We are extremely grateful to Ms. Jennifer Munguia for her artistic illustration of the schematic diagram. We thank Mr. Michael R. Honig at Houston&rsquo;s Community Public Radio Station KPFT for his editorial assistance. This study was supported by American Diabetes Association #1-15-BS-177 (YS), and NIH R56DK118334/R01DK118334 (YS). This work was also supported by the USDA National Institute of Food and Agriculture, Hatch project 1010840 (YS) and R01 DK095118 (SG).

All methods described here have been approved by the Animal Care and Use Committee (ACUC) of Texas A&#38;M University. The surgical tools need is shown in Figure 1 and the schematic diagram of the procedure is shown in Figure 2.
1. Solutions
<ol>
	<li>Prepare Hank&#8217;s Balanced Salt Solution (HBSS) by adding 100 mL of 10X HBSS (from stock) to 900 mL of distilled water to make 1 L HBSS (1X).</li>
	<li>Prepare STOP solution (must be made fresh and should be used within 1 h) by adding 50 mL of 100X fetal bovine serum (FBS) to 450 mL of ice cold 1X HBSS; this makes 500 mL STOP solution. Keep the STOP solution at 4 &#176;C.</li>
	<li>Prepare collagenase P solution (must be made fresh within 1 h of being used) by adding 1 mg/mL of collagenase P to ice cold 1X HBSS; use 6 mL/mouse.
	<ol>
		<li>Add 0.05% (w/v) bovine serum albumin (BSA) to collagenase P solution (this provides nutrients to the isolated islets). For example, use 3 mg BSA in 6 mL collagenase P solution. Keep on ice.</li>
		<li>Calculate and prepare the amount of collagenase P needed for all mice in one 50 mL tube.</li>
	</ol>
	</li>
	<li>Prepare complete RPMI 1640 medium by adding 10% FBS, 100 U/mL penicillin, 100 &#181;g/mL streptomycin, INS-1 cell supplement (10 mM HEPES, 2 mM L-glutamine, 1 mM sodium pyruvate, and 0.05 mM 2-mercaptoethanol) to 500 mL RPMI 1640 media containing 5.5&#160;mM glucose to be used for overnight culture and incubation.</li>
</ol>
2. Preparation
<ol>
	<li>Fill three 50 mL tubes of 25 mL RNase inhibiting solution, 70% ethanol or distilled H2O. These solutions will be used for cleaning surgical tools prior and during the procedure.</li>
	<li>Soak the tips of the tools in RNase inhibiting solution for 30 min before starting the protocol; this eliminates any potential RNase on the tools.</li>
	<li>Pre-cut absorbent pads to 6 in x 6 in size for use during surgery.</li>
	<li>Prepare 1X HBSS solution in advance and store at 4 &#176;C. Prepare STOP solution prior to surgery. Store at 4 &#176;C.</li>
	<li>Prepare collagenase P solution immediately prior to surgery and store on ice. 
	NOTE: This should be used within 2 h of preparation.</li>
	<li>Label 50 mL tubes for digestion and purification; prepare 2 tubes for each mouse, one for digestion and the other for islet purification. Ensure that the animal ID is on both tubes.</li>
	<li>Add 3 mL of collagenase P solution into the first 50 mL tube. The remaining 3 mL of collagenase P will be injected.</li>
	<li>Draw the remaining 3 mL of collagenase solution into a 3 mL syringe mounted with 30 G &#189; in needle. Place the syringe on ice.</li>
</ol>
3. Procedure
<ol>
	<li>Remove all the tools from RNase inhibiting solution, then dip them first in the tube with 70% ethanol, then in the tube containing distilled H2O, then air-dry on clean paper towel.</li>
	<li>Place the mouse in a chamber containing 0.5 mL of isoflurane until mouse is deeply anaesthetized.</li>
	<li>Remove mouse from the chamber and check the state of anesthesia by pinching a foot pad with forceps. Deep anesthetization is based on the observation that breathing become steadily slow and mouse is unreactive to foot pinching. After confirming that the mouse is deeply anaesthetized, euthanize the mouse with cervical dislocation, and then place the mouse on the absorbent pad.
	<ol>
		<li>Place anaesthetized mouse on its stomach, applying pressure to the neck and dislocating the spinal column from the brain by pulling tail.</li>
	</ol>
	</li>
	<li>Tape the limbs of the mouse in supine position to the absorbent pad, spray the body with 70% ethanol, and wipe excess off the excess ethanol.</li>
	<li>Use cover glass forceps and curved surgical scissors to make incisions. First make a horizontal incision on the skin of the abdominal area (~3 cm), pull the skin wide open to expose the abdominal wall. Then make a vertical incision (~3&#8211;4cm) on the abdominal peritoneum to fully expose the pancreas in abdominal cavity (Figure 3).</li>
	<li>Push the lobes of the liver superiorly to expose the bile duct, it will appear as a pale pink tube (Figure 3).</li>
	<li>Carefully move the intestines from the right lumbar/iliac region of the abdominal cavity to the right, exposing the bile duct and hepatic artery (Figure 3).</li>
	<li>Carefully clamp the common bile duct using the Schwartz micro serrefines (Figure 1) as close to the liver as possible.</li>
	<li>Identify the ampulla of Vater, which is located at the duodenal papilla, formed by the union of the pancreatic duct and the common bile duct. The ampulla of Vater appears swollen when viewed under a dissection microscope which is the entry point to the common bile duct (Figure 4). 
	NOTE: Adjusting intensity/angle of light of the dissection microscope can make it easier to locate.</li>
	<li>Insert the syringe with 3 mL of the collagenase P solution into the ampulla of Vater. Push the needle into the duct for about 1/4 of the length of the common bile duct (ampulla leads into duct) as shown in Figure 5.</li>
	<li>Once the needle is in the ampulla, ensure that the orientation of the needle is such that it is parallel with the duct.</li>
	<li>Stabilize the needle by clamping with micro Adson forceps to prevent it from puncturing the duct (Figure 5).</li>
	<li>Slowly and steadily inject 3 mL of the collagenase P solution from the syringe into the common bile duct (enough to feel resistance) as shown in Figure 6. The goal is to create backflow pressure to force the collagenase to enter the pancreatic duct. Injection is considered successful if the head, neck, body and tail region of the pancreas are all fully inflated. 
	NOTE: Islet yield will be low if either the pancreas is not fully inflated, or the splenic area is not fully inflated. The splenic area contains the highest number of islets6. Inflation can be confirmed by the appearance of open spaces between pancreatic tissue that are filled with solution.</li>
	<li>Carefully dissect out the inflated pancreas and place it in a 50 mL digestion tube containing 3 mL of ice-cold collagenase P solution.
	<ol>
		<li>Remove the pancreas using 2 forceps (curved and Micro Adson; See Figure 1): (starting from the spleen, pull the pancreas away from spleen and continue removing from the stomach and along the duodenum. 
		NOTE: No incisions required.</li>
		<li>Chop pancreas for 3&#8211;5 s in the digestion tube with 3 mL of ice-cold collagenase P solution using fine surgical scissors (Figure 7A).</li>
	</ol>
	</li>
	<li>Secure the tube to a rack in 37 &#176;C water bath and shake at 100&#8211;120 rpm for approximately 12&#8211;13 min.</li>
	<li>After incubation, gently shake the tubes by hand to disrupt the tissue until the collagenase P digestion solution becomes homogenous (Figure 7B). Homogeneity is confirmed by a sand-like appearance of fine particles of pancreas. About 30 s of gentle hand-shaking is usually enough. Hold the tube up to light to examine if the tissue is well homogenized; shake for another ~15 s if needed.</li>
	<li>Once digested, immediately place the tubes on ice and add 40 mL of ice-cold STOP solution to terminate the enzymatic digestion. 
	NOTE: At this point digestion tubes can be left on ice up to 2 h, if working on multiple mice.</li>
	<li>Centrifuge the tube in a swinging-bucket centrifuge at 300 x g for 30 s (temperature of centrifuge is flexible). 
	NOTE: Use a swinging-bucket centrifuge so that the tissue pellet is formed at the bottom of the 50 mL tube and not on the wall of the tube; this is critical for better islet yield.</li>
	<li>Decant and repeat the centrifugation with STOP solution 2 more times, decanting the solution after each spin. Use 20 mL of STOP solution for each subsequent wash.
	<ol>
		<li>Before each spin, disrupt the pellet by gently shaking the tissue pellet in the 50 mL tube in 20 mL STOP solution.</li>
	</ol>
	</li>
	<li>Re-suspend the tissue pellet with 40 mL of ice cold HBSS and centrifuge at 300 x g for 30 s.</li>
	<li>Decant and repeat the centrifugation using a swinging-bucket centrifuge with HBSS solution two more times, decanting the solution after each spin. Use 20 mL of HBSS for each wash.
	<ol>
		<li>Before each spin, disrupt the pellet, to detach it from the bottom of the tube by gently shaking the tube containing 20 mL HBSS solution.</li>
	</ol>
	</li>
	<li>After the last centrifugation remove all HBSS.</li>
	<li>Then add 5 mL of room temperature density gradient to the 50 mL tube containing the pellet. Vortex briefly at low speed until homogenized.</li>
	<li>Add another 5 mL of the room temperature density gradient to the 50 mL tube. Do not vortex/mix. 
	NOTE: It is critical to remain steady and still so as to allow better gradient to form without disruption.</li>
	<li>Pipette 10 mL of room temperature HBSS buffer into the tube (containing the density gradient), drop-by-drop gently and slowly to allow a gradient to form. Use a pipette gun with a 10 mL pipette to add HBSS dropwise.</li>
	<li>Using a swinging-bucket centrifuge, spin tubes at 1700 x g for 15 min. Make sure to change the speed of both acceleration/deceleration to the lowest setting to maintain the gradient (Figure 7C).</li>
	<li>After the spin, carefully remove the tubes without disturbing the gradient. Using a pipette gun pre-wetted with cold HBSS (pipette HBSS up and down), pipette out the layer of islets (5&#8211;10 mL) formed between the density gradient and HBSS into the new 50 mL islet collection tube. 
	NOTE: It is helpful to wet the pipette with cold HBSS prior to pipetting the islets to prevent the islets from sticking to the inner walls of the pipette.
	<ol>
		<li>In case the separation is incomplete, islets would be visible in the density gradient layer, pipette out the entire 10 mL of the density gradient (bottom layer) along with the islet layer formed at the interface (only to leave about 8&#8211;10 mL of the HBSS top layer behind). 
		NOTE: Collecting both the islet layer and the density gradient layer (bottom layer) can result in the collection of debris which may lengthen the islet picking time, but no other steps will be altered. Collecting both these layers is not necessary when islet layer is well formed.</li>
	</ol>
	</li>
	<li>Add 20 mL of ice cold HBSS to the new 50 mL tube containing islets, then centrifuge at 350 x g for 3 min in a swinging-bucket centrifuge.</li>
	<li>After the spin, carefully pipette (do not decant) out the supernatant (leave ~3 mL at the bottom) without disturbing the pellet containing the islets at the bottom. Discard the supernatant.</li>
	<li>Repeat washing and centrifuging at least 3 times. Add 20 mL of HBSS each time, and be sure to suspend the pellet before each spin.</li>
	<li>Warm the RPMI-1640 complete media bottle in a water bath at 37 &#176;C prior to use. After the last centrifugation, remove all of the HBSS and add 4 mL of previously prepared complete RPMI-1640 media (containing FBS, INS-1 cell supplement and penicillin/streptomycin) to the pellet.</li>
	<li>Dislodge the pellet by gently swirling the tube and immediately pour the RPMI-1640 media into a 100 mm Petri dish. Add another 5 mL of RPMI-1640 media to the tube and gently swirl it to wash off any remaining islets, then also pour the media into the same Petri dish.
	<ol>
		<li>Under a dissection microscope, pick healthy islets from the Petri dish using a 20 &#181;L pipette, and put them in a new Petri dish containing 10 mL of complete RPMI 1640 media. When viewed under a dissection microscope, islets should appear spherical/oblong and golden-brown color with a smooth surface compared to the relatively transparent, wispy exocrine tissue. 
		NOTE: Magnification of dissection microscope is usually set at 12.5&#8211;16x. Islet yield will vary depending on various factors including strain, age and sex of mouse. This protocol usually yields 250&#8211;350 healthy islets from healthy C57BL/6J mouse age 4&#8211;10 months old.</li>
	</ol>
	</li>
	<li>Incubate the islets in a sterile incubator at 37 &#176;C with 5% CO2 infusion and 95% humidified air overnight for experiments the next day, or freeze the islets for desired analysis at a later time.
	<ol>
		<li>Once islets are frozen, they cannot be used for secretion assays, only RNA or protein quantification. To collect cells to freeze, place them in HBSS buffer, collect all islets in 200&#8211;500 &#181;L of buffer, transfer to 1.5 mL tube, centrifuge 350 x g for 1&#8211;2 min, remove the supernatant leaving no more than 30&#8211;40 &#181;L solution, place in -20 &#176;C for short term storage (several days) or -80 &#176;C for long term storage.</li>
	</ol>
	</li>
</ol>

<ol>
	<li>Carter, J. D., Dula, S. B., Corbin, K. L., Wu, R., Nunemaker, C. S. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=A+practical+guide+to+rodent+islet+isolation+and+assessment.">A practical guide to rodent islet isolation and assessment.</a> Biological Procedures Online. 11, 3-31 (2009).</li><li>Gotoh, M., Maki, T., Kiyoizumi, T., Satomi, S., Monaco, A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=An+improved+method+for+isolation+of+mouse+pancreatic+islets.">An improved method for isolation of mouse pancreatic islets.</a> Transplantation. 40 (4), 437-438 (1985).</li><li>O'Dowd, J. F. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=The+isolation+and+purification+of+rodent+pancreatic+islets+of+Langerhans.">The isolation and purification of rodent pancreatic islets of Langerhans.</a> Methods in Molecular Biology. 560, 37-42 (2009).</li><li>Do, O. H., Low, J. T., Thorn, P. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Lepr(db)+mouse+model+of+type+2+diabetes:+pancreatic+islet+isolation+and+live-cell+2-photon+imaging+of+intact+islets.">Lepr(db) mouse model of type 2 diabetes: pancreatic islet isolation and live-cell 2-photon imaging of intact islets.</a> Journal of Visualized Experiments : JoVE. (99), e52632 (2015).</li><li>Stull, N. D., Breite, A., McCarthy, R., Tersey, S. A., Mirmira, R. G. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Mouse+islet+of+Langerhans+isolation+using+a+combination+of+purified+collagenase+and+neutral+protease.">Mouse islet of Langerhans isolation using a combination of purified collagenase and neutral protease.</a> Journal of Visualized Experiments : JoVE. (67), (2012).</li><li>Wang, X. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Regional+Differences+in+Islet+Distribution+in+the+Human+Pancreas+-+Preferential+Beta-Cell+Loss+in+the+Head+Region+in+Patients+with+Type+2+Diabetes.">Regional Differences in Islet Distribution in the Human Pancreas - Preferential Beta-Cell Loss in the Head Region in Patients with Type 2 Diabetes.</a> PLOS ONE. 8, (2013).</li><li>Li, D. S., Yuan, Y. H., Tu, H. J., Liang, Q. L., Dai, L. J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=A+protocol+for+islet+isolation+from+mouse+pancreas.">A protocol for islet isolation from mouse pancreas.</a> Nature Protocols. 4 (11), 1649-1652 (2009).</li><li>Neuman, J. C., Truchan, N. A., Joseph, J. W., Kimple, M. E. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=A+method+for+mouse+pancreatic+islet+isolation+and+intracellular+cAMP+determination.">A method for mouse pancreatic islet isolation and intracellular cAMP determination.</a> Journal of Visualized Experiments : JoVE. (88), e50374 (2014).</li><li>Scharp, D. W., Lacy, P. E., Finke, E., Olack, B. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Low-temperature+culture+of+human+islets+isolated+by+the+distention+method+and+purified+with+Ficoll+or+Percoll+gradients.">Low-temperature culture of human islets isolated by the distention method and purified with Ficoll or Percoll gradients.</a> Surgery. 107 (5), e50374 (1987).</li><li>Salvalaggio, P. R. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Islet+filtration:+a+simple+and+rapid+new+purification+procedure+that+avoids+ficoll+and+improves+islet+mass+and+function.">Islet filtration: a simple and rapid new purification procedure that avoids ficoll and improves islet mass and function.</a> Transplantation. 74 (66), 877-879 (2002).</li><li>Saliba, Y., Bakhos, J. J., Itani, T., Fares, N. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=An+optimized+protocol+for+purification+of+functional+islets+of+Langerhans.">An optimized protocol for purification of functional islets of Langerhans.</a> Laboratory Investigation. 97 (1), 70-83 (2017).</li><li>Pradhan, 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=Obestatin+stimulates+glucose-induced+insulin+secretion+through+ghrelin+receptor+GHS-R.">Obestatin stimulates glucose-induced insulin secretion through ghrelin receptor GHS-R.</a> Scientific Reports. 7 (1), 979 (2017).</li><li>Shapiro, A. M. J., Hao, E., Rajotte, R. V., Kneteman, N. M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=High+yield+of+rodent+islets+with+intraductal+collagenase+and+stationary+digestion--a+comparison+with+standard+technique.">High yield of rodent islets with intraductal collagenase and stationary digestion--a comparison with standard technique.</a> Cell Transplantation. 5 (6), 631-638 (1996).</li></ol>

The authors have nothing to disclose.

This protocol includes collagenase perfusion and digestion, followed by purification of islets. The most critical steps of this protocol are effective injection and complete perfusion of the pancreas1,4,7. The delivery method of this protocol allows the enzyme to traverse the anatomical routes to better digest the exocrine tissue surrounding the islets1. In addition, this technique is well suited for complete digestion of the splenic region, which has the highest concentration of islets4,6. This protocol, with well-controlled digestion time and carefully executed purification steps, can produce 250&ndash;350 healthy islets. The islets isolated from this protocol have been used successfully to study glucose-stimulated insulin secretion ex vivo12. From our experience, insulin secretion increased 4-fold upon high glucose stimulation (22.2 mM) compared to baseline (3.3 mM) after overnight incubation in 5.5 mM glucose-containing RPMI-1640 complete media. The survivability/functionality of the islets under prolonged incubation (2&ndash;7 days) has not been tested.
Even though the presented protocol includes detailed notes and visual demonstrations, some adjustments are needed to achieve the optimal conditions for high yield and high-quality islets. Two most common problems that may impede the success are improper cannulation of the ampulla of Vater or accidental puncture of the duct. To avoid these, one should ensure that the site of penetration is precisely where the ampulla meets with the duodenum. This area is bigger and relatively easy to identify, which allows for multiple punctures without seriously compromising the integrity of the duct. Once within the ampulla, the orientation of the needle should be parallel with the duct rather than angled. At this point, push the needle into the duct for about 1/4 of the duct&rsquo;s length, and then stabilize the needle with forceps while slowly injecting collagenase; this will help to prevent the needle from bending under the pressure and accidentally puncturing the duct. Other problems may include over- or under-digestion of the pancreas; this may require modification based on age, strain and sex of the mice. Damaged islets due to over-digestion (enzymatic and mechanical) or prolonged exposure to the density gradient may occur. These are common problems that exist for similar methods; some minor adjustments should yield significant improvements. A suggestion when dealing with these types of issues is to choose one variable to modify at a time (e.g., time of digestion or concentration of collagenase).
The main advantage of this protocol is the route of enzyme delivery: having collagenase P to directly digest the exocrine pancreas using an easier anatomical route which increases digestion efficiency1. This method has been reported to yield a 50% increase in number of islets compared to the method of excising the pancreas, chopping it, and exposing it to collagenase13. This protocol only requires the use of a single density gradient, making it significantly less labor-intensive and more cost-effective, as compared to other methods which require the preparation of multiple gradients at different densities, or the complex Percoll method that requires additional time1,8,11. The gradient method employed in this protocol has also be used in islet isolation by others4. This method of islet isolation provides the scientist with an improved tool for studying pancreatic islets. Future applications of this protocol include alteration to enhance the efficacy when dealing with diabetic mice. As Do et al. have observed, diabetic mice, depending on glucose levels, yield fewer islets (less than 100), with reduced size and appearance of islets4. We have observed this phenomenon and believe that diabetic islets are more vulnerable to enzymatic and mechanical digestion which require special care. Additionally, islet density may alter its appearance in the density gradient, further optimization of the protocol would help to increase the yield of diabetic islets.

There are two common methods in the literature for pancreatic islet isolation. One requires excising the pancreas and dicing it into small pieces using surgical scissors, and then digesting it in a collagenase solution1,2,3. Another more precise method is to use the network of ducts present in the pancreas to introduce digestive enzyme. The following sites have been used for digestive enzyme injection: the junction of the bile and cystic duct, the gallbladder into the common bile duct, or the common bile duct itself1,4,5. It is known that islets are not evenly distributed in the pancreas; the splenic region contains the most islets6. While the second method using anatomical routes to deliver digestive enzymes allows for a more complete perfusion of the pancreas, including the splenic region, this procedure often requires clamping or suturing of the ampulla of Vater that is technically challenging. In terms of islet purification, multiple density gradients, as well as cell strainers and magnetic retraction have been used to purify the islets3,7. The utilization of these gradients can be time consuming and the Ficoll gradients can result in toxic damage of islets8.
The current protocol is built on the method described by Li et al.7, with additional modifications added based on the experience of ourselves and others1,4. The most critical steps of our protocol are clamping of the common bile duct near the liver end, injecting collagenase P via the ampulla of Vater to digest the exocrine tissue, and then using a shaking water bath to expedite the digestion mechanically1,4,7. Subsequently, a 'STOP' solution is applied to inhibit further digestion of the islets; HBSS is used to wash off the remaining collagenase P and STOP solution. When the Ficoll method was used to purify human islets, yield was reported to be twice the islets with greater functional capability (e.g., insulin secretion) as compared to the use of Percoll gradients9. However, studies have questioned the use of Ficoll gradient due to its toxic effect on the islets1,10. It has been reported that the Histopaque gradient provides optimal purification kinetics for mouse islet isolation, which produces good yield of high quality islets with simpler steps and lower cost1. In our protocol, Histopaque-1077 is used to purify islets from other residual tissue8,11. The harvested islets can be cultured in complete RPMI-1640 media, or directly utilized in RNA/protein quantitation.
Our protocol, using a combination of collagenase P digestion and a single gradient purification step, is simpler than other published protocols. Our method does not require demanding surgical procedures and has just a few simple steps. More importantly, this protocol consistently produces a good yield of high quality functional islets (250-350/mouse) as we reported12.

<table>
	<tbody>
		<tr>
			<td>3 mL syringe</td>
			<td>BD</td>
			<td>309657</td>
			<td>Hoding collagenase P</td>
		</tr>
		<tr>
			<td>Coverglass forceps</td>
			<td>VWR</td>
			<td>82027-396</td>
			<td>Holding skin of mouse to aid incision procedure</td>
		</tr>
		<tr>
			<td>Curved forceps</td>
			<td>Sigma-Aldrich</td>
			<td>Z168696</td>
			<td>Holding tissues during pancreas removal</td>
		</tr>
		<tr>
			<td>Isoflurane</td>
			<td>Piramal</td>
			<td>B13B16A</td>
			<td>To anaesthetize mice prior surgery</td>
		</tr>
		<tr>
			<td>100 mm petri dishes</td>
			<td>VWR</td>
			<td>30-2041</td>
			<td>Used for islet culture</td>
		</tr>
		<tr>
			<td>30 G. &#189; inch needle</td>
			<td>BD</td>
			<td>305106</td>
			<td>For penetration of Ampulla of vater to deliver Collagenase P - this guage is used as it fits well in most CBDs</td>
		</tr>
		<tr>
			<td>50ml tube</td>
			<td>VWR</td>
			<td>89039-658</td>
			<td>Holding digested pancreatic tissue, collagenase P, and purified islets</td>
		</tr>
		<tr>
			<td>Absorbent pads with waterproof moisture barrier</td>
			<td>VWR</td>
			<td>82020-845</td>
			<td>To absorb blood from syurgical procesdudes</td>
		</tr>
		<tr>
			<td>Centrifuge 5810R with swing bucket and deceleration capability</td>
			<td>Eppendorf</td>
			<td>5811FJ478114</td>
			<td>Use for pelleting tissues, pellet is formed at bottom of conical tube - swing bucket centrifuge is needed. Also the decelaration feature is important to form the gradient layers.</td>
		</tr>
		<tr>
			<td>Collagenase P- 1g</td>
			<td>Roche Diagnostics</td>
			<td>11249002001</td>
			<td>For digestion of exocrine pancreas</td>
		</tr>
		<tr>
			<td>Curved surgical scissors</td>
			<td>Fisher-Scientific</td>
			<td>13-804-21</td>
			<td>For cutting open mouse abdomen</td>
		</tr>
		<tr>
			<td>Dissection microscope</td>
			<td>Olympus</td>
			<td>SZX16</td>
			<td>Used for identification of key anatomical structures to accurately deliver collagenase into pancreas</td>
		</tr>
		<tr>
			<td>Hank&#39;s Balanced Salt Solution 10x</td>
			<td>Corning</td>
			<td>20-023-CV</td>
			<td>Washing cells</td>
		</tr>
		<tr>
			<td>Histopaque-1077</td>
			<td>Sigma</td>
			<td>RNBF5100</td>
			<td>For gradient formation</td>
		</tr>
		<tr>
			<td>Light source</td>
			<td>Leeds</td>
			<td>LR92240</td>
			<td>Enhancing visibility of microscope</td>
		</tr>
		<tr>
			<td>RNaseZap</td>
			<td>Fisher-Scientific</td>
			<td>AM9780</td>
			<td>For removing RNase</td>
		</tr>
		<tr>
			<td>RPMI-1640 Media w/o L-Glutamine</td>
			<td>Corning</td>
			<td>15-040-CV</td>
			<td>Culturing Islets</td>
		</tr>
		<tr>
			<td>Schwartz micro serrefines (Microvascular clamp)</td>
			<td>Fine Science Tools</td>
			<td>18052-01</td>
			<td>Clamping common bile duct and hepatic artery</td>
		</tr>
		<tr>
			<td>Shaking waterbath</td>
			<td>Boekel/Grant</td>
			<td>8R0534008</td>
			<td>Important for mechanical digestion of exocrine tissue</td>
		</tr>
		<tr>
			<td>Small surgical scissors</td>
			<td>VWR</td>
			<td>82027-578</td>
			<td>Cuttitng tissue that atached to pancreas</td>
		</tr>
	</tbody>
</table>

a simple high efficiency protocol for pancreatic islet isolation from mice

Pancreatic islets, also called the Islets of Langerhans, are a cluster of endocrine cells which produces hormones for glucose regulation and other important biological functions. The islets primarily consist of five types of hormone-secreting cells: &#945; cells secrete glucagon, &#946; cells secrete insulin, &#948; cells secrete somatostatin, &#949; cells secrete ghrelin, and PP cells secrete pancreatic polypeptide. Sixty to 80% of the cells in the islets are &#946; cells, which are the most important cell population to study insulin secretion. Pancreatic islets are a crucial model system to study ex vivo insulin secretion. Acquiring high quality islets is of great importance for diabetes research. Most islet isolation procedures require technically difficult to access site of collagenase injection, harsh and complex digestion procedures, and multiple density gradient purification steps. This paper features a simple high yield mouse islet isolation method with detailed descriptions and realistic demonstrations, showing the following specific steps: 1) injection of collagenase P at the ampulla of Vater, a small area joining the pancreatic duct and the common bile duct, 2) enzymatic digestion and mechanical separation of the exocrine pancreas, and 3) a single gradient purification step. The advantages of this method are the injection of digestive enzyme using the more accessible ampulla of Vater, more complete digestion using combination of enzymatic and mechanical approaches, and a simpler single gradient purification step. This protocol produces approximately 250&#8212;350 islets per mouse; and islets are suitable for various ex vivo studies. Possible caveats of this procedure are potentially damaged islets due to enzymatic digestion and/or prolonged gradient incubation, all of which can be largely avoided by careful ad justification of incubation time.

Proper completion of this procedure requires some understanding of mouse anatomy in the abdominal cavity. This allows for proper identification of the ampulla of Vater and clamping of the common bile duct. The entire procedure normally takes 1&#8211;2 h. It is more efficient to isolate islets from 4&#8211;6 mice at the same time, so several samples can be centrifuged together. The time for islet-picking varies, depending on the number of islets and the efficiency of digestion; it may take roughly an hour to pick 250&#8211;350 islets from 1 mouse.
In this paper, a number of very realistic images are included: Figure 3 shows the abdominal cavity of the mouse, exposing the common bile duct and hepatic artery. Figure 4 shows the entire length of common bile duct, which appears to be a lighter color, as well as the ampulla of Vater, which is bigger and shinier near the juncture (where the needle will be inserted) between the pancreas and duodenum. A clamp is placed at the common bile duct and hepatic artery bundle close to the liver to block off the flow of collagenase P into liver. Failure to clamp the bile duct correctly or tight enough will result in leakage and incomplete perfusion of the pancreas. Figure 5 shows the needle inserted at the ampulla of Vater into the common bile duct. Once the needle is in the common duct, forceps are used to stabilize the needle to prevent it from puncturing the duct while injecting. Once the injection begins, the pancreas will begin to swell from proximal end to distal end; the splenic region should begin to inflate after about 1 mL of collagenase injection. Backflow into the intestines can lead to an undesirable inflation of the duodenum; this can be remedied by readjusting the placement of the needle (pull it out a little, or reinsert slightly deeper) and by properly stabilizing the needle using forceps. The injection is considered a success if all regions of the pancreas are inflated (duodenal, gastric, and splenic lobes) as shown in Figure 6. Removal of the pancreas should begin from the splenic region. The inflated pancreas is chopped into chunks using fine surgical scissors (Figure 7A). After the 12&#8211;13 min digestion and mixing by hand-shaking, the tissue-containing suspension appears more homogeneous (Figure 7B). Subsequently, the islets are purified by the density gradient after centrifugation. Figure 7C shows that an islet suspension layer is formed between HBSS and the density gradient after centrifugation. Good/healthy islets appear as smooth round-shaped; bad/damaged islets show rough edges, and undigested exocrine tissue shows irregular shape and appears more translucent as shown in Figure 8.
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/57048/57048fig01.jpg" /> 
Figure 1: Surgical tools. 
Curved surgical scissors, cover glass forceps, micro Adson forceps, curved forceps, small surgical scissors, and Schwartz micro serrefines (microvascular clamp) are shown. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57048/57048fig01large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/57048/57048fig02.jpg" /> 
Figure 2: Schematic illustration of the protocol. 
The most critical steps of this procedure are the clamping of the common bile duct near the liver, and injecting collagenase P via the ampulla of Vater into common bile duct to digest the pancreas. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57048/57048fig02large.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/57048/57048fig03.jpg" /> 
Figure 3: Location of common bile duct. 
Forceps hold up the common bile duct and hepatic artery bundle. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57048/57048fig03large.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/57048/57048fig04.jpg" /> 
Figure 4: Illustration of common bile duct and ampulla of Vater. A clamp is placed on the common bile duct and hepatic artery bundle near the liver. The black arrows point to the ampulla of Vater where the needle will be inserted. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57048/57048fig04large.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/57048/57048fig05.jpg" /> 
Figure 5: Cannulation of common bile duct. 
After proper cannulation of the common bile duct, the ampulla of Vater is injected with trypan blue (for demonstration purpose only) to better emphasize the placement of the common bile duct. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57048/57048fig05large.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/57048/57048fig06.jpg" /> 
Figure 6: Fully inflated pancreas. 
The dotted line shows the boundary of the fully perfused pancreas. Forceps hold up the splenic region where islets are most concentrated. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57048/57048fig06large.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/57048/57048fig07.jpg" /> 
Figure 7: Islet isolation and purification steps. 
(A) Mechanically chopped tissue pieces of pancreas before digestion. (B) Digested pancreas&#8212;homogeneous tissue suspension of collagenase-perfused pancreas after 13 min of incubation in a shaking water bath at 37 &#176;C, followed by 30 s of mixing by hand. (C) Islet suspension layer is formed between the HBSS and the density gradient after centrifugation. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57048/57048fig07large.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/57048/57048fig08.jpg" /> 
Figure 8: Representative islet images from Fluorescence Cell-Imager. 
(A) Good islets, bad islets and exocrine tissue are seen. (B) A cluster of good islets is shown. (C) Panel shows undigested exocrine tissue attached to a good islet. Good/healthy islets show smooth round edges, indicated by the red letter &#8220;G&#8221;; bad/damaged islets show irregular shape and rough edges, and are indicated by blue letter &#8220;B&#8221;. Undigested exocrine tissues appear translucent, often attached to islets, and are indicated by green letter &#8220;E&#8221;. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57048/57048fig08large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>

Watch this Scientific Journal Video about A Simple High Efficiency Protocol for Pancreatic Islet Isolation from Mice at JoVE.com

A Simple High Efficiency Protocol for Pancreatic Islet Isolation from Mice

This islet isolation protocol described a novel route of collagenase injection to digest the exocrine tissue and a simplified gradient procedure to purify the islets from mice. It involves enzymatic digestion, gradient separation/purification, and islet hand-picking. Successful isolation can yield 250&#8211;350 high quality and fully functional islets per mouse.

Pancreatic islets, also called the Islets of Langerhans, are a cluster of endocrine cells which produces hormones for glucose regulation and other ...

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28.8K Views.  Texas A&M University. This islet isolation protocol described a novel route of collagenase injection to digest the exocrine tissue and a simplified gradient procedure to purify the islets from mice. It involves enzymatic digestion, gradient separation/purification, and islet hand-picking. Successful isolation can yield 250–350 high quality and fully functional islets per mouse.

Video: A Simple High Efficiency Protocol for Pancreatic Islet Isolation from Mice

Murine Pancreatic Islet Isolation

Neutrophil Isolation Protocol

Neutrophil polymorphonuclear granulocytes (PMN) are the most abundant leukocytes in humans and among the first cells to arrive on the site of inflammatory immune response. Due to their key role in inflammation, neutrophil functions such as locomotion, cytokine production, phagocytosis, and tumor cell combat are extensively studied. To characterize the specific functions of neutrophils, a clean, fast, and reliable method of separating them from other blood cells is desirable for in vitro studies, especially since neutrophils are short-lived and should be used within 2-4 hours of collection. Here, we demonstrate a standard density gradient separation method to isolate human neutrophils from whole blood using commercially available separation media that is a mixture of sodium metrizoate and Dextran 500. The procedure consists of layering whole blood over the density gradient medium, centrifugation, separation of neutrophil layer, and lysis of residual erythrocytes. Cells are then washed, counted, and resuspended in buffer to desired concentration. When performed correctly, this method has been shown to yield samples of >95% neutrophils with >95% viability.

Neutrophils are among the first cells to arrive on the site of inflammatory immune response, and their functions and mechanisms have been studied extensively in vitro. We demonstrate a standard density gradient separation method to isolate human neutrophils from whole blood using commercially available separation media.

Neutrophil polymorphonuclear granulocytes (PMN) are the most abundant leukocytes in humans and among the first cells to arrive on the site of inflammatory ...

Human Pancreatic Islet Isolation: Part I: Digestion and Collection of Pancreatic Tissue

Management of Type 1 diabetes is burdensome, both to the individual and society, costing over 100 billion dollars annually. Despite the widespread use of glucose monitoring and new insulin formulations, many individuals still develop devastating secondary complications. Pancreatic islet transplantation can restore near normal glucose control in diabetic patients 1, without the risk of serious hypoglycemic episodes that are associated with intensive insulin therapy. Providing sufficient islet mass is important for successful islet transplantation. However, donor characteristic, organ procurement and preservation affect the isolation outcome 2. At University of Illinois at Chicago (UIC) we have developed a successful isolation protocol with an improved purification gradient 3. The program started in January 2004, and more than 300 isolations were performed up to November 2008. The pancreata were sent in cold preservation solutions (UW, University of Wisconsin or HTK, Histidine-Tryptophan Ketoglutarate) 4-7 to the Cell Isolation Laboratory at UIC for islet isolation. Pancreatic islets were isolated using the UIC method, which is a modified version of the method originally described by Ricordi et al 8. Briefly, after cleaning the pancreas from the surrounding tissue, it was perfused with enzyme solution (Serva Collagenase + Neutral Protease or Sigma V enzyme). The distended pancreas was then transferred to the Ricordi digestion chamber, connected to a modified, closed circulation tubing system, and warmed up to 37&deg;C. During the digestion, the chamber was shaken gently. Samples were taken continuously to monitor the digestion progress. Once free islets were detected under the microscope, the digestion was stopped by flushing cold (4&deg;C) RPMI dilution solution (Mediatech, Herndon, VA) into the circulation system to dilute the enzyme. After being collected and washed in M199 media supplemented with human albumin, the tissue was sampled for pre-purification count and incubated with UW solution before purification. Purification process will be described in Part II: Purification and Culture of Human Islets.

Achieving high quality and appropriate quantity of human islets is one of the prominent prerequisites for successful islet transplantation. In this video, we describe step by step the procedures for human pancreatic islet isolation (part I: digestion and collection of pancreatic tissue) using a modified automated method.

Management of Type 1 diabetes is burdensome, both to the individual and society, costing over 100 billion dollars annually. Despite the widespread use of ...

Human Pancreatic Islet Isolation: Part II: Purification and Culture of Human Islets

Management of Type 1 diabetes is burdensome, both to the individual and society, costing over 100 billion dollars annually. Despite the widespread use of glucose monitoring and new insulin formulations, many individuals still develop devastating secondary complications. Pancreatic islet transplantation can restore near normal glucose control in diabetic patients 1, without the risk of serious hypoglycemic episodes that are associated with intensive insulin therapy. Providing sufficient islet mass is important for successful islet transplantation. However, donor characteristics, organ procurement and preservation affect the isolation outcome 2. At University of Illinois at Chicago (UIC) we developed a successful isolation protocol with an improved purification gradient 3. The program started in January 2004 and more than 300 isolations were performed up to November 2008. The pancreata were sent in cold preservation solutions (UW, University of Wisconsin or HTK, Histidine-Tryptophan Ketoglutarate) 4-7 to the Cell Isolation Laboratory at UIC for islet isolation. Pancreatic islets were isolated using the UIC method, which is a modified version of the method originally described by Ricordi et al 8. As described in Part I: Digestion and Collection of Pancreatic Tissue, human pancreas was trimmed, cannulated, perfused, and digested. After collection and at least 30 minutes of incubation in UW solution, the tissue was loaded in the cell separator (COBE 2991, Cobe, Lakewood, CO) for purification 3. Following purification, islet yield (expressed as islet equivalents, IEQ), tissue volume, and purity was determined according to standard methods 9. Isolated islets were cultured in CMRL-1066 media (Mediatech, Herndon, VA), supplemented with 1.5% human albumin, 0.1% insulin-transferrin-selenium (ITS), 1 ml of Ciprofloxacin, 5 ml o f 1M HEPES, and 14.5 ml of 7.5% Sodium Bicarbonate in T175 flasks at 37&deg;C overnight culture before islets were transplanted or used for research.

Achieving high quality and appropriate quantity of human islets is one of the prominent prerequisites for successful islet transplantation. In this video, we describe step by step the procedures for human pancreatic islet isolation (part II: purification and culture of human islets) using a modified automated method.

Isolation of Stem Cells from Human Pancreatic Cancer Xenografts

Cancer stem cells (CSCs) have been identified in a growing number of malignancies and are functionally defined by their ability to undergo self-renewal and produce differentiated progeny1. These properties allow CSCs to recapitulate the original tumor when injected into immunocompromised mice. CSCs within an epithelial malignancy were first described in breast cancer and found to display specific cell surface antigen expression (CD44+CD24low/-)2. Since then, CSCs have been identified in an increasing number of other human malignancies using CD44 and CD24 as well as a number of other surface antigens. Physiologic properties, including aldehyde dehydrogenase (ALDH) activity, have also been used to isolate CSCs from malignant tissues3-5.
Recently, we and others identified CSCs from pancreatic adenocarcinoma based on
ALDH activity and the expression of the cell surface antigens CD44 and CD24, and CD1336-8. These highly tumorigenic populations may or may not be overlapping and display other functions. We found that ALDH+ and CD44+CD24+ pancreatic CSCs are similarly tumorigenic, but ALDH+ cells are relatively more invasive8. In this protocol we describe a method to isolate viable pancreatic CSCs from low-passage human
xenografts9. Xenografted tumors are harvested from mice and made into a single-cell suspension. Tissue debris and dead cells are separated from live cells and then stained using antibodies against CD44 and CD24 and using the ALDEFLUOR reagent,
a fluorescent substrate of ALDH10. CSCs are then isolated by fluorescence activated cell sorting. Isolated CSCs can then be used for analytical or functional assays requiring viable cells.

Cancer stem cells (CSCs) have been identified in a number of malignancies. In this protocol we describe a flow cytometric method utilizing aldehyde dehydrogenase activity and CD44 and CD24 expression to isolate CSCs from human pancreatic adenocarcinoma xenografts. These viable cells can then be used in functional and analytical studies.

Cancer stem cells (CSCs) have been identified in a growing number of malignancies and are functionally defined by their ability to undergo self-renewal ...

A Simple Protocol for Extracting Hemocytes from Wild Caterpillars

Insect hemocytes (equivalent to mammalian white blood cells) play an important role in several physiological processes throughout an insect's life cycle 1. In larval stages of insects belonging to the orders of Lepidoptera (moths and butterflies) and Diptera (true flies), hemocytes are formed from the lymph gland (a specialized hematopoietic organ) or embryonic cells and can be carried through to the adult stage. Embryonic hemocytes are involved in cell migration during development and chemotaxis regulation during inflammation. They also take part in cell apoptosis and are essential for embryogenesis 2. Hemocytes mediate the cellular arm of the insect innate immune response that includes several functions, such as cell spreading, cell aggregation, formation of nodules, phagocytosis and encapsulation of foreign invaders 3. They are also responsible for orchestrating specific insect humoral defenses during infection, such as the production of antimicrobial peptides and other effector molecules 4, 5. Hemocyte morphology and function have mainly been studied in genetic or physiological insect models, including the fruit fly, Drosophila melanogaster 6, 7, the mosquitoes Aedes aegypti and Anopheles gambiae 8, 9 and the tobacco hornworm, Manduca sexta 10, 11. However, little information currently exists about the diversity, classification, morphology and function of hemocytes in non-model insect species, especially those collected from the wild 12.
Here we describe a simple and efficient protocol for extracting hemocytes from wild caterpillars. We use penultimate instar Lithacodes fasciola (yellow-shouldered slug moth) (Figure 1) and Euclea delphinii (spiny oak slug) caterpillars (Lepidoptera: Limacodidae) and show that sufficient volumes of hemolymph (insect blood) can be isolated and hemocyte numbers counted from individual larvae. This method can be used to efficiently study hemocyte types in these species as well as in other related lepidopteran caterpillars harvested from the field, or it can be readily combined with immunological assays designed to investigate hemocyte function following infection with microbial or parasitic organisms 13.

Insect hemocytes carry out many important functions, both immune and non-immune, throughout all stages of insect development. Our present knowledge of hemocyte types and function comes from studies on insect genetic models. Here, we present a method for extracting, quantifying and visualizing hemocytes from wild caterpillars.

Insect hemocytes (equivalent to mammalian white blood cells) play an important role in several physiological processes throughout an insect's life cycle ...

A Method for Mouse Pancreatic Islet Isolation and Intracellular cAMP Determination

Uncontrolled glycemia is a hallmark of diabetes mellitus and promotes morbidities like neuropathy, nephropathy, and retinopathy. With the increasing prevalence of diabetes, both immune-mediated type 1 and obesity-linked type 2, studies aimed at delineating diabetes pathophysiology and therapeutic mechanisms are of critical importance. The &#946;-cells of the pancreatic islets of Langerhans are responsible for appropriately secreting insulin in response to elevated blood glucose concentrations. In addition to glucose and other nutrients, the &#946;-cells are also stimulated by specific hormones, termed incretins, which are secreted from the gut in response to a meal and act on &#946;-cell receptors that increase the production of intracellular cyclic adenosine monophosphate (cAMP). Decreased &#946;-cell function, mass, and incretin responsiveness are well-understood to contribute to the pathophysiology of type 2 diabetes, and are also being increasingly linked with type 1 diabetes. The present mouse islet isolation and cAMP determination protocol can be a tool to help delineate mechanisms promoting disease progression and therapeutic interventions, particularly those that are mediated by the incretin receptors or related receptors that act through modulation of intracellular cAMP production. While only cAMP measurements will be described, the described islet isolation protocol creates a clean preparation that also allows for many other downstream applications, including glucose stimulated insulin secretion, [3H]-thymidine incorporation, protein abundance, and mRNA expression.

Assaying in vitro &#946;-cell function using isolated mouse islets of Langerhans is an important component in the study of diabetes pathophysiology and therapeutics. While many&#160;downstream applications are available, this protocol specifically describes the measurement of intracellular cyclic adenosine monophosphate (cAMP) as an essential parameter determining &#946;-cell function.

Uncontrolled glycemia is a hallmark of diabetes mellitus and promotes morbidities like neuropathy, nephropathy, and retinopathy. With the increasing ...

Pancreatic Islet Embedding for Paraffin Sections

Experiments using isolated pancreatic islets are important for diabetes research, but islets are expensive and of limited abundance. Islets contain a mixed cell population in a structured architecture that impacts function, and human islets are widely variable in cell type composition. Current frequently used methods to study cultured islets include molecular studies performed on whole islets, lumping disparate islet cell types together, or microscopy or molecular studies on dispersed islet cells, disrupting islet architecture. For in vivo islet studies, paraffin-embedded pancreas sectioning is a powerful technique to assess cell-specific outcomes in the native pancreatic environment. Studying post-culture islets by paraffin sectioning would offer several advantages: detection of multiple outcomes on the same islets (potentially even the exact-same islets, using serial sections), cell-type-specific measurements, and maintaining native islet cell-cell and cell-substratum interactions both during experimental exposure and for analysis. However, existing techniques for embedding isolated islets post-culture are inefficient, time consuming, prone to loss of material, and generally produce sections with inadequate islet numbers to be useful for quantifying outcomes. Clinical pathology laboratory cell block preparation facilities are inaccessible and impractical for basic research laboratories. We have developed an improved, simplified bench-top method that generates sections with robust yield and distribution of islets. Fixed islets are resuspended in warm histological agarose gel and pipetted into a flat disc on a standard glass slide, such that the islets are distributed in a plane. After standard dehydration and embedding, multiple (10+) 4 - 5 &#181;m sections can be cut from the same islet block. Using this method, histological&#160;and immunofluorescent analyses can be performed on mouse, rat, and human islets. This is an effective, inexpensive, time-saving approach to assess cell-type-specific, intact-architecture outcomes from cultured islets.

Ex vivo pancreatic islet studies are important for diabetes research. Existing techniques to study cultured islets in their native 3-dimensional architecture are time consuming, inefficient, and infrequently used. This work describes a new, simple, and efficient method for generating high-quality paraffin sections of whole cultured islets.

Experiments using isolated pancreatic islets are important for diabetes research, but islets are expensive and of limited abundance. Islets contain a ...

Imaging Calcium Dynamics in Subpopulations of Mouse Pancreatic Islet Cells

Pancreatic islet hormones regulate blood glucose homeostasis. Changes in blood glucose induce oscillations of cytosolic calcium in pancreatic islet cells that trigger secretion of three main hormones: insulin (from &#946;-cells), glucagon (&#945;-cells) and somatostatin (&#948;-cells). &#946;-Cells, which make up the majority of islet cells and are electrically coupled to each other, respond to the glucose stimulus as one single entity. The excitability of the minor subpopulations, &#945;-cells and &#948;-cells (making up around 20% (30%) and 4% (10%) of the total rodent1 (human2) islet cell numbers, respectively) is less predictable and is therefore of special interest.
Calcium sensors are delivered into the peripheral layer of cells within the isolated islet. The islet or a group of islets is then immobilized and imaged using a fluorescence microscope. The choice of the imaging mode is between higher throughput (wide-field) and better spatial resolution (confocal). Conventionally, laser scanning confocal microscopy is used for imaging tissue, as it provides the best separation of the signal between the neighboring cells. A wide-field system can be utilized too, if the contaminating signal from the dominating population of &#946;-cells is minimized.
Once calcium dynamics in response to specific stimuli have been recorded, data are expressed in numerical form as fluorescence intensity vs. time, normalized to the initial fluorescence and baseline-corrected, to remove the effects linked to bleaching of the fluorophore. Changes in the spike frequency or partial area under the curve (pAUC) are computed vs. time, to quantify the observed effects. pAUC is more sensitive and quite robust whereas spiking frequency provides more information on the mechanism of calcium increase.
Minor cell subpopulations can be identified using functional responses to marker compounds, such as adrenaline and ghrelin, that induce changes in cytosolic calcium in a specific populations of islet cells.

Here, we present a protocol for imaging and quantifying calcium dynamics in heterogeneous cell populations, such as pancreatic islet cells. Fluorescent reporters are delivered into the peripheral layer of cells within the islet, which is then immobilized and imaged, and per-cell analysis of the dynamics of fluorescence intensity is performed.

Pancreatic islet hormones regulate blood glucose homeostasis. Changes in blood glucose induce oscillations of cytosolic calcium in pancreatic islet cells ...

An Antegrade Perfusion Method for Cardiomyocyte Isolation from Mice

In basic research using mouse heart, isolating viable individual cardiomyocytes is a crucial technical step to overcome. Traditionally, isolating cardiomyocytes from rabbits, guinea pigs or rats has been performed via retrograde perfusion of the heart with enzymes using a Langendorff apparatus. However, a high degree of skill is required when this method is used with a small mouse heart. An antegrade perfusion method that does not use a Langendorff apparatus was recently reported for the isolation of mouse cardiomyocytes. We herein report a complete protocol for the improved antegrade perfusion of the excised heart to isolate individual heart cells from adult mice (8 - 108 weeks old). Antegrade perfusion is performed by injecting perfusate near the apex of the left ventricle of the excised heart, the aorta of which was clamped, using an infusion pump. All procedures are carried out on a pre-warmed heater mat under a microscope, which allows for the injection and perfusion processes to be monitored. The results suggest that ventricular and atrial myocytes, and fibroblasts can be well isolated from a single adult mouse simultaneously.

We developed a simple method for isolating high quality individual mouse heart cells by the antegrade perfusion technique. This method is Langendorff-free and useful for isolating ventricular and atrial myocytes or interstitial cells, such as cardiac fibroblasts or progenitors.