Gowning and gloving

Closed gloving technique: step-by-step with supervised practice
Open gloving: when used and critical failure points
Gown donning without surface contamination
Double gloving: rationale and technique for orthopedic procedures

4. Patient preparation

Clipping timing and technique (immediate pre-op; clippers vs. razors)
Antiseptic agent selection by site and species
Centrifugal scrub direction and application count
Common preparation errors and their consequences

5. Sterile field principles

Boundaries of the sterile field: physical and procedural
Rules of the sterile field: what belongs, what does not
Instrument handling: passing, dropping below table level, replacement protocol
Draping: application, stability, no-reposition rule

6. OR behavior and environment

Movement in and around the sterile field
Traffic management during active procedures
OR door discipline during surgery
Talking, sneezing, and mask discipline

7. Break recognition and correction

What constitutes a break vs. an error
The designated field monitor role
Non-punitive naming and correction culture
The correct immediate response to each break category

Role-specific content

Role	Additional training focus
Surgeon	Decision-making in complex break scenarios; antibiotic prophylaxis timing
Scrub technician	Instrument table setup; sterile opening technique; instrument count protocol
Circulating nurse	Opening sterile supplies; monitoring OR entry; supporting field monitor
OR cleaner / support staff	Between-case disinfection protocols; what is and is not a sterile surface

Training delivery formats

Initial orientation training

All new surgical personnel should complete a structured orientation before participating in procedures, consisting of:

Didactic component: Lecture or self-directed module covering foundations, technique standards, and break recognition. Duration: 2 to 4 hours depending on role.
Demonstration: Supervised observation of correct scrub, gown, and glove technique by a trained observer.
Supervised practice: Repeated practice of hand antisepsis, gowning, and gloving until technique is correct without correction needed.
Assessed competency: Observed performance of a complete scrub-gown-glove sequence with structured scoring. Personnel should not participate in surgical cases without passing competency assessment.

Ongoing training and refresher cycles

Orientation training alone is insufficient to maintain performance. Refresher programs should include:

Annual competency re-assessment: Observed scrub, gown, and glove performance scored against a structured rubric
Case-specific debrief: After any case where an aseptic break is documented, a team debrief reviews what occurred and what the correct response was
SSI event review: When a post-operative SSI is identified, a structured case review examines all recorded perioperative aseptic practices
Protocol update training: When antiseptic agents, sterilization methods, or OR procedures change, training must precede implementation

For the checklist staff should follow after training, including the phase-by-phase verification tool that trained personnel use to apply their training consistently during every procedure, that guide provides the operational reference.

Competency assessment: standards and methods

What competency assessment must include

Written tests confirm knowledge. They do not confirm performance. Competency assessment in surgical asepsis must include direct observation of behavior.

Minimum competency assessment components:

Component	Method	Pass standard
Knowledge of asepsis principles	Written or oral examination	80% or higher
Surgical hand antisepsis	Observed performance with structured rubric	Zero critical errors
Gowning	Observed performance	Gown exterior not contaminated
Gloving	Observed performance (closed technique)	Bare skin not contacting glove exterior
Sterile field rules	Scenario-based questioning	Correct response to 4/5 scenarios
Break recognition	Observed or video-based identification	Identifies all presented breaks

Critical errors are those that would result in definite contamination of the sterile field: ungloved skin touching the glove exterior, gown exterior contacting the scrub suit, returning a dropped instrument to the sterile field.

Who conducts competency assessment

Assessment requires a trained observer who knows what correct technique looks like and can distinguish it from incorrect. This is not a self-assessment activity. Peer observation by another trained staff member, supervised by a senior surgeon or clinical director, is the appropriate structure.

Documenting competency

All competency assessments should be dated, signed, and filed. In the event of an SSI, documented competency records demonstrate due diligence and form part of the clinical governance record.

Building a training culture

The most consequential training outcome is not a passing score on a competency assessment. It is a surgical team that names and corrects breaks immediately, regardless of who made them, without judgment or delay.

This outcome requires explicit attention in training, not just technical skill instruction.

Elements of a correction culture that training should address:

The designated field monitor role is a legitimate function, not a policing one: Every team member should understand that the field monitor's job is patient safety, and naming a break is a clinical act, not a personal criticism.
Seniority does not protect against errors: Training should explicitly address the documented tendency for junior staff to avoid correcting senior personnel. The contamination consequences of a missed break are identical regardless of who made it.
Immediate correction is always the right response: There is no scenario in which naming a break later is better than naming it when it occurs.

For the breaks in asepsis that training prevents, including the full taxonomy of break categories, their mechanisms, and the response framework that trained staff should apply, that guide provides the reference material for break-specific training content.

Training scenarios built around specific break categories are more effective than general technique reminders. Simulated break identification exercises, where trainees watch a gowning or gloving sequence and name every deviation, build the observation skills that field monitoring depends on. This kind of scenario-based training also normalizes the act of naming breaks, reducing the cultural hesitation that allows violations to go uncorrected in real procedures.

For the errors addressed through staff training, including the published incidence data for each error category and why experience level does not predict error rate, that guide provides the evidence base for training priority decisions.

Connecting training to audit

Training and audit form a cycle. Training establishes the standard. Audit measures whether the standard is being met. Audit findings drive training refinement.

A clinic that trains without auditing does not know whether training is working. A clinic that audits without training does not have a systematic way to address identified gaps.

For auditing trained staff for compliance, including how to structure observation-based audits, what to measure, and how audit findings should feed back into training program revision, that guide covers the audit component of the training-audit cycle.

Frequently asked questions

How often should asepsis training be repeated?

At minimum annually for all surgical personnel, with additional training triggered by: any SSI event, any documented significant aseptic break, changes to antiseptic agents or sterilization equipment, or new procedures being introduced to the practice. High-volume practices may benefit from semi-annual refreshers.

Should asepsis training be role-specific or universal?

Both. A shared foundational curriculum ensures every person in the OR understands the same principles and the same correction expectations. Role-specific training then addresses the technical responsibilities of each position. Surgeons, scrub technicians, and OR cleaners share the foundation but have different intraoperative responsibilities.

Can online or self-directed training replace observed competency assessment?

No. Online training is an effective delivery format for foundational knowledge. It does not substitute for observed performance assessment. A person who completes an online module on closed gloving technique has not demonstrated that they can perform it correctly. Observed assessment is irreplaceable.

What should happen when a staff member fails a competency assessment?

Additional supervised practice followed by re-assessment. Failing a competency assessment is not a disciplinary event; it is a training event. The appropriate response is remedial practice, not penalty. Personnel should not participate in surgical cases until competency is confirmed.

How should training address MRSP and resistant organisms?

As part of the infection consequence module: explain that antibiotic-resistant organisms including MRSP are increasingly prevalent in veterinary surgical infections, that they are harder to treat when they do occur, and that consistent aseptic technique is the primary prevention strategy. This provides context for why technique rigor matters beyond routine infections.

For the core technique covered in training, including the complete technical reference for every step of aseptic technique that training must cover, that guide serves as the curriculum content source for the technical components.

Asepsis training works when it is designed as a continuous program rather than a one-time event, when competency is assessed through observed performance rather than knowledge tests alone, and when the cultural expectation of immediate, non-judgmental break correction is built into the program from the start. The training that produces the best aseptic outcomes is not the most comprehensive lecture. It is the one that most reliably changes behavior in the OR.

Resources

The following sources were used as reference and background for this article:

AVMA Journals. Aseptic protocol breaches are common among veterinary students. AJVR, 2025. avmajournals.avma.org
AVMA Journals. Surgical site infection definitions consensus in veterinary medicine. AJVR, 2026. avmajournals.avma.org
NIH/PMC. Assessing the effect of a canine surgical-neutering educational programme. ncbi.nlm.nih.gov
NIH/PMC. The effectiveness of aseptic non-touch technique audit cycle implementation on reducing SSI. ncbi.nlm.nih.gov
Improve Veterinary Education. VTCert Surgical Nursing module. improveinternational.com
Veterinary Practice. Infection control in the surgical environment. veterinary-practice.com

Get a Free Poster

Enhance your workspace with a high-quality radiographs reference poster, designed for veterinary professionals. This free physical poster will be shipped directly to you—just fill out the form to request your copy.

Request

Table of contents

Heading 2

Heading 3

Things to know

Maintaining a Sterile Field in Veterinary Surgery

The sterile field is established the moment the patient is draped. From that point forward, every action in the OR either maintains or compromises it.

A single unrecognized contamination event can introduce the organisms that cause a surgical site infection even when every preceding preparation step was performed perfectly.

Quick answer: The sterile field encompasses the draped patient, scrubbed personnel (front of gown chest to table, gloved hands), and all sterile instruments within the field. Only sterile personnel and items enter the field. Any item contacting a non-sterile surface is contaminated. All breaks are called out and corrected immediately regardless of who caused them.

Key takeaways

The sterile field is defined by the drapes: everything within the draped zone is sterile; everything outside is not
Only the front of the gown (chest to table level) and gloves are sterile; gown backs and cuffs are not
Any item falling below table level is contaminated: it is replaced, not retrieved
OR traffic must be minimized: each additional person increases airborne contamination; doors stay closed during surgery
Breaks in sterility must be called out immediately by any team member, regardless of seniority
A contaminated glove, instrument, or drape is replaced immediately: there are no exceptions

What constitutes the sterile field

Core distinction: asepsis is the prevention of contamination by maintaining a sterile or near-sterile environment.

The sterile field has four components:

1. The draped patient: the sterile drapes define the sterile zone on and around the patient. Only the window of the fenestrated drape over the surgical site is part of the sterile field. The undraped portions of the patient are not sterile.

2. Scrubbed personnel: Rigorous adherence to the principles of asepsis by all scrubbed personnel is the foundation of surgical site infection prevention. The sterile zones on a scrubbed team member are: front of the gown from chest to table level, gloved hands and wrists. The back of the gown is not sterile. Below table level is not sterile.

3. Draped instrument tables and Mayo stand: instrument tables draped with sterile covers are sterile on their horizontal surfaces. Side drapes hanging below the table edge are not sterile. Nonsterile equipment or furniture, such as the Mayo stand, should be covered appropriately with sterile barrier materials if it is to be used during the procedure. Only sterile items should touch or extend over sterile surfaces.

4. All items transferred onto the sterile field: instruments, implants, sutures, sponges, and solutions delivered onto the sterile field must be transferred using sterile technique.

The rules of the sterile field

Sterile-to-sterile only

Only sterile items contact sterile surfaces. A non-sterile hand reaching into the sterile field even briefly contaminates it. Non-scrubbed personnel do not reach across or into the sterile field.

Below table level = contaminated

Any instrument, sponge, or implant that falls below the table edge is contaminated. It is not picked up and returned to the field. A new item replaces it.

Wet = contaminated

Moisture wicking through a sterile drape (strike-through contamination) renders the overlying sterile surface contaminated.

This is why instruments are not left on wet drapes, and why maintaining dry sterile fields matters throughout the procedure.

No reaching across the sterile field

Scrubbed team members do not reach across the sterile field or across other scrubbed personnel. They position themselves to avoid this. Non-scrubbed personnel do not pass between scrubbed team members.

Dropped packages

If a sterile package is dropped, the item may be considered safe for immediate use only if it is enclosed in impervious packaging that was not punctured or torn on impact and the area of contact is dry. Dropped items wrapped in reusable woven fabric materials should not be transferred to the sterile field.

Traffic control in the OR

In the operating room, the major reason for iatrogenic microbial contamination is breaks in sterile technique. It is one of the key responsibilities of the technical staff to recognize and correct breaks in sterile technique made in preparation for and during a surgical procedure.

The risk of SSIs is significantly elevated with increased surgical time and increased persons present during surgery.

OR traffic rules:

OR doors remain closed during surgery; each opening releases positive-pressure filtered air and allows unfiltered air in
Only essential personnel enter the OR during a procedure
Anyone entering the OR during surgery must comply with OR attire requirements: cap, mask, appropriate footwear
Personnel entering must avoid passing between the surgical team and the sterile field
Conversations and movement near the sterile field are minimized

The operating room should be exposed to limited amounts of traffic, and those allowed into the operating room during procedures should be limited to essential personnel to avoid contamination.

Recognizing and calling out breaks

Any member of the surgical team scrubbed or not has a duty to recognize and call out breaks in sterile technique.

This includes identifying contamination caused by a surgeon, specialist, or more senior team member.

Common breaks requiring immediate action:

A glove perforated, torn, or contacting a non-sterile surface: replace the glove
A gown sleeve below table level: note that area is now contaminated
An instrument dropped below table level: do not retrieve; replace with a sterile instrument
Moisture striking through a drape: identify the area as contaminated; apply an additional sterile drape if needed
A circulating nurse reaching into the sterile field: identify the contamination; replace affected items
OR door opened and left ajar during the procedure: close immediately

The rule is: when in doubt, it is contaminated. Proceeding with a questionable item is never acceptable.

Transferring items onto the sterile field

Items are added to the sterile field by the circulating (non-scrubbed) nurse, who:

Opens packaging without contaminating the interior
Presents the item to the scrubbed team member or drops it onto the sterile field without touching the sterile surface
Pours solutions into sterile containers held or placed by the scrubbed team member (never reaching over the field)

The scrubbed team member receives the item without contact with the package exterior.

OR environment and ventilation

Surgical suites should be positioned to minimize patient transport through high-traffic clinical areas and to allow unidirectional patient flow.

Standard OR ventilation design maintains positive pressure relative to the corridor air flows out of the OR when the door opens, preventing corridor air from entering. HEPA filtration reduces airborne particle load.

Each opening of the OR door disrupts this positive-pressure environment.

Between-case disinfection of all horizontal surfaces, floor, and equipment is required before the next case. High-touch surfaces (light handles, table controls, anesthetic machine) are cleaned with appropriate hospital-grade disinfectant.

For the site preparation that establishes the basis for the sterile field, see surgical site preparation in dogs: complete guide and surgical site preparation in cats: complete guide.

For the draping sequence that creates the sterile field, see draping techniques in small animal surgery.

For the hand scrub that precedes entry into the sterile field, see veterinary surgical hand scrub protocol guide.

Frequently asked questions

If I am not sure whether something was contaminated, what should I do?

Treat it as contaminated. The principle is: when in doubt, it is contaminated. Proceeding with a potentially contaminated item and rationalizing that it was probably fine is never the correct decision.

Replace the item.

Who is responsible for calling out a break in sterile technique?

Everyone in the OR. This is a team responsibility, not a hierarchical one. A veterinary nurse who observes a break caused by the surgeon has a duty to call it out.

A junior team member who observes a senior team member breach technique must call it out.

Can I re-glove if my glove tears mid-surgery?

Yes.

Step back from the sterile field, remove the torn glove without contaminating the other glove, and have the circulating nurse open a new sterile glove for closed or open re-gloving as appropriate.

Do not continue with a torn glove.

The OR door was opened briefly during surgery. Is the sterile field compromised?

A brief opening of an OR door with positive-pressure ventilation functioning is not automatically a contamination event.

The concern is: prolonged opening, OR with inadequate ventilation, or personnel moving through the doorway passing near the sterile field.

Brief openings in a properly ventilated OR are of low risk, but the door should still be kept closed throughout as a standard practice.

What is the difference between asepsis and antisepsis?

Asepsis is the prevention of contamination keeping the field free of microorganisms through sterile technique. Antisepsis is the use of chemical agents to kill or inhibit microorganisms on skin or surfaces.

Surgical technique aims for asepsis; antiseptic agents (chlorhexidine, povidone-iodine) support it by reducing the microbial load on the patient's skin before the field is established.

Resources

VIN / WSAVA 2014. Maintaining a Sterile Operating Environment. vin.com
Infection Control Today. Guidelines for Maintaining the Sterile Field. infectioncontroltoday.com
Veterinary Practice. Infection Control in the Surgical Environment. veterinary-practice.com
MWIAH. Keep It Sterile. mwiah.com
The Veterinary Nurse. Surgical Site Infections: Preparation, Technique and Perioperative Prevention. theveterinarynurse.com

X min read

Asepsis During Orthopedic Surgery in Dogs

Orthopedic surgery in dogs carries higher SSI rates than most other surgical categories. The combination of complex anatomy, prolonged procedure times, tissue trauma from bone work, and the frequent use of implants creates a surgical environment where asepsis must be applied with particular rigor.

What this covers: The asepsis protocol for orthopedic surgery in dogs, including pre-operative preparation, intraoperative standards, and post-operative wound management. Both implant and non-implant orthopedic procedures are addressed, with specific attention to where requirements differ.Evidence base: TPLO SSI retrospective cohorts; veterinary orthopedic surgical site infection incidence data; intraoperative bacterial contamination survey (Vet Surg, Andrade et al., 2016); MRSP colonization as SSI risk factor.SSI rate context: SSI rates in veterinary orthopedic surgery range from approximately 3% to 18%, with the highest rates in procedures involving implants and joints (TPLO: 0.8 to 14.3%; arthrodesis: up to 25%). These rates are substantially higher than for clean soft tissue procedures (1 to 5%).

Key takeaways

Orthopedic SSI rates are higher than soft tissue SSI rates across all procedure types.
MRSP colonization is a documented significant risk factor for orthopedic SSI.
Prolonged procedure time increases SSI risk; minimize through efficient technique.
Bone work (saw, drill) generates aerosolized contamination near the sterile field.
Implant procedures require enhanced asepsis; non-implant procedures meet standard.
Intraoperative lavage is standard for all orthopedic procedures before closure.

Why orthopedic surgery carries elevated SSI risk

Several procedure-specific factors elevate SSI risk for canine orthopedic surgery beyond the baseline for clean soft tissue procedures:

1. Prolonged procedure time

Longer procedures increase SSI risk through cumulative contamination exposure, personnel fatigue leading to technique lapses, and extended anesthesia duration which may impair immune function. SSI risk increases with each additional hour of surgical time.

2. Bone and soft tissue trauma

Oscillating saws, drills, and osteotomes create significant local tissue trauma. Devitalized tissue is more susceptible to bacterial colonization. Thermal damage from bone cutting can further reduce local tissue viability and host defense.

3. Periosteal and soft tissue dissection

Extensive tissue dissection creates dead space. Blood and tissue fluid accumulation in dead space provides a culture medium for bacteria. Minimizing dead space through careful tissue handling and closure is part of the aseptic technique in orthopedic surgery.

4. Implant presence

When metal implants are used, the minimum infective dose required to establish infection drops dramatically. Implants provide an abiotic surface for biofilm formation that bypasses host immune defense. This is why implant procedures require a higher asepsis standard than non-implant procedures.

5. MRSP colonization

S. pseudintermedius, including MRSP strains, is commensal on canine skin and the most common cause of orthopedic SSI. MRSP colonization of the patient is a documented independent risk factor for SSI (OR 9.0 in one orthopedic cohort study).

Pre-operative asepsis: orthopedic-specific requirements

Patient preparation

Clipping:

Clip immediately before surgery. Clip margins should be generous: for extremity procedures, clip from the body wall to the distal limb. For stifle procedures (TPLO, cruciate repair), this typically means the entire limb from the groin to the paw.

A study by Andrade et al. (Vet Surg, 2016) surveyed intraoperative bacterial contamination in dogs undergoing elective orthopedic surgery, confirming that contamination is common and multifactorial. Generous clip margins reduce the zone of potential surface contamination adjacent to the incision.

Skin antisepsis:

Minimum three-pass centrifugal scrub with CHG-alcohol or PVI-alcohol combination. For limb procedures, the scrub extends to the entire clipped area.

Limb hanging:

After skin antisepsis, the limb is suspended (hung) for sterile draping to allow circumferential draping. The hanging apparatus should not contaminate the prepped site. The foot is typically covered with a sterile cohesive bandage or towel before suspension to reduce contamination from paw surfaces.

Pre-operative MRSP consideration:

For high-risk patients (previous MRSP positive culture, recent antimicrobial treatment, chronic skin disease, prior SSI at same site), pre-operative MRSP screening allows scheduling adjustments, decolonization where protocols exist, and enhanced intraoperative asepsis.

Surgical team preparation

Standard surgical hand antisepsis applies. Double gloving is recommended for all implant orthopedic procedures.

Orthopedic instrument sets:

Confirm all instruments are sterile before case start. Orthopedic instrument sets are often complex with many components; each must have chemical indicator confirmation and pack integrity verification before being opened onto the sterile field.

Intraoperative asepsis: orthopedic-specific requirements

Sterile field management

Draping for limb procedures:

Circumferential draping of the limb is standard for most extremity orthopedic procedures. This requires:

Limb hanging in a sterile loop or stockinette suspended from an IV stand
Initial circumferential draping with impervious drape material
Sterile stockinette or cohesive bandage over the distal limb
Final draping to isolate the surgical site within the sterile field

Once placed, drapes must not be repositioned. Any draped area contaminated during patient positioning must have a new sterile drape applied.

Powered instrument management:

Oscillating saws and drills generate bone and tissue debris that contaminates the surrounding sterile field. Management strategies:

Use irrigation during bone cutting to reduce heat generation and debris dispersion
Use sterile drapes positioned to capture contaminated material where possible
Surgical team members not directly holding the powered instrument should step back during cutting to reduce contamination exposure

Implant insertion:

The moment of implant insertion into bone is the highest-risk moment for contamination in orthopedic surgery. The implant transitions from the sterile field into the bone canal, and any contamination of the implant surface at this moment cannot be subsequently corrected.

Implant handling standards:

Grasped only with sterile instruments, never bare gloved hands unless using sterile technique
Not resting on any surface below sterile field level
Not touched by non-sterile personnel or instruments at any point

OR traffic:

Enforce strict traffic control throughout. Orthopedic procedures are often long (1 to 3+ hours). The temptation to allow additional personnel entry during extended procedures must be resisted. Each entry increases airborne contamination cumulatively across the procedure duration.

For aseptic technique applied during orthopedic procedures, including the sterile field rules, instrument handling, and personnel behavior standards that govern the intraoperative phase of all surgical procedures, that guide covers the intraoperative technique framework.

Intraoperative lavage

Wound lavage before closure is standard for all orthopedic procedures, both implant and non-implant.

Saline lavage:

Copious pulsatile or syringe-pressure saline irrigation removes:

Loose bone fragments (sequestra)
Blood clots and debris that would otherwise remain in dead space
Free-floating bacteria that accumulated during surgery

Volume: typically 500 mL to 1 L for a single joint procedure; more for larger procedures.

Antiseptic lavage:

For higher-risk procedures (implant placement, MRSP-positive patient, prolonged procedure), antiseptic lavage before closure addresses residual bacterial contamination that saline alone cannot eliminate. Non-antibiotic antiseptic lavage options targeting biofilm-forming organisms have been used in veterinary orthopedic settings to reduce bacteria, biofilm, and resistant organisms before suturing.

This is a non-antibiotic contamination control step aligned with antimicrobial stewardship principles.

For asepsis requirements when implants are involved, including the enhanced asepsis protocol and the clinical rationale for each enhancement in the context of implant-associated infection risk, that guide covers implant-specific asepsis.

Procedure-specific asepsis notes

TPLO (tibial plateau leveling osteotomy)

TPLO is the highest-volume and highest-SSI-rate procedure in veterinary small animal orthopedic surgery. Key asepsis considerations:

Entire limb prep from groin to paw
Prolonged procedure time warrants strict OR traffic management
Bone work with oscillating saw generates significant local contamination
MRSP risk is the primary driver of treatment-resistant SSI in TPLO patients
Implant presence (plate and screws) elevates the consequence of any contamination event

For TPLO-specific asepsis protocols, including the procedure-specific application of enhanced orthopedic asepsis to TPLO, that guide covers TPLO asepsis in detail.

Fracture stabilization

Trauma patients presenting for fracture repair often have wound contamination from the injury. Wound classification should be assessed before surgery:

Closed fracture: generally Class I (clean); standard asepsis applies
Open fracture: Class III (contaminated) or higher; enhanced protocols apply; antimicrobial therapy (not prophylaxis) indicated

Arthroscopy

Arthroscopic procedures have lower SSI rates than open orthopedic procedures. However, fluid distension media must be sterile, instruments must be sterile (high-level disinfection is not sufficient for instruments entering joint space), and skin antisepsis applies to all portal sites.

Joint replacement

Where performed, hip and elbow total joint replacement represents the highest-consequence orthopedic implant procedure. Full implant asepsis protocol, MRSP screening, and antiseptic lavage are all indicated.

For asepsis standards applied to orthopedic cases, including the five-domain surgical asepsis framework and how it applies across the full range of surgical procedures, that guide covers the broader surgical asepsis standard.

Post-operative wound management

Wound monitoring is more intensive after orthopedic surgery than after routine soft tissue procedures, reflecting the higher SSI rate and the greater treatment difficulty when infection does occur.

Monitoring schedule:

Wound check at 48 to 72 hours post-operatively
Suture/staple removal at 14 days
Follow-up radiographs at defined intervals for bone healing assessment

What to monitor:

Incision: redness, swelling, discharge, dehiscence
Systemic signs: fever, lethargy, reduced appetite
Limb use: sudden worsening of weight-bearing may indicate deep SSI

Early SSI (within 30 days): typically reflects intraoperative contamination.Late SSI (30 days to 12 months): may reflect biofilm maturation, licking-related contamination, or hematogenous seeding.

Any suspicion of SSI in an orthopedic patient warrants prompt veterinary assessment, bacterial culture, and sensitivity testing before antibiotic selection.

For breaks in asepsis during orthopedic procedures, including the specific break categories that are most common and consequential in orthopedic settings, that guide covers the break identification and response framework.

Frequently asked questions

Do all canine orthopedic procedures require implants?

No. Many orthopedic procedures are performed without permanent implants: cruciate ligament extracapsular repair, femoral head and neck excision, arthrotomy for joint exploration or fragment removal. Non-implant procedures carry lower SSI risk and do not require all of the implant-specific enhancements. They still require the full standard orthopedic asepsis protocol described above.

How does procedure duration affect SSI risk?

Longer procedures accumulate more contamination events, increase OR traffic needs, and may involve personnel fatigue affecting technique compliance. SSI risk increases measurably with each additional hour of surgical time. Efficient surgical technique that minimizes unnecessary tissue handling and procedure duration is itself an asepsis-related quality variable.

Is post-operative antimicrobial prophylaxis required for orthopedic procedures?

Current evidence and stewardship guidelines in both human and veterinary medicine recommend limiting prophylaxis to the perioperative period (within 60 minutes of incision; discontinued within 24 hours). Extended post-operative antimicrobial courses do not reduce SSI rates and contribute to resistance development. The goal is optimizing intraoperative asepsis and prophylaxis timing, not extending post-operative antibiotic coverage.

Orthopedic surgery in dogs demands asepsis that accounts for longer procedures, more tissue trauma, the specific risks of implants and biofilm, and the prevalence of MRSP as the dominant SSI pathogen. None of these factors are addressed by antibiotics alone. All of them are addressed by rigorous asepsis applied across every phase of the perioperative period.

Resources

The following sources were used as reference and background for this article:

NIH/PMC. Surgical site infection after 769 Tibial Plateau Leveling Osteotomies. pmc.ncbi.nlm.nih.gov
DVM360. Improving Infection Rates After TPLO. dvm360.com
Veterinary Practice News. Old and New Thoughts on Infection Control. veterinarypracticenews.com
Wiley Online Library. Surgeon and Patient Preparation to Minimize Surgical Site Complications in CCL Surgery. onlinelibrary.wiley.com
Springer Nature. Antimicrobial prophylaxis is sufficient for acceptable SSI rate in clean orthopaedic and neurosurgeries in dogs. link.springer.com

X min read

Surgical Site Preparation in Dogs: Complete Guide

Surgical site preparation is the first line of defense against surgical site infection (SSI).

The goal is to reduce the bacterial load on the skin to the lowest achievable level before the incision is made.

Every step in the preparation protocol matters a single shortcut can undermine the entire chain.

Quick answer: Canine surgical site preparation follows a fixed sequence: clip a wide area in the prep room, perform an initial scrub for gross decontamination, then in the OR perform the aseptic scrub center-to-periphery using chlorhexidine or povidone-iodine, then drape. Never clip or scrub in the OR.

Key takeaways

Clip a wide margin around the incision site: at minimum 5 to 10 cm on each side; more is better
Clip in the prep room, not the OR: loose hair and dander are OR contaminants
Initial scrub removes gross contamination (oils, bacteria, debris) before the aseptic scrub begins in the OR
Aseptic scrub technique: target pattern center to periphery, discard gauze after each pass, never return toward center
Chlorhexidine and povidone-iodine are both acceptable: do not mix them on the same patient due to potential chemical incompatibility
Alcohol rinsing between antiseptic applications improves bacterial kill; contact time for each application must be respected

Why site preparation matters

Translocation of endogenous microbial flora is the most common route of surgical site infection. Skin preparation and aseptic techniques aim to reduce or eliminate the growth of resident and transient flora at the wound site, thereby reducing the morbidity and mortality rates from SSIs.

The skin surface harbors resident flora (permanently colonizing microorganisms) and transient flora (recently deposited organisms). Both can contaminate the wound at the moment of incision if not adequately reduced by preparation.

The preparation protocol addresses both.

Step 1: Pre-clipping assessment

Before clipping, assess the skin in the intended surgical field:

Note any existing wounds, abrasions, or skin conditions
Identify regional lymph nodes for palpation
Confirm the surgical site with the team before hair removal

Step 2: Hair clipping

Clipping is performed in the designated preparation area, not in the operating room. Loose hair shed into the OR environment is a contamination source.

Technique:

Use electric clippers with a surgical blade (size 40 preferred: finer cut, closer to skin)
Clip the direction of hair growth first, then against it for a closer result
Clip a wide field minimum 5 to 10 cm beyond the proposed incision on all sides
Do not clip the skin itself guard against clipper trauma which creates skin breaks and increases SSI risk

Blade size evidence: studies have evaluated different blade sizes for SSI risk. A size 40 blade (finer cut) has been associated with more SSIs in some studies due to skin microtrauma; a size 10 blade (less close) may reduce this risk. Practice varies; the key is avoiding visible skin irritation.

Male dog prepuce management: if the surgical field includes or borders the prepuce, flush it with 0.05% chlorhexidine diacetate solution for 2 minutes and displace it laterally in the field before draping.

Step 3: Initial scrub (gross decontamination)

Wear examination gloves and remove gross debris from the surgical site using gauze sponges and an antiseptic solution such as chlorhexidine gluconate 4% or povidone-iodine. Scrub the site gently until little to no gross debris remains. The use of clean, but not sterile, supplies for initial surgical site cleaning does not affect infection rates when the skin is intact.

The initial scrub is performed in the prep room before the patient enters the OR. It removes surface oils, organic matter, and loose debris.

This is not the aseptic scrub it prepares the skin for it.

Step 4: Patient transfer to OR

The patient is moved to the OR and positioned on the surgical table. The prepared site must not contact non-sterile surfaces during transfer.

Limbs may be loosely wrapped or positioned to avoid contact.

Step 5: Aseptic scrub in the OR

Once the patient is properly positioned, secured to the operating room table, and connected to all anesthetic monitoring equipment, the aseptic scrub can be performed.

The target pattern:

Begin scrubbing at the center of the proposed incision site, working outward in a circular target pattern until the edge of the clipped area is reached. Use a gentle motion to produce a lather. Discard the gauze and repeat the scrub as needed to allow for the appropriate contact time recommended by the scrub solution manufacturer.

Critical rules:

Always work center to periphery never return toward the incision center with a used gauze
Discard each gauze after a single outward pass
The scrubbing team wears sterile gloves
Contact time must be respected do not wipe off prematurely

Number of scrub cycles: typically three alternating cycles of antiseptic scrub and alcohol rinse (for chlorhexidine-based protocols) or antiseptic scrub and saline rinse (for povidone-iodine). Confirm your specific protocol with your clinic's surgical guidelines.

Antiseptic selection

Chlorhexidine gluconate (CHG)

Chlorhexidine kills a wide range of bacteria and has residual activity, meaning it continues working after application.

Chlorhexidine gluconate is often considered superior to povidone-iodine because of its longer residual action.

CHG is the more commonly recommended agent for veterinary surgical site preparation based on human medicine data showing superiority over PI, particularly with alcoholic formulations.

Povidone-iodine (PI)

Povidone-iodine is effective against bacteria, viruses, and fungi, and is commonly used in veterinary surgery.

Povidone-iodine has an excellent immediate antimicrobial effect. Most samples collected at post-asepsis did not present bacterial growth, both for animals subjected to povidone-iodine (74%) or chlorhexidine (70%) protocols.

PI has excellent immediate kill but minimal residual activity once dry.

Do not mix antiseptics

There is some evidence to suggest it is important not to mix the two on the same patient do not use chlorhexidine gluconate for initial prep and then povidone-iodine for the final prep. Chlorhexidine gluconate is cationic and povidone-iodine is anionic, which together are chemically unsuited. There is concern that when used together, they may provide limited or no skin antisepsis as the iodine inactivates the chlorhexidine.

Choose one antiseptic and use it throughout the entire preparation protocol.

Step 6: Draping

After the aseptic scrub, the sterile team applies four corner drapes secured with towel clamps, followed by a large fenestrated drape over the patient and table.

Draping rules: drapes can only be moved away from the incision site. A drape moved toward the incision contaminates the sterile field.

For the full draping guide, see draping techniques in small animal surgery. For the surgical hand scrub that precedes site preparation, see veterinary surgical hand scrub protocol guide.

For the SSI prevention overview, see how to prevent surgical site infections in dogs.

Frequently asked questions

Can I clip and scrub in the operating room?

No. Clipping should always be performed in a designated prep area separate from the OR. Loose hair contaminated with skin bacteria sheds into the OR environment and settles on sterile surfaces.

Clipping in the OR is a recognized SSI risk factor.

How wide should the clip area be?

At minimum 5 to 10 cm beyond the proposed incision on all sides.

In practice, clip wider than you think you need running out of prepared skin during surgery is worse than clipping a little more than necessary.

Should I use chlorhexidine or povidone-iodine?

Both are acceptable. Chlorhexidine has longer residual activity; povidone-iodine has excellent immediate kill. Do not mix them.

Most current guidance leans toward chlorhexidine (ideally in alcoholic formulation) based on human surgery data showing superior SSI reduction, though veterinary-specific evidence is more limited.

How many scrub cycles are required?

Protocol varies by clinic. A typical approach is three antiseptic scrub cycles with alcohol rinse between each.

The key is achieving the required contact time for your chosen antiseptic and removing each gauze after a single outward pass. Follow the antiseptic manufacturer's contact time recommendation.

Can I scrub toward the incision center if I see a missed area?

Never. Once a gauze has passed outward, it is contaminated with the organisms it picked up from the skin periphery.

A new gauze must be used for any additional scrubbing of the central area. Returning inward with a used gauze violates the core principle of aseptic scrub technique.

Resources

Clinician's Brief. Preoperative Surgical Site Preparation in Veterinary Medicine. cliniciansbrief.com
PMC. Comparative Clinical Effectiveness of Preoperative Skin Antiseptic Preparations of CHG and PI for Preventing SSIs in Dogs. pmc.ncbi.nlm.nih.gov
PMC. Skin Asepsis Protocols as a Preventive Measure of SSI in Dogs: Chlorhexidine-Alcohol versus Povidone-Iodine. pmc.ncbi.nlm.nih.gov
The Veterinary Nurse. Surgical Site Infections: Preparation, Technique and Perioperative Prevention. theveterinarynurse.com
VetNurse. Surgical Skin Preparation: Best Practice Protocol. vetnurse.com.au

X min read

Asepsis for IV Catheter Placement in Dogs and Cats

IV catheter placement is one of the most frequently performed procedures in veterinary medicine. It is also one of the most frequently performed with insufficient aseptic technique.

Catheter-related bloodstream infection (CRBSI) is a well-documented complication in veterinary patients. It is almost entirely preventable with correct aseptic placement and maintenance technique.

What this covers: The asepsis standards for peripheral and central IV catheter placement in dogs and cats, based on AAHA 2018 Infection Control, Prevention and Biosecurity (ICPB) Guidelines, including site preparation, glove type selection, catheter handling, and dwell time management.Scope: Peripheral IV catheters, jugular catheters, and peripherally inserted central catheters (PICCs) in small animal patients. Both placement and maintenance asepsis are addressed.Key distinction: Peripheral short-term catheters and central/long-term catheters require different asepsis standards. Peripheral catheters: examination gloves. Central, jugular, and PICC catheters: sterile gloves. This distinction is clinically significant and frequently overlooked.

Key takeaways

AAHA 2018 ICPB Guidelines are the current evidence base for veterinary IV catheter asepsis.
Peripheral catheters: examination gloves and 0.5 to 2% CHG scrub diluted with saline.
Central, jugular, and PICC catheters: sterile gloves and full aseptic prep.
Do not palpate the insertion site after antiseptic prep without sterile gloves.
Dwell time beyond 72 hours significantly elevates CRBSI risk; replace or reassess.
Catheter site inspection at least once daily is required for all indwelling catheters.
Disconnection and reconnection events are major contamination opportunities.

The asepsis risk from IV catheters

An IV catheter creates a direct pathway from the skin surface into the vascular system. Any bacteria present at the insertion site, on the catheter surface, or introduced through the catheter hub can travel directly into the bloodstream.

In veterinary critical care settings, CRBSI causes:

Bacteremia and septicemia
Extension of hospitalization
Requirement for systemic antibiotic therapy
Increased morbidity and mortality

Unlike SSI after surgery, CRBSI develops over the dwell time of the catheter. The risk accumulates with each hour of catheter presence, each disconnection and reconnection event, and each site care interaction performed without adequate technique.

AAHA 2018 ICPB Guidelines: the evidence framework

The American Animal Hospital Association 2018 Infection Control, Prevention and Biosecurity (ICPB) Guidelines provide the current veterinary standard for IV catheter asepsis.

Key AAHA 2018 ICPB requirements for peripheral IV catheterization:

Remove hair from the insertion area
Don examination gloves
Use chlorhexidine scrub diluted with saline to 0.5 to 2% working concentration for skin preparation

Key requirements for central, jugular, and PICC catheters:

Sterile gloves required for catheter placement
Full aseptic preparation of the site (more extensive than peripheral prep)
Sterile draping of the site

VETgirl's review of these guidelines notes: "For peripheral central venous catheters (PICC) or jugular central line catheters, following aseptic preparation I don sterile gloves for the cannulation procedure, as aseptic technique is very important with these longer dwelling catheters."

Site preparation: peripheral catheters

Hair removal

Clip or shave the insertion area. VETgirl recommends clipping around the entire circumference of the limb at the catheter site to prevent hair being dragged into the insertion site when taping.

Hair removal is not just aesthetic: hair carries surface bacteria that can contaminate the insertion site during catheter placement and securing.

Antiseptic application

Agent: CHG diluted with sterile 0.9% saline to a working concentration of 0.5 to 2%.

Zoetis guidance (via veterinary percutaneous IV catheter guide): "Following removal of hair and organic debris, chlorhexidine antiseptic scrub diluted with sterile 0.9% saline to a working concentration of 0.5 to 2.0% should be used to prepare the skin. Isopropyl alcohol (70% or greater) antiseptic can also be used in combination with the chlorhexidine scrub."

Technique: Circular motion from center of insertion site outward. At least two to three application passes.

Contact time: Allow the antiseptic to fully dry before insertion. Wet antiseptic is partially diluted at the point of contact and does not achieve its labeled kill claim.

Critical error: Do not palpate the insertion site after antiseptic preparation without sterile gloves. VETgirl specifically notes: "After the scrub has been performed, palpation of the insertion site should be avoided." Palpation to find the vein after prepping recontaminates the prepped site with finger flora.

Gloves

Examination (clean, non-sterile) gloves for peripheral catheter placement. Sterile gloves are not required for short-term peripheral catheters per AAHA 2018 ICPB.

Hand hygiene before gloving is required regardless of glove type.

Site preparation: central, jugular, and PICC catheters

Central venous catheters, jugular catheters, and PICCs have longer dwell times, larger caliber vessels, and more direct cardiac proximity than peripheral catheters. The consequence of contamination is more severe.

Full aseptic prep required:

Larger clip area than for peripheral catheters
Antiseptic preparation of broader site area
Sterile gloves for placement
Sterile draping of the site where possible

CHG concentration: 0.5 to 2% CHG-alcohol or CHG-saline combination. For cats, diluted CHG only (CHG-alcohol combinations may be appropriate; confirm CHG does not contact mucous membranes or ear canals).

Sterile glove technique: Once sterile gloves are donned, no contact with non-sterile surfaces before catheter placement. If the vein must be palpated after prep, use the sterile-gloved finger (which must not then contact non-sterile surfaces).

For comparing IV catheter asepsis to urinary catheter asepsis in dogs, including the parallel clean-to-sterile technique framework applied to urinary catheterization and how the two catheter types compare in asepsis requirement, that guide covers urinary catheter asepsis.

IV catheter placement and maintenance are medical asepsis procedures, not surgical asepsis. Understanding this distinction clarifies which standard governs each phase of care. For medical asepsis in veterinary clinics, including how the medical asepsis standard that governs IV catheter care differs from the surgical asepsis standard for OR procedures, that guide covers the medical asepsis framework.

Catheter handling and insertion

Catheter sterility

IV catheters are supplied sterile in individual packaging. Inspect each catheter before use:

Packaging intact (no tears, moisture, or seal failure)
Expiry date not exceeded
Visual inspection of catheter: no kinking or visible contamination

Once the catheter is removed from its packaging, the catheter surface must not contact any non-sterile surface before vascular insertion.

Hub handling

The catheter hub is the most common contamination point during insertion and subsequent use. After placement:

Apply a sterile cap or T-port immediately
Do not allow the hub to rest against non-sterile surfaces
Flush with sterile heparinized saline or sterile saline immediately to confirm patency

Catheter maintenance asepsis

Placement asepsis determines the starting bacterial load at the insertion site. Maintenance asepsis determines whether that load increases over the dwell period.

Site inspection

At minimum daily (more frequently in critical care patients): inspect the insertion site for:

Redness, swelling, heat, or discharge at the site
Catheter movement or partial displacement
Occlusion or resistance to flushing

Any sign of local inflammation is an indication for catheter removal.

Dressing changes

Change the catheter dressing when soiled, wet, or lifting at the edges
At each dressing change: hand hygiene, examination gloves, fresh sterile primary contact material
Inspect the insertion site before applying the new dressing

Disconnection and reconnection

Each disconnection and reconnection of the catheter hub is a contamination event. Protocols to minimize risk:

Scrub the hub with 70% alcohol and allow to dry before any connection or disconnection
Use needleless connectors (when available) to reduce disconnection frequency
Minimize disconnections to clinically necessary events only

Dwell time

Peripheral IV catheter dwell time should not routinely exceed 72 hours in small animal veterinary patients. Beyond this threshold, CRBSI risk increases substantially.

In practice, replace or reassess catheters at 72 hours. If the catheter is still clinically necessary and the site appears healthy, reassessment by a clinician determines whether replacement or extension is appropriate. Do not extend dwell time by default without clinical assessment.

For common aseptic errors in catheter and clinical procedures, including the error categories most commonly identified in IV catheter placement and management, that guide covers the error taxonomy.

Feline-specific considerations

CHG for cats

CHG is appropriate for feline IV catheter site preparation at 0.5 to 2% concentration. Avoid contact with:

Ear canals
Mucous membranes
Eyes

Cats that remove their IV catheters and groom the insertion site are at risk of CHG ingestion. Monitor all feline IV catheter sites; use protective bandaging and E-collars where cats persistently interfere.

Vein selection in cats

The cephalic and saphenous veins are standard peripheral sites in cats. Jugular catheters in cats require sterile placement technique as for dogs.

For IV catheter asepsis compared to urinary catheter asepsis in cats, including the specific sterile technique required for urinary catheterization in cats and how it compares to the IV catheter standard, that guide covers urinary catheter asepsis in cats.

IV catheter site preparation uses antiseptic agents (specifically CHG) within an aseptic technique framework. Understanding the difference between these two concepts clarifies why antisepsis of the insertion site is a component of, not a substitute for, the overall aseptic catheter placement procedure.

Asepsis vs. antisepsis in IV catheterization

For the distinction between asepsis and antisepsis, including how IV catheter site preparation uses antiseptic agents within an aseptic technique framework, and how these two concepts operate together in clinical practice, that guide covers the conceptual relationship.

Common catheter placement errors

Error	Consequence	Correction
Palpating site after antiseptic prep	Recontamination of prepped site	No palpation post-prep without sterile gloves
Non-sterile gloves for jugular/PICC	Direct flora transfer at insertion	Sterile gloves for all central lines
Antiseptic not allowed to dry	Reduced kill efficacy	Full dry time before insertion
Hub contact with non-sterile surface	Hub contamination; CRBSI risk	Handle hub only with sterile gloves; cap immediately
Dwell time exceeding 72 hours without reassessment	Elevated CRBSI risk	72-hour reassessment protocol
Disconnection without hub scrub	Hub contamination at each connection event	70% alcohol scrub and dry before every connection

Frequently asked questions

Should diluted CHG be mixed fresh each day?

Yes. Pre-diluted CHG solutions can become contaminated during storage, particularly if non-sterile water was used for dilution or if the dispensing container is not kept clean. Published CRBSI outbreaks in human medicine have been traced to contaminated pre-diluted CHG. Mix fresh diluted CHG daily using sterile 0.9% saline.

Is povidone-iodine acceptable as an alternative to CHG for catheter site prep?

Yes, where CHG is contraindicated (documented allergy, specific patient contraindication). PVI provides adequate antisepsis but has less residual activity than CHG and is more readily inactivated by blood or plasma at the insertion site. CHG is preferred by most current guidelines for peripheral vascular access site preparation.

Can IV catheter extension sets be reused between connections?

Extension sets should be changed per the manufacturer's recommendation or at catheter replacement, and whenever they are visibly contaminated or soiled. Reusing extension sets across multiple days without replacement increases the contamination burden at the catheter hub with each connection event.

IV catheter asepsis is medical asepsis applied to an invasive device. The principles are straightforward: prepare the site correctly, use the right gloves for the right catheter type, handle the hub as the sterile-critical point it is, monitor the site daily, and replace on schedule. The CRBSI that develops from inadequate IV catheter asepsis is as preventable as the SSI that develops from inadequate surgical asepsis. The only difference is that it happens more slowly and in a patient who is already compromised.

Resources

The following sources were used as reference and background for this article:

VETgirl. Best Practices for Aseptic Skin Preparation for IV Catheter Placement. vetgirlontherun.com
Zoetis US. How To Place A Percutaneous Intravenous Catheter in Canine and Feline Patients. zoetisus.com
VETgirl. How to Place a Peripheral IV Catheter. vetgirlontherun.com
Virginia Tech ARCD. SOP: Placing an Intravenous Catheter in Dogs and Cats. research.vt.edu
AAHA. 2018 Infection Control, Prevention and Biosecurity Guidelines. aaha.org

X min read

Preventing Post-Operative Infections in Cats

Cats are exceptional at hiding discomfort, and they're equally determined to groom themselves the moment you look away. Both of these traits make post-operative infection prevention in cats more demanding than in dogs.

The good news: most post-surgical infections in cats are preventable. The majority require the same foundational measures: keeping the wound protected, monitoring it daily, and getting your cat to their follow-up appointments.

Quick answer: Preventing post-operative infections in cats comes down to three owner responsibilities: keeping the E-collar on at all times to prevent licking and grooming of the incision, checking the surgical site daily for redness, swelling, or discharge, and following all medication and follow-up instructions from your vet. Cats that lick their incisions develop secondary infections at a much higher rate than those kept properly protected.

Key takeaways

Licking is the leading preventable cause of post-operative infection in cats at home.
E-collar compliance is non-negotiable until the vet confirms the incision is fully healed.
Daily incision checks help you catch early infection signs before they become serious.
Cats hide illness well: behavioral changes (hiding, reduced appetite) may be the first sign of trouble.
FIV or FeLV positive cats carry higher infection risk and need closer post-surgical monitoring.
Normal healing vs. early infection has clear distinguishing signs covered in the monitoring section below.

Why cats are at particular risk after surgery

Cats present specific challenges in post-surgical infection prevention that differ from dogs.

Grooming instinct: cats are compulsive self-groomers. The moment an E-collar is removed, most cats will attempt to access the incision site. Their tongue is rough enough to pull sutures and introduce oral bacteria directly into the healing wound.

Hiding pain: cats conceal discomfort as a survival instinct. By the time a cat is visibly unwell, the infection may be more established than it would be in a dog who shows pain more obviously. This is why daily visual inspection of the wound matters more than watching for behavioral signs alone.

FIV and FeLV: cats with feline immunodeficiency virus or feline leukemia virus have compromised immune systems that make infection more likely and harder to resolve. Post-surgical monitoring must be more intensive for these cats.

PetMD confirms: "Grooming and licking the surgical site can cause secondary complications such as infections, irritation, and damage to the sutures."

The E-collar: your most important tool

No single measure prevents more post-operative infections in cats than consistent E-collar use.

Revel Vet explains: "You should generally keep an e-collar on your cat until the incision has healed, unless you receive other instructions from your veterinarian."

When the E-collar must be worn

At all times when unsupervised
During the night
When you're in the same room but not actively watching the cat
During the full healing period, typically 10 to 14 days for routine incisions

The E-collar comes off for eating and drinking if you can watch directly and return it immediately after. It does not come off because your cat hates it or seems distressed. Cats adjust to E-collars far faster than owners expect, particularly if the alternative (infection and re-suturing) is considered.

E-collar alternatives

If your cat is extremely distressed by a traditional cone-style E-collar, alternatives include:

Inflatable recovery collars: softer and more tolerable for some cats, but verify the cat can't access the wound
Recovery body suits/onesies: cover abdominal and some thoracic incisions; not suitable for all wound locations
Neck collars: a softer version that prevents head rotation to reach the body

Confirm any alternative with your vet before substituting, as the incision location determines which option adequately protects it.

Daily wound monitoring: what to look for

Check the incision every day at the same time, in good lighting.

Normal healing appearance

Timeframe	Normal signs
Days 1 to 3	Mild redness at wound edges, slight swelling, possible clear or pink-tinged fluid
Days 3 to 7	Redness fading, swelling reducing, wound edges closing
Days 7 to 14	Wound edges fully closed, minimal redness, hair beginning to grow back

Signs that require a vet call

Contact your vet the same day if you notice:

Redness spreading beyond the immediate wound margin
Yellow, green, or opaque discharge
Foul smell from the wound site
Increasing rather than decreasing swelling after day 3
The wound opening or sutures separating
The cat obsessively pawing at or trying to reach the wound despite the E-collar

Behavioral signs to watch for

Because cats hide pain, watch for:

Reduced appetite or refusing food for more than 24 hours
Hiding more than usual or unwillingness to engage
Increased or decreased grooming elsewhere (compensatory behavior)
Vocalizing when the wound area is touched
Fever (temperature above 39.5°C / 103.1°F)

For how to distinguish healing from infection in feline surgical wounds, see distinguishing healing from infection after surgery.

Home environment and wound care

Activity restriction

Cats recovering from surgery need restricted movement. Jumping, climbing, and running all place mechanical stress on incisions that can cause wound breakdown.

Practical measures:

Confine to one room or a large crate during the initial recovery period
Remove access to furniture they jump from
Block stairs if the incision could be strained by stair use
Keep children and other pets away to prevent accidental trauma to the wound

Wound hygiene

Unless your vet specifically instructs otherwise:

Do not clean the incision with antiseptics, hydrogen peroxide, or any product not explicitly recommended by your vet
Keep the wound dry: no bathing until fully healed
Don't apply creams or ointments unless prescribed
Keep bedding clean: change it regularly to reduce environmental bacterial load

Pooler Veterinary Hospital advises: "Keep the incision site clean and dry at all times. Avoid bathing your dog (or cat) until your vet gives approval."

Medications

Give all medications for the full prescribed course. Stopping antibiotics early when the cat appears improved is one of the most common owner errors that leads to recurrence and, in resistant bacteria, to selection pressure that makes retreatment harder.

Comparing cat and dog post-operative infection prevention

Cat post-operative infection prevention shares core principles with dogs but has cat-specific considerations:

Factor	Cats	Dogs
Grooming instinct	Very strong; E-collar critical	Strong; E-collar also critical
Pain expression	Hides it; harder to detect early	More obvious behavioral signs
Immune risk factors	FIV, FeLV	Diabetes, Cushing's, old age
Activity compliance	Easier to confine	More difficult in active dogs
Wound licking	Tongue causes more suture damage	Equally damaging

For post-operative infection prevention in dogs specifically, see post-operative infection prevention in dogs for comparison. For the timing of when infections typically appear, see when to watch for post-operative infections in cats.

When to seek emergency care

Go to an emergency vet immediately if:

Your cat is unresponsive or collapses
The wound has opened significantly with visible tissue
Rapidly spreading redness or warmth covers a large area
Your cat has a high fever and severe lethargy together
Bleeding from the wound site that doesn't stop within 5 minutes

These signs indicate the infection or wound complication has progressed beyond what can wait for a regular appointment.

For the specific surgical site infection prevention protocols vets use in cats, see surgical site infection prevention specifically in cats.

Frequently asked questions

My cat is acting normally but the wound looks a little red. Should I be worried?

Mild redness at the wound margin is normal for the first 2 to 3 days. If it's fading rather than spreading, and there's no discharge or odor, it's likely normal healing. If redness is spreading beyond the wound margin or appearing on day 5 or later when it should be diminishing, call your vet.

Can I take the E-collar off at night if I'm watching my cat sleep?

No. Cats move during sleep and can access wounds in positions you won't notice. The E-collar must stay on during sleeping hours. Remove it only for eating and drinking under direct supervision.

My cat had surgery two days ago and hasn't eaten much. Is that normal?

Reduced appetite for 24 to 48 hours post-surgery is common due to the effects of anesthesia and the stress of the procedure. By day 2 to 3, most cats return to normal or near-normal eating. If your cat is still refusing food at 72 hours post-surgery, contact your vet: this may indicate pain, nausea from medications, or early infection.

The owner's role in preventing post-operative infection in cats is more active than many people expect. The surgeon controls the intraoperative environment. You control everything that happens once your cat comes home, and for most preventable infections, that's where the critical work is done.

Resources

PetMD. Cat Surgery Aftercare FAQs. petmd.com
Revel Vet. Signs of Infection in Cats After Surgery. revelvet.com
Pooler Veterinary Hospital. Pet Wound Care at Home. poolervet.com
The Pet Vet. Post-Surgical Infection in Cats. thepetvet.com

X min read

Draping Techniques in Small Animal Surgery

Draping is the step in surgical preparation that defines the sterile field.

It isolates the prepared skin at the incision site from all surrounding contaminated surfaces the patient's hair and skin, the surgical table, and the anesthetic equipment.

Done incorrectly, draping is just a gesture. Done correctly, it is the final barrier between the sterile surgical wound and the contaminated world around it.

Quick answer: Standard small animal draping uses four corner drapes to frame the incision, secured with towel clamps, then one large fenestrated drape over the patient and table. Drapes move only away from the incision. Orthopedic limb surgery uses free-draping for full limb manipulation.

Key takeaways

Four corner drapes frame the incision site first; a large fenestrated drape is placed on top as the final layer
Drapes can only move away from the incision site: moving toward the center contaminates the sterile field
Towel clamps become unsterile once they pierce skin: hand off to a non-sterile assistant before reusing
Drapes must never be shaken or fanned: air currents from rapid handling contaminate the prepared field
Free-draping is used for orthopedic limb surgery to allow full limb manipulation within a sterile field
Key sheet draping (single-drape method) is an alternative that eliminates the need for corner drapes and towel clamps

Why draping matters

Virtual Vet Surgery (University of Melbourne): "Draping isolates the surgical site from contamination from non-sterile areas including the surrounding hair and skin. The drapes should ideally cover the entire patient and table."

The prepared skin has been decontaminated by clipping and antisepsis. But it still sits next to:

Unclipped hair at the edges of the prep zone
The patient's non-sterile body
The surgical table surface
Anesthetic circuit tubing
Any unsterile equipment around the patient

Drapes isolate the sterile island (prepared skin) from all of these contamination sources.

Drape types

Rectangular (utility / corner) drapes

These are the standard-size rectangular drapes used to frame the incision site during the initial four-corner step.

Animal Hospital Supply: "Corner drapes are doubled over at one end (9 to 10 cm) and placed at the periphery of the surgical field one at a time."

The drape edge is wrapped around the gloved hands to prevent contamination while covering the four corners.

The doubled-over edge faces toward the surgeon to protect the glove from contact with the non-sterile surface as the drape is applied.

Fenestrated drapes

A large drape with a pre-cut opening (fenestration) placed over the patient and table after the four corner drapes.

McCurnin's Clinical Textbook: "For final draping, a large fenestrated or unfenestrated drape is placed over the animal and the table.

The fenestration is placed over the incision site, or a slit is cut into the unfenestrated drape at the incision site."

Animal Hospital Supply: "A large sterile drape is placed over and above the four square-off drapes.

This large drape is then fenestrated, the fenestration through which the sterile surgical procedure is then performed."

SustainableVet: "Fenestrated drapes should be large, covering as much of the patient and table as possible."

Disposable vs. reusable drapes

Disposable drapes are made from synthetic non-woven material, single-use, and are discarded after each procedure. They eliminate the risk of inadequate sterilization between uses.

Virtual Vet Surgery: "Significant reductions in the numbers of bacteria in surgical wounds have been documented using disposable (single-use) and Opsite drapes."

Reusable linen drapes can be laundered and autoclaved. They are more economical over time but require careful inspection for holes and worn areas before each use.

Key sheets (single-drape method)

Animal Hospital Supply: "As in nearly every human surgical procedure in the US, some veterinary surgeries have moved toward a single drape or key sheet draping method.

The key sheet eliminates the need for all underneath draping and the need to clamp the drapes to the patient skin."

Key sheets are procedure-specific and often incorporate additional features: adhesive edges to secure to the patient, tube holders, fluid collection pouches for arthroscopy, and absorbent zones.

Four-corner draping: the standard sequence

McCurnin's: "Four quarter drapes are secured with towel clamps approximate to the incision."

Step 1: Apply corner drape 1 at the cranial edge of the proposed incision site.

Veterinary Surgery Online: "The first drape is generally applied at the cranial edge of the proposed incision site.

Once the drape is unfolded, it should not be turned around in order to maintain the most sterile portion (close to the hands) sterile."

Step 2: Apply corner drapes 2, 3, and 4, framing the other three sides.

The sequence "top, tail, near, far" is a common convention. Virtual Vet Surgery: "A placement pattern of top, tail, near, and far.

The reason for this: in deep-chested dogs, holding a lateral drape in place is difficult because a second drape has to be applied before it can be secured by a towel clamp."

Step 3: Secure with towel clamps.

McCurnin's: "If Backhaus towel clamps are positioned directly in the corners of a four-toweled drape set, the edges will lie flat and not bulge up."

Critical rule on towel clamps: McCurnin's: "The Backhaus towel clamps are considered unsterile once they have penetrated the skin. If you need to remove towel clamps for readjustments, do not touch the contaminated tips; hand them off the table to a nonsterile assistant and use a new clamp."

Step 4: Apply the large fenestrated drape as the final layer over the entire patient and table.

Critical draping rules

Drapes only move away from the incision

Veterinary Surgery Online: "As drapes are applied, they can be moved away from the proposed incision site, towards the edge of the prepared area (without exposing hair).

Conversely, a drape cannot be moved from the site of application towards the center of the prepared area since this may lead to contamination of the prepared field."

This rule is absolute. Moving a drape toward the incision drags contamination with it.

Do not shake or fan drapes

Veterinary Surgery Online: "Drapes should not be shaken, fanned, or flipped rapidly when handled as this will create air currents and promote contamination of the prepared surgical field."

Drapes must be gently unfolded and placed never snapped open.

Drapes must cover the entire patient and table

SustainableVet: "Fenestrated drapes should be large, covering as much of the patient and table as possible." Any exposed surface represents a contamination risk.

Special situations

Orthopedic limb surgery: free-draping

For limb surgeries requiring full manipulation (TPLO, fracture repair), the limb is draped to allow it to move freely within the sterile field.

Virtual Vet Surgery: "For many orthopaedic procedures on the limbs, a 'free-draping' technique may be used to help surgical manipulation of the limb.

To isolate the limb, the limb is suspended using a drip stand with the foot enclosed inside a clean latex glove. The glove is secured to the foot with adhesive tape."

The limb is then clipped and prepared. Three corner drapes are placed around the base of the limb to isolate it from the trunk.

A sterile cohesive bandage is applied over the glove and up the limb before the final draping layer.

Male dog abdominal surgery: prepuce management

Veterinary Surgery Online: "If draping the abdomen of a male dog, the prepuce should be displaced laterally and held with a towel clamp to decrease contamination risk.

This should be done prior to draping the area in order to drape over the tip of the prepuce."

Procedure-specific draping

SustainableVet: "Orthopedic surgeries: Often require fenestrated drapes that expose limbs while covering the rest of the body. Abdominal surgeries: Use large non-fenestrated drapes to cover the entire abdomen.

Thoracic surgeries: Require careful draping to isolate the chest area, often using multiple drapes."

For the site preparation that precedes draping, see surgical site preparation in dogs. For the sterile field context draping creates, see maintaining a sterile field in veterinary surgery.

For the PPE worn during draping, see PPE use and barrier protection in veterinary clinics.

Frequently asked questions

Why can drapes move away from the incision but not toward it?

Moving a drape toward the incision site drags whatever the drape previously contacted (potentially contaminated area) toward the sterile field. Moving away simply extends coverage over already-covered non-sterile area.

This is a fundamental aseptic principle with no exceptions.

What happens if a drape becomes contaminated during application?

A contaminated drape must be replaced. If a drape contacts a non-sterile surface (the floor, an unsterile piece of equipment, the patient's non-prepped hair), it cannot be used further.

A new sterile drape replaces it.

Can the surgeon reposition a towel clamp once it has been placed?

If the clamp has penetrated skin, its tips are unsterile. McCurnin's: it must be handed off to a non-sterile assistant. A new sterile clamp is used for repositioning.

What is the advantage of key sheet draping over four-corner draping?

Key sheets are faster, eliminate the towel clamp skin-penetration issue, and are procedure-specific with integrated features like fluid pouches and tube holders. The tradeoff is higher per-use cost.

Why do drapes need to cover the entire patient and table, not just the immediate area?

The entire table surface around the patient is a potential contamination source. Any instrument, sponge, or implant that falls onto an uncovered table surface is contaminated.

Draping the full patient and table prevents these incidental contaminations.

Can a drape that has slipped during surgery be pushed back into place?

No. If a drape slips, alert the circulating nurse. A new sterile drape is placed over the exposed area. The slipped drape cannot be repositioned, regardless of how small the movement needed.

Resources

Veterinary Surgery Online. Draping. vetsurgeryonline.com
Virtual Vet Surgery (University of Melbourne). Construction of Surgical Instruments. lms.vet.unimelb.edu.au
Animal Hospital Supply. Veterinary Draping 101. animalhospitalsupply.com
McCurnin's Clinical Textbook for Veterinary Technicians. Elsevier. elsevier.com
Clinician's Brief. Preoperative Surgical Site Preparation in Veterinary Medicine. cliniciansbrief.com

X min read

Skin Antisepsis Protocol for Dogs

Skin antisepsis is the step that bridges medical and surgical asepsis. It is the last contamination-reduction opportunity before the incision, and the most frequently incorrectly performed step in surgical site preparation.

A 2018 study in dogs (BMC Veterinary Research, PMC5852956) found that both chlorhexidine-alcohol and povidone-iodine protocols produced no bacterial growth in 70 to 74% of post-antisepsis samples. In the remaining 9% of cases, a significant bacterial reduction was not achieved, indicating possible resistance or incomplete technique.

What this covers: The complete skin antisepsis protocol for dogs undergoing surgical procedures, including clipping standards, agent selection, scrub technique, application count, contact time, and transition to draping.Scope: Applies to all dogs undergoing surgery involving skin incision. Some elements (agent selection, dilution) also apply to wound preparation and IV catheter site preparation.Evidence base: BMC Veterinary Research (2018) comparative study in 46 dogs; PMC6149254 comparative study of chlorhexidine + cetrimide vs. povidone-iodine in 15 dogs; vetnurse.au best practice protocol for veterinary surgical skin preparation.Key clinical point: Alcohol is the component of combined antiseptic preparations (CHG-alcohol, PVI-alcohol) that provides the majority of the immediate bactericidal effect. Chlorhexidine provides the residual activity. Understanding this separation clarifies why agent selection and combination matter.

Key takeaways

Clipping timing matters: Immediate pre-operative clipping (within minutes of surgery) consistently outperforms night-before clipping due to recolonization of the prepared site during the interval.
Clippers, not razors: Razor blades create micro-abrasions that increase bacterial colonization at the wound margin. Clippers are the current standard.
Centrifugal direction is not optional: Scrubbing toward the incision center after working away from it recontaminates the prepared site. Direction must be maintained throughout.
Contact time is frequently skipped: The antiseptic must remain in contact with the skin for the required duration to achieve its labeled kill claim. Immediate drying negates the antimicrobial action.
Alcohol in combination adds immediate efficacy: Pure chlorhexidine or povidone-iodine without alcohol has slower onset than the alcohol-containing combination. Alcohol-based combinations are increasingly preferred.
Chlorhexidine must not contact ears, eyes, or open peritoneal/pleural cavities at surgical concentrations: These are the primary safety constraints for canine skin antisepsis agent selection.

Step 1: Timing and patient preparation

Clip-to-incision interval

Immediate pre-operative clipping is the current standard. The rationale:

Shaved or clipped skin begins recolonizing within hours
Night-before clipping allows sufficient recolonization time to partially negate the antisepsis step
Micro-abrasions from clipping (particularly with razors) increase rapidly over the hours following hair removal
In the OR or immediately before patient transport to the OR is optimal

Hair removal: clippers, not razors

Razors are contraindicated for pre-surgical hair removal in dogs.

A 2019 study (AJVR, Messiaen et al.) evaluated colony-forming unit counts on dog skin after clipping with two clipper blade sizes. Blade selection affects the closeness of the clip and the degree of skin microtrauma. Regardless of blade size, clippers produced substantially less skin microtrauma than razors.

Clipping protocol:

Use clean, appropriately sized clipper blades
Clip in the direction of hair growth first, then against if needed for a close clip
Clip a generous margin around the anticipated incision: minimum 5 to 10 cm beyond the longest anticipated incision extent
Vacuum or remove clipped hair from the patient before moving to the prep area
Do not wet the site before clipping (increases skin trauma and introduces moisture that complicates antiseptic application)

Step 2: Gross cleaning (pre-prep wash)

If the skin is visibly soiled (mud, feces, blood), a gross cleaning step precedes antiseptic application:

Rinse the area with warm water
Apply a mild soap or surgical scrub solution; gentle cleaning to remove visible contamination
Rinse thoroughly with sterile water or saline
Pat dry with sterile gauze before proceeding to antiseptic application

Do not use the antiseptic scrub solution for gross cleaning. Reserve it for the antiseptic phase after gross contamination is removed.

Step 3: Antiseptic agent selection

Chlorhexidine gluconate (CHG)

Why it is generally preferred for canine skin antisepsis:

Broad spectrum against gram-positive and gram-negative bacteria, yeasts, and fungi
Excellent residual (persistent) activity: binds to skin proteins and continues killing after application
Better-tolerated on canine skin than povidone-iodine in studies showing higher contact dermatitis rates with PVI

Concentrations for surgical prep:

Use	Concentration
Standard surgical scrub	2 to 4% CHG scrub solution
Final antiseptic solution	0.5 to 2% CHG in 70% isopropyl alcohol
Wound irrigation (if used)	0.05% CHG (dilute from concentrate: 1 mL CHG 5% to 99 mL water)

Contraindications:

Ear canals and tympanic membrane: ototoxic
Open pleural or peritoneal cavities at surgical concentrations: tissue toxic
Eyes and corneal contact: irrigate immediately if accidental contact occurs

Povidone-iodine (PVI)

Broad spectrum including bacteria, fungi, viruses, and spores at active concentrations
Less residual activity than CHG (inactivated by blood and organic material)
Higher incidence of acute contact dermatitis in dogs compared to CHG in some studies
Remains the preferred agent for ophthalmic surgical preparation (safe for corneal contact at 0.5 to 5% diluted solution)

Alcohol combination

Adding 70% isopropyl or ethyl alcohol to either CHG or PVI preparation provides:

Rapid immediate bactericidal action (alcohol is fast-acting)
Enhancement of the companion antiseptic's efficacy at the skin surface

A systematic review and meta-analysis (PMC3434203) noted that outcomes from chlorhexidine-alcohol combinations are often attributed to CHG alone, when alcohol contributes substantially to the observed efficacy. The combination is clinically superior to either agent used alone.

For antisepsis as part of the broader asepsis framework, including how surgical skin antisepsis relates to instrument sterilization and aseptic technique in the perioperative infection control chain, that guide covers the conceptual framework.

Step 4: Antiseptic application technique

The centrifugal scrub

Direction: Start at the center of the incision site and work outward in expanding circles. Never reverse direction (working back toward the center after moving outward recontaminates the center).

Method:

Apply antiseptic scrub to sterile gauze
Begin at the intended incision center
Work in concentric circles outward to the clip margin
Discard the gauze and use a fresh piece for each application pass
Repeat for the required number of applications

Application count

Minimum standard: three complete application passes. Each pass uses a fresh piece of gauze and covers the full prep area from center outward.

Some protocols specify alternating scrub (CHG or PVI) and solution (alcohol), with the final step being the antiseptic solution rather than the scrub:

Alternating protocol:

Pass 1: CHG or PVI scrub (outward)
Pass 2: 70% alcohol (outward)
Pass 3: CHG or PVI scrub (outward)
Final: CHG-alcohol solution applied and allowed to dry

Contact time

The antiseptic must remain in contact with the skin surface for its required duration. Common error: patting dry immediately after application.

CHG scrub: minimum 2 minutes total contact time across the application sequence
PVI scrub: minimum 5 minutes total contact time (PVI has slower onset than CHG)
Final alcohol or CHG-alcohol solution: allow to fully evaporate before draping (fire risk from electrosurgery if alcohol has not fully evaporated)

Note from vetnurse.au: "When unsure, the rule of thumb is to leave the solutions on for at least 5 minutes and remember iodine needs longer than chlorhexidine."

Step 5: Transition to draping

Once the antiseptic prep is complete:

Confirm the prep site is fully dry (alcohol evaporated; no visible moisture)
Transfer the patient to the OR or final surgical position
A gowned, gloved scrub technician applies sterile drapes
Drapes are placed from the incision site outward; once placed, not repositioned
The draped site becomes part of the sterile field

Any contamination of the prepped site during patient transfer requires restarting the prep sequence.

The sterile draping step is the bridge between skin antisepsis and the intraoperative aseptic technique that governs the rest of the procedure. For antisepsis as part of aseptic technique, including how skin antisepsis integrates with gowning, gloving, sterile field establishment, and intraoperative technique in the full perioperative sequence, that guide covers the complete intraoperative framework.

Common preparation errors

Error	Consequence	Correction
Night-before clipping	Significant bacterial recolonization before antisepsis	Clip immediately pre-operatively
Razor use	Micro-abrasions increase colonization	Use clippers only
Reversed scrub direction	Center recontaminated after prep	Centrifugal direction only; discard gauze after each pass
Insufficient contact time	Antiseptic kill claim not achieved	Observe required contact time for agent used
Single-pass prep	Inadequate bacterial reduction	Minimum three application passes
Wrong agent for site	Ear/eye toxicity with CHG; poor residual with PVI	Match agent to anatomical location
Alcohol not dry before draping	Fire risk with electrosurgery	Confirm full evaporation before draping

For skin antisepsis within surgical asepsis, including where skin antisepsis fits within the five-domain surgical asepsis framework and how it relates to the other perioperative steps, that guide covers the full context.

Frequently asked questions

Is chlorhexidine or povidone-iodine better for dogs?

Both achieve good bacterial reduction (74% and 70% no-bacterial-growth post-prep respectively in the BMC 2018 canine study). CHG is generally preferred for most canine surgical sites due to its superior residual activity and lower incidence of contact dermatitis. PVI is specifically preferred for ophthalmic surgery sites. Combined CHG-alcohol or PVI-alcohol preparations outperform either agent alone.

How wide should the prep area be?

At minimum, the clip and prep should extend 5 to 10 cm beyond the longest anticipated incision in every direction. For orthopedic procedures with potential for incision extension or implant manipulation, err generously. The prep area cannot be extended intraoperatively without contaminating the surgical field.

Can we use povidone-iodine for wound irrigation?

Dilute PVI (0.1 to 1%) has been used for wound irrigation, but its efficacy is significantly reduced by blood and tissue fluid. Sterile saline is the standard baseline for wound irrigation. For procedures where contamination control at closure is a priority, antiseptic lavage agents specifically designed for intraoperative use may be appropriate.

Should we scrub in circles or lines?

Published evidence from a feline study (PMC11195503) comparing circular and linear scrub methods found no significant difference in bacterial reduction between the two methods. The critical variable is technique consistency and ensuring full coverage of the prep area rather than the specific motion pattern. Centrifugal direction (outward from incision) is the consistent requirement regardless of circular or linear motion.

For skin antisepsis in cats for comparison, including how feline-specific anatomical considerations and agent sensitivity constraints differ from the canine protocol, that guide covers the feline skin antisepsis protocol in detail.

Skin antisepsis is where asepsis meets antisepsis: the step where the patient's own bacterial flora is reduced before the sterile field is established over the preparation. Every error in this step, wrong direction, insufficient contact time, night-before clipping, compromises the starting condition that all subsequent aseptic technique is designed to protect. The protocol matters as much as the agents.

Resources

The following sources were used as reference and background for this article:

NIH/PMC. Skin asepsis protocols as a preventive measure of SSI in dogs: chlorhexidine-alcohol versus povidone-iodine. ncbi.nlm.nih.gov
NIH/PMC. Comparative clinical effectiveness of chlorhexidine gluconate and povidone iodine for preventing SSI in dogs. ncbi.nlm.nih.gov
NIH/PMC. The Forgotten Role of Alcohol: Systematic Review and Meta-Analysis of Chlorhexidine in Skin Antisepsis. ncbi.nlm.nih.gov
VetNurse.com.au. Surgical Skin Preparation: Best Practice Protocol for Veterinary Nurses. vetnurse.com.au
The Veterinary Nurse. Surgical site infections: preparation, technique and perioperative prevention. theveterinarynurse.com

X min read

Surgical Site Preparation in Cats: Complete Guide

Surgical site preparation in cats follows the same fundamental sequence as in dogs clip, initial scrub, aseptic scrub, drape but cats present unique challenges that require specific adaptations.

Feline skin is more delicate than canine skin, cats are more stress-reactive in the clinical environment, and feline-specific anatomical features require attention during preparation.

Quick answer: Feline surgical site preparation follows the same sequence as dogs: clip in the prep room, initial gross scrub, then aseptic target-pattern scrub in the OR using chlorhexidine or diluted povidone-iodine, then sterile draping. Key differences: gentler clipping to avoid feline skin trauma, proactive stress management, and caution with alcohol in small cats.

Key takeaways

SSI rate in cats is approximately 1.5% vs 2.8% in dogs; same principles apply but feline skin tolerates scrubbing less well
Feline skin is more delicate: excessive pressure, concentrated alcohol, or dull blades cause skin trauma more readily than in dogs
Stress management before preparation improves cooperation: pheromones, minimal waiting time, and anxiolytic premedication reduce struggling during prep
The aseptic scrub sequence is identical to dogs: center to periphery, target pattern, discard gauze after each outward pass
Chlorhexidine and diluted povidone-iodine are both appropriate for cats; avoid full-strength alcohol on feline skin without prior antiseptic application
Prepuce flushing does not apply in female cats: focus perineal prep on the perianal and vulvar area

Why cats are different

In veterinary medicine, SSI rates are approximately 2.8% in dogs, 1.5% in cats, and 1.6% in horses.

Cats have a lower baseline SSI rate than dogs, which reflects both their fastidious grooming behavior and the generally shorter, more straightforward procedures commonly performed in feline surgery.

However, the lower rate does not mean preparation can be abbreviated. The same principles apply, adapted for feline anatomy and behavior.

Key feline-specific considerations:

Thinner, more sensitive skin prone to clipper trauma
Higher baseline stress level in the clinical environment
Dense, double-layered coat (longhaired breeds) requires more careful clipping
Smaller body size means smaller prep fields and less margin for error
Unique anatomy in perineal procedures (no prepuce; different perianal structure than dogs)

Step 1: Stress management before preparation

Pheromone therapy: synthetic feline facial pheromones may be used to reduce anxiety and promote relaxation. Pre-medication: in some cases, mild sedatives or anxiolytics are given before preparation to calm very anxious cats safely. Proper stress management protects both the cat and veterinary staff during surgical site preparation.

Cats that are struggling during preparation produce a substandard prep quality inconsistent coverage, skin trauma from clippers, and potential contamination from patient movement. Addressing stress before preparation begins produces better outcomes.

Pre-preparation stress management:

Minimize waiting time in the clinic before induction
Use Feliway or equivalent synthetic pheromone in the prep room
Allow the cat to reach an appropriate depth of anesthesia before beginning preparation
Use low-stress handling throughout: minimal restraint, no scruffing unless essential

Step 2: Hair clipping

General technique:

Use electric clippers with a clean, sharp blade
A size 40 blade is standard for most feline surgical sites
Clip gently feline skin is thin and more susceptible to clipper burns than canine skin
Clip a generous margin: at minimum 5 cm beyond the proposed incision on all sides
Vacuum or remove clipped hair before moving to the prep room antiseptic scrub step

Longhaired breeds: Maine Coons, Persians, Norwegian Forest Cats, and Ragdolls have coats that may require a coarser blade for initial length reduction before the fine blade. Take extra care to avoid tangling and skin pulling.

Do not use razors: Do not use razors, which can cause micro-lacerations that may promote infection.

Perineal and perianal prep in female cats: clip the perianal area broadly and flush the vaginal vestibule with 0.05% chlorhexidine diacetate for procedures in this region.

Step 3: Initial scrub (gross decontamination)

Performed in the prep room before the cat enters the OR.

In cats, apply the initial scrub with gentle pressure. Feline skin is thinner than canine skin and excessive scrubbing at this stage causes irritation that compromises the aseptic scrub in the OR.

Step 4: Transfer to OR and positioning

Position the cat on the surgical table and connect anesthetic monitoring before beginning the aseptic scrub. The cat must be fully immobile during the aseptic scrub.

Step 5: Aseptic scrub in the OR

The technique is identical to dogs:

Target pattern: begin at the center of the proposed incision site and work outward in concentric circles to the edge of the clipped field. Discard each gauze after a single outward pass. Never return toward the center with a used gauze.

Number of cycles: typically three alternating cycles of antiseptic scrub and rinse. Contact time for each antiseptic application must be respected.

Circular vs linear scrub: A feline study (PMC11195503) comparing circular and linear scrub methods found no significant difference in bacterial reduction between the two methods. The critical variable is technique consistency and ensuring full coverage of the prep area rather than the specific motion pattern.

Antiseptic selection in cats

Chlorhexidine gluconate

Chlorhexidine at appropriate dilution is the preferred antiseptic for most feline surgical site preparation. It has residual activity (continues working after application) and is well-tolerated by feline skin at correct concentrations.

Chlorhexidine and diluted povidone-iodine are the best antiseptics for cats. They effectively kill bacteria while being gentle on sensitive feline skin.

Povidone-iodine (diluted)

Povidone-iodine is appropriate for cats when used at the correct dilution. Full-strength PI can cause significant skin irritation in cats. The standard dilution for wound and skin use is 0.1 to 1%.

Alcohol

Isopropyl alcohol (70%) is used as a rinse between antiseptic applications in some protocols.

In cats, exercise caution with alcohol: apply only after an initial antiseptic application, and avoid prolonged contact or pooling.

Evaporative heat loss is significant in small cats and can cause hypothermia.

Do not mix antiseptics

As with dogs, do not use chlorhexidine and povidone-iodine on the same patient in the same preparation session due to potential chemical incompatibility.

Step 6: Draping

After the aseptic scrub, the sterile surgical team applies corner drapes followed by a large fenestrated drape.

In cats, the relative smallness of the prep field means drape placement must be precise the margin between the clipped edge and the incision is smaller than in large-breed dogs.

For the equivalent guide for dogs, see surgical site preparation in dogs: complete guide. For the sterile field principles that follow draping, see maintaining a sterile field in veterinary surgery.

For the full SSI prevention overview, see surgical site preparation in cats: complete guide.

Frequently asked questions

Is surgical site preparation the same in cats as in dogs?

The sequence is identical.

The differences are in execution: gentler clipping, more attention to stress management, more careful alcohol use, and awareness that feline skin tolerates scrubbing less well than canine skin.

Do cats need sedation before surgical site preparation?

Cats are anesthetized before preparation begins, so the question is really about the depth and timing of anesthesia induction. Allow adequate anesthetic depth before starting prep.

For very anxious cats, anxiolytic premedication before induction reduces struggling and stress and improves prep quality.

Can I use the same antiseptic for cats as I use for dogs?

Yes. Chlorhexidine gluconate and diluted povidone-iodine are appropriate for both species. The same rule applies: do not mix them on the same patient.

Take care with alcohol rinse in small cats where evaporative cooling is a hypothermia risk.

How wide should the clip field be in cats?

At minimum 5 cm beyond the proposed incision on all sides. This is a smaller absolute area than in large-breed dogs but the same relative principle.

For small cats and kittens, the absolute size of the prep field is smaller but the same proportional margin applies.

Should I bathe a cat before surgery?

Some clinics recommend bathing 24 hours before elective surgery to reduce skin bacterial load.

Never bathe on the day of surgery wet fur causes hypothermia under anesthesia and may cause skin irritation that increases SSI risk. Confirm your clinic's policy with the supervising veterinarian.

Resources

Clinician's Brief. Preoperative Surgical Site Preparation in Veterinary Medicine. cliniciansbrief.com
The Veterinary Nurse. Surgical Site Infections: Preparation, Technique and Perioperative Prevention. theveterinarynurse.com
VetNurse Australia. Surgical Skin Preparation: Best Practice Protocol. vetnurse.com.au
VIN / WSAVA 2014. Maintaining a Sterile Operating Environment. vin.com

X min read

Isolation Protocols for Infectious Dogs

When a dog arrives at a veterinary clinic with a suspected contagious disease, the default action is immediate isolation. Not after triage. Not after confirmation. Immediately.

Every contact point the infectious patient makes on the way to an isolation room is a potential contamination event.

Dogs with suspected parvovirus, kennel cough, or leptospirosis that are walked through a general reception area can leave contamination that persists for hours or, in the case of parvovirus, months.

Quick answer: Suspected infectious dogs go directly to isolation on arrival, bypassing reception and general wards. Parvovirus needs strict isolation, parvocidal disinfectants, and full PPE. Leptospirosis is zoonotic and requires face protection. Kennel cough requires both contact and respiratory precautions.

Key takeaways

Move suspected infectious dogs directly to isolation on arrival; do not walk them through general areas or reception
Canine parvovirus survives for months in the environment: only accelerated hydrogen peroxide or bleach at correct dilution eliminates it
Leptospirosis is zoonotic: spreads via contact with urine on mucous membranes or wounds; face protection and dedicated footwear are mandatory
Kennel cough (CIRDC) spreads via droplets and fomites: respiratory precautions and contact precautions are both required
Only staff directly involved in care should enter isolation; pet owners should not enter the isolation ward
No equipment from outside isolation (stethoscopes, thermometers, cell phones) enters the isolation room; all equipment is dedicated

Which diseases require dog isolation?

Canine parvovirus (CPV)

The most serious canine infectious disease in hospital settings.

AVMA: "Canine parvovirus is easily spread by direct contact with infected dogs, contact with their feces, or virus-contaminated surfaces like kennels, food bowls, and the clothing of people who handle infected dogs."

Indiana State Board of Animal Health: "Parvo is very stable in the environment, able to withstand freezing temperatures and many disinfectants.

The organism can live in the environment as long as seven months."

UC Davis IDC Protocol: "Move patient directly to examination room or cage in isolation. Notify the infectious disease control personnel." Disinfection: "Cleaning and disinfection with 1:16 dilution of accelerated hydrogen peroxide."

ASPCA Pro: "Promptly isolate diagnosed cases from the remainder of the population. Effectively sanitize or discard any exposed areas or items."

Minimum isolation duration: at least 14 days from resolution of clinical signs, given environmental virus persistence.

Canine infectious respiratory disease complex (CIRDC / kennel cough)

CIRDC is caused by multiple pathogens including Bordetella bronchiseptica, canine parainfluenza virus, canine influenza virus, and others. It spreads via droplets and fomites.

Animal Urgent Care: "Kennel cough, or canine infectious respiratory disease complex, is one of the most well-known contagious illnesses in dogs.

It often appears like a dog has something stuck in its throat when it is actually just the irritation from the infection."

UC Davis IDC Protocol (for distemper and respiratory disease): "Strict isolation if any respiratory signs are noted. House dogs in isolation at least 4 feet away from other patients."

Both droplet precautions (mask for staff within 3 to 5 feet) and contact precautions (gloves, gown) apply.

Canine distemper

UC Davis IDC: "Major disease manifestations: Fever, ocular and nasal discharge, coughing, tachypnea, vomiting, diarrhea, neurological signs, immunosuppression." Transmission: droplet secretions from saliva, tears, urine, and contaminated fomites.

Full isolation with respiratory precautions. Disinfection with routine hospital-grade disinfectants is effective distemper virus is not environmentally persistent like parvovirus.

Leptospirosis

Leptospirosis is a bacterial zoonosis with significant implications for staff safety.

Veterinary Practice: "The infection can spread through any form of contact with wounds or mucous membranes, directly or indirectly through urine, and can survive up to three months in contaminated water supplies."

Veterinary Practice: "Ideally, the possibility of leptospirosis should be flagged before the appointment to allow staff to create a plan.

The kennel and isolation area can be prepped for the patient's arrival and the owner will know to call ahead when they arrive.

The patient can then enter through a separate exterior door."

Veterinary Practice: "It is important to keep track of where the patient has been kennel logs are particularly useful to ensure the correct hygiene and cleaning procedures are followed."

Leptospirosis PPE: full contact precautions plus face protection are required. The pathogen enters through mucous membranes. Eye protection is mandatory when any contact with urine is possible.

Canine influenza

Rare in most regions but when present, highly contagious via droplets and aerosols. Full respiratory and contact precautions; separate airflow from other wards.

Multidrug-resistant organisms (MDRO)

Mississippi State IDC Manual: dogs with multidrug-resistant infections require restricted access, separate from other patients. This includes MRSA, extended-spectrum beta-lactamase (ESBL) producers, and other MDR organisms.

Setting up the isolation space

PMC: "Laboratory coats should be removed, and personnel must put on protective wear such as a disposable gown, gloves, and booties when entering the isolation ward.

Face protection may also be required, depending on the situation. A notice that outlines the required precautions should be posted on the door."

PMC: "Only the individuals directly involved in the care of the patient should enter isolation. Pet owners should not be allowed into the isolation ward.

No equipment used outside isolation (pens, thermometers, stethoscopes, cell phones) should be brought into isolation."

Required elements for a canine isolation room:

Separate from general wards with a closed door at all times
Separate ventilation where possible; if not, keep HVAC vent closed
Dedicated equipment: stethoscope, thermometer, food and water bowls, leash
Hand hygiene station immediately outside the room
Full PPE supply at the door: gowns, gloves, shoe covers, and masks or face shields
Biohazard waste disposal inside or directly adjacent to the room
Kennel log to track all contacts and cleaning events

PPE by disease category

Disease	Gloves	Gown	Mask	Face shield	Shoe covers
Parvovirus	Yes	Yes	Not required	No	Yes
CIRDC/kennel cough	Yes	Yes	Yes	Optional	Yes
Distemper	Yes	Yes	Yes	Optional	Yes
Leptospirosis	Yes	Yes	Yes	Yes	Yes (dedicated)
Canine influenza	Yes	Yes	Yes	Yes	Yes
MDRO	Yes	Yes	As applicable	As applicable	Yes

ASPCA Pro: "Follow good personal protective equipment practices. Utilize shoe covers or dedicated boots in isolation areas. Do not use foot baths, which can spread disease rather than prevent it."

Disinfection by pathogen

Pathogen	Effective disinfectants	Contact time
Parvovirus	Accelerated hydrogen peroxide (AHP); 1:16 dilution; 1:32 bleach	Per label
Bordetella/respiratory pathogens	Quaternary ammonium; AHP; bleach	Per label
Distemper virus	Most hospital-grade disinfectants	Per label
Leptospira	Quaternary ammonium; bleach; AHP	Per label
Canine influenza	Most hospital-grade disinfectants; AHP	Per label

Critical for parvovirus: standard quaternary ammonium compounds alone are not reliably effective against CPV. Only bleach at appropriate dilution or accelerated hydrogen peroxide should be used for confirmed or suspected parvovirus cases.

Cleaning sequence: remove gross contamination (feces, vomit, blood) first by mechanical scrubbing. Apply disinfectant after thorough cleaning disinfectants cannot penetrate organic material effectively.

Terminal cleaning after discharge of an infectious patient requires a complete two-cycle clean and disinfect of all surfaces, including walls, floor, ceiling fixtures, cage bars, and all equipment.

Isolation duration

Disease	Minimum isolation duration
Parvovirus	14 days after resolution of clinical signs
CIRDC (kennel cough)	Until 7 days after no clinical signs
Distemper	Until veterinarian confirms non-infectious; variable
Leptospirosis	Until 48 hours after initiating appropriate antibiotics; vet clearance
Canine influenza	14 days from onset or 7 days after clinical resolution

For the PPE guide covering all isolation-relevant equipment selection, see PPE use and barrier protection in veterinary clinics. For isolation protocols for cats, see isolation protocols for infectious cats.

For sterile field maintenance in the surgical context, see maintaining a sterile field in veterinary surgery.

Frequently asked questions

My dog has parvovirus. Can it be treated at home instead of the hospital?

Home treatment is sometimes elected for mild cases. In-hospital care gives better survival for moderate-to-severe disease. If home isolation is elected: full PPE, parvocidal disinfectants, and 14-day isolation from other animals.

Can a vaccinated dog get kennel cough?

Yes. Vaccines cover common strains but CIRDC has multiple causative agents. A vaccinated dog can still contract and transmit kennel cough from uncovered strains. Isolation applies regardless of vaccination status.

Is leptospirosis dangerous to the people treating my dog?

Yes. Leptospirosis is a significant zoonosis. Staff wear full PPE including face protection for suspected or confirmed cases. Any staff with potential exposure should report it to occupational health.

Can the parvo virus remain in the clinic after the dog is discharged?

Yes, if disinfection is inadequate. Parvovirus survives for months. Thorough cleaning followed by accelerated hydrogen peroxide or bleach at correct dilution is required. Absorbent materials that cannot be disinfected must be discarded.

How do I know when it is safe to end isolation?

Duration depends on the disease; veterinary clearance is required. Clinical resolution alone is not sufficient; parvovirus shedding can persist for 3 to 4 weeks after recovery.

My dog was exposed to a parvovirus case at the clinic. What should I know?

Contact your vet to assess vaccination status. Vaccinated adult dogs are generally well-protected. Unvaccinated or incompletely vaccinated dogs are at high risk. Incubation is 3 to 7 days.

Resources

ASPCA Pro. Canine Parvovirus. aspcapro.org
PMC. Infection Control Programs for Dogs and Cats. ncbi.nlm.nih.gov
UC Davis. Small Animal Infectious Disease Control/Biosecurity Protocol. safety.vetmed.ucdavis.edu
Veterinary Practice. Best Practice Infection Control. veterinary-practice.com
AVMA. Canine Parvovirus. avma.org

X min read

Quality Control Measures for Surgical Asepsis

Quality control in surgical asepsis is the structured system that confirms aseptic standards are being met, not just described.

Training tells the team what to do. Checklists document that it was done. Auditing confirms it was done correctly. SSI surveillance tells the clinic whether the cumulative effect is working. Each component is necessary; none is sufficient alone.

What this covers: The quality control framework for surgical asepsis in small animal veterinary practice, covering the specific QC measures, how they interact, and how quality data should feed back into protocol improvement.Core principle: Quality control in asepsis is a system, not a checklist. The measures described here form an integrated cycle: establish standards, monitor compliance, identify gaps, intervene, and re-assess.Evidence base: AJVR 2026 SSI definitions consensus confirmed the "surveillance effect": the act of participating in an SSI surveillance program increases compliance independently of specific findings. AJVR 2025 breach data confirmed that training alone does not maintain asepsis performance without external monitoring.

Key takeaways

QC is a cycle, not a checklist: Standards, monitoring, gap identification, intervention, and re-assessment form a continuous loop.
Auditing is the most sensitive QC tool for technique compliance.
Biological indicator testing is the most critical QC measure for sterilization.
SSI surveillance quantifies the patient outcome of all asepsis QC measures combined.
The surveillance effect is real: monitoring improves compliance independently of findings.
QC data must feed back into training and protocol revision to close the quality loop.

The quality control framework

Surgical asepsis quality control operates across four interconnected domains:

Standards: Defined protocols for every asepsis component (patient prep, instrument sterilization, team technique, OR environment)
Monitoring: Ongoing measurement of compliance against those standards
Analysis: Identifying gaps between standard and practice, distinguishing individual from systemic failures
Improvement: Training, protocol revision, and environmental changes that address identified gaps

The framework only works when all four domains are active. Standards without monitoring is assumption. Monitoring without analysis is data collection. Analysis without improvement is documentation of ongoing problems.

QC measure 1: Surgical safety checklists

Checklists convert protocol standards into verified, documented action. They are the most accessible and consistently evidence-supported QC tool for improving surgical safety outcomes.

A Veterinary Practice (2022) publication on infection control in the surgical environment notes that surgical checklists should be used to identify patient risks before surgery and improve team communication, while providing a standardized approach to theatre management.

What checklists quality-control:

Instrument pack indicator inspection before opening
Patient prep completion and technique
Surgical hand antisepsis completion
Pre-incision time-out including antimicrobial prophylaxis timing
Instrument count before closure
Between-case disinfection documentation

For checklists as quality control tools, including the phase-by-phase surgical asepsis checklist and how to implement it as a formal QC document, that guide provides the operational reference.

QC measure 2: Intraoperative auditing

Checklists verify that steps were completed. Auditing verifies that steps were completed correctly.

This distinction is significant. A team can complete a checklist item ("surgical hand antisepsis performed") while the technique used was incorrect. Auditing by a trained observer identifies technique compliance that self-reporting cannot.

Published evidence:

AJVR 2025 found that 46.3% of observed veterinary surgical procedures involved at least one aseptic protocol breach during scrubbing, gowning, and gloving alone. These breaches were largely undetected by the personnel themselves. External observation identified them.

Audit structure:

Trained observer present during a sample of procedures (minimum 10% of cases per month)
Standardized observation tool covering hand antisepsis technique, gloving, sterile field maintenance, OR behavior
Non-punitive debrief after case completion (not during surgery)
Audit findings documented with date, case type, and specific deviations noted
Results reviewed monthly to identify patterns

For auditing as a quality control method, including the full audit framework with sampling strategy, observation tools, and feedback protocols, that guide covers intraoperative auditing in comprehensive detail.

QC measure 3: Autoclave validation

Sterilization quality control has its own specific monitoring hierarchy. Instrument sterility is the prerequisite for everything else in surgical asepsis; if sterilization fails, no amount of correct technique downstream compensates.

The three-level autoclave QC system:

Mechanical monitoring (every cycle): Cycle records confirm temperature, pressure, and time parameters were met
Chemical indicators (every pack): External and internal indicators confirm the pack was processed and the sterilizing agent penetrated
Biological indicators (weekly minimum): Spore tests confirm the cycle killed G. stearothermophilus: the only direct confirmation of functional sterility

Class 5 chemical integrating indicators are valuable but cannot substitute for biological indicators. Dispomed (2026): "Class 5 indicators can demonstrate that certain cycle parameters were reached, but they cannot confirm that all microorganisms were killed."

Documentation: Every biological indicator result, positive or negative, must be logged with the date, cycle number, and technician initials. Failed results trigger immediate autoclave removal from service.

For autoclave validation as quality control, including the validation protocol, monitoring schedules, and failed indicator response procedure, that guide covers sterilization QC in full.

QC measure 4: SSI surveillance

SSI surveillance is the outcome measure that validates whether all other QC measures are working. It is also the most powerful single driver of compliance improvement through the surveillance effect.

The surveillance effect:

AJVR 2026 notes that in human healthcare, clear temporal associations between implementation of SSI surveillance programs and decreases in SSI rates have been demonstrated. "Simply the act of participating" in surveillance increases compliance with SSI prevention practices. This surveillance effect operates independently of any specific findings.

SSI surveillance components:

Standardized SSI definition applied consistently (AVMA Journal 2026 consensus definitions for veterinary use)
Post-operative follow-up protocol (14-day wound check as minimum)
SSI data recorded by procedure type, wound class, personnel, and outcome
Monthly or quarterly SSI rate review
Trend analysis to identify clusters or increases warranting investigation

Using SSI data:

SSI rate by procedure type provides the clearest signal. A clean-wound SSI rate consistently above 5% in a veterinary practice indicates a systemic asepsis problem requiring investigation across all QC domains.

For errors that quality control aims to prevent, including the most common aseptic error categories with published incidence data and what QC measures are most effective at detecting each, that guide covers the error taxonomy that QC is designed to address.

QC measure 5: Environmental monitoring

OR environmental quality control confirms that the physical environment supports aseptic technique rather than undermining it.

Environmental QC components:

Surface swabs: Taken from high-contact OR surfaces after between-case disinfection; quarterly baseline with increased frequency after any SSI cluster
Air sampling: Settle plates or volumetric sampling during occupied OR conditions; provides baseline contamination data
Positive pressure verification: Smoke pencil or manometer confirmation that the OR maintains positive pressure relative to adjacent spaces
HVAC maintenance records: Filter replacement, service history, and any pressure differential anomalies documented

Environmental monitoring data should be reviewed alongside SSI rates. An SSI cluster coinciding with a documented HVAC failure or positive pressure loss provides a clear causal relationship requiring investigation.

Connecting QC measures to the improvement cycle

Quality control data has no value unless it drives improvement. The improvement connection requires:

For checklist findings: Any consistently missed checklist item should trigger a review of whether the step is practically achievable within the surgical workflow or requires scheduling/resource changes.

For audit findings: Individual technique deviations → targeted training and observed re-assessment. Systemic pattern across multiple personnel → protocol review or environmental change (e.g., ABHR placement, gloving technique resource).

For autoclave failures: Immediate investigation and repair. Post-repair validation before return to service. Review of all cases in the quarantine window for SSI monitoring.

For SSI rate increases: Structured case review. Cross-reference with audit findings, environmental monitoring, and any protocol changes that preceded the increase. Root cause analysis before intervention.

Documentation of improvement actions: Every identified gap should have a corresponding documented action, responsible person, and follow-up date. Without documentation, quality improvement is anecdotal.

Frequently asked questions

How often should the full QC program be formally reviewed?

Annually at minimum, or whenever a significant SSI event occurs, a new surgical procedure type is introduced, major staff changes occur, or any audit or surveillance data shows a consistent negative trend. An annual comprehensive review covers all four QC domains and assesses whether improvement actions from the prior year produced the expected results.

Should QC findings be shared with all surgical staff?

Yes. Aggregate findings (not individual-level unless performance management is involved) should be shared with the team regularly. Transparency about QC findings builds the culture of quality and accountability that is prerequisite for the surveillance effect to work. Staff who understand QC outcomes and their own contribution to them are more likely to maintain compliance.

Is QC documentation a regulatory requirement?

In many jurisdictions and institutional settings, yes. Autoclave validation records, biological indicator logs, and SSI surveillance data are specifically required by IACUC protocols, veterinary regulatory bodies, and accreditation standards in various countries. Even where not formally required, documentation demonstrates due diligence and supports medicolegal defense if an SSI event results in a complaint or claim.

Quality control in surgical asepsis does not guarantee zero SSI. It guarantees that the practice knows what its aseptic standards are, is actively measuring whether they are being met, and is consistently acting on the gaps it finds. That is the difference between a practice that assumes it is doing well and one that knows it is.

Resources

The following sources were used as reference and background for this article:

AVMA Journals. Surgical site infection definitions consensus in veterinary medicine. AJVR, 2026. avmajournals.avma.org
AVMA Journals. Aseptic protocol breaches are common among veterinary students. AJVR, 2025. avmajournals.avma.org
Dispomed. The Gold Standard of Sterilization: Why Biological Indicators Matter in Veterinary Practice. dispomed.com
Veterinary Practice. Infection control in the surgical environment. veterinary-practice.com

X min read

We'd love you to
Join Us!

Thank you! Your submission has been received!

Oops! Something went wrong while submitting the form.

Taking Great TPLO Radiographs

Click Below to Watch Live Video Demos

We'll send you a Free Wall Poster with all the steps

Now that you are a pro at TPLO rads

Let's take your infection control to the next level

Watch these videos!

Step #1

Getting Ready

Ensuring a clean surgical field starts with proper skin preparation. This video demonstrates the best practices for:

Shaving the patient – Achieving a close, even shave while minimizing skin irritation
The Dirty Scrub – The initial skin prep step to remove surface debris and reduce bacterial load before the sterile scrub.

Following these techniques helps reduce infection risk and improve surgical outcomes. Watch the video to see how it’s done effectively!

Step #2

Reduce Your Risks

Many surgeons are shocked to find out that their patients are not protected from biofilms and resistant bacteria when they use saline and post-op antibiotics.

That’s Where Simini Comes In.

‍Why leave these risks and unmanaged? Just apply Simini Protect Lavage for one minute. Biofilms and resistant bacteria can be removed, and you can reduce two significant sources of infection.

Protect Your Patients

Step #3

Take the Course

Preventing surgical infections is critical for patient safety and successful outcomes. This course covers:

Aseptic techniques – Best practices to maintain a sterile field.
Skin prep & draping – Proper methods to minimize contamination.
Antibiotic stewardship – When and how to use perioperative antibiotics effectively.

Stay up to date with the latest evidence-based protocols. Click the link to start learning and earn CE credits!

Things to know

Asepsis

5 min read

Isolation Protocols for Infectious Cats

Learn effective isolation protocols for infectious cats to prevent disease spread and protect your home and pets.

When a cat arrives at a veterinary clinic with a contagious disease or is suspected of having one isolation is the most important immediate action.

Every minute a contagious patient spends in the general population is an opportunity for transmission.

Isolation protocols protect other patients in the hospital, protect staff, and protect the community's cats whose owners have not yet vaccinated them against the pathogens circulating in the clinic.

Quick answer: Suspected infectious cats go directly to isolation on arrival. Isolation needs dedicated equipment, full PPE for all staff entering, daily disinfection, and airflow separation from general wards. FPV requires at least 14 days isolation; URI typically 3 to 7 days after clinical improvement.

Key takeaways

Move suspected infectious cats directly to isolation on arrival do not route them through reception or general wards
FPV requires at least 14 days isolation; the virus survives on surfaces for months and needs parvocidal disinfectants
Feline URI spreads via droplets up to 5 feet and via fomites (hands, clothing, equipment) standard contact precautions are required
Ringworm is zoonotic: staff handling ringworm-positive cats need full contact PPE; precautions extend to the home
Dedicated equipment (stethoscope, thermometer, food dishes, bedding) stays in the isolation room; shared equipment brings contamination in and out
Separate airflow from the general ward is recommended; if unavailable, keep the door closed and minimize ventilation exchange

Which diseases require cat isolation?

Feline panleukopenia (FPV)

The most serious feline infectious disease in hospital settings.

ASPCA Pro: "Cats with FPV must be moved to an isolation area separate from unaffected and unexposed populations of cats.

Skilled staff with clinical treatment experience and knowledge of biosecurity should be assigned to the isolation ward."

ASPCA Pro: "Cats under treatment should remain in isolation for at least 14 days."

FPV is transmitted through fecal-oral contact and contaminated fomites. The virus is extremely environmentally stable it can survive on surfaces for months.

Only specific disinfectants (accelerated hydrogen peroxide, bleach at appropriate dilution) are effective against parvovirus.

ASPCA Pro: "If isolation is not available, animals with panleukopenia should be removed from the facility for treatment or euthanized to curtail their suffering and minimize disease spread."

Feline upper respiratory infection (URI)

The most common feline contagious disease encountered in clinical settings.

ASPCA Pro: "Feline URI easily spreads in shelter environments via fomites including hands, scrub tops, stethoscopes, toys, and shoes.

Feline URI can also be transmitted by droplets over distances of 5 feet or less."

Causative agents include feline herpesvirus (FHV-1) and feline calicivirus (FCV). Both can be transmitted via fomites and direct contact.

Calicivirus can also cause virulent systemic disease (FCV-VSD) a more severe form with skin lesions that has been reported as a post-surgical complication.

Best Friends Animal Society protocol: "PPE/handling restrictions lifted after 3 days" of no clinical signs in mild URI cases. Moderate to severe cases require longer isolation.

Ringworm (dermatophytosis)

Ringworm is a fungal infection not a worm caused by Microsporum canis in most feline cases. It is highly contagious between cats, between cats and dogs, and between cats and humans.

Animal Urgent Care: "Ringworm spreads through direct contact as well as contaminated bedding, furniture, and grooming tools."

Ringworm is zoonotic.

Staff handling ringworm-positive cats must use full contact precautions and should be aware that environmental contamination is extensive spores shed from infected cats can survive in the environment for months.

UC Davis IDC Protocol: disinfection requires an accelerated hydrogen peroxide product or dilute bleach; many common disinfectants are ineffective against dermatophyte spores.

Feline leukemia virus (FeLV) and feline immunodeficiency virus (FIV)

FeLV spreads through close contact and bodily fluids; FIV primarily through bite wounds. These viruses are not environmentally stable and standard contact precautions (gloves, hand hygiene) are sufficient.

Full isolation is not required for FeLV/FIV-positive cats in most hospital settings, but they should not be housed with FeLV/FIV-negative cats. Separate housing or adequate physical separation is required.

Setting up the isolation space

PMC (Infection Control Programs): "Isolation areas for sick animals should be present and these should have separate airflow from areas that house healthy animals."

PMC: "Isolation rooms may be poorly visible and/or accessible and may not provide access to an oxygen source or be amenable to intensive monitoring."

Minimum requirements for a feline isolation room:

Separate from all general ward areas
Door kept closed at all times when the room is occupied
Separate ventilation where possible; if not, close the HVAC vent serving the room
Dedicated equipment that never leaves the room: stethoscope, thermometer, food and water dishes, bedding, litter box and scoop
Hand hygiene station immediately outside the room (or inside if space allows)
PPE supply stocked outside the door: gowns, gloves, shoe covers, and masks or face shields where respiratory transmission is possible
Biohazard waste disposal within or immediately adjacent to the room

PPE requirements by disease category

Disease	Gloves	Gown	Mask	Shoe covers
FPV (panleukopenia)	Yes	Yes	Not required	Yes
URI (herpes/calicivirus)	Yes	Yes	Yes (within 5 feet)	Yes
Ringworm	Yes	Yes	Not required	Yes
FeLV/FIV	Yes	Recommended	Not required	Optional

Animal Urgent Care identifies the core elements as: wearing PPE when handling infectious patients, minimizing exposure within the facility, and maintaining separate isolation rooms sanitized after every patient.

Staff and workflow protocols

Assign dedicated staff to the isolation room whenever possible. Staff who have handled an isolation patient should not return to the general ward without removing PPE, performing hand hygiene, and changing contaminated scrubs.

UC Davis IDC Protocol: "Within Hospital: Move patient directly to examination room or cage in isolation. Notify the infectious disease control personnel."

Handling sequence:

Put on full PPE before entering
Complete all care for the isolation patient
Remove PPE inside or immediately outside the room (remove gloves last)
Perform hand hygiene
Change contaminated scrubs before entering general ward

Visit isolation patients last in the daily ward round, not between general patients.

Disinfection and cleaning

PMC: "Cages should be cleaned and disinfected at least daily." For FPV and ringworm cases, more frequent cleaning may be required.

Disinfectant selection by pathogen:

Pathogen	Effective agents
FPV (parvovirus)	Accelerated hydrogen peroxide; 1:32 bleach (sodium hypochlorite)
Feline herpesvirus	Accelerated hydrogen peroxide; quaternary ammonium compounds
Feline calicivirus	Accelerated hydrogen peroxide; bleach; some oxidizing agents
Ringworm spores	Accelerated hydrogen peroxide; 1:10 bleach

Standard quaternary ammonium compounds (common hospital disinfectants) are NOT effective against parvovirus or ringworm spores. Choosing the correct disinfectant is critical.

Terminal cleaning after discharge: a thorough cleaning of all surfaces, including walls, floor, ceiling fixtures, and all equipment. For parvovirus and ringworm cases, this requires two full cleaning and disinfection cycles.

Isolation duration guidelines

Disease	Minimum isolation duration
FPV (panleukopenia)	14 days after resolution of clinical signs
URI (mild)	3 days after no clinical signs
URI (moderate/severe)	7 days after no clinical signs
Ringworm	Until two consecutive negative fungal cultures
FeLV/FIV	Ongoing; separated housing, not full isolation

ASPCA Pro (FPV): "Cats under treatment should remain in isolation for at least 14 days."

Best Friends protocol: "PPE/handling restrictions lifted after 3 days" for mild URI cases.

For isolation protocols for infectious dogs, see isolation protocols for infectious dogs. For the PPE selection guide that applies to isolation work, see PPE use and barrier protection in veterinary clinics.

Frequently asked questions

My cat has a suspected URI. Does it need to be in a separate room at the vet clinic?

Yes, ideally. Feline URI spreads via droplets and fomites within 5 feet.

Cats with respiratory signs should be examined in a dedicated room or a drape-separated exam space, not in an open area near other cats.

Can I visit my cat while it is in isolation?

Policies vary by clinic. Many hospitals allow owner visits with PPE and staff supervision. The visit is typically brief and conducted in the isolation room itself.

Ask your clinic what their isolation visiting policy is.

How long does FPV survive in the environment?

Parvovirus is extremely hardy. ASPCA Pro notes it can survive for extended periods on contaminated surfaces.

This is why terminal cleaning with a parvocidal disinfectant, not just standard cleaning, is essential after a confirmed FPV case.

Is feline calicivirus dangerous to staff?

Feline calicivirus does not infect humans. However, staff can transmit it to other cats via their hands, clothing, and equipment. Standard contact precautions protect other feline patients, not necessarily staff health.

My cat was diagnosed with ringworm. What precautions should I take at home?

Wear gloves when handling your cat and cleaning the litter box. Wash hands after contact. Avoid sharing bedding or brushes. Vacuum and disinfect regularly with a product effective against ringworm spores.

Does a confirmed FeLV or FIV-positive cat need to be in a separate isolation room?

Not usually. FeLV/FIV-positive cats need physical separation from negative cats, not a full isolation room. Standard contact precautions apply. Full isolation is reserved for acutely contagious diseases like FPV and URI.

Resources

ASPCA Pro. Feline Panleukopenia. aspcapro.org
ASPCA Pro. Feline Upper Respiratory Infection. aspcapro.org
PMC. Infection Control Programs for Dogs and Cats. ncbi.nlm.nih.gov
Animal Urgent Care. Isolation Protocols: A Necessary Safeguard for Common Infectious Diseases. animalurgentcare.vet
UC Davis. Small Animal Infectious Disease Control/Biosecurity Protocol. safety.vetmed.ucdavis.edu

Read Blog Post

Surgical Site Infection Prevention in Dogs

Asepsis

5 min read

Surgical Site Infection Prevention in Dogs

Learn effective surgical site infection prevention in dogs with expert tips on hygiene, antibiotics, and wound care for safer surgeries.

Surgical site infections are among the most studied complications in veterinary surgery, and the evidence base for preventing them has matured significantly in the last decade.

SSIs are not inevitable. They are the outcome of cumulative failures in preparation, sterile technique, wound management, and post-operative care. Addressing each phase systematically produces the consistently low infection rates that characterize high-quality surgical centers.

Quick answer: Surgical site infection prevention in dogs requires coordinated measures across three phases. Pre-operatively: patient screening and proper skin preparation. Intraoperatively: antibiotic prophylaxis timed 30 to 60 minutes before incision, sterile technique with iodine-impregnated drapes, orthopedic gloves, and intraoperative lavage. Post-operatively: E-collar use, incision monitoring, activity restriction, and follow-up attendance. Extended surgery time is the strongest identified patient-level SSI risk factor in clean surgical procedures.

Key takeaways

Extended surgery time is the strongest SSI risk factor in clean procedures per published veterinary evidence.
MRSP carrier status significantly raises SSI risk: one study found a 9x higher odds ratio.
Perioperative antibiotic prophylaxis without postoperative extension is sufficient for clean procedures.
Iodophore-impregnated adhesive drapes and orthopedic gloves reduce contamination risk intraoperatively.
The E-collar at home is the most important owner-controlled variable in post-operative infection prevention.
SSI rates in canine clean surgery range from 0.8% to 21.3% depending on procedure, center, and protocol quality.

Why SSI prevention matters: the clinical and financial stakes

Surgical site infections in dogs cause measurable harm beyond the immediate complication. A study referenced by Clinician's Brief reported the economic impact of SSIs after TPLO surgery in dogs as ranging from $110.21 to $3,817.12 USD per case, depending on the intervention required. Beyond cost, SSIs extend recovery, increase antibiotic exposure, and in cases involving orthopedic implants, may require hardware removal.

SSI rates in canine surgery vary widely: Clinician's Brief reports published rates ranging from 0.8% to 21.3% of surgical cases depending on procedure type, setting, and protocol quality. This range demonstrates that SSI is not a fixed background risk: it is heavily influenced by practice decisions at every phase of surgical care.

Pre-operative SSI prevention

Patient screening and risk factor management

Not all surgical patients carry equal SSI risk. Identifying and modifying controllable risk factors before surgery reduces baseline risk:

Active skin infections (pyoderma): must be fully resolved before elective surgery. Skin bacteria can contaminate the surgical field directly.
MRSP carrier status: a Finnish veterinary teaching hospital study (PMC7495856) identified MRSP carriage as a significant SSI risk factor with an odds ratio of 9.0. Dogs known or suspected to carry MRSP warrant specific pre-operative screening.
Obesity: impairs blood flow to wound edges and slows healing.
Metabolic conditions: diabetes, Cushing's disease, and hypothyroidism all compromise immune function and wound repair.
Higher body temperature: the same Finnish study found higher pre-operative body temperature was associated with increased SSI risk (mean difference of +0.4°C compared to dogs without SSI).

Skin preparation

The skin harbors the microorganisms most likely to contaminate a wound during surgery. Reducing skin flora at the operative site is a fundamental pre-operative measure:

Hair is clipped, not shaved (shaving creates micro-abrasions that increase bacterial colonization)
Chlorhexidine gluconate-based prep solution applied in a scrub-then-paint sequence
The prepared area extends well beyond the planned incision margins
A minimum skin preparation contact time is observed before draping

The Veterinary Nurse confirms: "Skin preparation and aseptic techniques aim to reduce or eliminate the growth of resident and transient flora at the wound site."

Intraoperative SSI prevention

Antibiotic prophylaxis: timing and duration

The evidence consistently supports perioperative antibiotic prophylaxis without postoperative extension for clean orthopedic and neurosurgical procedures in dogs.

The Finnish study (PMC7495856) found: "Antimicrobial prophylaxis without postoperative antimicrobials is sufficient to maintain the overall rate of SSI at a level similar to published data in canine clean orthopedic and neurosurgeries." Of 406 dogs reviewed, 92.9% received antimicrobial prophylaxis and only 1.1% received postoperative antimicrobials: the SSI rate was comparable to international benchmarks.

The correct protocol: intravenous cefazolin given 30 to 60 minutes before skin incision, repeated every 90 to 120 minutes intraoperatively if surgery exceeds the dosing interval.

For how antibiotic prophylaxis works within the broader SSI prevention framework, see prophylactic antibiotics in SSI prevention.

Sterile field management

Beyond antibiotics, maintaining a sterile intraoperative environment requires:

Iodophore-impregnated adhesive drapes applied to the skin at the operative field to prevent migration of skin flora into the wound
Orthopedic surgical gloves for implant procedures to reduce perforation risk
Double-gloving with glove changes after draping and at the 60-minute mark for extended procedures
Rigorous instrument handling by all operating room personnel
Limiting operating room traffic during the procedure

Managing surgery time

Extended surgery time is the only variable identified as a significant SSI risk factor in a large-scale European study of 1,550 dogs undergoing clean procedures (ScienceDirect). Every additional minute of open wound time increases cumulative bacterial exposure. Efficient surgical technique is an infection control measure, not just a quality-of-care issue.

Intraoperative wound lavage

Lavage with sterile isotonic saline before wound closure removes blood, bone debris, and bacteria that accumulate during surgery. This is particularly important in orthopedic procedures where implant surfaces provide an adhesion substrate for bacteria.

For how biofilm forms on implants and why lavage matters, see biofilm as a driver of surgical site infections.

Wound closure technique

Anatomical layer closure without dead space prevents the fluid accumulation that bacteria exploit post-operatively. Antimicrobial suture materials (triclosan-coated) inhibit bacterial colonization of the suture itself. The published TPLO protocol change study (PMID 29878479) demonstrated that replacing staples with antimicrobial intradermal sutures was one component of a bundle that reduced implant-associated infection from 8.5% to 1.3%.

Post-operative SSI prevention

At the hospital before discharge

Antimicrobial ointment (mupirocin) applied to the wound before bandaging
Soft-padded bandage protecting the wound during in-hospital recovery
E-collar placed before the dog recovers from anesthesia
Single-use gloves for all staff handling the post-operative wound

Owner responsibilities at home

The dog's owner becomes the primary infection control agent once the dog leaves the hospital. The key measures:

E-collar compliance: the most important single owner-controlled factor. Licking delivers oral bacteria directly to the incision and can bypass every intraoperative precaution. The E-collar must remain on whenever the dog is unsupervised.

Incision monitoring: daily visual inspection to identify redness, swelling, discharge, or odor early enough to intervene before deep infection establishes.

Activity restriction: running and jumping create mechanical stress on healing tissue and can open wound layers before they've fully healed, creating dead space and infection opportunity.

Follow-up attendance: post-operative rechecks are not optional. The 10 to 14 day recheck confirms wound healing and removes sutures. The 6 to 8 week recheck (for orthopedic procedures) confirms bone healing and implant stability.

For the practical SSI prevention guide owners use at home, see practical SSI prevention guide. For comparison with SSI prevention in cats, see SSI prevention in cats for comparison. For when infections appear despite prevention, see when surgical site infections typically emerge.

For how SSI prevention in dogs specifically applies to orthopedic cases, see reducing SSI risk in orthopedic cases.

The team culture dimension

The Veterinary Nurse notes: "It is increasingly recognised that team culture can significantly affect the perioperative management of the patient and hence, the SSI risk. A proactive team culture must be cultivated and maintained."

SSI prevention isn't solely a technical matter. Every member of the surgical team must understand their role in maintaining sterile conditions. Compliance with hand hygiene, barrier precautions, and protocol steps must be consistent across all personnel and all cases, not just the highest-profile ones.

Frequently asked questions

What is the most common source of surgical site infections in dogs?

The most common source is translocation of the patient's own skin flora into the wound. The Veterinary Nurse confirms: "Translocation of endogenous microbial flora is the most common route of surgical site infection." This is why skin preparation and sterile draping matter more than environmental contamination, which is a secondary concern.

My dog had SSI after a clean surgery. What likely went wrong?

The most common contributing factors in published veterinary SSI cases are: extended surgery time, inadequate skin preparation, break in sterile technique (often glove perforation or field contamination), failure of E-collar compliance at home leading to licking, and MRSP carriage that wasn't identified pre-operatively. A culture and sensitivity test of the infection identifies the pathogen and guides appropriate treatment.

Does my dog need antibiotics to go home after surgery to prevent SSI?

For clean orthopedic procedures, the published evidence does not support routine post-operative antibiotic courses. Perioperative dosing is sufficient when technique is correct. However, individual circumstances may warrant a post-operative course: contaminated or dirty wounds, immunocompromised patients, or cases where intraoperative contamination occurred. Ask your surgeon for the specific rationale if a post-operative antibiotic course is prescribed.

SSI prevention is a system, not a single action. The surgeon controls most variables intraoperatively, but the perioperative window spans days before and weeks after. When every phase is managed well, consistently low SSI rates are achievable across a broad range of surgical procedures in dogs.

Resources

Gronkjaer et al. Risk factors for SSI associated with clean surgical procedures in dogs. Vet J, 2021. sciencedirect.com
Heikkinen et al. Antimicrobial prophylaxis is sufficient in clean orthopaedic and neurosurgeries in dogs. BMC Vet Res, 2020. ncbi.nlm.nih.gov
Clinician's Brief. Bacterial Biofilms. cliniciansbrief.com
The Veterinary Nurse. Surgical site infections: preparation, technique and perioperative prevention. theveterinarynurse.com

Read Blog Post

Asepsis

5 min read

Draping Techniques in Small Animal Surgery

Explore essential draping techniques in small animal surgery to ensure sterile fields and reduce infection risks during procedures.

Draping is the step in surgical preparation that defines the sterile field.

It isolates the prepared skin at the incision site from all surrounding contaminated surfaces the patient's hair and skin, the surgical table, and the anesthetic equipment.

Done incorrectly, draping is just a gesture. Done correctly, it is the final barrier between the sterile surgical wound and the contaminated world around it.

Quick answer: Standard small animal draping uses four corner drapes to frame the incision, secured with towel clamps, then one large fenestrated drape over the patient and table. Drapes move only away from the incision. Orthopedic limb surgery uses free-draping for full limb manipulation.

Key takeaways

Four corner drapes frame the incision site first; a large fenestrated drape is placed on top as the final layer
Drapes can only move away from the incision site: moving toward the center contaminates the sterile field
Towel clamps become unsterile once they pierce skin: hand off to a non-sterile assistant before reusing
Drapes must never be shaken or fanned: air currents from rapid handling contaminate the prepared field
Free-draping is used for orthopedic limb surgery to allow full limb manipulation within a sterile field
Key sheet draping (single-drape method) is an alternative that eliminates the need for corner drapes and towel clamps

Why draping matters

The prepared skin has been decontaminated by clipping and antisepsis. But it still sits next to:

Unclipped hair at the edges of the prep zone
The patient's non-sterile body
The surgical table surface
Anesthetic circuit tubing
Any unsterile equipment around the patient

Drapes isolate the sterile island (prepared skin) from all of these contamination sources.

Drape types

Rectangular (utility / corner) drapes

These are the standard-size rectangular drapes used to frame the incision site during the initial four-corner step.

Animal Hospital Supply: "Corner drapes are doubled over at one end (9 to 10 cm) and placed at the periphery of the surgical field one at a time."

The drape edge is wrapped around the gloved hands to prevent contamination while covering the four corners.

The doubled-over edge faces toward the surgeon to protect the glove from contact with the non-sterile surface as the drape is applied.

Fenestrated drapes

A large drape with a pre-cut opening (fenestration) placed over the patient and table after the four corner drapes.

McCurnin's Clinical Textbook: "For final draping, a large fenestrated or unfenestrated drape is placed over the animal and the table.

The fenestration is placed over the incision site, or a slit is cut into the unfenestrated drape at the incision site."

Animal Hospital Supply: "A large sterile drape is placed over and above the four square-off drapes.

This large drape is then fenestrated, the fenestration through which the sterile surgical procedure is then performed."

SustainableVet: "Fenestrated drapes should be large, covering as much of the patient and table as possible."

Disposable vs. reusable drapes

Disposable drapes are made from synthetic non-woven material, single-use, and are discarded after each procedure. They eliminate the risk of inadequate sterilization between uses.

Virtual Vet Surgery: "Significant reductions in the numbers of bacteria in surgical wounds have been documented using disposable (single-use) and Opsite drapes."

Reusable linen drapes can be laundered and autoclaved. They are more economical over time but require careful inspection for holes and worn areas before each use.

Key sheets (single-drape method)

Animal Hospital Supply: "As in nearly every human surgical procedure in the US, some veterinary surgeries have moved toward a single drape or key sheet draping method.

The key sheet eliminates the need for all underneath draping and the need to clamp the drapes to the patient skin."

Key sheets are procedure-specific and often incorporate additional features: adhesive edges to secure to the patient, tube holders, fluid collection pouches for arthroscopy, and absorbent zones.

Four-corner draping: the standard sequence

McCurnin's: "Four quarter drapes are secured with towel clamps approximate to the incision."

Step 1: Apply corner drape 1 at the cranial edge of the proposed incision site.

Veterinary Surgery Online: "The first drape is generally applied at the cranial edge of the proposed incision site.

Once the drape is unfolded, it should not be turned around in order to maintain the most sterile portion (close to the hands) sterile."

Step 2: Apply corner drapes 2, 3, and 4, framing the other three sides.

The sequence "top, tail, near, far" is a common convention. Virtual Vet Surgery: "A placement pattern of top, tail, near, and far.

The reason for this: in deep-chested dogs, holding a lateral drape in place is difficult because a second drape has to be applied before it can be secured by a towel clamp."

Step 3: Secure with towel clamps.

McCurnin's: "If Backhaus towel clamps are positioned directly in the corners of a four-toweled drape set, the edges will lie flat and not bulge up."

Step 4: Apply the large fenestrated drape as the final layer over the entire patient and table.

Critical draping rules

Drapes only move away from the incision

Veterinary Surgery Online: "As drapes are applied, they can be moved away from the proposed incision site, towards the edge of the prepared area (without exposing hair).

Conversely, a drape cannot be moved from the site of application towards the center of the prepared area since this may lead to contamination of the prepared field."

This rule is absolute. Moving a drape toward the incision drags contamination with it.

Do not shake or fan drapes

Veterinary Surgery Online: "Drapes should not be shaken, fanned, or flipped rapidly when handled as this will create air currents and promote contamination of the prepared surgical field."

Drapes must be gently unfolded and placed never snapped open.

Drapes must cover the entire patient and table

SustainableVet: "Fenestrated drapes should be large, covering as much of the patient and table as possible." Any exposed surface represents a contamination risk.

Special situations

Orthopedic limb surgery: free-draping

For limb surgeries requiring full manipulation (TPLO, fracture repair), the limb is draped to allow it to move freely within the sterile field.

Virtual Vet Surgery: "For many orthopaedic procedures on the limbs, a 'free-draping' technique may be used to help surgical manipulation of the limb.

To isolate the limb, the limb is suspended using a drip stand with the foot enclosed inside a clean latex glove. The glove is secured to the foot with adhesive tape."

The limb is then clipped and prepared. Three corner drapes are placed around the base of the limb to isolate it from the trunk.

A sterile cohesive bandage is applied over the glove and up the limb before the final draping layer.

Male dog abdominal surgery: prepuce management

Veterinary Surgery Online: "If draping the abdomen of a male dog, the prepuce should be displaced laterally and held with a towel clamp to decrease contamination risk.

This should be done prior to draping the area in order to drape over the tip of the prepuce."

Procedure-specific draping

Thoracic surgeries: Require careful draping to isolate the chest area, often using multiple drapes."

For the site preparation that precedes draping, see surgical site preparation in dogs. For the sterile field context draping creates, see maintaining a sterile field in veterinary surgery.

For the PPE worn during draping, see PPE use and barrier protection in veterinary clinics.

Frequently asked questions

Why can drapes move away from the incision but not toward it?

This is a fundamental aseptic principle with no exceptions.

What happens if a drape becomes contaminated during application?

A contaminated drape must be replaced. If a drape contacts a non-sterile surface (the floor, an unsterile piece of equipment, the patient's non-prepped hair), it cannot be used further.

A new sterile drape replaces it.

Can the surgeon reposition a towel clamp once it has been placed?

If the clamp has penetrated skin, its tips are unsterile. McCurnin's: it must be handed off to a non-sterile assistant. A new sterile clamp is used for repositioning.

What is the advantage of key sheet draping over four-corner draping?

Key sheets are faster, eliminate the towel clamp skin-penetration issue, and are procedure-specific with integrated features like fluid pouches and tube holders. The tradeoff is higher per-use cost.

Why do drapes need to cover the entire patient and table, not just the immediate area?

The entire table surface around the patient is a potential contamination source. Any instrument, sponge, or implant that falls onto an uncovered table surface is contaminated.

Draping the full patient and table prevents these incidental contaminations.

Can a drape that has slipped during surgery be pushed back into place?

No. If a drape slips, alert the circulating nurse. A new sterile drape is placed over the exposed area. The slipped drape cannot be repositioned, regardless of how small the movement needed.

Resources

Veterinary Surgery Online. Draping. vetsurgeryonline.com
Virtual Vet Surgery (University of Melbourne). Construction of Surgical Instruments. lms.vet.unimelb.edu.au
Animal Hospital Supply. Veterinary Draping 101. animalhospitalsupply.com
McCurnin's Clinical Textbook for Veterinary Technicians. Elsevier. elsevier.com
Clinician's Brief. Preoperative Surgical Site Preparation in Veterinary Medicine. cliniciansbrief.com

Read Blog Post

Asepsis

5 min read

Asepsis During Wound Management

Learn essential asepsis techniques during wound management to prevent infections and promote healing in pets.

Wound management in veterinary practice spans a wide contamination spectrum, from simple laceration repair in the clinic to complex open wound management over weeks of repeated bandaging. The asepsis standard applied must match the wound and procedure type.

Not all wound management requires surgical-level sterility. Much of it requires clean technique, which is a defined standard, not simply "fairly clean."

What this covers: The asepsis principles applied during wound assessment, lavage, debridement, dressing, and redressing in small animal veterinary practice, with the distinction between clean technique and sterile technique across different wound types.Scope: Applies to all wound management procedures in dogs and cats, from acute traumatic wounds through chronic open wounds requiring repeated bandage changes.Key distinction: Surgical asepsis (sterile technique) aims to maintain a contamination-free field during invasive procedures. Wound management asepsis uses clean technique for most non-surgical wound care, with sterile technique applied to specific components (irrigation fluids, instruments contacting wound bed).

Key takeaways

Not all wound management requires sterile technique; clean technique is the standard for most bandage changes.
Irrigation fluid must always be sterile; non-sterile lavage introduces contamination.
Instruments contacting the wound bed require sterile-level handling or single use.
Hand hygiene before any wound contact is non-negotiable regardless of glove use.
Dressings must be sterile at point of contact with the wound; non-sterile outer layers are acceptable.
Wound class determines the antimicrobial and closure strategy, not just the asepsis approach.
Owner-performed home wound care requires explicit asepsis education; compliance reduces SSI risk.

Wound classification and asepsis standard

The same wound classification framework that applies in surgery applies to wound management:

Wound class	Examples	Asepsis approach
Clean	Sutured surgical wound requiring bandage change	Clean technique; sterile primary contact layer
Clean-contaminated	Traumatic wound less than 6 hours old	Clean technique; sterile lavage and instruments; debridement
Contaminated	Traumatic wound 6 to 12 hours old; GI contamination	Copious sterile lavage; debridement; no primary closure
Dirty-infected	Established infection; devitalized tissue; abscesses	Lavage; culture; debridement; appropriate antimicrobials

The wound class should be assessed and documented at each evaluation, as wounds may progress from contaminated to dirty-infected without adequate management, or improve toward clean-contaminated with effective treatment.

The clean technique standard for wound management

Clean technique for wound management involves:

Hand hygiene before any wound contact (minimum: alcohol-based hand rub; soap and water if hands visibly soiled or if Clostridium contamination is possible)
Clean gloves (not necessarily sterile) for handling the outer wound dressing layers
Sterile gloves when directly contacting the wound bed or primary dressing layer
Sterile supplies for any item contacting the wound surface (primary dressings, irrigation fluids, instruments used on the wound)
Clean but not necessarily sterile outer layers and bandaging materials

This standard differs from sterile surgical technique in that:

Clean (non-sterile) gloves may be used for outer bandage layers
The environment does not need to be a sterile OR
The person managing the wound does not require surgical scrub technique

Clean technique does not mean casual or careless technique. The same attention to preventing contamination events applies; the environment and some personnel requirements are less demanding.

Wound lavage: the highest-priority asepsis component in wound management

Why lavage matters

Wound lavage is the single most effective contamination reduction intervention in wound management. Merck Veterinary Manual states: "Wounds should be irrigated (lavage) with an appropriate solution at appropriate pressure, to remove contamination (bacteria and debris) and improve visibility for wound inspection."

The mechanical action of lavage physically dislodges and removes bacteria, debris, and devitalized material that chemical antiseptics cannot address.

Irrigation fluid

Sterile saline (0.9% sodium chloride): The standard. Isotonic, non-cytotoxic, no antibacterial activity that could delay healing, widely available.

Sterile water: Acceptable where saline is not available; hypotonic, so longer-term use on open wounds may affect healing tissue.

Dilute povidone-iodine (0.1 to 1%): Acceptable for contaminated or infected wounds. Reduces bacterial load including some organisms not addressed by saline alone. Avoid in fresh granulation tissue.

Dilute chlorhexidine (0.05%): As above. Effective against a broad spectrum including biofilm-forming organisms. Avoid in body cavities at concentrations above 0.05%.

Non-sterile tap water: Not acceptable for wound irrigation. Tap water contains microorganisms and mineral contamination that introduce additional bacterial load into the wound.

Irrigation pressure

Wound irrigation should be performed at sufficient pressure to dislodge debris and bacteria:

Syringe and 18-gauge needle or irrigation catheter: Produces approximately 8 psi of pressure: the range shown to be effective for bacterial removal without tissue damage
Bulb syringe: Lower pressure; adequate for maintenance irrigation of healing wounds; insufficient for initial contaminated wound lavage
Pressure irrigation devices: Mechanical wound irrigation at 8 to 15 psi for heavily contaminated wounds

Volume

There is no single correct lavage volume. Volume should be sufficient to visibly clear debris and produce clear runoff. For contaminated traumatic wounds at initial presentation: minimum 200 to 500 mL per site; more for heavily contaminated wounds.

Lavage frequency

For open wounds undergoing repeated management: at each bandage change, lavage before applying the new primary dressing.

For asepsis principles during wound management, including how these principles apply to the specific wound management context of abscess drainage where contamination management is most demanding, that guide covers abscess-specific wound management.

Debridement and asepsis

Debridement (removal of necrotic, contaminated, or non-viable tissue) is performed using sterile instruments: scissors, scalpel, curettes, or forceps.

Asepsis requirements during debridement:

Sterile instruments for each debridement session; reused instruments between sessions must be re-sterilized or replaced
Sterile or clean gloves depending on the procedure depth
Lavage before and after debridement to clear removed material from the wound
Culture of wound tissue or exudate where infection is suspected or non-responsive

Dressing technique: clean and sterile components

Primary dressing (wound contact layer)

Must be sterile. This layer directly contacts the wound surface and is the contamination-critical interface.

Types of primary dressings:

Non-adherent sterile dressings (Telfa equivalent)
Sterile saline-moistened gauze for moist wound healing
Foam dressings with sterile wound contact surfaces
Antimicrobial primary dressings (silver-containing, honey-impregnated) where indicated

Opening primary dressings: Use aseptic technique. Handle the wound contact surface using sterile gloves. Do not touch the wound contact layer with clean (non-sterile) gloves.

Secondary and outer layers

Secondary and tertiary bandage layers (padding, conforming gauze, cohesive bandage) do not directly contact the wound. These may be handled with clean gloves.

Changing frequency

Wound type and dressing type determine change interval:

Heavily exudating wounds: daily or more frequently
Granulating wounds with low exudate: every 48 to 72 hours
Follow manufacturer guidelines for specialized dressings (e.g., silver foam, Manuka honey dressings)

Common asepsis errors in wound management

Error	Consequence	Correction
Skipping hand hygiene before wound contact	Hand flora introduced to wound	Mandatory hand hygiene before every contact
Using non-sterile irrigation fluid (tap water)	Contamination introduced	Sterile saline only for wound lavage
Touching wound contact layer with non-sterile gloves	Primary dressing contaminated	Use sterile gloves for primary dressing handling
Reusing instruments between sessions without resterilization	Cross-contamination between sessions	Re-sterilize or use single-use instruments
Insufficient lavage pressure for contaminated wounds	Debris not adequately removed	Syringe and 18-gauge needle for contaminated wounds

For aseptic errors during wound management, including the broader error taxonomy for all aseptic procedures in small animal practice, that guide covers the error categories and prevention strategies.

Wound management asepsis for specific wound types

Bite wounds

Cat bites (small, deep puncture wounds) frequently become infected and must be treated as potential abscesses. Dog bites have variable presentation from superficial to penetrating.

Asepsis approach:

Explore under appropriate analgesia or sedation to identify full wound extent
Generous clip around entry and exit wounds
Copious lavage with sterile saline at pressure
Culture of wound content where infection is present or suspected
Open wound management preferred over primary closure in contaminated bite wounds

Traumatic lacerations

Acute (under 6 hours): Lavage, debridement, primary closure if wound bed is clean and viable. Clean technique throughout.

Delayed presentation (over 6 to 12 hours): Treat as contaminated; open wound management or delayed primary closure after initial lavage and debridement.

Open wounds requiring repeated management

Wounds managed by second-intention healing over days to weeks require consistent clean technique at every bandage change. Each change represents a contamination opportunity. Consistent hand hygiene, sterile primary dressings, and sterile lavage at each change maintain the wound environment conducive to healing.

For aseptic technique applied to wound care, including how the sterile field principles developed for surgical settings adapt to the wound management context, that guide covers the technique framework.

Skin antisepsis before wound management procedures

When a skin incision is required for wound management (drainage, debridement under general anesthesia), standard skin antisepsis applies around the wound margin.

For skin antisepsis before wound management, including the centrifugal scrub technique, agent selection, and contact time requirements that apply when surgical-level preparation is needed around a wound site, that guide covers the skin antisepsis protocol.

Frequently asked questions

Can tap water be used to irrigate wounds in an emergency?

In a true field emergency without access to sterile saline, clean running potable water is preferable to no irrigation at all. However, at any point where sterile saline or sterile water is available, it should be used. Tap water contains bacteria and should not be used for wound irrigation in a clinical setting.

Do bandage changes require the same sterile environment as surgery?

No. Bandage changes use clean technique, not sterile technique. The key distinction is that primary dressings (wound-contact materials) must be sterile, but outer layers and the environment can be clean rather than sterile. The procedure area should be clean and disinfected, but it does not need to meet OR environmental standards.

When should wound cultures be taken for antibiotic guidance?

For any wound that is infected (discharge, odor, local inflammation beyond expected healing response), cultures should be taken before initiating or changing antibiotic therapy. Superficial swabs are less informative than deep tissue or purulent material samples. Submit for aerobic and anaerobic culture with sensitivity testing.

Wound management asepsis is not a scaled-down version of surgical asepsis. It is a parallel discipline with its own standard, clean technique, applied precisely. The critical variables are sterile irrigation fluids, sterile primary dressings, correct lavage pressure, hand hygiene at every contact, and the consistent discipline of treating a non-sterile approach as a patient safety failure, not a minor shortcut.

Resources

The following sources were used as reference and background for this article:

Merck Veterinary Manual. Initial Wound Management in Small Animals. merckvetmanual.com
Merck Veterinary Manual. Management of Specific Wounds in Small Animals. merckvetmanual.com
University of Minnesota Clinical Skills Compendium. Abscess Management in Cat/Dog. open.lib.umn.edu
WoundSource. Clean Dressing Technique Principles: Clean vs. Asepsis Wound Dressing Change. woundsource.com

Read Blog Post

Asepsis

5 min read

Surgical Site Preparation in Cats: Complete Guide

Learn essential steps and tips for effective surgical site preparation in cats to ensure safe and successful veterinary surgeries.

Surgical site preparation in cats follows the same fundamental sequence as in dogs clip, initial scrub, aseptic scrub, drape but cats present unique challenges that require specific adaptations.

Feline skin is more delicate than canine skin, cats are more stress-reactive in the clinical environment, and feline-specific anatomical features require attention during preparation.

Quick answer: Feline surgical site preparation follows the same sequence as dogs: clip in the prep room, initial gross scrub, then aseptic target-pattern scrub in the OR using chlorhexidine or diluted povidone-iodine, then sterile draping. Key differences: gentler clipping to avoid feline skin trauma, proactive stress management, and caution with alcohol in small cats.

Key takeaways

SSI rate in cats is approximately 1.5% vs 2.8% in dogs; same principles apply but feline skin tolerates scrubbing less well
Feline skin is more delicate: excessive pressure, concentrated alcohol, or dull blades cause skin trauma more readily than in dogs
Stress management before preparation improves cooperation: pheromones, minimal waiting time, and anxiolytic premedication reduce struggling during prep
The aseptic scrub sequence is identical to dogs: center to periphery, target pattern, discard gauze after each outward pass
Chlorhexidine and diluted povidone-iodine are both appropriate for cats; avoid full-strength alcohol on feline skin without prior antiseptic application
Prepuce flushing does not apply in female cats: focus perineal prep on the perianal and vulvar area

Why cats are different

In veterinary medicine, SSI rates are approximately 2.8% in dogs, 1.5% in cats, and 1.6% in horses.

Cats have a lower baseline SSI rate than dogs, which reflects both their fastidious grooming behavior and the generally shorter, more straightforward procedures commonly performed in feline surgery.

However, the lower rate does not mean preparation can be abbreviated. The same principles apply, adapted for feline anatomy and behavior.

Key feline-specific considerations:

Thinner, more sensitive skin prone to clipper trauma
Higher baseline stress level in the clinical environment
Dense, double-layered coat (longhaired breeds) requires more careful clipping
Smaller body size means smaller prep fields and less margin for error
Unique anatomy in perineal procedures (no prepuce; different perianal structure than dogs)

Step 1: Stress management before preparation

Pre-preparation stress management:

Minimize waiting time in the clinic before induction
Use Feliway or equivalent synthetic pheromone in the prep room
Allow the cat to reach an appropriate depth of anesthesia before beginning preparation
Use low-stress handling throughout: minimal restraint, no scruffing unless essential

Step 2: Hair clipping

General technique:

Use electric clippers with a clean, sharp blade
A size 40 blade is standard for most feline surgical sites
Clip gently feline skin is thin and more susceptible to clipper burns than canine skin
Clip a generous margin: at minimum 5 cm beyond the proposed incision on all sides
Vacuum or remove clipped hair before moving to the prep room antiseptic scrub step

Do not use razors: Do not use razors, which can cause micro-lacerations that may promote infection.

Perineal and perianal prep in female cats: clip the perianal area broadly and flush the vaginal vestibule with 0.05% chlorhexidine diacetate for procedures in this region.

Step 3: Initial scrub (gross decontamination)

Performed in the prep room before the cat enters the OR.

In cats, apply the initial scrub with gentle pressure. Feline skin is thinner than canine skin and excessive scrubbing at this stage causes irritation that compromises the aseptic scrub in the OR.

Step 4: Transfer to OR and positioning

Position the cat on the surgical table and connect anesthetic monitoring before beginning the aseptic scrub. The cat must be fully immobile during the aseptic scrub.

Step 5: Aseptic scrub in the OR

The technique is identical to dogs:

Number of cycles: typically three alternating cycles of antiseptic scrub and rinse. Contact time for each antiseptic application must be respected.

Antiseptic selection in cats

Chlorhexidine gluconate

Chlorhexidine and diluted povidone-iodine are the best antiseptics for cats. They effectively kill bacteria while being gentle on sensitive feline skin.

Povidone-iodine (diluted)

Povidone-iodine is appropriate for cats when used at the correct dilution. Full-strength PI can cause significant skin irritation in cats. The standard dilution for wound and skin use is 0.1 to 1%.

Alcohol

Isopropyl alcohol (70%) is used as a rinse between antiseptic applications in some protocols.

In cats, exercise caution with alcohol: apply only after an initial antiseptic application, and avoid prolonged contact or pooling.

Evaporative heat loss is significant in small cats and can cause hypothermia.

Do not mix antiseptics

As with dogs, do not use chlorhexidine and povidone-iodine on the same patient in the same preparation session due to potential chemical incompatibility.

Step 6: Draping

After the aseptic scrub, the sterile surgical team applies corner drapes followed by a large fenestrated drape.

In cats, the relative smallness of the prep field means drape placement must be precise the margin between the clipped edge and the incision is smaller than in large-breed dogs.

For the equivalent guide for dogs, see surgical site preparation in dogs: complete guide. For the sterile field principles that follow draping, see maintaining a sterile field in veterinary surgery.

For the full SSI prevention overview, see surgical site preparation in cats: complete guide.

Frequently asked questions

Is surgical site preparation the same in cats as in dogs?

The sequence is identical.

The differences are in execution: gentler clipping, more attention to stress management, more careful alcohol use, and awareness that feline skin tolerates scrubbing less well than canine skin.

Do cats need sedation before surgical site preparation?

Cats are anesthetized before preparation begins, so the question is really about the depth and timing of anesthesia induction. Allow adequate anesthetic depth before starting prep.

For very anxious cats, anxiolytic premedication before induction reduces struggling and stress and improves prep quality.

Can I use the same antiseptic for cats as I use for dogs?

Yes. Chlorhexidine gluconate and diluted povidone-iodine are appropriate for both species. The same rule applies: do not mix them on the same patient.

Take care with alcohol rinse in small cats where evaporative cooling is a hypothermia risk.

How wide should the clip field be in cats?

At minimum 5 cm beyond the proposed incision on all sides. This is a smaller absolute area than in large-breed dogs but the same relative principle.

For small cats and kittens, the absolute size of the prep field is smaller but the same proportional margin applies.

Should I bathe a cat before surgery?

Some clinics recommend bathing 24 hours before elective surgery to reduce skin bacterial load.

Never bathe on the day of surgery wet fur causes hypothermia under anesthesia and may cause skin irritation that increases SSI risk. Confirm your clinic's policy with the supervising veterinarian.

Resources

Clinician's Brief. Preoperative Surgical Site Preparation in Veterinary Medicine. cliniciansbrief.com
The Veterinary Nurse. Surgical Site Infections: Preparation, Technique and Perioperative Prevention. theveterinarynurse.com
VetNurse Australia. Surgical Skin Preparation: Best Practice Protocol. vetnurse.com.au
VIN / WSAVA 2014. Maintaining a Sterile Operating Environment. vin.com

Read Blog Post

Common Aseptic Errors in Small Animal Surgery

Asepsis

5 min read

Common Aseptic Errors in Small Animal Surgery

Learn about common aseptic errors in small animal surgery and how to prevent infections for safer pet care.

Aseptic errors are not rare occurrences in poorly run clinics. They are common events in every surgical environment, including well-run ones.

Published data from the American Journal of Veterinary Research (2025) found that 46.3% of observed veterinary surgical procedures involved at least one aseptic protocol breach during scrubbing, gowning, and gloving alone. These breaches frequently went undetected without trained observers.

The implication is clear: errors are not primarily a training problem. They are a monitoring and culture problem.

What this covers: The most frequent categories of aseptic error in small animal surgery, the mechanisms through which each leads to SSI, and the evidence-based prevention strategies for each category.Evidence base: AJVR 2025 breach data; Veterian Key surgical asepsis principles; WSAVA sterile field maintenance guidelines.Key distinction: An aseptic error is any departure from correct technique. An aseptic break is a specific breach of sterility during a procedure. Errors can occur without an immediate break; breaks always constitute an error. Both matter.Clinical relevance: SSI risk increases 3.5-fold when there are lapses in aseptic principles during surgery, even for non-obvious contamination events such as general movement and OR visitors (AJVR 2025, citing human surgical data).

Key takeaways

The most common errors occur during scrubbing, gowning, and gloving: These are the highest-traffic steps for human-origin contamination and the least reliably monitored.
Instrument contamination is the highest-consequence single-error category: A contaminated instrument delivers bacteria directly to the wound.
Patient preparation errors are frequently underestimated: Inadequate clip margins and reversed antiseptic technique recontaminate the surgical site before incision.
Most errors are not detected by the person making them: Self-monitoring is unreliable. External observation and structured checklists are required.
Errors accumulate: SSI is rarely caused by one catastrophic failure. The literature describes a pattern of recurring minor infractions that collectively exceed the infection threshold.
Team culture determines error rates more than individual skill: Environments where errors are named and corrected immediately maintain better asepsis than those where naming a breach feels confrontational.

Error category 1: Surgical hand antisepsis failures

What happens

Inadequate scrub technique leaves transient and resident flora at counts sufficient to contaminate the surgical field through glove micro-perforations or breaches during gloving.

Specific errors

Insufficient scrub duration (under 3 minutes for first case of day)
Substandard nail hygiene (dirt or debris under fingernails)
Failure to scrub all surfaces of fingers, interdigital spaces, and forearm
Touching the faucet, sink edge, or scrub brush holder with scrubbed hands before gloving
Sterile towel dripping onto the gown or gloves during hand drying
Using ABHR without allowing full manufacturer-specified contact time

Published incidence

The AJVR 2025 study of 96 veterinary surgical procedures identified improper scrubbing technique in 17.4% of observed cases. This was one of the four most frequent breach categories.

Prevention

Standardize scrub protocol with a posted visual guide at each scrub sink
Require first-case scrubs of minimum 3 to 5 minutes, timed
Conduct periodic competency observation of scrub technique for all team members
Confirm ABHR contact time with timer when transitioning from traditional scrub

Error category 2: Gowning and gloving violations

What happens

Incorrect gowning or gloving technique introduces hand or body-surface contamination onto the exterior sterile surface of the gown or glove before the procedure begins.

Specific errors

Contacting non-sterile surfaces with the exterior gown surface during donning
Pushing hands through gown cuffs before gloving (precluding closed technique)
Touching the exterior glove surface with ungloved skin during open gloving
Sterile towel contacting the gown or gloves before drying is complete
Gown back tie touching the front sterile zone during wrapping

Published incidence

AJVR 2025 found contact of the sterile towel onto non-sterile surfaces in 17.7% of procedures, and contact of the gown with non-sterile surfaces in another 17.7%. Touching sterile objects with bare hands occurred in 12.5% of procedures.

The total aseptic protocol breach rate during this single preparation phase was 46.3% of all observed procedures.

Prevention

Train closed gloving technique as the default method for all scrub personnel
Conduct observed gowning and gloving competency assessments at orientation and periodically thereafter
Assign a circulating nurse specifically to monitor the gowning/gloving phase and name any breach immediately
Designate a second sterile towel for redundancy if the first is compromised

For the correct technique these errors violate, including the step-by-step standards for surgical hand antisepsis, gowning, and gloving with closed technique, that guide provides the technical reference.

Error category 3: Patient preparation errors

What happens

Inadequate clipping or incorrect antiseptic application leaves residual bacteria on the surgical site that are inoculated into the wound at incision.

Specific errors

Clipping errors:

Clipping performed the night before surgery rather than immediately pre-operatively
Clip margins too narrow (inadequate buffer around anticipated incision)
Use of a razor rather than clippers (creates micro-abrasions; increases recolonization)
Clipper blades contaminated with debris from previous patient

Antiseptic scrub errors:

Scrub direction reversed (scrubbing outward then back inward recontaminates the center)
Insufficient number of scrub applications (minimum two applications is standard)
Wrong antiseptic agent for body location (chlorhexidine in contact with ear canal, open peritoneal cavity, or cornea)
Allowing antiseptic to dry incompletely before draping
Alcohol pooling under the patient, creating fire risk with electrosurgery

Prevention

Establish a standardized clip-to-incision interval policy (immediate preoperative only)
Post visual guides showing correct centrifugal scrub technique in every prep area
Confirm agent selection in the pre-incision time-out for body location-specific risks
Verify alcohol is fully evaporated before electrosurgery or laser use

Error category 4: Instrument and sterile supply errors

What happens

Instruments or supplies that are not sterile, or that become contaminated during handling, introduce bacteria directly to the surgical site.

Specific errors

Pack used despite failed chemical indicator (indicator not checked before use)
Pack used past expiry date
Instrument pack with compromised seal, moisture penetration, or tear used
Non-sterile item introduced to sterile field without sterile opening technique
Instrument passed across non-sterile surface during transfer to surgeon
Instrument falling below table level and returned to use without replacement
Biological indicators not used or results not reviewed before using autoclave batch

Consequence severity

This error category carries the highest direct contamination consequence. A contaminated instrument transfers organisms directly into deep tissue, bypassing the skin defense layer entirely.

For errors to avoid that compromise instrument sterility, the surgical asepsis checklist includes specific verification steps for pack indicators, expiry dates, and seal integrity at each use.

Error category 5: Sterile field maintenance errors

What happens

Actions or events during the procedure that introduce non-sterile material into the established sterile field.

Specific errors

Non-gowned personnel reaching over or across the sterile field
Drapes displaced and not replaced or covered
Gowned personnel turning their back to the sterile field or stepping below table level
Glove perforation undetected and not replaced
Items introduced to the field without sterile opening technique
OR door opened repeatedly during procedure, increasing airborne contamination
Talking or sneezing across the sterile field by personnel without masks

The role of the field monitor

The most important structural prevention for this error category is a designated, named field monitor: one team member whose explicit responsibility during the procedure is to observe the sterile field and name breaches immediately.

Without designation, field monitoring becomes everyone's responsibility, which in practice means no one's.

For the breaks in asepsis that lead to errors and how to categorize, respond to, and prevent them within a systematic approach to sterile field management, that guide covers the break taxonomy in detail.

Error category 6: Environmental and behavioral errors

What happens

OR environment or team behavior creates conditions that elevate airborne or surface contamination beyond what the sterile field can absorb without risk.

Specific errors

Excessive personnel in OR during procedure
Frequent OR door openings during active surgery
Personnel movement that generates air currents across the sterile field
Failure to disinfect OR surfaces between cases
Use of fans or non-surgical forced air systems in the OR
Wet floors or surfaces that aerosolize bacteria with foot traffic

Prevention framework

Error type	Primary prevention	Secondary prevention
Traffic excess	Written OR entry policy	Real-time enforcement by circulating nurse
Door openings	Pre-procedure supply confirmation	Signage and physical barriers
Between-case contamination	Documented between-case disinfection protocol	Checklist sign-off before next case
Airflow disruption	HEPA-filtered positive-pressure ventilation	Restrict fan use in OR

Why errors persist despite training

The evidence is consistent: error rates in surgical asepsis do not correlate with experience or length of training. The AJVR 2025 study found no association between aseptic protocol breaches and previous scrub experience or rotation stage.

This finding has a direct operational implication: training alone is not sufficient to maintain aseptic standards. What reduces error rates is:

Structured external observation rather than self-monitoring
Checklists actively used rather than assumed
Team culture that expects and normalizes immediate, non-judgmental error correction
Audit programs that identify recurring patterns rather than isolated incidents

For training that prevents common errors, including the evidence-based elements of effective asepsis training programs in veterinary practice and how to build competency assessment into staff development, that guide covers the training design component.

Training that addresses the cultural dimension of error correction, not just the technical components of correct technique, consistently produces better long-term asepsis performance than skills-only curricula. The combination of observed competency assessment and ongoing peer monitoring is the most supported approach in the veterinary surgical literature.

For auditing to identify repeated errors, including the structured audit methods that identify systematic versus individual error patterns, that guide provides the compliance monitoring framework.

Frequently asked questions

Are experienced surgeons as likely to make aseptic errors as trainees?

The published data suggest yes. Error rates in human surgical literature are consistently high across experience levels. In veterinary surgery, the AJVR 2025 study found no significant association between breach rates and prior experience. Complacency may actually elevate risk in experienced practitioners, since automatic behavior bypasses deliberate checking.

Should a procedure be halted when an aseptic error is identified?

Not necessarily halted, but addressed immediately. The correct response depends on what was contaminated and whether it can be corrected. A contaminated glove is changed. A contaminated instrument is replaced. A significantly compromised sterile field may require reopening sterile supplies before continuing. The decision rests with the primary surgeon, informed by the field monitor's observation.

How should aseptic errors be documented?

Every identified intraoperative aseptic breach should be documented in the surgical record, including the nature of the breach, what corrective action was taken, and whether the sterile field was considered compromised. This documentation serves quality improvement, regulatory compliance, and medicolegal purposes if SSI develops post-operatively.

Aseptic errors are the rule in surgical practice, not the exception. The surgical team that acts as though errors are impossible is the team most likely to miss them. The team that builds external monitoring, immediate correction, and audit feedback into its standard operation is the one that keeps error consequences minimal.

Resources

The following sources were used as reference and background for this article:

AVMA Journals. Aseptic protocol breaches are common among veterinary students. AJVR, 2025. avmajournals.avma.org
PubMed. Aseptic protocol breaches during SGG in veterinary students. pubmed.ncbi.nlm.nih.gov
Veterian Key. Principles of Surgical Asepsis. veteriankey.com
WSAVA 2014. Maintaining a Sterile Operating Environment. vin.com

Read Blog Post

Asepsis

5 min read

Auditing Asepsis Compliance in Veterinary Clinics

Learn how to audit asepsis compliance in veterinary clinics to ensure infection control and patient safety effectively.

Asepsis training establishes the standard. Audit determines whether the standard is being met.

Without audit, a clinic cannot distinguish between a team that maintains correct aseptic technique and one that has normalized gradual deviations from it. Both teams may describe their practices as compliant. Only observation-based audit can determine which is actually true.

What this covers: The design and implementation of asepsis compliance auditing in small animal veterinary practice, including observation-based audits, SSI surveillance, autoclave validation, environmental monitoring, and audit cycle management.Evidence base: AJVR 2026 SSI consensus data confirms that implementation of surveillance programs produces a "surveillance effect": the act of monitoring itself increases compliance. Simply participating in an audit program reduces SSI rates independent of any other intervention.Key finding: Higher care-bundle compliance yields fewer SSI cases. A quality improvement study reported a moderate negative correlation (r = −0.31) between care-bundle compliance and SSI incidence, with SSI rates dropping from 0.3% to 0.1% following structured audit implementation.Audit goal: Identify gaps between stated protocol and actual practice, distinguish individual errors from systemic patterns, and drive targeted improvement.

Key takeaways

Audit detects what self-reporting misses: Personnel consistently overreport their own compliance. Direct observation is the only reliable method for identifying intraoperative technique gaps.
The surveillance effect is real and significant: Documented in both veterinary and human surgical literature, the mere presence of an active audit program increases compliance independent of the specific findings.
SSI rate alone is an inadequate compliance metric: SSI is a lagging indicator influenced by many variables. Process compliance metrics are more actionable because they are directly modifiable.
Audits should distinguish individual from systemic errors: A single practitioner making a specific error is a training issue. Multiple practitioners making the same error repeatedly is a protocol or system design issue.
Audit findings must be fedback to the team: An audit that produces a report that no one acts on does not improve compliance. Feedback, action planning, and re-audit complete the cycle.
Autoclave monitoring is a distinct audit domain: Biological indicator validation is the most critical sterilization audit and must be performed regularly, not just when a problem is suspected.

Audit domain 1: Intraoperative technique observation

What it measures

Direct observation of surgical personnel during active procedures, assessing adherence to correct aseptic technique across scrubbing, gowning, gloving, sterile field maintenance, and OR behavior.

Why self-reporting is unreliable

Personnel who are asked whether they followed correct technique will almost universally report yes. AJVR 2025 found that 46.3% of observed procedures involved at least one aseptic protocol breach, yet the breach rate identified by self-report would be substantially lower.

The gap between self-report and observation is not primarily a matter of dishonesty. Most people genuinely do not notice their own minor technique violations. External observation is irreplaceable.

Observation method

Structured observation audit:

Assign a trained auditor (a senior clinician or designated compliance officer) to observe a sample of procedures
Use a standardized observation tool with defined scoring criteria for each technique element
Record all observed deviations without interrupting the procedure (except in cases of significant patient risk)
Debrief the team after the case, not during, to avoid disrupting active surgery
Document all findings with date, case type, personnel observed, and specific deviations

Sampling strategy:

Minimum: observe 10% of surgical procedures per month, distributed across procedure types and personnel
Higher risk: observe 100% of procedures after an SSI event, a new team member starts, or a significant breach is reported
Longitudinal: track the same personnel across multiple observations to assess improvement after training

For quality control measures evaluated in audits, including how auditing fits within the broader quality control framework for surgical asepsis, that guide covers the quality assurance architecture.

Audit domain 2: SSI surveillance

What it measures

Post-operative infection rates by procedure type, personnel, patient risk category, and time period.

Why SSI surveillance matters

SSI is the outcome that asepsis is designed to prevent. Tracking SSI rates provides the ultimate performance indicator and can identify temporal clusters that signal a systemic problem.

Key published benchmarks:

Veterinary SSI rates: 1.5% to 18% depending on procedure type and setting (Veterinary Nurse, 2023)
Clean wound class expected SSI rate: 1 to 5%
Clean-contaminated: 5 to 10%
Contaminated: 10 to 17%
Dirty-infected: 27%+

A clinic whose clean-wound SSI rate consistently exceeds 5% has a systemic problem that audit should help identify.

SSI definition consistency

The AJVR (2026) published a consensus on SSI definitions for veterinary medicine, noting that implementation of uniform definitions may initially appear to increase SSI rates as surveillance improves. This is the surveillance effect in action: more rigorous definition and counting does not mean more infections, but it does mean more accurate detection.

Clinics should adopt a standardized SSI definition and apply it consistently across all cases to enable meaningful trend analysis.

Surveillance infrastructure

Post-operative follow-up protocol: All surgical cases should have a defined follow-up contact at 10 to 14 days post-procedure to assess wound status
SSI recording system: A standardized case record capturing wound class, personnel involved, procedure duration, prophylaxis use, and outcome
Periodic analysis: Monthly or quarterly review of SSI rate by procedure type and by surgeon

For auditing OR standards compliance, including how SSI surveillance connects to OR environment standards assessment and the physical infrastructure audits that complement technique observation, that guide provides the OR-specific audit components.

Audit domain 3: Autoclave and sterilization validation

What it measures

Whether sterilization equipment is reliably producing sterile loads, and whether loads are being used within validated shelf life.

The three levels of sterilization monitoring

Chemical indicators (Class 1 to 6):

Chemical indicators on the outside and inside of instrument packs change color or appearance when exposed to the sterilization conditions. They confirm exposure to the sterilizing agent but do not confirm sterility.

External indicators confirm the pack has been through a sterilization cycle
Internal indicators confirm the agent penetrated the interior of the pack
Class 5 and 6 integrating indicators provide the closest chemical approximation to a sterility confirmation

Biological indicators (spore tests):

Biological indicators contain Geobacillus stearothermophilus spores that are killed only if sterilization conditions were sufficient to achieve sterility. A killed spore test confirms functional sterility of the autoclave cycle.

Biological indicators are the only method that directly confirms sterilization efficacy.

Recommended frequency: at minimum weekly in active veterinary surgical practices; after any autoclave service or malfunction; after any pack with a failed chemical indicator is identified.

Mechanical monitoring:

Temperature, pressure, and time records from each autoclave cycle should be logged and reviewed. Many modern autoclaves print cycle records automatically. These should be filed and reviewed periodically.

Sterilization audit checklist

[ ] Biological indicator run within the past week; result documented
[ ] Chemical indicator status checked on all packs before use
[ ] Pack integrity (no tears, no moisture) checked before use
[ ] Expiry dates on all packs confirmed
[ ] Autoclave service record current
[ ] Instrument reprocessing log maintained

Audit domain 4: Patient preparation compliance

What it measures

Adherence to clipping, antiseptic agent selection, scrub technique, and transport protocols.

Common preparation compliance gaps

Step	Common deviation	SSI consequence
Clipping timing	Night-before clipping rather than immediate pre-op	Significant: bacteria recolonize the surgical site overnight
Antiseptic direction	Reversed or random rather than centrifugal	Moderate: recontaminates the prepared center
Antiseptic application count	Single application rather than minimum two	Moderate: reduces antiseptic efficacy
Agent selection	Chlorhexidine applied near ears or eyes	Patient safety risk
Transport	Prepared site contacting non-sterile transfer surface	Low to moderate depending on contact

Observation method

Preparation compliance is best audited during the prep phase, not intraoperatively. A designated observer documents whether each preparation step was performed correctly before the patient is transported to the OR.

Audit domain 5: Environmental compliance

What it measures

Between-case disinfection, OR access control, airflow system function, and surface cleanliness.

Environmental audit items

[ ] Between-case floor mop and surface wipe documented
[ ] OR door access log (if maintained) reviewed for traffic during procedures
[ ] HEPA filtration system maintenance current
[ ] Positive pressure differential confirmed functional
[ ] Environmental surface swabs taken periodically (quarterly recommended for active ORs)
[ ] Humidity and temperature log reviewed

For breaks detected through auditing, including the specific break categories that observation-based auditing is most effective at detecting and the response protocols for each, that guide provides the break-level detail that audit findings map to.

Audit cycle management

The audit cycle

An effective asepsis audit program operates as a continuous cycle, not a one-time event:

Baseline audit: Establish current compliance rates across all audit domains
Gap identification: Identify specific areas where practice deviates from protocol
Root cause analysis: Determine whether gaps are individual (training issue) or systemic (protocol or equipment issue)
Targeted intervention: Training for individual gaps; protocol revision for systemic ones
Re-audit: Assess whether the intervention produced improvement
Monitoring: Continue sampling to confirm improvement is sustained

Audit frequency recommendations

Audit type	Recommended frequency
Intraoperative observation	Monthly (10% case sample minimum)
SSI rate review	Monthly
Autoclave biological indicator	Weekly
Patient preparation observation	Quarterly
Environmental compliance	Quarterly
Comprehensive program review	Annually

Feedback to the team

Audit findings that are not shared with the team do not produce change. Feedback should be:

Timely: Shared within one to two weeks of the audit observation, while the case is recent
Specific: Referenced to the specific deviation observed, not generalized
Non-punitive: Framed as performance data, not disciplinary input
Actionable: Accompanied by a clear corrective step

For errors identified in audits, including the most common error categories and the evidence for why training and audit together outperform training alone, that guide provides the error-level reference for interpreting audit findings.

The relationship between audit findings and training response should be direct and documented. When an audit identifies a recurring error in a specific category, the training calendar should reflect a targeted refresher for that category within 30 days. This closes the quality loop rather than leaving findings as reports without action.

For training that audits assess for compliance, including how the training program and audit program should be designed as complementary elements of a single quality system rather than independent activities, that guide covers the training-audit integration.

Frequently asked questions

How is an audit different from routine supervision?

Routine supervision is ongoing and informal. An audit is structured, documented, and comparative. Audits use standardized tools, record findings systematically, and compare results to defined standards and to previous audit cycles. Supervision catches problems in the moment; auditing identifies patterns over time.

Who should conduct asepsis audits in a veterinary clinic?

The clinical director, a senior surgeon, or a designated compliance officer. The auditor should be familiar with correct aseptic technique and must be credible to the team being audited. External auditors (visiting specialists or consultants) provide valuable perspective for annual comprehensive reviews.

Should audit findings be used in performance reviews?

With caution. If audit findings are linked to disciplinary consequences, personnel may under-disclose breaches or become resistant to the audit process. The most effective audit programs frame findings as quality improvement data rather than individual performance metrics. Pattern-level findings (repeated errors by the same person despite training) may eventually warrant a performance conversation, but this should not be the primary audit framing.

What should happen when an autoclave biological indicator fails?

Remove all packs sterilized since the last successful biological indicator result from use. Do not use any instruments from those packs. Have the autoclave serviced and repaired. Run a new biological indicator before returning the autoclave to service. Review all cases performed using instruments from potentially non-sterile packs for SSI monitoring. Document the incident and corrective actions taken.

For the checklist used to standardize audits, including the structured verification tool that serves as the reference standard against which audit observations are compared, that guide provides the operational baseline for compliance measurement.

Audit is the discipline that closes the gap between what a clinic believes its aseptic standards are and what they actually are. Without it, compliance is an assumption. With it, compliance becomes a measured, improvable performance metric. The clinics with the best surgical infection rates are invariably those that measure their performance systematically and act on what they find.

Resources

The following sources were used as reference and background for this article:

AVMA Journals. Surgical site infection definitions consensus in veterinary medicine. AJVR, 2026. avmajournals.avma.org
NIH/PMC. The effectiveness of aseptic non-touch technique audit cycle implementation on reducing SSI. ncbi.nlm.nih.gov
NIH/PMC. Quality improvement approach for SSI prevention. ncbi.nlm.nih.gov
Veterinary Practice. Infection control in the surgical environment. veterinary-practice.com
The Veterinary Nurse. Surgical site infections: preparation, technique and perioperative prevention. theveterinarynurse.com

Read Blog Post

Asepsis

5 min read

Draping Techniques in Small Animal Surgery

Explore essential draping techniques in small animal surgery to ensure sterile fields and reduce infection risks during procedures.

Draping is the step in surgical preparation that defines the sterile field.

It isolates the prepared skin at the incision site from all surrounding contaminated surfaces the patient's hair and skin, the surgical table, and the anesthetic equipment.

Done incorrectly, draping is just a gesture. Done correctly, it is the final barrier between the sterile surgical wound and the contaminated world around it.

Quick answer: Standard small animal draping uses four corner drapes to frame the incision, secured with towel clamps, then one large fenestrated drape over the patient and table. Drapes move only away from the incision. Orthopedic limb surgery uses free-draping for full limb manipulation.

Key takeaways

Four corner drapes frame the incision site first; a large fenestrated drape is placed on top as the final layer
Drapes can only move away from the incision site: moving toward the center contaminates the sterile field
Towel clamps become unsterile once they pierce skin: hand off to a non-sterile assistant before reusing
Drapes must never be shaken or fanned: air currents from rapid handling contaminate the prepared field
Free-draping is used for orthopedic limb surgery to allow full limb manipulation within a sterile field
Key sheet draping (single-drape method) is an alternative that eliminates the need for corner drapes and towel clamps

Why draping matters

The prepared skin has been decontaminated by clipping and antisepsis. But it still sits next to:

Unclipped hair at the edges of the prep zone
The patient's non-sterile body
The surgical table surface
Anesthetic circuit tubing
Any unsterile equipment around the patient

Drapes isolate the sterile island (prepared skin) from all of these contamination sources.

Drape types

Rectangular (utility / corner) drapes

These are the standard-size rectangular drapes used to frame the incision site during the initial four-corner step.

Animal Hospital Supply: "Corner drapes are doubled over at one end (9 to 10 cm) and placed at the periphery of the surgical field one at a time."

The drape edge is wrapped around the gloved hands to prevent contamination while covering the four corners.

The doubled-over edge faces toward the surgeon to protect the glove from contact with the non-sterile surface as the drape is applied.

Fenestrated drapes

A large drape with a pre-cut opening (fenestration) placed over the patient and table after the four corner drapes.

McCurnin's Clinical Textbook: "For final draping, a large fenestrated or unfenestrated drape is placed over the animal and the table.

The fenestration is placed over the incision site, or a slit is cut into the unfenestrated drape at the incision site."

Animal Hospital Supply: "A large sterile drape is placed over and above the four square-off drapes.

This large drape is then fenestrated, the fenestration through which the sterile surgical procedure is then performed."

SustainableVet: "Fenestrated drapes should be large, covering as much of the patient and table as possible."

Disposable vs. reusable drapes

Disposable drapes are made from synthetic non-woven material, single-use, and are discarded after each procedure. They eliminate the risk of inadequate sterilization between uses.

Virtual Vet Surgery: "Significant reductions in the numbers of bacteria in surgical wounds have been documented using disposable (single-use) and Opsite drapes."

Reusable linen drapes can be laundered and autoclaved. They are more economical over time but require careful inspection for holes and worn areas before each use.

Key sheets (single-drape method)

Animal Hospital Supply: "As in nearly every human surgical procedure in the US, some veterinary surgeries have moved toward a single drape or key sheet draping method.

The key sheet eliminates the need for all underneath draping and the need to clamp the drapes to the patient skin."

Key sheets are procedure-specific and often incorporate additional features: adhesive edges to secure to the patient, tube holders, fluid collection pouches for arthroscopy, and absorbent zones.

Four-corner draping: the standard sequence

McCurnin's: "Four quarter drapes are secured with towel clamps approximate to the incision."

Step 1: Apply corner drape 1 at the cranial edge of the proposed incision site.

Veterinary Surgery Online: "The first drape is generally applied at the cranial edge of the proposed incision site.

Once the drape is unfolded, it should not be turned around in order to maintain the most sterile portion (close to the hands) sterile."

Step 2: Apply corner drapes 2, 3, and 4, framing the other three sides.

The sequence "top, tail, near, far" is a common convention. Virtual Vet Surgery: "A placement pattern of top, tail, near, and far.

The reason for this: in deep-chested dogs, holding a lateral drape in place is difficult because a second drape has to be applied before it can be secured by a towel clamp."

Step 3: Secure with towel clamps.

McCurnin's: "If Backhaus towel clamps are positioned directly in the corners of a four-toweled drape set, the edges will lie flat and not bulge up."

Step 4: Apply the large fenestrated drape as the final layer over the entire patient and table.

Critical draping rules

Drapes only move away from the incision

Veterinary Surgery Online: "As drapes are applied, they can be moved away from the proposed incision site, towards the edge of the prepared area (without exposing hair).

Conversely, a drape cannot be moved from the site of application towards the center of the prepared area since this may lead to contamination of the prepared field."

This rule is absolute. Moving a drape toward the incision drags contamination with it.

Do not shake or fan drapes

Veterinary Surgery Online: "Drapes should not be shaken, fanned, or flipped rapidly when handled as this will create air currents and promote contamination of the prepared surgical field."

Drapes must be gently unfolded and placed never snapped open.

Drapes must cover the entire patient and table

SustainableVet: "Fenestrated drapes should be large, covering as much of the patient and table as possible." Any exposed surface represents a contamination risk.

Special situations

Orthopedic limb surgery: free-draping

For limb surgeries requiring full manipulation (TPLO, fracture repair), the limb is draped to allow it to move freely within the sterile field.

Virtual Vet Surgery: "For many orthopaedic procedures on the limbs, a 'free-draping' technique may be used to help surgical manipulation of the limb.

To isolate the limb, the limb is suspended using a drip stand with the foot enclosed inside a clean latex glove. The glove is secured to the foot with adhesive tape."

The limb is then clipped and prepared. Three corner drapes are placed around the base of the limb to isolate it from the trunk.

A sterile cohesive bandage is applied over the glove and up the limb before the final draping layer.

Male dog abdominal surgery: prepuce management

Veterinary Surgery Online: "If draping the abdomen of a male dog, the prepuce should be displaced laterally and held with a towel clamp to decrease contamination risk.

This should be done prior to draping the area in order to drape over the tip of the prepuce."

Procedure-specific draping

Thoracic surgeries: Require careful draping to isolate the chest area, often using multiple drapes."

For the site preparation that precedes draping, see surgical site preparation in dogs. For the sterile field context draping creates, see maintaining a sterile field in veterinary surgery.

For the PPE worn during draping, see PPE use and barrier protection in veterinary clinics.

Frequently asked questions

Why can drapes move away from the incision but not toward it?

This is a fundamental aseptic principle with no exceptions.

What happens if a drape becomes contaminated during application?

A contaminated drape must be replaced. If a drape contacts a non-sterile surface (the floor, an unsterile piece of equipment, the patient's non-prepped hair), it cannot be used further.

A new sterile drape replaces it.

Can the surgeon reposition a towel clamp once it has been placed?

If the clamp has penetrated skin, its tips are unsterile. McCurnin's: it must be handed off to a non-sterile assistant. A new sterile clamp is used for repositioning.

What is the advantage of key sheet draping over four-corner draping?

Key sheets are faster, eliminate the towel clamp skin-penetration issue, and are procedure-specific with integrated features like fluid pouches and tube holders. The tradeoff is higher per-use cost.

Why do drapes need to cover the entire patient and table, not just the immediate area?

The entire table surface around the patient is a potential contamination source. Any instrument, sponge, or implant that falls onto an uncovered table surface is contaminated.

Draping the full patient and table prevents these incidental contaminations.

Can a drape that has slipped during surgery be pushed back into place?

No. If a drape slips, alert the circulating nurse. A new sterile drape is placed over the exposed area. The slipped drape cannot be repositioned, regardless of how small the movement needed.

Resources

Veterinary Surgery Online. Draping. vetsurgeryonline.com
Virtual Vet Surgery (University of Melbourne). Construction of Surgical Instruments. lms.vet.unimelb.edu.au
Animal Hospital Supply. Veterinary Draping 101. animalhospitalsupply.com
McCurnin's Clinical Textbook for Veterinary Technicians. Elsevier. elsevier.com
Clinician's Brief. Preoperative Surgical Site Preparation in Veterinary Medicine. cliniciansbrief.com

Read Blog Post

Asepsis

5 min read

Quality Control Measures for Surgical Asepsis

Explore essential quality control measures for surgical asepsis to ensure safe, infection-free surgeries and protect patient health.

Quality control in surgical asepsis is the structured system that confirms aseptic standards are being met, not just described.

What this covers: The quality control framework for surgical asepsis in small animal veterinary practice, covering the specific QC measures, how they interact, and how quality data should feed back into protocol improvement.Core principle: Quality control in asepsis is a system, not a checklist. The measures described here form an integrated cycle: establish standards, monitor compliance, identify gaps, intervene, and re-assess.Evidence base: AJVR 2026 SSI definitions consensus confirmed the "surveillance effect": the act of participating in an SSI surveillance program increases compliance independently of specific findings. AJVR 2025 breach data confirmed that training alone does not maintain asepsis performance without external monitoring.

Key takeaways

QC is a cycle, not a checklist: Standards, monitoring, gap identification, intervention, and re-assessment form a continuous loop.
Auditing is the most sensitive QC tool for technique compliance.
Biological indicator testing is the most critical QC measure for sterilization.
SSI surveillance quantifies the patient outcome of all asepsis QC measures combined.
The surveillance effect is real: monitoring improves compliance independently of findings.
QC data must feed back into training and protocol revision to close the quality loop.

The quality control framework

Surgical asepsis quality control operates across four interconnected domains:

Standards: Defined protocols for every asepsis component (patient prep, instrument sterilization, team technique, OR environment)
Monitoring: Ongoing measurement of compliance against those standards
Analysis: Identifying gaps between standard and practice, distinguishing individual from systemic failures
Improvement: Training, protocol revision, and environmental changes that address identified gaps

QC measure 1: Surgical safety checklists

Checklists convert protocol standards into verified, documented action. They are the most accessible and consistently evidence-supported QC tool for improving surgical safety outcomes.

What checklists quality-control:

Instrument pack indicator inspection before opening
Patient prep completion and technique
Surgical hand antisepsis completion
Pre-incision time-out including antimicrobial prophylaxis timing
Instrument count before closure
Between-case disinfection documentation

For checklists as quality control tools, including the phase-by-phase surgical asepsis checklist and how to implement it as a formal QC document, that guide provides the operational reference.

QC measure 2: Intraoperative auditing

Checklists verify that steps were completed. Auditing verifies that steps were completed correctly.

Published evidence:

Audit structure:

Trained observer present during a sample of procedures (minimum 10% of cases per month)
Standardized observation tool covering hand antisepsis technique, gloving, sterile field maintenance, OR behavior
Non-punitive debrief after case completion (not during surgery)
Audit findings documented with date, case type, and specific deviations noted
Results reviewed monthly to identify patterns

QC measure 3: Autoclave validation

The three-level autoclave QC system:

Mechanical monitoring (every cycle): Cycle records confirm temperature, pressure, and time parameters were met
Chemical indicators (every pack): External and internal indicators confirm the pack was processed and the sterilizing agent penetrated
Biological indicators (weekly minimum): Spore tests confirm the cycle killed G. stearothermophilus: the only direct confirmation of functional sterility

For autoclave validation as quality control, including the validation protocol, monitoring schedules, and failed indicator response procedure, that guide covers sterilization QC in full.

QC measure 4: SSI surveillance

SSI surveillance is the outcome measure that validates whether all other QC measures are working. It is also the most powerful single driver of compliance improvement through the surveillance effect.

The surveillance effect:

SSI surveillance components:

Standardized SSI definition applied consistently (AVMA Journal 2026 consensus definitions for veterinary use)
Post-operative follow-up protocol (14-day wound check as minimum)
SSI data recorded by procedure type, wound class, personnel, and outcome
Monthly or quarterly SSI rate review
Trend analysis to identify clusters or increases warranting investigation

Using SSI data:

QC measure 5: Environmental monitoring

OR environmental quality control confirms that the physical environment supports aseptic technique rather than undermining it.

Environmental QC components:

Surface swabs: Taken from high-contact OR surfaces after between-case disinfection; quarterly baseline with increased frequency after any SSI cluster
Air sampling: Settle plates or volumetric sampling during occupied OR conditions; provides baseline contamination data
Positive pressure verification: Smoke pencil or manometer confirmation that the OR maintains positive pressure relative to adjacent spaces
HVAC maintenance records: Filter replacement, service history, and any pressure differential anomalies documented

Connecting QC measures to the improvement cycle

Quality control data has no value unless it drives improvement. The improvement connection requires:

For autoclave failures: Immediate investigation and repair. Post-repair validation before return to service. Review of all cases in the quarantine window for SSI monitoring.

Frequently asked questions

How often should the full QC program be formally reviewed?

Should QC findings be shared with all surgical staff?

Is QC documentation a regulatory requirement?

Resources

The following sources were used as reference and background for this article:

AVMA Journals. Surgical site infection definitions consensus in veterinary medicine. AJVR, 2026. avmajournals.avma.org
AVMA Journals. Aseptic protocol breaches are common among veterinary students. AJVR, 2025. avmajournals.avma.org
Dispomed. The Gold Standard of Sterilization: Why Biological Indicators Matter in Veterinary Practice. dispomed.com
Veterinary Practice. Infection control in the surgical environment. veterinary-practice.com

Read Blog Post

Asepsis

5 min read

Asepsis for Spay and Neuter Surgery

Learn essential asepsis techniques for spay and neuter surgery to ensure safe, infection-free procedures for your pet.

Spay and neuter surgery is the highest-volume surgical category in small animal veterinary practice. In most practices, these procedures are performed multiple times daily. The combination of high volume, relatively short procedures, and the perception of routine can erode aseptic standards over time.

SSI rates after elective spay and neuter in healthy patients range from 1 to 5% when asepsis is correctly applied. Rates above this in a practice typically indicate systematic asepsis gaps rather than patient-level risk.

What this covers: The complete perioperative asepsis protocol for ovariohysterectomy and castration in dogs and cats, including pre-operative preparation, intraoperative technique, MRSP considerations, and antimicrobial stewardship alignment.Scope: Applies to elective spay/neuter in healthy patients, including high-volume clinic settings. Modified protocols for higher-risk patients (concurrent infection, retroviral disease, immunosuppression) are noted.Clinical relevance: High-volume procedures are the highest-risk settings for asepsis normalization: the gradual, unnoticed relaxation of standards that occurs when procedures feel routine. Checklists and periodic auditing counteract this risk.

Key takeaways

Clean wound class (elective, healthy patient): expected SSI rate 1 to 5% with correct asepsis.
MRSP is a risk even in spay/neuter patients; carrier rate in dogs is approximately 4.4%.
Asepsis normalization is a real risk in high-volume settings; checklists counteract it.
Antimicrobial prophylaxis is not routinely indicated for clean spay/neuter in healthy patients.
Immediate pre-operative clipping is required; night-before clipping increases SSI risk.
Post-operative licking is the most common cause of SSI in spay/neuter patients.

Wound classification and SSI risk

Elective spay and neuter in healthy patients is a Class I (clean) procedure:

No inflammation present
No body tracts entered under uncontrolled conditions
Elective, not urgent
Primary closure anticipated

Expected SSI rate for Class I procedures: 1 to 5% in veterinary patients.

SSI rates exceeding this in spay/neuter cases within a practice typically reflect:

Asepsis normalization (gradual reduction in compliance with high-volume procedures)
Licking access post-operatively
Patient-level risk factors (concurrent skin disease, MRSP colonization, immunosuppression)

Patient preparation

Clipping

Timing: Immediate pre-operative. Do not clip the night before. Recolonization of the clipped site begins within hours; night-before clipping allows sufficient time for significant bacterial reestablishment.

Area:

Dogs - ovariohysterectomy (midline):

Clip from mid-sternum to pubis
Lateral extension: bilateral, to mid-flank
Include ventral vulvar margin in the prep area

Dogs - castration:

Clip the scrotum and prepuce; extend anteriorly to the inguinal area
Clip below the planned scrotal incision site

Cats - ovariohysterectomy (flank approach):

Clip the relevant flank from last rib to hindlimb; generous dorsal and ventral margins
Note: flank approach is common in cats; midline also used

Cats - ovariohysterectomy (midline):

Clip from mid-sternum to pubis; lateral extension to flanks

Cats - castration:

Clip scrotum; extend into perineal region

Skin antisepsis

Standard three-pass centrifugal scrub sequence.

Agent: CHG-alcohol combination preferred for most spay/neuter sites. PVI for periocular or ear canal-adjacent sites.

Feline considerations: 2% CHG-alcohol combination appropriate. Confirm CHG does not contact ear canals. Post-operative E-collar to prevent licking and grooming of the CHG-treated area.

Application: Centrifugal direction throughout (incision center to periphery; never reversing). Minimum three passes with fresh gauze for each pass. Contact time observed (minimum 2 minutes for CHG-alcohol). Full evaporation before draping.

Surgical team preparation

Standard surgical hand antisepsis applies:

Full surgical scrub (minimum 3 minutes for first case of day) or validated ABHR application
Sterile gown and gloves
Surgical cap and mask

High-volume settings: Each case requires fresh surgical preparation. Using the same gown across multiple consecutive spay/neuter cases without resterilizing or replacing it does not meet the sterile technique standard and is a common asepsis normalization error.

Intraoperative asepsis

Sterile field maintenance

Standard sterile field principles apply:

Sterile drapes isolate the surgical site
Sterile instruments used throughout
Any instrument dropped or contacting a non-sterile surface is removed and replaced
Non-sterile personnel do not contact the sterile field

Draping for spay/neuter:

For abdominal spay (dogs and cats): four-corner draping or a single fenestrated drape. For scrotal castration in cats: towel draping around the scrotal region with the remainder of the perineum excluded.

Instruments

Spay/neuter instrument packs should be confirmed sterile (chemical indicator checked, pack integrity verified, expiry confirmed) before each use.

High-volume settings: Individual packs per patient. Sharing instruments between patients during a multi-case session, even with rinsing between patients, does not meet the sterilization standard.

Tissue handling

Gentle atraumatic tissue handling applies regardless of procedure perceived simplicity. Excessive tissue trauma increases local inflammatory response and devitalized tissue, elevating SSI risk.

For the intraoperative technique framework that governs sterile field maintenance, instrument handling, and break response during spay/neuter procedures:

For core aseptic technique for the procedure, including the intraoperative sterile field rules and instrument handling standards that apply during spay/neuter as for all surgical procedures, that guide covers the technique framework.

Spay and neuter are soft tissue procedures and share the same wound classification and risk stratification framework as other canine and feline soft tissue surgery. For soft tissue asepsis applied to spay/neuter, including the wound classification table, patient risk factors, prophylaxis decision framework, and GI-entry protocols that apply across all canine soft tissue procedures, that guide covers the full soft tissue asepsis context.

MRSP and spay/neuter

MRSP colonization is relevant to spay/neuter SSI risk as for all canine surgical procedures. The approximately 4.4% carrier rate in dogs means that approximately 1 in 22 spay/neuter patients may be MRSP-positive on skin.

Standard CHG-alcohol skin antisepsis significantly reduces surface MRSP load before incision. The BMC Veterinary Research (2018) study found no MRSP in post-antisepsis samples from dogs prepared with either CHG or PVI protocols, suggesting that correct antisepsis technique effectively addresses surface MRSP before surgery.

For MRSP-positive dogs identified pre-operatively, enhanced skin antisepsis, consideration of intraoperative lavage, and close post-operative monitoring are appropriate.

For preventing post-spay/neuter MRSP through asepsis, including the MRSP epidemiology relevant to spay/neuter patients and the asepsis-based prevention strategy, that guide covers MRSP prevention.

Antimicrobial prophylaxis for spay/neuter

Standard recommendation

Antimicrobial prophylaxis is not routinely indicated for elective spay/neuter in healthy dogs and cats classified as Class I (clean) wounds. Standard aseptic technique applied correctly maintains SSI rates within the expected 1 to 5% range without prophylaxis.

This position is consistent with:

Current veterinary antimicrobial stewardship guidelines
Human surgical infection prevention guidelines for clean procedures
The evidence that prophylaxis provides no significant SSI reduction in clean procedures in healthy patients

When prophylaxis is indicated

Prophylaxis is appropriate for:

Concurrent infection at another site (dental disease, skin infection, urinary infection)
Pyometra or other pre-existing reproductive tract infection (reclassifies wound from Class I)
Immunosuppression (retroviral disease in cats, hyperadrenocorticism in dogs)
Procedure duration anticipated to exceed 90 minutes significantly

When indicated: cefazolin IV within 60 minutes of incision; discontinued within 24 hours post-operatively.

For skin antisepsis before spay/neuter in dogs, including the detailed centrifugal scrub technique and agent selection for canine spay/neuter preparation, that guide covers the canine skin prep protocol.

Feline spay/neuter skin antisepsis follows the same centrifugal technique but requires attention to CHG dilution safety constraints and the risk of post-operative licking of residual antiseptic from accessible skin surfaces. The 2% CHG-alcohol combination is appropriate for cats at this concentration; higher concentrations should not be applied near ear canals or wound contact surfaces.

For skin antisepsis before spay/neuter in cats, including feline-specific agent constraints and dilution requirements for cat spay/neuter preparation, that guide covers the feline skin prep protocol.

Post-operative asepsis: licking prevention

Post-operative licking is the most common preventable cause of spay/neuter SSI.

E-collar requirements:

Must be fitted and applied before the patient recovers from anesthesia
Must extend 2 inches past the nose tip (shorter cones allow most cats and many dogs to access the wound)
Must be worn at all times until the veterinarian confirms adequate healing at the recheck

Recovery suit:

A well-fitted recovery suit can substitute for or supplement the E-collar for trunk and abdominal incisions. The suit must be confirmed to prevent access to the incision.

Owner education:

Owner compliance with E-collar use is frequently insufficient. Direct communication that even a single licking session can introduce enough bacteria to start an SSI, and that the risk is highest in the first 48 to 72 hours, improves compliance.

High-volume clinic asepsis considerations

High-volume spay/neuter clinics (shelters, voucher programs, MASH clinics) perform procedures at a pace that creates specific asepsis risks:

Time pressure and asepsis normalization:

When the same procedure is performed 10 to 20 times per day, steps that are perceived as not immediately consequential may be informally abbreviated. Common normalization examples:

Reducing scrub duration for subsequent cases
Reusing gowns across cases
Skipping the clipping timing protocol (clipping before the session, not immediately before each case)

These shortcuts individually may seem minor. Cumulatively, they produce SSI rates above the expected range.

Structure that counteracts normalization:

Written protocol for each procedure step
Designated case-start checklist
Periodic competency observation even for experienced high-volume teams

Frequently asked questions

Should all cats and dogs be tested for MRSP before spay/neuter?

Universal pre-operative MRSP screening for routine spay/neuter in healthy patients is not currently standard practice. Screening is most valuable for patients with known risk factors (prior MRSP positive, chronic skin disease, recent antibiotics). Correct skin antisepsis technique effectively addresses surface MRSP in most cases regardless of carrier status.

Is night-before clipping acceptable in high-volume settings to save time?

No. Night-before clipping is associated with higher SSI rates than immediate pre-operative clipping across all surgical categories and is not acceptable regardless of workflow pressures. The clip-to-incision interval should be as short as possible. Workflow scheduling should be adjusted to allow immediate pre-operative clipping, not the reverse.

Can spay/neuter instruments be cleaned and reused between patients in the same session without re-sterilization?

No. Between-patient instrument reuse without re-sterilization does not meet the sterile technique standard. Each patient requires fresh sterile instruments. In high-volume settings, sufficient instrument packs must be prepared in advance to cover all cases in a session.

Spay and neuter are the most frequently performed surgeries in veterinary practice. That frequency, not despite it, is the strongest argument for maintaining rigorous asepsis. The procedures that feel routine are the procedures where standards erode. The SSI in patient number 15 of the day is as consequential as the SSI in patient number one.

Resources

The following sources were used as reference and background for this article:

NIH/PMC. Skin asepsis protocols in dogs: chlorhexidine-alcohol versus povidone-iodine. ncbi.nlm.nih.gov
ATDove. Surgical Site Infection. atdove.org
ASPCA Pro. Sterile Surgical Techniques. aspcapro.org
The Veterinary Nurse. Surgical site infections: preparation, technique and perioperative prevention. theveterinarynurse.com
Veterian Key. Principles of Surgical Asepsis. veteriankey.com

Read Blog Post

Asepsis

5 min read

Medical Asepsis During Routine Veterinary Exams

Learn how medical asepsis protects pets during routine veterinary exams with practical steps and expert tips.

Routine companion animal appointments represent the highest-volume, lowest-perceived-risk clinical interactions in veterinary practice. They are also the clinical setting with the most documented medical asepsis failures.

The combination of high patient volume, time pressure, and low perceived infection risk consistently produces poor hand hygiene compliance, inconsistent surface disinfection, and inadequate PPE use in exam room settings.

What this covers: The practical application of medical asepsis during routine companion animal examinations, including the WHO Five Moments framework adapted to veterinary appointments, PPE selection, between-patient disinfection, and what the evidence shows about current compliance.Evidence base: A video observation study across 38 Ontario veterinary clinics documented 10,894 hand hygiene opportunities during routine appointments (PMC4108058). A Swiss companion animal clinic study found overall hand hygiene compliance of 36.6% (PMC8623950). Both confirm that compliance during routine exams is substantially below recommended levels.Clinical relevance: Routine exams are the primary setting for patient-to-patient pathogen transmission in companion animal practice. MRSP, MRSA, and MDR gram-negative organisms circulate through exam rooms via inadequate hand hygiene and surface disinfection.

Key takeaways

Routine exams are high-risk medical asepsis settings, not low-risk ones: High appointment volume and inadequate compliance amplifies transmission risk despite the low-acuity nature of individual appointments.
Documented hand hygiene compliance in companion animal clinics is approximately 36 to 40%: This means that in the majority of patient contacts, hand hygiene is either not performed or performed incorrectly.
The exam table is a primary transmission vehicle: Studies in human healthcare settings confirm that contaminated examination surfaces transfer pathogens to subsequently examined patients. The mechanism is identical in veterinary exam rooms.
ABHR at point of care is the most effective compliance intervention: Placement of ABHR dispensers at the exam room entrance and inside the exam room consistently improves compliance rates in human and veterinary healthcare settings.
Between-patient disinfection of the exam table and stethoscope is non-negotiable: These surfaces contact every patient and serve as cross-contamination vehicles when not disinfected between patients.
Clean gloves do not replace hand hygiene: Donning clean gloves without prior hand hygiene and removing gloves without performing hand hygiene afterward both represent medical asepsis failures.

The appointment as an asepsis sequence

A routine companion animal appointment involves multiple patient contacts, each with specific hand hygiene requirements. Mapping the WHO Five Moments to a typical appointment:

Typical appointment structure

A patient is received by a veterinary technician, examined by the veterinarian, and a vaccination is administered.

Hand hygiene moments:

Moment	Who	When
Moment 1: Before patient contact	Technician	Before touching the patient on intake
Moment 1: Before patient contact	Veterinarian	Before beginning the physical examination
Moment 2: Before aseptic procedure	Veterinarian	Before administering the vaccination
Moment 4: After patient contact	Technician	After handling the patient on intake
Moment 4: After patient contact	Veterinarian	After completing the examination
Moment 5: After contact with patient surroundings	Both	After touching the exam table, leash, carrier, or kennel door

In a typical appointment with one technician and one veterinarian, the Canadian video observation study identified five hand hygiene opportunities. The study observed 10,894 such opportunities across 38 clinics.

Where compliance fails

Published data and observational research consistently identify the same failure patterns:

Most commonly missed moments:

Moment 2 (before a clean/aseptic procedure): most frequently missed in human and veterinary healthcare data
Moment 5 (after contact with patient surroundings): frequently omitted because contamination from environmental surfaces is not intuitively associated with patient risk

Most commonly performed moments:

Moment 4 (after patient contact): performed more reliably because the contamination is perceived as coming directly from the patient

The asymmetry is clinically important: the moments that are skipped are the ones that prevent the staff member from introducing contamination rather than acquiring it.

Applying medical asepsis: step-by-step for a routine exam

Before the appointment

[ ] Previous patient's exam table disinfected (top, sides, any raised edge)
[ ] Stethoscope diaphragm and earpieces cleaned with ABHR or appropriate disinfectant
[ ] Any equipment from previous patient removed or disinfected
[ ] ABHR available at point of care (inside exam room preferred; entrance as minimum)

On patient arrival

[ ] Hand hygiene (Moment 1) before touching the patient or their belongings
[ ] Gloves if indicated (body fluid contact anticipated; patient with known infectious disease)

During the physical examination

[ ] Examination proceeds with clean technique: no non-indicated glove removal; no touching of non-patient surfaces unnecessarily
[ ] If gloves are worn: remove before touching clean surfaces (keyboard, record, door handle); perform hand hygiene after removal

Before any invasive step (injection, blood draw, IV catheter)

[ ] Hand hygiene (Moment 2) if not already wearing gloves; or ensure gloves are on and clean
[ ] Site antisepsis: clip hair if needed; apply isopropyl alcohol or appropriate antiseptic
[ ] For IV catheter placement: aseptic site preparation (more rigorous than standard injection site prep)

After examination

[ ] Hand hygiene (Moment 4) after completing patient contact
[ ] Hand hygiene (Moment 5) after touching the exam table, leash, carrier, scale, or any patient-zone surface

Between patients

[ ] Exam table disinfected with hospital-grade disinfectant; contact time observed
[ ] Stethoscope diaphragm cleaned
[ ] Any single-use items from previous patient disposed of
[ ] If infectious disease suspected: enhanced disinfection; all surfaces in patient zone

For medical asepsis principles applied broadly in veterinary clinics, including the five domains of medical asepsis (hand hygiene, PPE, surface disinfection, waste management, and environmental cleaning) with the published compliance data context, that guide covers the full medical asepsis framework.

Minor invasive procedures during routine exams, including IV catheter placement and urinary catheterization, require an aseptic step within the otherwise medical-asepsis context of the appointment. For asepsis for IV catheter placement, including the site preparation, clean technique, and aseptic barrier requirements that apply when catheter placement occurs outside the OR setting, that guide covers the specific asepsis requirements for this common clinic procedure.

The stethoscope problem

The stethoscope is among the most persistently under-disinfected clinical tools in both human and veterinary medicine.

Multiple studies in human healthcare settings have documented stethoscope contamination rates between 80 and 100% in routine clinical use, with organisms including MRSA, Clostridium difficile, and gram-negative pathogens.

In veterinary practice, the stethoscope contacts multiple patients per day, is worn around the neck between patients (contacting clothing and skin), and is rarely disinfected between every patient contact.

Minimum requirement: ABHR applied to the diaphragm between each patient. A single application of 70% isopropyl alcohol (which is present in ABHR) achieves greater than 99% bacterial reduction on stethoscope diaphragm surfaces.

Practical approach: ABHR application to the diaphragm as the last step of each patient encounter, immediately before leaving the exam room.

Point-of-care ABHR: the most impactful compliance intervention

The single environmental factor most consistently associated with improved hand hygiene compliance in both human and veterinary healthcare settings is point-of-care availability of ABHR.

When ABHR requires staff to leave the exam room or walk across the room to a sink, the moment-of-use convenience is lost and compliance drops. When ABHR is within arm's reach at the point of care, the behavioral barrier to compliance is minimized.

Recommended placement:

Inside each exam room, near the exam table
Outside exam room entrances
At ward entry points
At treatment room entries

Wall-mounted dispensers are preferable to countertop bottles, which can contaminate the hand during pumping if the pump itself is not cleaned regularly.

For how exam asepsis differs from surgical asepsis, including the formal comparison of clean technique vs. sterile technique standards across the full range of veterinary clinical settings, that guide covers the distinction in comprehensive detail.

Infectious disease patients in the routine exam setting

Patients presenting with suspected infectious disease require modified medical asepsis protocols in the exam room:

Enhanced protocols:

Contact precautions: gown and gloves for all patient contact
Dedicated exam room if possible; if not, schedule as last patient of day in that room
Enhanced between-patient disinfection: intermediate-level agent with appropriate contact time
Patient handled directly from carrier to scale to exam table without floor contact (reduces environmental contamination spread)
Staff perform hand hygiene after removing gloves and gown; both must be disposed before leaving the exam area

Infectious disease categories of particular concern in companion animal practice:

Suspected Salmonella or Campylobacter (zoonotic risk)
Known MRSP colonization
Respiratory disease (Bordetella, influenza, feline URI pathogens)
Parvovirus (highly resistant environmental pathogen)
Giardia and other enteric protozoa (zoonotic risk in immunocompromised owners)

For antisepsis applied in exam settings, including how antiseptic agents used in routine exam procedures (injection site prep, minor wound care) relate to the broader asepsis framework, that guide covers the antisepsis component applicable to routine clinical settings.

Frequently asked questions

Should veterinary staff wear gloves for all routine physical examinations?

No. Routine glove use for every examination without indication is not supported by infection control evidence and may paradoxically reduce hand hygiene compliance (by creating a false sense of protection). Gloves are indicated for contact with body fluids, non-intact skin, mucous membranes, and patients with known infectious disease. For routine examination of a healthy patient, hand hygiene before and after contact is the appropriate medical asepsis approach.

Is it necessary to disinfect the exam table between every patient?

Yes. The exam table is a confirmed pathogen transfer surface. Between-patient disinfection is not optional. Time pressure does not exempt this step; it should be factored into appointment scheduling.

How should we manage an exam room after a patient with suspected parvovirus?

Immediate enhanced disinfection with a parvovirus-effective agent (such as dilute sodium hypochlorite/bleach at appropriate concentration, or an accelerated hydrogen peroxide product with parvovirus label claim). Standard quaternary ammonium compounds are not effective against parvovirus. The room should remain disinfected and the surface wet for the full required contact time before the next patient enters.

What should we do if we discover a staff member has not been performing hand hygiene consistently?

Address this as a training and compliance issue, not a disciplinary one. Provide reinforcement of the Five Moments framework and point-of-care ABHR placement. Monitor compliance prospectively. The response to non-compliance should be educational and systemic rather than punitive, as punitive responses reduce disclosure and worsen overall compliance culture.

Routine appointments are the volume backbone of companion animal practice and the primary site of nosocomial pathogen transmission. The hand hygiene compliance rate of approximately 37% documented in published veterinary studies represents a substantial and addressable patient safety gap. Point-of-care ABHR availability, Five Moments training, and between-patient surface disinfection are the three highest-impact interventions available. None of them are expensive. All of them are consistently underimplemented.

Resources

The following sources were used as reference and background for this article:

NIH/PMC. Video observation of hand hygiene practices during routine companion animal appointments. pmc.ncbi.nlm.nih.gov
NIH/PMC. Hand Hygiene Evaluation Using Two Different Tools in a Swiss Companion Animal Clinic. ncbi.nlm.nih.gov
Australian Veterinary Association. Infection prevention and control in veterinary workplaces. ava.com.au
WHO. My 5 Moments for Hand Hygiene. who.int
Merck Veterinary Manual. Overview of Antiseptics and Disinfectants for Use With Animals. merckvetmanual.com

Read Blog Post

PPE Use and Barrier Protection in Veterinary Clinics

Asepsis

5 min read

PPE Use and Barrier Protection in Veterinary Clinics

Learn about PPE use and barrier protection in veterinary clinics to keep staff and pets safe from infections and hazards.

Personal protective equipment (PPE) in veterinary practice serves two simultaneous purposes: protecting staff from patients, and protecting patients from staff and from each other.

Neither direction of protection can be neglected. Failure in either direction puts patients, staff, or the public at risk.

Quick answer: Veterinary PPE includes exam gloves, surgical gloves, bite-resistant gloves, masks, N95 respirators, gowns, and eye protection. Selection depends on the procedure, the patient's disease status, and splash or aerosol risk. Fewer than 40% of veterinary staff use appropriate PPE consistently.

Key takeaways

Exam gloves are the baseline PPE for any patient contact involving bodily fluids, non-intact skin, feces, or mucous membranes
Surgical gloves differ from exam gloves: they are sterile, thinner, and used only for sterile procedures
Eye protection is required whenever splash is possible dental procedures, wound lavage, necropsy, and many laboratory procedures
N95 respirators are required for aerosol-generating procedures in patients with suspected respiratory pathogens; surgical masks do not filter aerosols
OSU CVM: fewer than 40% of veterinary staff use appropriate PPE consistently compliance is a recognized gap
PPE removal sequence matters as much as donning sequence: incorrect removal contaminates skin and clothing

Why PPE compliance matters

OSU CVM: "Less than 40% of veterinarians and staff reported using the appropriate PPE for given situations."

OSU CVM: "When observing PPE removal by healthcare providers in one study, almost 50% inadvertently contaminated their skin or clothing."

OSU CVM: "Failure to properly use PPE puts you, your staff, and patients at increased risk for disease.

In some cases, disease outbreaks can occur in clinics and illness can be very severe, even leading to death."

PPE use is not optional for high-risk situations.

AVMA: "Drawing blood from a dog suspected or known to have leptospirosis poses greater biological health hazards than drawing blood from a clinically healthy dog.

The disease transmission risk warrants elevated caution and PPE."

Gloves: types and selection

Exam gloves (nitrile or latex)

The baseline barrier for general clinical work.

CVMA: "Nitrile gloves should be worn routinely when contact with feces, body fluids, vomitus, exudates, and non-intact skin is likely.

They should be worn when performing dental or obstetric procedures, resuscitations, and necropsies and when handling diagnostic specimens."

Nitrile is preferred over latex due to lower allergy risk for both staff and clients.

Indications:

All patient examinations involving bodily fluids
Wound assessment and dressing changes
Handling fecal samples, urine, aspirates, or swabs
Dental procedures (high splash risk)
Any contact with animals of unknown infectious status

Surgical gloves

Sterile, powderless, and considerably thinner than exam gloves for tactile sensitivity. Used exclusively for sterile procedures.

Surgical gloves are donned using closed gloving technique after a full surgical scrub or ABHR. They are not interchangeable with exam gloves for sterile procedures.

Bite-resistant gloves

Mahan Law: "Staff members should have access to bite-resistant gloves for working with potentially fractious animals."

These are not sterile and not appropriate for aseptic work. They protect against puncture and laceration. They should be accessible in reception, examination rooms, and kennels.

Masks: surgical masks vs. N95 respirators

These two types of masks serve fundamentally different purposes and are not interchangeable.

Surgical masks

OSU CVM: "Face masks (surgical) are used to prevent exposure of the mucous membranes of the eyes, nose, and mouth to pathogens."

Surgical masks block large droplets and splatter. They are appropriate for:

Routine surgical procedures (as part of full surgical attire)
Procedures with splash risk to the mouth or nose
General barrier between staff and patient

Surgical masks do not filter aerosols. They do not provide respiratory protection against airborne pathogens.

N95 respirators

N95 respirators filter at least 95% of airborne particles 0.3 microns or larger.

They are required when:

A patient has confirmed or suspected airborne infectious disease (e.g., influenza, bordetella in kennel situations with active outbreak)
Aerosol-generating procedures are performed on patients with respiratory pathogens
Staff work in high-risk situations such as necropsy of animals with zoonotic pathogens

N95 respirators require fit testing to be effective. An N95 that does not fit correctly provides negligible protection over a surgical mask.

Eye and face protection

OSU CVM: "Face protection such as masks, goggles, and full-face shields prevent exposure of the mucous membranes of the eyes, nose, and mouth to pathogens."

OSU CVM: "These items are warranted whenever there is a risk for splashes or sprays onto a person's mucous membranes."

Situations requiring eye protection:

Procedure	Recommended protection
Dental scaling	Face shield or goggles + mask
Wound lavage with syringe	Goggles or face shield
Necropsy	Full face shield
Blood draws from leptospirosis-suspected dogs	Goggles + mask
Ear flushing/irrigation	Goggles
Surgery (routine)	Surgical mask minimum; goggles optional

OSU CVM: "Items used for the above should be single-use disposable (surgical mask) or reusable after cleaned and disinfected (face shield, goggles)."

Protective outerwear: gowns, lab coats, and aprons

CVMA: "The purpose of protective outerwear is to limit the transfer of pathogens between the wearer and the patient, and to limit contamination of the wearer's clothing."

Lab coats:Baseline protection for routine clinical work. They prevent contamination of personal clothing and can be laundered. They are not fluid-resistant without specific coating.

Disposable gowns:Used for higher-risk situations: isolation cases, procedures with significant fluid exposure, or when the lab coat cannot be immediately changed between contaminated patients.

IndeVets: "Gowns/coveralls lab coats, cloth surgical gowns, change of scrubs, and even trash bags work in a pinch."

Sterile surgical gowns:Used exclusively for sterile surgical procedures. Not interchangeable with non-sterile disposable gowns.

Waterproof aprons:For procedures with heavy fluid volume necropsy, parturition, large wound irrigation.

PPE for specific high-risk situations

Isolation patients (suspected or confirmed contagious disease)

AVMA: patients with suspected leptospirosis warrant "double glove, face shields or the combination of masks and eye protection, disposable gown, isolation ward."

Full isolation PPE protocol:

Disposable gown (new for each entry)
Double gloves (outer pair removed on exit, inner pair with glove disposal)
Goggles or face shield
N95 if respiratory transmission is possible
Dedicated footwear or disposable shoe covers

All PPE is removed before leaving the isolation area. AAHA Infection Control Guidelines specify a defined sequence: PPE is removed inside the room before touching the door handle.

Necropsy

CVMA: necropsy warrants full PPE due to "potential contact with infectious body fluids, aerosols, and contaminated sharps."

Full necropsy PPE: double gloves, face shield, gown or waterproof apron, N95 if respiratory pathogen is possible, cut-resistant gloves when opening body cavities in large animals.

Radiography

AVMA PPE list: "Lead-lined radiology thyroid guard, lead-lined radiology apron, radiology eyewear, lead-lined radiology gloves." These are not infection control items but physical hazard PPE required for radiation safety.

They require annual inspection and replacement when damaged.

PPE donning and removal sequence

Donning order: gown first, then mask/respirator, then eye protection, then gloves last.

Removal order is the reverse and equally critical. Gloves are removed first (the most contaminated item), then eye protection, then gown, then mask. Each step should avoid touching the contaminated outer surfaces.

OSU CVM: "Almost 50% of healthcare providers inadvertently contaminated their skin or clothing" during PPE removal. Removal should be practiced with deliberate attention until the sequence becomes automatic.

Hand hygiene at minimum, glove removal followed by hand washing or ABHR is performed after PPE removal is complete.

For the surgical scrubbing and sterile gloving that applies specifically to aseptic surgical procedures, see veterinary surgical hand scrub protocol. For isolation protocols for infectious patients, see isolation protocols for infectious dogs.

For aseptic technique in the operating room, see aseptic technique in dog and cat surgery.

Frequently asked questions

Do I need gloves for every patient interaction?

Not every interaction petting or walking a healthy dog does not require gloves.

Gloves are required when there is realistic risk of contact with bodily fluids, non-intact skin, feces, or mucous membranes, or when the patient's infectious status is unknown.

Can I reuse disposable gloves between patients if I use hand sanitizer on them?

No. Single-use gloves are designed for one patient contact. OSHA and AVMA guidelines do not support decontaminating and reusing exam gloves. A new pair is used for each patient.

My clinic does not have face shields. Can I use safety glasses instead?

Safety glasses without side panels provide minimal splash protection. OSU CVM specifies goggles that "wrap around the sides of the face or include side-protectors" as the appropriate choice.

Standard safety glasses are not equivalent to clinical goggles.

Are surgical masks sufficient for working with a dog that may have leptospirosis?

No. AVMA: leptospirosis-suspected dogs warrant "face shields or the combination of masks and eye protection." A surgical mask alone does not provide adequate protection for a high-risk zoonotic patient.

How often should PPE training be refreshed?

IndeVets recommends asking what PPE protocols are in place at any new practice and reviewing them on arrival. AVMA recommends regular refresher training.

Staff training at hiring and at least annually when protocols change is a reasonable minimum standard.

What PPE is needed when handling a dog with suspected parvovirus?

Full contact precautions: disposable gown and exam gloves (double-glove recommended), with eye protection if splash is possible.

Parvovirus is environmentally stable; PPE must be removed before leaving isolation, and contaminated surfaces must be disinfected with a parvocidal agent.

Resources

AVMA. Personal Protective Equipment (PPE). avma.org
OSU CVM. Types of PPE and Indications for Use Based on Risk Assessment. ohiostate.pressbooks.pub
OSU CVM. Risk Assessment and Introduction to PPE Part 2. ohiostate.pressbooks.pub
Mahan Law. Health and Safety Risks in Veterinary Practices. mahanlaw.com
CVMA. Personal Protective Equipment. cvma-watchdog.net

Read Blog Post

Get Your
‍Free Poster!

We will work on your request shortly.

Oops! Something went wrong while submitting the form.

What’s your role in animal care?

Tell us who you are so we can guide you to the most relevant information.

Pet Owner

Veterinary Professional