The authors wish to acknowledge those employees and research personnel who have participated in the Rabbit Handling and Anesthesia Training sessions for their feedback while learning this intubation technique.

The intubation procedure outlined below was approved by the Mayo Clinic Institutional Animal Care and Use Committee.
1. Preparation (Figure 1)
<ol>
	<li>Obtain a 5 French polypropylene catheter and cut the non-rounded end so the total length is 8-10 inches. Mark the cut end of the tubing to clearly indicate which end should not be inserted into the trachea (arrow, Figure 1).</li>
	<li>Place a size 0 or 1 Miller laryngoscope blade on the laryngoscope and verify that the light is functioning.</li>
	<li>Draw 0.25 mL of 2% lidocaine into a 1 mL syringe.</li>
	<li>Apply sterile lubricant to the end of an appropriately sized uncuffed endotracheal tube (typically 2.5-4.0 mm ID).</li>
	<li>Prepare supplies for securing the endotracheal tube in place once it is inserted (e.g., umbilical tape).</li>
	<li>Obtain a device to detect air flow at the end of the procedure to confirm successful intubation (#5, Figure 1). This is Optional.</li>
</ol>
2. Anesthesia
<ol>
	<li>Administer injectable anesthesia, such as 35 mg/kg ketamine and 5 mg/kg xylazine intramuscularly using a 3 mL syringe with a 25 gauge needle in the quadriceps muscle of the hind leg of an approximately 4 month old, 3.0-3.5 kg, New Zealand White rabbit. 
	NOTE: This anesthetic regimen is a commonly used injectable combination in young, healthy, specific pathogen-free research rabbits, but based upon clinical condition and/or experimental objectives, a different protocol may be more appropriate.</li>
	<li>After the rabbit is anesthetized, apply sterile ophthalmic lubricant to the eyes to preserve the corneal tissue.</li>
</ol>
3. Endotracheal Intubation
<ol>
	<li>Measure the endotracheal tube from the incisors to the thoracic inlet to determine the proper length for insertion of the endotracheal tube. Placement of the end of the tube at the level of the thoracic inlet assures that the tube opening is past the larynx but cranial to the tracheal bifurcation.</li>
	<li>Position the rabbit sternally on the preparation table with its head slightly extended over the edge of the table (Figure 2). The rabbit should be positioned square with the head and spine in straight alignment.</li>
	<li>Lifting the head up, use a gauze pad to pull the rabbit&#39;s tongue lateral to the rabbit&#39;s right lower incisors (in the diastema), taking care to avoid trauma from the incisors.</li>
	<li>Grasp the laryngoscope and blade with the right hand and place it into the mouth behind the incisors, entering from the rabbit&#39;s left.</li>
	<li>Follow the roof of the mouth with the tip of the blade in a caudal direction until the soft palate is visible.</li>
	<li>With the right hand, tip the laryngoscope forward (bend the wrist, holding the laryngoscope downward) while extending the rabbit&#39;s head back and the neck forward to maintain an open airway and view the larynx (Figure 3A). As obligate nasal breathers, the epiglottis is often above the soft palate, and use of this method compresses the base of the tongue to displace the epiglottis and expose the glottis. To prevent oxygen desaturation, it is important to keep the neck extended as described to maintain an open airway during intubation.</li>
	<li>Release the tongue and switch the laryngoscope blade to the left hand to free up the right hand for placement of the guide catheter.</li>
	<li>While holding the laryngoscope and maintaining view of the glottis (Figure 3B), advance the rounded tip of the guide catheter through the opening past the larynx (Figure 4). The catheter will come to a natural stop at the tracheal bifurcation.</li>
	<li>While maintaining hold of the guide catheter, grasp the endotracheal tube and thread it over the catheter, taking care not to apply force to the catheter by catching it on the endotracheal tube connector. Advance the tube until there is resistance from the vocal cords (Figure 5).</li>
	<li>Instill 0.25 mL of 2% lidocaine into the opening of the endotracheal tube. The lidocaine will travel down the endotracheal tube to locally anesthetize the vocal cords, preventing laryngospasm22 (Figure 6).</li>
	<li>Allow approximately two minutes for the topical anesthesia to take effect, and proceed by gently twisting the endotracheal tube, advancing it through the vocal cords (Figure 7). Once the tube has passed the vocal chords, remove the laryngoscope blade and catheter, taking care not to dislodge the tube.</li>
	<li>Verify placement of the endotracheal tube by observing airflow. There are multiple ways to accomplish this, including placement of a tissue or fur at the end of the tube to detect airflow, looking for fogging of the tube or fogging of a glass/mirror at the end of the tube, and listening for airflow. Devices designed to detect airflow23 or respirations may also be used (Figure 8) to determine whether intubation was successful (see Materials Table for options). Secure the endotracheal tube using a preferred method, such as umbilical tape tied around the tube and head. Attach the anesthesia circuit and auscult both sides of the thorax while giving breaths to assure ventilation to both sides of the lung.</li>
</ol>

<ol>
	<li>Quesenberry, K. E., Carpenter, J. W. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=.">.</a> Ferrets, rabbits, and rodents : clinical medicine and surgery. 3rd edn . , (2012).</li><li>Dugdale, A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=.">.</a> Veterinary Anaesthesia: Principles to Practice. , (2010).</li><li>Yamamoto, Y., Inoue, S., Abe, R., Kawaguchi, M., Furuya, H. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Airway+management+with+the+laryngeal+tube+in+rabbits.">Airway management with the laryngeal tube in rabbits.</a> Lab animal. 36 (5), 33-35 (2007).</li><li>Belena, J. M., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Laryngeal+mask,+laryngeal+tube,+and+Frova+introducer+in+simulated+difficult+airway.">Laryngeal mask, laryngeal tube, and Frova introducer in simulated difficult airway.</a> J Emerg Med. 48 (2), 254-259 (2015).</li><li>Smith, J. C., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Endotracheal+tubes+versus+laryngeal+mask+airways+in+rabbit+inhalation+anesthesia:+ease+of+use+and+waste+gas+emissions.">Endotracheal tubes versus laryngeal mask airways in rabbit inhalation anesthesia: ease of use and waste gas emissions.</a> Contemp Top Lab Anim Sci. 43 (4), 22-25 (2004).</li><li>Kazakos, G. M., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Use+of+the+laryngeal+mask+airway+in+rabbits:+placement+and+efficacy.">Use of the laryngeal mask airway in rabbits: placement and efficacy.</a> Lab Anim (NY). 36 (4), 29-34 (2007).</li><li>Crotaz, I. R. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Initial+feasibility+investigation+of+the+v-gel+airway:+an+anatomically+designed+supraglottic+airway+device+for+use+in+companion+animal+veterinary+anaesthesia.">Initial feasibility investigation of the v-gel airway: an anatomically designed supraglottic airway device for use in companion animal veterinary anaesthesia.</a> Vet Anaesth Analg. 37 (6), 579-580 (2010).</li><li>Bateman, L., Ludders, J. W., Gleed, R. D., Erb, H. N. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Comparison+between+facemask+and+laryngeal+mask+airway+in+rabbits+during+isoflurane+anesthesia.">Comparison between facemask and laryngeal mask airway in rabbits during isoflurane anesthesia.</a> Veterinary Anaesthesia and Analgesia. 32 (5), 280-288 (2005).</li><li>Johnson, D. H. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Endoscopic+intubation+of+exotic+companion+mammals.">Endoscopic intubation of exotic companion mammals.</a> The veterinary clinics of North America. Exotic animal practice. 13 (2), 273-289 (2010).</li><li>Tranquilli, W. J., Thurmon, J. C., Grimm, K. A., Lumb, W. V. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=.">.</a> Lumb &amp; Jones' veterinary anesthesia and analgesia. 4th edn. , (2007).</li><li>Worthley, S. G., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Rapid+oral+endotracheal+intubation+with+a+fibre-optic+scope+in+rabbits:+a+simple+and+reliable+technique.">Rapid oral endotracheal intubation with a fibre-optic scope in rabbits: a simple and reliable technique.</a> Laboratory Animals. 34 (2), 199-201 (2000).</li><li>Miranda, A., Pego, J. M., Correia-Pinto, J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Animal+facility+videoendoscopic+intubation+station:+tips+and+tricks+from+mice+to+rabbits.">Animal facility videoendoscopic intubation station: tips and tricks from mice to rabbits.</a> Laboratory animals. , (2016).</li><li>Irazuzta, J., Hopkins, J., Gunnoe, P., Brittain, E. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Simple+method+of+multipurpose+airway+access+through+percutaneous+tracheostomy+in+rabbits+(Oryctolagus+cuniculus).">Simple method of multipurpose airway access through percutaneous tracheostomy in rabbits (Oryctolagus cuniculus).</a> Lab Anim Sci. 47 (4), 411-413 (1997).</li><li>Bertolet, R. D., Hughes, H. C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Endotracheal+intubation:+an+easy+way+to+establish+a+patent+airway+in+rabbits.">Endotracheal intubation: an easy way to establish a patent airway in rabbits.</a> Lab Anim Sci. 30 (2), 227-230 (1980).</li><li>Gilroy, B. A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Endotracheal+intubation+of+rabbits+and+rodents.">Endotracheal intubation of rabbits and rodents.</a> J Am Vet Med Assoc. 179 (11), 1295 (1981).</li><li>Morgan, T. J., Glowaski, M. M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Teaching+a+new+method+of+rabbit+intubation.">Teaching a new method of rabbit intubation.</a> J Am Assoc Lab Anim Sci. 46 (3), 32-36 (2007).</li><li>Inglis, S., Strunk, A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Rabbit+anesthesia.">Rabbit anesthesia.</a> Lab Anim (NY). 38 (3), 84-85 (2009).</li><li>Falcao, S. C., Pereira Junior, J. R., Coelho, A. R. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Technique+of+blind+tracheal+intubation+in+rabbits+(Oryctolagus+cuniculi)+supported+by+previous+maneuver+of+esophageal+cannulization.">Technique of blind tracheal intubation in rabbits (Oryctolagus cuniculi) supported by previous maneuver of esophageal cannulization.</a> Acta Cir Bras. 26 (5), 352-356 (2011).</li><li>Su, H. P., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=A+miniature+lighted+stylet+for+fast+oral+endotracheal+intubation+in+rabbits.">A miniature lighted stylet for fast oral endotracheal intubation in rabbits.</a> Vet J. 195 (2), 254-256 (2013).</li><li>Weinstein, C. H., Fujimoto, J. L., Wishner, R. E., Newton, P. O. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Anesthesia+of+six-week-old+New+Zealand+White+rabbits+for+thoracotomy.">Anesthesia of six-week-old New Zealand White rabbits for thoracotomy.</a> Contemp Top Lab Anim Sci. 39 (3), 19-22 (2000).</li><li>Stephens DeValle, J. M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Successful+Management+of+Rabbit+Anesthesia+Through+the+Use+of+Nasotracheal+Intubation.">Successful Management of Rabbit Anesthesia Through the Use of Nasotracheal Intubation.</a> Journal of the American Association for Laboratory Animal Science. 48, 166-170 (2009).</li><li>. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=.">.</a> A Guidance on the Use of Topical Anesthetics for Naso/Oropharyngeal and Laryngotracheal Procedures. , (2006).</li><li>Cook, R. T., Stene, J. K., Marcolina, B. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Use+of+a+Beck+Airway+Airflow+Monitor+and+controllable-tip+endotracheal+tube+in+two+cases+of+nonlaryngoscopic+oral+intubation.">Use of a Beck Airway Airflow Monitor and controllable-tip endotracheal tube in two cases of nonlaryngoscopic oral intubation.</a> Am J Emerg Med. 13 (2), 180-183 (1995).</li><li>Fish, R. E., Brown, M. J., Danneman, P. J., Karas, A. Z. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=.">.</a> Anesthesia and Analgesia in Laboratory Animals. , (2008).</li><li>Gografe, S. I., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Successful+management+of+long-term+general+anesthesia+in+rabbits+used+as+an+animal+model+of+human+disease.">Successful management of long-term general anesthesia in rabbits used as an animal model of human disease.</a> Contemp Top Lab Anim Sci. 42 (2), 16-19 (2003).</li><li>Nordin, U. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=The+trachea+and+cuff-induced+tracheal+injury.+An+experimental+study+on+causative+factors+and+prevention.">The trachea and cuff-induced tracheal injury. An experimental study on causative factors and prevention.</a> Acta Otolaryngol Suppl. 345, 1-71 (1977).</li><li>Phaneuf, L. R., Barker, S., Groleau, M. A., Turner, P. V. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Tracheal+injury+after+endotracheal+intubation+and+anesthesia+in+rabbits.">Tracheal injury after endotracheal intubation and anesthesia in rabbits.</a> J Am Assoc Lab Anim Sci. 45 (6), 67-72 (2006).</li><li>Grint, N. J., Sayers, I. R., Cecchi, R., Harley, R., Day, M. J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Postanaesthetic+tracheal+strictures+in+three+rabbits.">Postanaesthetic tracheal strictures in three rabbits.</a> Lab Anim. 40 (3), 301-308 (2006).</li><li>Squire, R., Siddiqui, S. Q., DiNunizio, G., Brodsky, L. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Quantitative+study+of+the+tracheotomy+and+endotracheal+intubation+on+the+rabbit+tracheobronchial+tree.">Quantitative study of the tracheotomy and endotracheal intubation on the rabbit tracheobronchial tree.</a> Ann Otol Rhinol. , (1990).</li><li>Kumar, R. A., Boyer, M. I., Bowen, C. V. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=A+reliable+method+of+anesthesia+for+extensive+surgery+in+small+rabbits.">A reliable method of anesthesia for extensive surgery in small rabbits.</a> Lab Anim Sci. 43 (3), 265-266 (1993).</li></ol>

The authors have nothing to disclose.

Here we provide a detailed description of a rabbit intubation technique that can be easily mastered in any clinical setting. This technique is similar to previously published direct visualization techniques10,15,20,25 with some additional refinements, including use of a 3.5 mm uncuffed endotracheal tube, and a 5 French urinary catheter as our chosen guide, which has been cut and marked with a permanent marker at the cut end. The rabbit trachea is easily prone to injury and thus the use of uncuffed endotracheal tubes is generally recommended when intubating rabbits to prevent damage to the tracheal mucosa from the pressure of the cuff.26 The 5 French urinary catheter we chose as a guide is small enough to easily pass through the vocal folds without obstructing the view during direct visualization of the larynx. While small, this catheter is stiff enough to remain in place as a guide for the endotracheal tube. The distal tip of the catheter is rounded to help reduce trauma when the bifurcation is reached. The proximal end of the catheter is cut so that the catheter is at a workable length (not excessively long) and to remove the end that widens for attachment to a syringe. The cut end is marked with permanent marker as a visual indicator to not insert this end into the trachea, which may cause damage to the tracheal mucosa.
The primary limitation of this technique is that, because it does require the use of a laryngoscope blade, it may not be feasible for very young rabbits or very small breeds due to smaller mouth size. In addition, some facilities may not have this size of laryngoscope blade readily available. At the author&#39;s institution, this method is used for New Zealand White (&#8805;6 weeks) and adult Dutch Belted rabbits, but we have not attempted this method in younger animals or smaller breeds. In situations where the rabbit patient is small, or if a laryngoscope with a small Miller blade is unavailable, an alternative option is to use a handheld otoscope rather than the laryngoscope.15,20 Using an otoscope with a #5 ear speculum, the larynx is visualized, the guide catheter is placed by direct visualization, and the speculum is removed prior to proceeding following the same steps as outlined above.
It is important to use great care when the guide catheter is placed to avoid the possibility of causing trauma or bronchospasm as the end of the catheter passes into the trachea and touches the tracheal bifurcation. The risk of these complications can be reduced or avoided by feeding the catheter with very gentle movements, stopping as soon as there is resistance, and avoiding movement of the head and neck once the catheter is in place. In addition, when advancing the endotracheal tube over the catheter, there is the potential for the catheter to catch on the endotracheal tube connector. Thus, it is important to make sure that the catheter slides through the connector without catching; alternatively, the connector can be removed and replaced when securing the endotracheal tube or attaching to the anesthetic circuit.
With any method of intubation, there is the potential for complications and adverse effects. Using the direct visualization method with a laryngoscope, improper insertion of the laryngoscope blade or aggressive placement of the endotracheal tube can result in laryngeal, tongue, or tooth injuries. Correct positioning of the animal is the first critical step in minimizing trauma during visualization of the larynx. The spine should be straight, with the head in direct alignment with the spine; if the animal is not straight, or if the neck is twisted to the left or right, this will make visualization of the larynx more difficult and may result in excessive trauma with the laryngoscope blade. Another critical key to success when using this technique is to follow the roof of the mouth towards the larynx, and once the soft palate is visualized, shift the blade into a proper position by bending at the wrist. This keeps the head in place, while moving the tip of the blade into optimal viewing position of the vocal cords, which are located quite ventral in the rabbit20,24.
Because direct visualization of the larynx can be tricky if the precise techniques we outline above are not followed, the use of alternative intubation strategies that do not require visualization of the larynx can be appealing. For example, the blind technique is one possible option that does not require use of a laryngoscope16,17,18,19,20. However, use of this technique relies on the ability to detect airflow through the endotracheal tube in order to direct the placement of the tube, and if the animal&#39;s breaths are very shallow or arrested, use of this method is not reliable. Supraglottic devices may also be considered, since placement of these devices does not require visualization of the larynx and they are generally very easy to place. These devices do not directly enter the trachea, however, and thus there is potential for lack of direct flow to the airway, inability to ventilate if laryngospasm develops, lack of a seal tight enough for ventilation during open-chest procedures or emergency resuscitation, and development of gastric tympany3,4,8. Newer devices specifically designed for rabbits may offer a promising alternative, but more studies are needed to evaluate these devices, and the concerns regarding lack of entry into the trachea still remain. Gastric tympany can also be a potential complication in an intubated animal if the endotracheal tube is accidentally placed into the esophagus; however, use of a direct visualization technique minimizes the risk of this complication by verifying proper placement of the guide catheter into the larynx.
Trauma to the arytenoid and/or tracheal mucosa is another potential concern when inserting an endotracheal tube, particularly when using inflatable cuffed tubes26,27,28. The trachea in rabbits may be easily injured, which can lead to complications such as subcutaneous emphysema, pneumothorax, and even death10,27,28,29. While performing the technique we describe here, care should be taken to prevent tracheal injury by use of uncuffed endotracheal tubes, ensuring the rounded tip of the guide catheter is inserted into the trachea, and not forcing the guide catheter into the glottis. In addition, selection of an appropriately sized endotracheal tube is of critical importance. Endotracheal tube size should be considered against the size of the animal, as well as compared to the opening of the laryngeal inlet since it is smaller in diameter than the trachea. An endotracheal tube too large in diameter may result in trauma to the arytenoid mucosa or cartilage. On the other hand, use of a smaller endotracheal tube results in increased airway resistance and increases the chances of obstruction due to mucus or a kink. For this reason, respiratory monitoring is very important in intubated rabbits. In addition to pulse oximetry, measurement of airflow should be monitored with capnography; if a capnograph is unavailable, airway monitors are an alternative that can be used to detect flow of air (but do not provide measurements of exhaled carbon dioxide). In addition, provision of assisted ventilation can be valuable, particularly in cases when smaller diameter tubes are used24,30.
In addition to the already mentioned benefits of using this technique, another major advantage of this method is that it can be performed by a single individual without the need for an assistant, which can be important in a busy clinical setting. In this situation, it is important to gather all necessary supplies and have them within easy reach during the intubation process, particularly when the guide catheter is in place and movement of the head should be avoided.
The technique we describe here is used by the veterinary and research staff in our institution for all rabbit intubations, which amounts to approximately 200-400 intubations per year. It is very easily taught in a typical rabbit anesthesia training session, which takes approximately 30 minutes. We have found that it is relatively easy to learn, with students learning it within their first 3 attempts and generally able to repeat the process successfully in the next additional attempt.For future study, it would be valuable to compare time to proficiency and ability to maintain proficiency over time for this method compared to other intubation techniques. While this has been studied for variations of blind techniques16, a comprehensive assessment of the learning curve for a wide variety of intubation techniques has not yet been performed. Another potential future direction of study could include comparing direct endotracheal intubation to the newer species-specific supraglottic airway devices, particularly concerning function during positive pressure ventilation.
In conclusion, the technique for intubation of rabbits we describe here is non-invasive, reliable, does not require the use of specialized equipment, is easy to master, and can be performed by a single individual without the need for an assistant. All airway access techniques present some level of risk, but by using a direct visualization technique and following the steps we describe above to minimize complications, the risks are far outweighed by the benefits of having an adequate airway during anesthesia.

Rabbits have a narrow, deep oral cavity that restricts visibility of the larynx for endotracheal intubation. They also have a very large fleshy tongue and cheek teeth which, when combined with the narrow oral cavity, can cause issues when inserting a laryngoscope and visualizing the glottis to insert an endotracheal tube1. Great care must be taken to avoid causing injury to the oral cavity and airway when attempting intubation. The laryngeal tissues are very friable and excessive trauma from repeated attempts to intubate can cause significant inflammation, making intubation more difficult2.
For these reasons, a variety of alternative techniques have been described, most notably supraglottic airway devices including the laryngeal tube3,4, the laryngeal mask airway (LMA)4,5,6 and a species-specific supraglottic airway device7. A laryngeal tube consists of a tube with two balloons that direct air flow into the trachea: a larger balloon in the middle of the tube forms a seal in the upper pharynx and a smaller balloon at the distal end seals the esophageal inlet3. The LMA consists of a tube with an elliptical mask at the distal end that is inflated to form an airtight seal over the glottis4,5,6. The species-specific device is the first veterinary species-specific supraglottic airway device, currently available for cats and rabbits, designed to fit the anatomical structures for each species to create a pressure seal in the pharynx7. However, because these devices do not directly enter the trachea, they may present risks for complications such as gastric tympany. The lack of a proper seal within the trachea presents a concern regarding the adequacy for use of these devices for positive pressure ventilation for respiratory support, emergencies, or thoracic surgery3,8. In addition, lack of direct intubation of the trachea may result in personnel exposure to waste anesthetic gases5.
Many methods for direct endotracheal intubation have been described9,10,11,12,13,14,15. One popular method is the blind technique, which may decrease the chance of injury to the oropharyngeal cavity since insertion of a laryngoscope isn&#39;t necessary16,17,18,19,20. As a visually blind technique, this method requires monitoring for air flow through the endotracheal tube and careful manipulation to guide placement. Although this method is commonly used in research and clinical veterinary practice, in the authors&#39; experience, this technique can be time consuming and not always successful, and thus is more difficult to teach and may require extra dosing of anesthetic agents9,10. In addition, because monitoring for respiration is used to guide proper placement of the tube, this method would be more difficult and less reliable during respiratory arrest. Another popular method is to use a traditional laryngoscope technique to intubate as is done with larger species. However, the traditional laryngoscope technique in rabbits is difficult in that the view of the vocal cords is obstructed when the endotracheal tube is inserted into the mouth. Therefore, use of this method can result in repeated intubation attempts, increased anesthetic dosing, and injury to the oral cavity and airway10.
More expensive and technically challenging options for intubation also exist. The fiberoptic laryngoscope allows easy insertion of the endotracheal tube by inserting the laryngoscope into the tube and visualizing the insertion into the trachea on a screen. Similarly, endoscopes can be used to visualize the laryngeal area and guide placement of the tube. However, both of these methods require the use of expensive equipment that may not be readily available in typical clinical settings9,11,12. Intubation via the nasal cavity is an alternative method that has been described, though this presents a risk of introducing opportunistic pathogens from the nasal cavity into the lungs, particularly in rabbits that are not specific-pathogen-free21. Lastly, more invasive methods of intubation have also been published, including retrograde insertion of a guide catheter through a needle placed percutaneously into the trachea, as well as the use of a needle cricothyroidotomy followed by placement of a guide wire, vessel dilator, and sheath introducer13,14. As invasive techniques, these methods have potential complications such as post-procedural pain and infection. The technique we describe here, using a laryngoscope and guide catheter, can be taught with minimal training with a short time to proficiency, is non-invasive, can be performed by a single individual without the need for an assistant, and does not require the use of specialized equipment.

<table><tbody><tr><td>Ketalar&lt;br/&gt; Ketamine HCl Inj.</td><td>JHP Pharmaceuticals</td><td>NDC 42023-113-10</td><td>35mg/kg IM in epaxial muscles or quadriceps muscle (preferred)</td></tr><tr><td>Anased&lt;br/&gt; Xylazine (100mg/ml)</td><td>Lloyd Labs</td><td>NADA #139-236</td><td>5mg/kg IM in epaxial muscles or quadriceps muscle (preferred)</td></tr><tr><td>Welch Allyn Laryngoscope Handle</td><td>Welch Allyn</td><td>60300</td><td>Requires 2 size C alkaline batteries</td></tr><tr><td>Size 0 or 1 Miller Laryngoscope Blade</td><td>Welch Allyn</td><td>68040</td><td></td></tr><tr><td>2.5 &amp;ndash; 4.0 mm ID uncuffed endotracheal tube</td><td>Jorgenson</td><td>J0149V</td><td>Suitable for 2.5-5 kg rabbits&lt;br/&gt; 3.5 mm most commonly used</td></tr><tr><td>Sovereign polypropylene catheter, 5 Fr x 22&amp;rdquo;</td><td>Medtronic</td><td>8890703310</td><td>Cut to 8-10 inches&lt;br/&gt; Mark the cut end with permanent marker to indicate which end not to insert</td></tr><tr><td>Lidocaine 2% HCL Inj</td><td>VetOne</td><td>L-2000-04</td><td></td></tr><tr><td>4-Ply Nonsterile, Bulk Packed Versalon Sponges (Gauze pads)</td><td>Covidien</td><td>KC9024A</td><td></td></tr><tr><td>Tape, Twill, Bleached &amp;frac12;&amp;rdquo; x 72 yds</td><td>Encompass Textiles</td><td>48210-025</td><td>Used for securing endotracheal tube</td></tr><tr><td>HR Lubricating Jelly</td><td>HR Pharmaceuticals</td><td>201</td><td>For lubricating endotracheal tube tip</td></tr><tr><td>Great Plains Ballistics: BAAM (Beck Airway Airflow Monitor) 22</td><td>BoundTree Medical</td><td>21410</td><td>For confirmation of successful intubation</td></tr><tr><td>Ambu Pediatric Co2 Detector</td><td>AMBU INC</td><td>172713</td><td>For confirmation of successful intubation</td></tr></tbody></table>

endotracheal intubation of rabbits using a polypropylene guide catheter

Endotracheal intubation in rabbits can be challenging due to their unusual anatomy. Achieving a patent airway during anesthesia is critical for the avoidance of airway obstruction, prevention of gastric tympany, and to allow ventilatory support. Due to the difficulty of intubation, alternative methods such as the use of laryngeal mask airways or laryngeal tubes have been explored. However, these methods do not result in direct access to the trachea and thus may present a risk for development of complications. In addition, lack of direct intubation of the trachea can result in personnel exposure to waste anesthetic gases. Numerous methods for endotracheal intubation have been described, including blind placement, use of a fiberoptic laryngoscope or endoscope, and cricoid placement. Despite these numerous publications, many still struggle to achieve success. Here we provide a detailed description of an intubation technique that can be taught with minimal training with a short time to proficiency. Briefly, after administration of injectable anesthesia and proper positioning of the rabbit, a polypropylene catheter is placed into the trachea by direct visualization using a laryngoscope. The catheter is then used as a guide to direct the endotracheal tube into the trachea. This method allows for intubation without the need for expensive equipment and can be performed by a single individual without the need for an assistant. In conclusion, this technique can be easily taught and performed at very little cost in any clinical or research setting.

At the authors&#39; institution, this technique is typically taught to laboratory and veterinary personnel during training sessions on rabbit handling and anesthesia techniques. Teaching sessions are performed with dedicated training animals. The trainer demonstrates the technique once and then trainees perform the technique under the guidance of the trainer. Trainees typically achieve success within 1-3 attempts. After they have successfully intubated the rabbit once, individuals are required to perform the intubation a second time, and are typically able to successfully intubate the rabbit again on the first additional attempt. Feedback during these training sessions, particularly from individuals who have been previously trained with alternative techniques, consistently includes comments on how easy this technique is to learn and complete successfully.
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/56369/56369fig1.jpg" /> 
Figure 1. Supplies for endotracheal intubation: 1) Laryngoscope with size 0 or 1 Miller laryngoscope blade, 2) umbilical tape (or other supplies for securing endotracheal tube), 3) 0.25 mL of 2% lidocaine, 4) 5-French polypropylene catheter cut to 8-10 inches with the non-rounded end marked with a permanent marker to clearly indicate which end should not be inserted into the trachea (arrow), 5) air flow detection device, 6) sterile lubricant to be applied to the distal end of the tube, 7) uncuffed endotracheal tube.&#160;<a href="https://cloudflare.jove.com/files/ftp_upload/56369/56369fig1large.jpg" style="font-size: 14px;" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/56369/56369fig2.jpg" /> 
Figure 2: Sternal positioning for endotracheal intubation. The rabbit is positioned sternally with the forelimbs extended to the end of the table. The hind limbs are extended back, and the rabbit&#39;s head is aligned with the spine. The left hand is used to elevate the head into extension in preparation for insertion of the laryngoscope. <a href="https://cloudflare.jove.com/files/ftp_upload/56369/56369fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/56369/56369fig3.jpg" /> 
Figure 3: Insertion of laryngoscope. A) The laryngoscope is inserted into the left diastema using the right hand, following the roof of the mouth with the tip of the blade until the soft palate is visible. Once the soft palate is visible, the laryngoscope is tipped forward while extending the rabbit&#39;s head back and neck forward to visualize the larynx. B) Visualization of the larynx. <a href="https://cloudflare.jove.com/files/ftp_upload/56369/56369fig3large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 4" class="xfigimg" src="/files/ftp_upload/56369/56369fig4.jpg" /> 
Figure 4: Advancement of the guide catheter. A) After switching the laryngoscope blade to the left hand, the right hand advances the rounded tip of the guide catheter through the opening past the larynx. B) The guide catheter is passed through the vocal chords with direct visualization. <a href="https://cloudflare.jove.com/files/ftp_upload/56369/56369fig4large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 5" class="xfigimg" src="/files/ftp_upload/56369/56369fig5.jpg" /> 
Figure 5: Advancement of the tracheal tube. The endotracheal tube is threaded over the guide catheter and is advanced until there is resistance from the vocal cords. <a href="https://cloudflare.jove.com/files/ftp_upload/56369/56369fig5large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 6" class="xfigimg" src="/files/ftp_upload/56369/56369fig6.jpg" /> 
Figure 6: lidocaine instillation. Lidocaine (2%, 0.25 mL) is instilled into the opening of the endotracheal tube. <a href="https://cloudflare.jove.com/files/ftp_upload/56369/56369fig6large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 7" class="xfigimg" src="/files/ftp_upload/56369/56369fig7.jpg" /> 
Figure 7: Endotracheal tube advancement. Two minutes after instillation of the lidocaine, the endotracheal tube is advanced by gently twisting it to pass through the vocal cords. <a href="https://cloudflare.jove.com/files/ftp_upload/56369/56369fig7large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 8" class="xfigimg" src="/files/ftp_upload/56369/56369fig8.jpg" /> 
Figure 8: Verification of air flow through the endotracheal tube. An airflow detection device may be used to verify air flow through the endotracheal tube, or a dental mirror may also be used to detect the condensation from breaths indicating successful intubation.&#160;<a href="https://cloudflare.jove.com/files/ftp_upload/56369/56369fig8large.jpg" style="font-size: 14px;" target="_blank">Please click here to view a larger version of this figure.</a>

Watch this Scientific Journal Video about Endotracheal Intubation of Rabbits Using a Polypropylene Guide Catheter at JoVE.com

Endotracheal Intubation of Rabbits Using a Polypropylene Guide Catheter

Endotracheal intubation in rabbits is challenging due to their unusual anatomy. Here we present a technique for direct intubation of the trachea using a polypropylene catheter as a guide. This method utilizes relatively inexpensive supplies, requires minimal training, and can be easily performed in any clinical setting.

Endotracheal intubation in rabbits can be challenging due to their unusual anatomy. Achieving a patent airway during anesthesia is critical for the ...

endotracheal-intubation-rabbits-using-polypropylene-guide

Research

JoVE Journal

Biology

33.3K Views.  Mayo Clinic. Endotracheal intubation in rabbits is challenging due to their unusual anatomy. Here we present a technique for direct intubation of the trachea using a polypropylene catheter as a guide. This method utilizes relatively inexpensive supplies, requires minimal training, and can be easily performed in any clinical setting.

Video: Endotracheal Intubation of Rabbits Using a Polypropylene Guide Catheter

Endotracheal Intubation in Mice via Direct Laryngoscopy Using an Otoscope

Mice, both wildtype and transgenic, are the principal mammalian model in biomedical research currently. Intubation and mechanical ventilation are necessary for whole animal experiments that require surgery under deep anesthesia or measurements of lung function. Tracheostomy has been the standard for intubating the airway in these mice to allow mechanical ventilation. Orotracheal intubation has been reported but has not been successfully used in many studies because of the substantial technical difficulty or a requirement for highly specialized and expensive equipment. Here we report a technique of direct laryngoscopy using an otoscope fitted with a 2.0 mm speculum and using a 20 G&#160;intravenous catheter as an endotracheal tube. We have used this technique extensively and reliably to intubate and conduct accurate assessments of lung function in mice. This technique has proven safe, with essentially no animal loss in experienced hands. Moreover, this technique can be used for repeated studies of mice in chronic models.

Endotracheal Intubation in Mice via Direct Laryngoscopy Using an Otoscope

We have developed a simple, reliable, and relatively inexpensive method for endotracheal intubation in mice via direct laryngoscopy using an otoscope with a 2.0 mm speculum. This technique is atraumatic and can be used for repeated measurements in chronic experiments. We find it superior to tracheostomy or previously reported nonsurgical techniques.

Mice, both wildtype and transgenic, are the principal mammalian model in biomedical research currently. Intubation and mechanical ventilation are ...

Medicine

A Reversible, Non-invasive Method for Airway Resistance Measurements and Bronchoalveolar Lavage Fluid Sampling in Mice

Airway hyperreactivity (AHR) measurements and bronchoalveolar lavage (BAL) fluid sampling are essential to experimental asthma models, but repeated procedures to obtain such measurements in the same animal are generally not feasible.  Here, we demonstrate protocols for obtaining from mice repeated measurements of AHR and bronchoalveolar lavage fluid samples.  Mice were challenged intranasally seven times over 14 days with a potent allergen or sham treated.  Prior to the initial challenge, and within 24 hours following each intranasal challenge, the same animals were anesthetized, orally intubated and mechanically ventilated.  AHR, assessed by comparing dose response curves of respiratory system resistance (RRS) induced by increasing intravenous doses of acetylcholine (Ach) chloride between sham and allergen-challenged animals, were determined.  Afterwards, and via the same intubation, the left lung was lavaged so that differential enumeration of airway cells could be performed.  These studies reveal that repeated measurements of AHR and BAL fluid collection are possible from the same animals and that maximal airway hyperresponsiveness and airway eosinophilia are achieved within 7-10 days of initiating allergen challenge.  This novel technique significantly reduces the number of mice required for longitudinal experimentation and is applicable to diverse rodent species, disease models and airway physiology instruments.  

Repeated measurements of rodent respiratory physiology and sampling of airway inflammatory cells are desirable, but generally not feasible. Here we describe a repeatable method for orally intubating mice that permits repeated measurements of airway hyperreactivity and sampling of airway inflammatory cells.

Airway hyperreactivity (AHR) measurements and bronchoalveolar lavage (BAL) fluid sampling are essential to experimental asthma models, but repeated ...

Blind Endotracheal Intubation in Neonatal Rabbits

The newborn rabbit is a useful animal model for various pathologies and procedures. Airway management of the rabbit is complex due to its anatomical characteristics, which is further complicated in the case of the newborn. Of the different methods of advanced airway management, endotracheal intubation is less aggressive than tracheostomy, and is more feasible than supraglottic management given the lack of supraglottic devices of such a small size. As direct glottis visualization is very difficult in animals this size, this blind intubation model is presented as an effective alternative, especially for experiments requiring prolonged anesthesia. Using this method, we performed blind intubations with a 90% success rate.

We describe a technique of endotracheal intubation in newborn rabbits after esophageal catheterization with a gastric tube.

The newborn rabbit is a useful animal model for various pathologies and procedures. Airway management of the rabbit is complex due to its anatomical ...

Simplifying Transcutaneous Intratracheal Drug Delivery in the Newborn Preterm Rabbit

Intratracheal (IT) drug delivery allows the direct delivery of pharmaceutical substances to the lung, maximizing potential pulmonary benefit and minimizing systemic drug exposure. The transcutaneous technique is simple and allows for the IT delivery of substances to the lung of prematurely born rabbits shortly after birth. Newborn pups are anesthetized with inhaled Isoflurane before being placed in a supine position with the neck extended. The larynx is identified and stabilized before transcutaneous placement of a 26-gauge (G) catheter into the trachea. Following catheterization of the trachea, a 30 G blunt needle attached to a Hamilton syringe is introduced into the IT catheter and is used for delivering a precise volume into the trachea during spontaneous respiration. After the IT injection is completed, the needle and catheter are withdrawn, and the pup is allowed to recover from anesthesia. Transcutaneous IT injection delivers a large proportion of the injected substance to the lung, with the majority remaining in the lung 3 hours after the intervention. The injections are well tolerated from the day of birth and can be repeated for multiple consecutive days without influencing survival. This technique can be used to investigate the effect of pharmaceutical agents on lung development and in the prevention of neonatal lung injury in preterm rabbits.

Transcutaneous intratracheal injection allows for effective intrapulmonary drug delivery during spontaneous respiration. Single and multiple injections are well tolerated with no effect on survival. The technique is simple to perform and can examine the effect of substances on lung development and the prevention of lung injury in newborn rabbits.

Intratracheal (IT) drug delivery allows the direct delivery of pharmaceutical substances to the lung, maximizing potential pulmonary benefit and ...

Isolated Lung Perfusion System in the Rabbit Model

The isolated lung perfusion system has been widely used in pulmonary research, contributing to elucidate the lungs&#39; inner workings, both micro and macroscopically. This technique is useful in the characterization of pulmonary physiology and pathology by measuring metabolic activities and respiratory functions, including interactions between circulatory substances and the effects of inhaled or perfused substances, as in drug testing. While in vitro methods involve the slicing and culturing of tissues, the isolated ex vivo lung perfusion system allows to work with a complete functional organ making possible the study of a continuous physiological function while recreating ventilation and perfusion. However, it should be noted that the effects of the absence of central innervation and lymphatic drainage still have to be fully assessed. This protocol aims to describe the assembly of the isolated lung apparatus, followed by the surgical extraction and cannulation of lungs and heart from experimental lab animals, as well as to display the perfusion technique and signal processing of data. The average viability of the isolated lung ranges between 5-8 h; during this period, the pulmonary capillary permeability increases, causing edema and lung injury. The functionality of preserved pulmonary tissue is measured by the capillary filtration coefficient (Kfc), used to determine the extent of pulmonary edema through time.

The isolated rabbit lung preparation is a gold standard tool in pulmonary research. This publication aims to describe the technique as developed for the study of physiological and pathological mechanisms involved in airway reactivity, lung preservation, and preclinical research in lung transplantation and pulmonary edema.

The isolated lung perfusion system has been widely used in pulmonary research, contributing to elucidate the lungs&#39; inner workings, both micro and ...

Endotracheal Intubation Using a Flexible Intubation Endoscope as a Standardized Model for Safe Airway Management in Swine

Endotracheal intubation is often a basic requirement for translational research in porcine models for various interventions that require a secured airway or high ventilation pressures. Endotracheal intubation is a challenging skill,&#160;requiring a minimum number of successful endotracheal intubations to achieve a high success rate under optimal conditions, which is often unachievable for non-anaesthesiology researchers. Due to the specific porcine airway anatomy, a difficult airway can usually be assumed. The impossibility of establishing a secure airway can result in injury, adverse events, or death of the laboratory animal. Using a prospective, randomized, controlled evaluation approach, it has been shown that fiberoptic-assisted endotracheal intubation takes longer but has a higher first-pass success rate than conventional intubation without causing clinically relevant drops in oxygen saturation. This model presents a standardized regimen for endoscopically guided endotracheal intubation, providing a secured airway, especially for researchers who are inexperienced in the technique of endotracheal intubation via direct laryngoscopy. This procedure is expected to minimize animal suffering and unnecessary animal losses.

The use of pigs in research has increased in recent years. Nevertheless, pigs are characterized by difficult airway anatomy. By demonstrating how to perform endoscopically guided endotracheal intubation, the present protocol aims to further increase laboratory animals' safety to avoid animal suffering and unnecessary death.

Endotracheal intubation is often a basic requirement for translational research in porcine models for various interventions that require a secured airway ...

Model of Ischemia and Reperfusion Injury in Rabbits

The protocol here provides a simple, highly replicable methodology to induce in situ acute regional myocardial ischemia in the rabbit for non-survival and survival experiments. New Zealand White adult rabbit is sedated with atropine, acepromazine, butorphanol, and isoflurane. The animal is intubated and placed on mechanical ventilation. An intravenous catheter is inserted into the marginal ear vein for the infusion of medications. The animal is pre-medicated with heparin, lidocaine, and lactated Ringer&#39;s solution. A carotid cut-down is performed to obtain arterial line access for blood pressure monitoring. Select physiologic and mechanical parameters are monitored and recorded by continuous real-time analysis.
With the animal sedated and fully anesthetized, either a fourth intercostal space small left thoracotomy (survival) or midline sternotomy (non-survival) is performed. The pericardium is opened, and the left anterior descending (LAD) artery is located.
A polypropylene suture is passed around the second or third diagonal branch of the LAD artery, and the polypropylene filament is threaded through a small vinyl tube, forming a snare. The animal is subjected to 30 min of regional ischemia, achieved by occluding the LAD by tightening the snare. Myocardial ischemia is confirmed visually by regional cyanosis of the epicardium. Following regional ischemia, the ligature is loosened, and the heart is allowed to re-perfuse.
For both survival and non-survival experiments, the myocardial function can be assessed via an echocardiography (ECHO) measurement of the fractional shortening. For non-survival studies, data from sonomicrometry collected using three digital piezoelectric ultrasonic probes implanted within the ischemic area and the left ventricle developed pressure (LVDP) using an apically inserted left ventricle (LV) catheter can be continuously acquired for evaluating the regional and global myocardial function, respectively.
For survival studies, the incision is closed, a left needle thoracentesis is performed for pleural air evacuation, and postoperative pain control is achieved.

The present study demonstrates a highly reproducible animal model of acute regional myocardial ischemia and reperfusion injury in rabbits using a left mini-thoracotomy for survival cases or a midline sternotomy for non-survival cases.

The protocol here provides a simple, highly replicable methodology to induce in situ acute regional myocardial ischemia in the rabbit for non-survival and ...

Tracheotomy-Based Endotracheal Intubation Protocol for Non-Survival Rat Models

Endotracheal Intubation via Tracheotomy and Subsequent Thoracotomy in Rats for Non-Survival Applications

Endotracheal intubation and subsequent ventilation are often basic requirements for translational research in rat models for various interventions that require controlled or high ventilation pressures or access to the thoracic cavity and organs. Conventional endoorotracheal intubation using the anatomically existing route through the mouth is well suited for survival experiments. However, this procedure poses some challenges, including generally higher levels of the required experience and technical skill, more advanced equipment, and greater time effort with relevant intubation failure rates and complications such as tracheal perforation, temporary systemic hypooxygenation, and relevant aerial leakage.
This manuscript, therefore, presents a detailed step-by-step protocol for endotracheal intubation through tracheotomy in non-survival rat models when guaranteed intubation success, constant oxygenation levels, high ventilation pressures, or open thoracotomy are required.
The protocol emphasizes the importance of meticulous surgical technique to ensure consistent and reliable outcomes, especially for researchers who are inexperienced or lack routine in the technique of endoorotracheal intubation via direct laryngoscopy. This procedure is, therefore, expected to minimize animal suffering and unnecessary animal losses.

Here we introduce a standardized procedure for endotracheal intubation via tracheotomy followed by thoracotomy in rats, aimed at enhancing the precision and reproducibility of non-survival applications requiring invasive ventilation and exposure of thoracic organs in in vivo rat models.

Endotracheal intubation and subsequent ventilation are often basic requirements for translational research in rat models for various interventions that ...

Tracheal Cannulation in Rabbit Model: A Procedure to Insert Tracheal Cannula into the Rabbit Trachea

Source: Pacheco-Baltazar A, et al. <a href="https://jove.unicartagenaproxy.elogim.com/v/62734">Isolated Lung Perfusion System in the Rabbit Model.</a> J. Vis. Exp. (2021).
This video demonstrates the surgical creation of an opening in the rabbit trachea to insert a tracheal cannula for artificially ventilating the lungs.

Source: Pacheco-Baltazar A, et al. Isolated Lung Perfusion System in the Rabbit Model. J. Vis. Exp. (2021).
This video demonstrates the surgical creation ...

JoVE Encyclopedia of Experiments

Large Animal Models

Leporine

Tracheal Intubation for Mechanical Ventilation: A Procedure to Insert Endotracheal Tube in Trachea of Rabbit Model

Source: Marger, L. et al, <a href="https://jove.unicartagenaproxy.elogim.com/v/59976">Calvarial Model of Bone Augmentation in Rabbit for Assessment of Bone Growth and Neovascularization in Bone Substitution Materials.</a> J. Vis. Exp. (2019)
In this video, we demonstrate the tracheal intubation &#8212; an invasive procedure for insertion of an endotracheal tube through the mouth in a rabbit model. This procedure allows for mechanical ventilation of the lungs.

Endotracheal Intubation of Rabbits Using a Polypropylene Guide Catheter

Summary

Explore More Videos

Chapters in this video

Endotracheal Intubation in Mice via Direct Laryngoscopy Using an Otoscope

A Reversible, Non-invasive Method for Airway Resistance Measurements and Bronchoalveolar Lavage Fluid Sampling in Mice

Blind Endotracheal Intubation in Neonatal Rabbits

Simplifying Transcutaneous Intratracheal Drug Delivery in the Newborn Preterm Rabbit

Isolated Lung Perfusion System in the Rabbit Model

Endotracheal Intubation Using a Flexible Intubation Endoscope as a Standardized Model for Safe Airway Management in Swine

Model of Ischemia and Reperfusion Injury in Rabbits

Endotracheal Intubation via Tracheotomy and Subsequent Thoracotomy in Rats for Non-Survival Applications

Tracheal Cannulation in Rabbit Model: A Procedure to Insert Tracheal Cannula into the Rabbit Trachea

Tracheal Intubation for Mechanical Ventilation: A Procedure to Insert Endotracheal Tube in Trachea of Rabbit Model