Name: Murine Kidney Transplant Technique (Video) | JoVE Journal
Uploaded: 2015-10-20T14:00:00.000+00:00
Duration: 8 min 58 s
Description: Learn a modified arterial anastomosis technique for kidney transplants in mice using the heel and toe cuff method. This approach reduces arterial thrombosis and improves surgical outcomes in transplantation research.

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5 minutes

This work was supported in part by 1R03DK096151.&#160;We acknowledge the UAB-UCSD O&#8217;Brien Center (NIH P30 DK079337) for providing initial technical assistance with setting up this model.

All mice were purchased from The Jackson Laboratory (Bar Harbor, ME) and were housed under pathogen free conditions at the University of Colorado Denver, Barbara Davis Center Animal Facility according to NIH Guidelines and with approval of the University of Colorado Denver IACUC.
1. Donor Kidney Harvest
<ol>
	<li>Sterilize all instruments, wear sterile gloves throughout the procedure and maintain a sterile field. Perform all surgeries with the use of an operating microscope.</li>
	<li>Surgically remove mouse donor kidneys from pentobarbital-anesthetized (60mg/kg IP) donors. Ascertain depth of anesthesia by toe-pinch, and observe the respiratory rate.</li>
	<li>Clip the fur then immobilize the mouse by 4-way restraints. Prepare the skin with povidone-iodine and drape the mouse in a sterile fashion.</li>
	<li>Make a 2 cm midline vertical abdominal incision and enter the abdominal cavity. Retract the bowel superiorly and externalize it on to the chest. Keep the bowel wrapped in sterile moist gauze throughout the procedure.</li>
	<li>Identify the great abdominal vessels and mobilize them, identify any lumbar branches and either cauterize or ligate them with 10/0 nylon suture.</li>
	<li>Immediately distal to the left renal vessels tease the inferior vena cava (IVC) and abdominal aorta (AA) apart by blunt dissection over approximately 2mm. Ligate with 10/0 nylon and divide small arterial and venous branches from the renal vessels.</li>
	<li>Now separate the renal vein from the renal artery carefully by blunt dissection of these structures. This allows for the accurate creation of a Carrel patch at the proximal end of the renal vein, which will be used to form an end-to-side anastomosis to the recipients IVC.</li>
	<li>Identify, ligate and divide the left adrenal vessels. This permits access to the suprarenal aorta and a 6-0 silk suture is placed around the aorta in preparation for ligation, but not tied at this time.</li>
	<li>Mobilize the kidney, vessels and ureter from the surrounding facia. Rotate the kidney to the right and ligate/divide any posterior branches. Then return the kidney to the left.</li>
	<li>Now direct attention to the ureter. Without disturbing the renal hilum free the ureter from the surrounding facia taking care to preserve the ureteric vessels. Divide the ureter at the level of the ductus deferens. The kidney is now ready for recovering.</li>
	<li>Slowly inject 300 units of heparin into the distal IVC thereby heparinizing the donor. Tie down the 6-0 silk suture placed around the suprarenal AA and perfuse the left kidney via the distal abdominal aorta with 0.8ml of heparin saline solution (100 U/ml).</li>
	<li>Once the perfusion has ceased create a venous Carrel patch immediately to eliminate backflow into the kidney. Retract the renal vein toward the kidney revealing the AA and renal artery beneath.</li>
	<li>Divide the aorta adjacent to the renal artery creating a heel and toe cuff as shown in Figure&#160;1. Remove the kidney, vessels and ureter from the donor.</li>
	<li>Remove the kidney directly to a pre-prepared recipient (0 min&#160;cold ischemia time) or stored at 4&#160;oC in a solution of choice for a pre-determined time until time of implantation. Euthanized the donors by exsanguanation and cervical dislocation. Total time to recover donor kidney is approx. 15-20 min.</li>
</ol>
2. Kidney Implant Technique
<ol>
	<li>Anesthetize the recipient mouse with pentobarbital (60mg/kg IP initial dose, 25mg/kg IP supplemental dose if required). Ascertain depth of anesthesia by toe-pinch, and observe the respiratory rate. Clip the fur then immobilize the mouse by 4-way restraints and apply ophthalmic ointment to the eyes. Prepare the skin with povidone-iodine and drape the mouse in a sterile fashion.</li>
	<li>Make a 2 cm midline vertical abdominal incision and enter the abdominal cavity. Retract the bowel superiorly and externalize on to the chest. Keep the bowel wrapped in sterile moist gauze throughout the procedure.</li>
	<li>At this time perform a right nephrectomy. Ligate the renal artery and vein with 6-0 silk sutures. Excise the kidney distal to the sutures. Ligate the ureter with 6-0 silk and then divide proximal to the kidney.</li>
	<li>Isolate the abdominal aorta and inferior vena cava (IVC) below the renal vessels. Place 4-0 cotton ties around the aorta and IVC superior then inferior to the anastomosis site. Identify and ligate any lumbar vessels within the field with 10-0 nylon suture.</li>
	<li>Knot the cotton ties, first the inferior followed by the superior. In this way some blood is retained in the aorta making the aortotomy easier.</li>
	<li>Form the aortotomy with a 30G needle to enter the lumen of the aorta. Extend the incision with fine micro scissors to a length of approximately 2mm.</li>
	<li>Make an end to side anastomosis of the donor aortic heel-and-toe cuff to the recipient aorta in the following fashion. Place a 10-0 nylon suture stay stitch in the donor aorta and to the inferior angle of the incision in the recipient aorta and tie.</li>
	<li>Place a second 10-0 nylon opposite the first in the donor aorta and the superior corner of the incision in the abdominal aorta and tie. Make a running suture line from superior to inferior in the lateral wall of the aorta and tie against the previously placed stay stitch. Then suture the medial wall in a running fashion and tie.</li>
	<li>Make an end to side anastomosis of the donor renal vein to the recipient IVC in the following fashion. Puncture the IVC with a 30G needle and extend the incision with fine micro scissors. Tie the donor renal vein to the inferior corner of the incision in the IVC with 10-0 nylon. Make a running suture line between the renal vein and the IVC and tie. 
	NOTE: It is also vitally important that full thickness passes of the suture needle including the vascular adventitia and the intima are achieved. Eversion of the edges also ensures that there is intima-to-intima contact, which aids in sealing and healing of the anastomoses. While a hemostatic clotting agent can be useful for reducing leaks, we recommend that a surgeon instead rely on good technique.</li>
	<li>Ensure that the anastomoses are &#8220;clean&#8221;. That is, that the opposing walls are not caught when placing stitches. This will cause a significant constriction to flow that will result in a failed graft and in extreme cases to hind limb paralysis. 
	NOTE: Another vitally important factor is ensuring that the tension of the anastomotic suture lines is also optimal. Too loose and there will be irreversible leaking, too tight and stricture to flow will result. If on the arterial side this will result in poor perfusion of the graft, if on the venous side a congested kidney will result.</li>
	<li>Release the distal 4-0 cotton tie re-establishing venous flow. Once hemostasis of the venous anastomosis has been observed gradually loosen the proximal 4-0 cotton tie and observe the arterial anastomosis for hemostasis.</li>
	<li>Remove the cotton ties from the mouse once both anastomoses are considered secure. Pierce the bladder with a 20 G needle creating two holes.</li>
	<li>Pass the tips of curved forceps through the holes and pull the donor ureter through the bladder with the forceps with the proximal end of the ureter being anchored to the bladder wall with two 10-0 nylon sutures. Trim the excess length of ureter protruding from the second hole allowing the ureter to retract within the bladder and close the hole with two 10-0 nylon sutures.</li>
	<li>Return the bowel to the abdomen. Close the abdominal wall in two layers using 5-0 Silk suture in a running fashion.</li>
	<li>Administer a 1.0 ml bolus of sterile, warm normal saline into the abdomen as fluid resuscitation upon closing, and inject 0.8 ml of normal saline subcutaneously post-operatively. No other supportive measures are required during the surgery.</li>
	<li>Recover the animal on a warming blanket. Total implant time is approx. 35-45 min. Administer analgesics such as buprenorphine, 0.05 mg/kg, SC, 0.1-0.2 ml at the beginning of the procedure and every 6-12 hr for 72 hr post-op.</li>
</ol>
3. Contralateral Nephrectomy
<ol>
	<li>Depending on the protocol requirements, several days after the implant procedure, perform a contralateral nephrectomy under isoflurane anesthesia (5% inhaled isoflurane for induction, 1.5-2.0% for maintenance).</li>
	<li>Enter the abdominal cavity and gently retract the bowel to the animal&#8217;s right. Expose the left kidney and blunt dissect from the surrounding fascia.</li>
	<li>Ligate the renal artery, vein and ureter with 6-0 silk sutures and then excise the kidney above the sutures and remove the kidney. Total operative time is approx. 10 min.</li>
</ol>
4. Graft Assessment
<ol>
	<li>Measure serum creatinine using the alkaline picrate method (Jaffe reaction).</li>
</ol>

<ol><li>Skoskiewicz, M., Chase, C., Winn, H. J., Russell, P. S. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Kidney+transplants+between+mice+of+graded+immunogenetic+diversity%5BTitle%5D)+AND+%22Transplant+Proc%22%5BJournal%5D)">Kidney transplants between mice of graded immunogenetic diversity.</a> Transplant Proc. 5 (1), 721-725 (1973).</li>
<li>Kalina, S. L., Mottram, P. L. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((A+microsurgical+technique+for+renal+transplantation+in+mice%5BTitle%5D)+AND+%22Aust+N+Z+J+Surg%22%5BJournal%5D)">A microsurgical technique for renal transplantation in mice.</a> Aust N Z J Surg. 63 (3), 213-216 (1993).</li>
<li>Han, W. R., Murray-Segal, L. J., Mottram, P. L. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Modified+technique+for+kidney+transplantation+in+mice%5BTitle%5D)+AND+%22Microsurgery%22%5BJournal%5D)">Modified technique for kidney transplantation in mice.</a> Microsurgery. 19 (6), 272-274 (1999).</li>
<li>Ge, F., Gong, W. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Strategies+for+successfully+establishing+a+kidney+transplant+in+a+mouse+model%5BTitle%5D)+AND+%22Exp+Clin+Transplant%22%5BJournal%5D)">Strategies for successfully establishing a kidney transplant in a mouse model.</a> Exp Clin Transplant. 9 (5), 287-294 (2011).</li>
<li>Martins, P. N. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Learning+curve%2C+surgical+results+and+operative+complications+for+kidney+transplantation+in+mice%5BTitle%5D)+AND+%22Microsurgery%22%5BJournal%5D)">Learning curve, surgical results and operative complications for kidney transplantation in mice.</a> Microsurgery. 26 (8), 590-593 (2006).</li>
<li>Corry, R. J., Winn, H. J., Russell, P. S. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Primarily+vascularized+allografts+of+hearts+in+mice.+The+role+of+H-2D%2C+H-2K%2C+and+non-H-2+antigens+in+rejection%5BTitle%5D)+AND+%22Transplantation%22%5BJournal%5D)">Primarily vascularized allografts of hearts in mice. The role of H-2D, H-2K, and non-H-2 antigens in rejection.</a> Transplantation. 16 (4), 343-350 (1973).</li>
<li>Zhang, Z. Kidney Transplantation in Mice. <a target="_blank" href="http://scholar.google.com/scholar?hl=en&safe=off&q=author%3aZhang%2C+Z+%22Experimental+Organ+Transplantation%22">Experimental Organ Transplantation</a>. Chen, H., Qian, S. , Nova Science Publishers. 45-64 (2013).</li>
<li>Zhang, L., Moskovitz, M., Piscatelli, S., Longaker, M. T., Siebert, J. W. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Hemodynamic+study+of+different+angled+end-to-side+anastomoses%5BTitle%5D)+AND+%22Microsurgery%22%5BJournal%5D)">Hemodynamic study of different angled end-to-side anastomoses.</a> Microsurgery. 16 (2), 114-117 (1995).</li>
<li>Liu, Q., Mirc, D., Fu, B. M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Mechanical+mechanisms+of+thrombosis+in+intact+bent+microvessels+of+rat+mesentery%5BTitle%5D)+AND+%22J+Biomech%22%5BJournal%5D)">Mechanical mechanisms of thrombosis in intact bent microvessels of rat mesentery.</a> J Biomech. 41 (12), 2726-2734 (2008).</li>
<li>Chesnutt, J. K., Han, H. C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Tortuosity+triggers+platelet+activation+and+thrombus+formation+in+microvessels%5BTitle%5D)+AND+%22J+Biomech+Eng%22%5BJournal%5D)">Tortuosity triggers platelet activation and thrombus formation in microvessels.</a> J Biomech Eng. 133 (12), 121004(2011).</li>
<li>Han, H. C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Blood+vessel+buckling+within+soft+surrounding+tissue+generates+tortuosity%5BTitle%5D)+AND+%22J+Biomech%22%5BJournal%5D)">Blood vessel buckling within soft surrounding tissue generates tortuosity.</a> J Biomech. 42 (16), 2797-2801 (2009).</li>
<li>Gutierrez-Diaz, J. A., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Intraluminal+thrombus+and+neointimal+hyperplasia+after+microvascular+surgery%5BTitle%5D)+AND+%22Surg+Neurol%22%5BJournal%5D)">Intraluminal thrombus and neointimal hyperplasia after microvascular surgery.</a> Surg Neurol. 24 (2), 153-159 (1985).</li>
<li>Khouri, R. K., Cooley, B. C., Kenna, D. M., Edstrom, L. E. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Thrombosis+of+microvascular+anastomoses+in+traumatized+vessels%3A+fibrin+versus+platelets%5BTitle%5D)+AND+%22Plast+Reconstr+Surg%22%5BJournal%5D)">Thrombosis of microvascular anastomoses in traumatized vessels: fibrin versus platelets.</a> Plast Reconstr Surg. 86 (1), 110-117 (1990).</li>
<li>Johnson, P. C., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Initial+platelet+deposition+at+the+human+microvascular+anastomosis%3A+effect+on+downstream+platelet+deposition+to+intact+and+injured+vessels%5BTitle%5D)+AND+%22Plast+Reconstr+Surg%22%5BJournal%5D)">Initial platelet deposition at the human microvascular anastomosis: effect on downstream platelet deposition to intact and injured vessels.</a> Plast Reconstr Surg. 90 (4), 650-658 (1992).</li>
</ol>

The authors have nothing to disclose.

Mastering this transplant technique is difficult, but once accomplished it is a very powerful research tool. The patient surgeon/researcher will be rewarded by attention to detail and consistency of technique, which is the key to mastering any surgical procedure, even more so in small animal models. The technical difficulties of mastering the mouse kidney transplant are many folds, and it is highly probable that experience in other small animal transplant models must be gained before tackling this procedure.
<p class...

Since 1973 the kidney transplant model in mice has been a valuable research tool, but technical issues have hampered its widespread use. Over the years several papers have been published detailing improvements/refinements to this procedure. As a model of primarily vascularized solid organ transplantation this procedure is probably second only to the heterotopic heart transplant model which was also devised by the Russell laboratory in 1973 6. Both models lend themselves to research into allogeneic rejection responses, the development of delayed graft function and ischemia reperfusion injury.
One of the most common issues to be reported with kidney transplantation is the relatively high incidence of arterial thrombosis 4,5,7 which we also experienced in our laboratory. Therefore we set out to perform a literature review of thrombus formation and possibly find the cause of this technical issue and to also devise a possible solution. The most likely cause of thrombosis is the somewhat tortuous path the blood takes from the recipient aorta, into the donor renal aorta then on to the donor renal artery. This path causes turbulence in the renal artery which can lead to platelet activation and thrombus formation. Based on the recent observations and a search of relevant literature 8-14 we came up with a new technique that has reduced thrombosis to 0%.
The technique described here varies from previously reported techniques in the formation of an arterial heel-and-toe cuff which facilities improved blood flow and significantly reduces thrombus formation. The cuff is formed by dividing the infra-renal aorta across the face of the renal arterial ostium at an angle less than 45o to the longitudinal axis of the aorta (Figure 1A &#38; 1B). This results in a cuff approximately 2mm in length. A venous Carrel patch is formed by transecting the renal vein into the IVC thereby increasing the diameter of the cuff. The infra-renal donor abdominal aorta heel-and-toe cuff is end-to-side anastomosed to the recipient abdominal aorta and the donor renal vein/IVC patch is end-to-side anastomosed to the recipient abdominal inferior vena cava (IVC). The ureter is then introduced into and anchored to the bladder as described by Han et al 3.
For this study untreated transplants with warm ischemia times only (i.e., no cold ischemia) are compared. In this case warm ischemia refers to the time from the cessation of blood flow through the donor kidney (step 1.11 below) and reperfusion of the graft in the recipient (step 2.11 below). Cold ischemia refers to the time that the kidney is not perfused and is kept in cold storage until the beginning of the implant procedure.

<table><tbody><tr><td>Instrument</td><td>Roboz #</td><td>Fine Science Tools #</td><td>Arosurgical #</td></tr><tr><td>Straight micro-dissecting forcep #5</td><td>RS-5015</td><td>11295-51</td><td></td></tr><tr><td>Curved micro-dissecting forcep #7</td><td>RS-5047</td><td>11297-00</td><td></td></tr><tr><td>Curved serrated forcep</td><td>RS-5137</td><td>11052-10</td><td></td></tr><tr><td>Vannas micro-dissecting scissors, short</td><td>RS-5610</td><td></td><td>09.140.08</td></tr><tr><td>Micro-dissecting scissors, straight, sharp, long</td><td></td><td>11.602.11</td><td></td></tr><tr><td>Micro spring handle needle holder</td><td></td><td></td><td>11.549.15</td></tr><tr><td>Straight mosquito forcep</td><td></td><td>91308-12</td><td></td></tr><tr><td>Micro-dissecting scissors, straight, blunt</td><td>RS-5962</td><td>14078-10</td><td></td></tr><tr><td>Micro-dissecting scissors, curved, blunt</td><td>RS-5981</td><td>14079-10</td><td></td></tr><tr><td>Micro retractor</td><td>RS-6540</td><td></td><td></td></tr><tr><td>Instrument tray, 10&amp;rdquo; x 6 &amp;frac12;&amp;rdquo; x &amp;frac34;&amp;rdquo;</td><td>RT-1350S</td><td></td><td></td></tr><tr><td>Silk suture, 5/0, 22.5m spool</td><td></td><td>18020-50</td><td></td></tr><tr><td>Suture</td><td></td><td></td><td></td></tr><tr><td>10/0 nylon</td><td></td><td></td><td>T4A10Q07</td></tr><tr><td>5/0 silk</td><td></td><td></td><td>E19A05N</td></tr><tr><td>Gloves</td><td></td><td>Drapes</td><td></td></tr><tr><td>Biogel from Medex Supply</td><td></td><td>Precept, #64-9012-9</td><td></td></tr><tr><td>Syringes</td><td></td><td>Cotton applicators</td><td></td></tr><tr><td>B-D 1cc insulin, #329424</td><td></td><td>Fisher-brand, #23-400-100</td><td></td></tr><tr><td>Povidone-Iodine swabs</td><td></td><td></td><td></td></tr><tr><td>PDI, #B40600</td><td></td><td></td><td></td></tr><tr><td>4/0 Cotton ties</td><td></td><td></td><td></td></tr><tr><td>Domestic cotton autoclaved with instruments</td><td></td><td></td><td></td></tr></tbody></table>

murine kidney transplant technique

Murine Kidney Transplant Technique

The first mouse kidney transplant technique was published in 19731 by the Russell laboratory. Although it took some years for other labs to become proficient in and utilize this technique, it is now widely used by many laboratories around the world. A significant refinement to the original technique using the donor aorta to form the arterial anastomosis instead of the renal artery was developed and reported in 1993 by Kalina and Mottram 2 with a further advancement coming from the same laboratory in 1999 3. While one can become proficient in this model, a search of the literature reveals that many labs still experience a high proportion of graft loss due to arterial thrombosis. We describe here a technique that was devised in our laboratory that vastly reduces the arterial thrombus reported by others 4,5. This is achieved by forming a heel-and-toe cuff of the donor infra-renal aorta that facilitates a larger anastomosis and straighter blood flow into the kidney.

This surgical technique allows for either simple graft survival/rejection studies, or quite complex experimental protocols. In the figures below we demonstrate the advantages of using this improved arterial anastomosis technique. Using this technique we have significantly reduced the incidence of arterial thrombosis from 35% to 0% thus increasing productivity. We have used this technique for over one year with the same 0% thrombosis result maintained. Figure 1 describes the method for the formation of th...

The goal of this manuscript is to describe the steps required to perform a kidney transplant in a mouse, paying particular attention to the details of the arterial anastomosis.

The first mouse kidney transplant technique was published in 19731 by the Russell laboratory. Although it took some years for other labs to become ...

The overall goal of this procedure is to demonstrate a modified arterial anastomosis technique for kidney transplants in the mouse. This is accomplished by first carefully dissecting the relevant vessels in the donor. The second step is to create a heel and toe cuff of the donor abdominal aorta adjacent to the renal artery.Next, this heel and toe cuff is used to form the arterial anastomosis in the recipient. Ultimately, this technique should result in very low instances of arterial thrombosis. This video will show you how to create an arterial heel and toe cuff to facilitate kidney transplants in the mouth.The main advantage of this technique of resisting methods is that the blood flow path from the recipient aorta into the donor renal artery is straightened, resulting in a reduction of platelet activation and thrombosis formation Using sterile technique under an operating microscope, harvest the donor's kidney, perform properly. The harvest time will be 15 to 20 minutes. Remove the fur and then restrain the animal.Prepare the surgical site by washing the skin with povidone iodine, drape the mouse and begin the surgery with a two centimeter midline abdominal incision. Retract the bowel onto the chest and wrap it in moist gauze. Keep the gauze moist throughout the procedure.Now, find the great abdominal vessels and mobilize them. Any lumbar branches should be either cauterized or ligated with 10 zero nylon suture. Next bluntly, dissect a two millimeter division of the inferior vena cava and the aorta distal to the left renal vessels.Then ligated and divide any small arterial and venous branches that attach to the renal vessel. Continue the blunt dissection to separate the renal vein from the renal artery, thus allowing for the later creation of a Carroll patch at the proximal end of the renal vein, this patch will be used for the formation of the venous anastomosis. Next like it and divide the left adrenal vessels to access the supra renal aorta.Once accessed, loop six zero silk. Suture around the supra renal aorta for later use. Now mobilize the kidney vessels and ureter from the surrounding fascia.Rotate the kidney to the right on the posterior side, ligate and divide any vascular branches focusing in on the ureter. Carefully free the ureter from the surrounding fascia. Do not disturb the renal hilum and preserve the eretic vessels.Next, divide the ureter at the level of the ductus deens. The kidney can now be recovered. First, slowly inject 300 units of heparin into the distal IVC to heparinized the donor.Second, tie down the six zero suture around the supra renal aa. Then perfuse the left kidney from the abdominal aorta, injecting 0.8 milliliters of heparin saline solution at 100 units per milliliter. After the perfusion, immediately create the venous caryl patch, thereby avoiding backflow into the kidney.Retract the renal vein toward the kidney to reveal the AA and renal artery. Now divide the aorta adjacent to the renal artery. Make a heel and to cuff.Then if zero minutes of cold ischemia is required, transfer the recovered kidney into a prepared recipient. Alternatively, transfer the organs to a four degree Celsius storage chamber and then euthanize the donors as indicated in the text protocol. This procedure will take 35 to 45 minutes as done for the donor anesthetize.The recipient also supplement the initial bolus as needed. Provide the recipient with ophthalmic cream. Then give the animal an injection of buprenorphine and continue its administration after the procedure, after making the initial incision and displacing the bowel as done with the donor, proceed with a right nephrectomy, ligate the renal artery and vein with six zero suture ligate and divide the ureter proximal to the kidney with six zero suture.Then excise the kidney distal to the vascular suture. Now below the renal vessels, isolate the AA and IVC then superior to the anastomosis site. Place a four zero cotton tie around the aorta and IVC do the same inferior to the site.Any lumbar vessels found in the region should either be cauterized or ligated with 10 zero nylon suture tightly not the suture that is inferior and then tightly not the suture that is superior. This will retain some blood in the aorta facilitating the AOR autotomy. Perform the atomy with a 30 gauge needle, then extend the incision to be about two millimeters long using fine micro scissors.The next step is to make an endo anastomosis from the donor heel and toe cuff to the recipient's aorta. First, put a stay stitch in the heel of the donor aorta with 10 zero suture. Continue this through the inferior end of the incision in the recipient's aorta and tie off.Second, place a 10 zero suture in the superior end of the aortic incision and continue this through the toe of the donor cuff and tie off. Thirdly, starting at the superior end, make a runny suture in the lateral wall of the aorta and tie off against the previously placed inferior stay stitch. Then flip the kidney and continue a running suture along the medial wall and tie off against the superior stay stitch.Complete the venous anastomosis by puncturing the IVC using the needle and then extending the incision with fine micro scissors. Using 10 zero nylon, tie the donor renal vein to the inferior corner of the IVC. Place another 10 zero suture at the superior end of the IVC and donor vein and make a running suture along both sides.As with the arterial anastomosis, aversion of the tissue edges helps with seal and healing. Now, check your work. Opposing walls should not be caught by the stitches or blood flow will be too constricted.Another vitally important factors ensuring that the tension of the anastomotic suture line is optimal too loose and there will be irreversible leaking too tight and there will be stricture to flow. If on the arterial side, this will result in poor profusion of the graft. If on the venous side a congested kidney will result.Once the anastomosis are complete, release the distal cotton tie to establish venous flow. Then gradually loosen the proximal tie and wash for hemostasis at the arterial anastomosis. When both anastomosis are confirmed as secure, here's the recipient's bladder with a 20 gauge needle making two holes pass forceps through the holes and pull the donor ureter through the bladder.Then anchor the proximal end of the ureter to the bladder wall with 2 10 0 sutures. Trim the excess length of protruding ureter so it retracts within the bladder. Then close the other hole in the bladder with 10 zero suture.Complete the surgery by replacing the bowel, closing the abdomen in two layers with running five zero silk suture and injecting one microliter of saline into the abdomen before closing. After closing the abdomen inject another 0.8 milliliters of saline subcutaneously and recover the animal on a warm blanket In one year of data collection, this technique significantly reduced the incidence of arterial thrombosis from 35%to 0%and this rate of 0%thrombosis has been maintained since immunohistochemistry was performed on a non-transplant kidney and a kidney transplanted. Using the described technique, a periodic acid shift stain revealed normal proximal tubular cells in the control and donor.The cells are cuboidal with a clear cytoplasm and a round light nucleus in the middle of the cell for both the arrows. Point out evidence of a mild brush border injury, but the majority of brush borderers are regular and well preserved. After watching this video, you should have a good understanding of how to perform an arterial heel and toe cup anastomosis that will result in reduced instances of thrombosis and more successful kidney transplants.

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In this video, we describe the procedure for kidney extraction from the retroperitoneal space of the mouse. The extracted kidney can further be microdissected to obtain an intact kidney without a renal capsule and the surrounding fat layer.

Extracting Intact Kidney from Mouse: A Technique to Obtain Kidney Without Renal Capsule from Murine Models

This video describes orthotopic kidney auto-transplantation in a porcine model. This surgical procedure involves the transplantation of an animal's kidney graft at its original anatomical location. The model is used to investigate new treatments for end-stage kidney diseases in humans.

Orthotopic Porcine Kidney Transplantation: A Technique to Transplant Graft Kidney in Porcine Model

Here, we present a protocol to study the immunology of rejection. The surgical model presented reports a short operating time and a concise technique. Depending on the donor-recipient strain combination, the transplanted kidney may develop acute cellular rejection or chronic allograft damage, defined by interstitial fibrosis and tubular atrophy.

Mouse Kidney Transplantation: Models of Allograft Rejection

This report provides a detailed description of transplanting murine thymi from different aged donor mice under the kidney capsule of immunodeficient mouse recipients. The goal of this approach is to model T cell development and thymic selection events in vivo.

Isolation and Transplantation of Different Aged Murine Thymic Grafts.

The purpose of this manuscript and protocol is to explain and demonstrate in detail the surgical procedure of orthotopic kidney transplantation in rats. This method is simplified to achieve the correct perfusion of the donor kidney and shorten the reperfusion time by using the venous and ureteral cuff anastomosis technique.

Orthotopic Rat Kidney Transplantation: A Novel and Simplified Surgical Approach

We provide a simple and efficient method to transplant 2’-deoxyguanosine treated E18.5 thymus into the renal capsule of a nude mouse. This method should aide in the study of both thymic epithelial cells function and T cells maturation.

Renal Subcapsular Transplantation of 2'-Deoxyguanosine-Treated Murine Embryonic Thymus in Nude Mice

This protocol presents a new surgical technique of mouse kidney transplantation focusing on a modified arterial anastomosis strategy. A vascular suture technique including a simple and safer ureter-bladder anastomosis method is also presented. These modifications shorten the operation time and improve the success rate of the mouse kidney transplantation procedure.

A Modified Surgical Technique for Kidney Transplantation in Mice

The rat orthotopic renal transplantation model contributes to investigating the mechanism of renal allograft rejection. The current model increases the recipients' survival without interference with blood supply and venous reflux of the lower body using an end-to-end anastomosis of kidney implantation and an end-to-side "tunnel" method of ureter-bladder anastomosis.

A Rat Orthotopic Renal Transplantation Model for Renal Allograft Rejection

Learn a modified arterial anastomosis technique for kidney transplants in mice using the heel and toe cuff method. This approach reduces arterial thrombosis and improves surgical outcomes in transplantation research.

Murine Kidney Transplant Technique

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