The authors would like to thank Curtis Vande Stouwe for his technical assistance. The research underlying development of the protocols was supported by grants from the National Institute on Alcohol Abuse and Alcoholism (5P60AA009803-25, 5T32AA007577-20 and 1F31AA028459-01).

All obtained tissues and procedures were approved by the Institutional Animal Care and Use Committee at the Louisiana State University Health Sciences Center and were performed in accordance with the guidelines of the National Institute of Health (NIH publication No. 85-12, revised 1996).
1. Preparation of buffers and solutions
<ol>
	<li>Prepare sterile 5-phosphate-buffered saline wash buffer (5-PBS) solution by adding 5% penicillin/streptomycin (pen/strep) and 0.25 &#956;g/mL of fungal inhibitor to 1x PBS. Prepare sterile 2-PBS wash buffer (2-PBS) solution by adding 2% pen/strep and 0.25 &#956;g/mL of fungal inhibitor in 1x PBS. Wash buffers can be stored at 4 &#176;C for future use and must be used within 4 weeks. 
	NOTE: 5-PBS buffer is used for adipose tissue collection and initial washing to minimize possible contamination as tissue samples obtained at necropsy are collected in a non-sterile environment.</li>
	<li>Prepare sterile collagenase buffer (CB) by combining 0.075% collagenase Type I (125 units/mg activity), 2% pen/strep, and 0.25 &#956;g/mL of fungal inhibitor in Hank&#8217;s balanced salt solution (HBSS) with 1% Bovine Serum Albumin. CB must be used within 1 h.</li>
	<li>Prepare sterile ADSC growth medium using &#945;-MEM buffer. Combine 100 mL of fetal bovine serum (FBS), 5 mL of 200 mM L-glutamine solution, 500 &#956;L of 0.25 &#956;g/mL of fungal inhibitor and 10 mL of pen/strep solution in 394 mL of &#945;-MEM buffer. ADSC growth medium can be stored at 4 &#176;C and must be used within 4 weeks. 
	NOTE: Heat inactivation of FBS is not necessary.</li>
	<li>Prepare sterile ADSC differentiation medium by combining ADSC growth medium as prepared above and induction agents to achieve final concentration of 0.5 &#956;g/mL dexamethasone, 0.5 mM isobutyl methylxanthine and 50 &#956;M indomethacin.</li>
</ol>
2. ADSC isolation
<ol>
	<li>Tissue preparation and digestion
	<ol>
		<li>Pipette ~10 mL of 5-PBS buffer into four 100 mm cell culture dishes.</li>
		<li>Transfer ~50 g of adipose sample to one of the 100 mm dishes containing 5-PBS. Wash the collected adipose tissue sample four times by transferring it sequentially across the four culture dishes containing 5-PBS.</li>
		<li>Transfer adipose sample to a clean 100 mm culture dish and thoroughly mince adipose tissue using scissors or two sterile scalpels. Mincing allows for increasing the surface area for efficient and complete enzymatic digestion.</li>
		<li>Transfer the minced adipose tissue to 50 mL plastic conical tube containing 13 mL of CB (1&#8211;3 cm section of tissue per 15 mL of CB).</li>
		<li>Rinse the culture dish with 2 mL of CB and transfer the medium to the 50 mL plastic conical tube. 
		NOTE: At this point, there should be a total of 15 mL of CB with tissue in a 50 mL plastic conical tube.</li>
		<li>Pipette up and down several times using 25 mL serological pipette to facilitate mechanical tissue digestion.</li>
		<li>Incubate the 50 mL plastic conical tube containing tissue in CB on a rocker at medium speed at 37 &#176;C for 30&#8211;60 min.</li>
	</ol>
	</li>
	<li>ADSC plating for culture
	<ol>
		<li>Add 10 mL of ADSC growth medium to the 50 mL tube containing tissue to neutralize enzyme activity. Pipette up and down several times using 25 mL serological pipette to separate any adipose tissue aggregates.</li>
		<li>Transfer the liquid portion to a new sterile 50 mL conical tube leaving the solids behind. Wash the original 50 mL tube 3 times with ~7 mL of 2-PBS buffer and transfer the liquid portion to the 50 mL tube.</li>
		<li>Centrifuge at 500 x g for 5 min to obtain a cell pellet. Carefully remove as much supernatant as possible using a serological pipette without disturbing the cell pellet. Do not decant.</li>
		<li>Resuspend the cell pellet in 1 mL of 1x red blood cell (RBC) lysis buffer and incubate at room temperature for 10 min. Add 5 mL of ADSC growth medium to the tube and centrifuge at 500 x g for 5 min, then carefully remove and discard the supernatant.</li>
		<li>Add 5 mL of ADSC growth medium and centrifuge at 500 x g for 5 min to wash cell pellet. Discard the supernatant.</li>
		<li>Resuspend the pellet in 2 mL of ADSC growth medium and filter through a 70 &#956;m cell strainer into a new sterile 50 mL plastic conical tube.</li>
		<li>Rinse the cell strainer with an additional 2 mL of ADSC growth medium. Transfer 4 mL of the suspension containing ADSCs from the 50 mL conical tube to a sterile 100 mm culture dish.</li>
		<li>Wash the 50 mL conical tube 2 times with 3 mL of ADSC growth medium and transfer the liquid into the 100 mm culture dish containing ADSCs for a total of 10 mL of medium in culture dish.</li>
		<li>View cells under an inverted microscope at 10x magnification to check for floating cells in the media as shown in Figure 1A. Cells should be maintained in a CO2 incubator at 37 &#176;C at 5% CO2 and 100% relative humidity.</li>
		<li>After 24 h, view cells under an inverted microscope to check for cell adherence. Aspirate ADSC growth medium from the plate and replace with 10 mL of fresh, warm (37 &#176;C) media. Remove and replace media every 48 h until cells are 80%&#8211;90% confluent (Figure 1B). 
		NOTE: At least 10&#8211;20 % of cells will be adherent by 24 h. Check the cell culture for signs of contamination such as cell granularity, turbidity of the media, or growth of spores. Once cells are 80% confluent, they can be harvested for proliferation and cryopreservation or induced to differentiate. ADSCs can be expanded to 4&#8211;6 passages before losing their ability to efficiently proliferate or differentiate.</li>
	</ol>
	</li>
</ol>
3. ADSC proliferation
<ol>
	<li>Cell detachment
	<ol>
		<li>Remove ADSC growth medium using an aspirator/pipette. Rinse confluent ADSCs 2 times with 2 mL of sterile, room temperature PBS.</li>
		<li>Aspirate PBS and add 2 mL of 0.25 % trypsin-EDTA per 100 mm culture plate. Ensure that the entire surface area is covered with trypsin.</li>
		<li>Incubate plate for ~7 min at 37 &#176;C in 5% CO2 until ADSCs are detached. Remove plate from incubator and mechanically dislodge cells by forcefully pipetting the trypsin solution in the plate.</li>
		<li>Add 2 mL of ADSC growth medium to the dislodged cells and gently pipette to mix. Transfer cells to sterile 50 mL plastic conical tube. To ensure maximal cell recovery, rinse culture dish with another 2 mL of ADSC growth medium, and transfer medium to the conical tube containing detached cells.</li>
		<li>Centrifuge the 50 mL conical tube at 500 x g for 5 min at room temperature to obtain a cell pellet. Carefully decant supernatant without disturbing the cell pellet.</li>
		<li>Resuspend cell pellet in 5&#8211;6 mL of ADSC growth medium per 1 x 106 cells.</li>
	</ol>
	</li>
	<li>Cell count and plating
	<ol>
		<li>In a 1.5 mL microcentrifuge tube, dilute 10 &#956;L of cell solution from above and 10 &#956;L of 0.04% trypan blue solution (0.4% trypan blue diluted 1:10 in PBS) and count cells using a hemocytometer.</li>
		<li>Resuspend the desired number of ADSCs in growth medium. For 100 mm culture dish, plate ~3.0 x 105 cells in 10 mL ADSC growth media to allow for 80% confluence in 72 h or 100% confluency in 96 h.</li>
		<li>View the dish under an inverted microscope at 10x magnification prior to incubation to ensure presence of suspended cells. Maintain the cells at 37 &#176;C at 5% CO2 and 100% relative humidity.</li>
		<li>Every 48 h aspirate the growth medium and replace with warm (37 &#176;C) medium until cells are 80% to 90% confluent as shown in Figure 1B.</li>
		<li>Repeat steps from sections 3.1 and 3.2 for appropriate number of passages to obtain desired cell number. 
		NOTE: After passages 5 to 6, primary cells appear to undergo senescence; therefore, aim to obtain desired cell numbers by passage 4.</li>
	</ol>
	</li>
</ol>
4. ADSC adipogenic differentiation
<ol>
	<li>Aspirate ADSC growth medium from adhered ADSCs that have reached 80% to 90% confluence.</li>
	<li>Quickly rinse ADSC cell layer with sterile, room temperature PBS.</li>
	<li>Add ADSC differentiation medium. For 100 mm culture dish, add 10 mL of ADSC differentiation medium.</li>
	<li>Replace medium every 3 days for approximately 14&#8211;21 days. Mature adipocytes are generally observed after 14 days of differentiation.</li>
	<li>Examine cells under an inverted light microscope at 40x magnification to confirm the presence of lipid droplet as shown in Figure 2A.</li>
</ol>
5. Adipocyte detection
NOTE: This section will describe staining protocols used for lipid droplet detection in differentiated adipocytes, however, immunofluorescent staining for CD105, a mesenchymal stem cell marker, can also be used for ADSC confirmation.
<ol>
	<li>Oil Red O staining
	<ol>
		<li>Prepare 0.5% Oil Red O stock solution in isopropanol. For 20 mL of Oil Red O stock solution, dissolve 100 mg Oil Red O in 20 mL of isopropanol. Filter the solution through a sterile syringe filter with 0.2 &#956;m membrane.</li>
		<li>Carefully aspirate the differentiation medium and wash cells 2 times by adding PBS along the sides of the well to not disturb the cell monolayer.</li>
		<li>Carefully aspirate PBS from cells and add enough neutral buffered formalin (NBF, 10%) to cover cell layer. Incubate at room temperature for 30&#8211;60 min.</li>
		<li>During the formalin fixation step, prepare Oil Red O working solution by diluting 3 parts of Oil Red O stock solution with 2 parts of distilled water. Mix the solution and filter through a sterile syringe filter with 0.2 &#956;m membrane. Working solution is stable for up to 2 h.</li>
		<li>Carefully aspirate NBF and quickly wash (~ 15 s) the cell layer with distilled water. Add enough 60% isopropanol to cover the cell layer after aspirating water and incubate at room temperature for 5 min.</li>
		<li>Carefully aspirate isopropanol after 5 min incubation and add enough Oil Red O working solution to cover the cell layer and incubate at room temperature for 10&#8211;15 min.</li>
		<li>Carefully aspirate off the Oil Red O working solution and wash the cell layer several times with distilled water until the water becomes clear.</li>
		<li>Add PBS to the cell culture dish and examine cells under an inverted microscope for indication of differentiation and presence of lipid droplets (Figure 2B).</li>
	</ol>
	</li>
	<li>BODIPY Staining
	<ol>
		<li>Prepare 5 mM BODIPY stock solution by dissolving 1.3 g of BODIPY in 1 mL of DMSO. Prepare 2 &#956;g/mL BODIPY working solution by diluting the stock solution 1:25,000 times in PBS.</li>
		<li>Carefully aspirate the differentiation medium and wash cells 2 times by adding PBS along the sides of the well to not disturb the cell monolayer.</li>
		<li>Carefully aspirate PBS and add enough BODIPY working solution to cover the cell layer and incubate at 37 &#176;C for 30 min. 
		NOTE: From this point, protect cells from light by covering plate with foil.</li>
		<li>Carefully aspirate the BODIPY working solution and wash the cell layer 3 times with PBS.</li>
		<li>Fix cells by adding 4% paraformaldehyde and incubating at room temperature for 15 min.</li>
		<li>Carefully aspirate the fixation buffer and wash cells 2 times by adding PBS along the sides of the well to not disturb the cell monolayer.</li>
		<li>Add PBS to cell culture dish and examine cells under an inverted fluorescent microscope for evidence of differentiation and presence of lipid droplet (Figure 2C). Image cells using a FITC/EGFP/Bodipy Fl/Fluo3/DiO Chroma filter set. Excitation wavelength is at 480 nm with a band width of 40 nm and emission wavelength is at 535 nm with a bandwidth of 50 nm. A similar or appropriate filter set, and microscope can be used.</li>
	</ol>
	</li>
</ol>

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ADSC isolation, proliferation and differentiation protocols are straight-forward and reproducible, but they require careful technique to ensure adequate isolation, healthy expansion, and efficient differentiation. A sterile working environment is critical for all cell culture experiments. Bacteria or fungi may be introduced into cell cultures through contaminated tools, media or work environment. Fungal contamination is indicated by spore growth in the culture, while bacterial contamination is indicated by the presence o...

Adipose tissue is comprised of a heterogeneous mixture of cells, predominantly mature adipocytes and a stromal vascular fraction including fibroblasts, immune cells and adipose-derived stem cells (ADSCs)1,2,3. Primary ADSCs can be isolated directly from white adipose tissue and stimulated to differentiate into adipocytes, cartilage or bone cells4. ADSCs exhibit classical stem cell characteristics such as maintenance of multipotency in vitro and self-renewal; and are adherent to plastic in culture5,6. ADSCs are of important interest for the use in regenerative medicine due to their multipotency and ability to be easily harvested in large quantities using non-invasive techniques7. Adipogenic differentiation of ADSCs produces cells that functionally mimic mature adipocytes including lipid accumulation, insulin-stimulated glucose uptake, lipolysis, and adipokine secretion8. Their resemblance to mature adipocytes has led to the widespread use of ADSCs for physiological investigation of cellular characteristics and metabolic function of adipocytes. There is increasing evidence&#160;supporting the idea that the development of metabolic dysfunction and disorders originates at the cellular or tissue level9,10,11,12. Optimal ADSC differentiation is required for sufficient adipose tissue expansion, proper adipocyte function, and effective metabolic regulation13.
Protocols described in this manuscript are straightforward techniques utilizing standard laboratory equipment and basic reagents. The manuscript first describes the protocol for the isolation of primary ADSCs from fresh adipose tissue using mechanical and enzymatic digestion. Next, the protocol for proliferation and passaging of ADSCs in stromal medium is described. Lastly, the protocol for adipogenic differentiation of ADSCs is described. Following differentiation, these cells can be used for studies to better understand adipocyte metabolism and mechanisms of dysfunction. The protocols for confirmation of adipogenic differentiation and lipid droplet detection using Oil Red O and boron-dipyrromethene (BODIPY) staining are also described. The details of these protocols focused on primary ADSCs isolated from fresh omental adipose tissue of rhesus macaques. We and others have used this protocol to successfully isolate ADSCs from rhesus macaque subcutaneous and omental adipose tissues depots14,15. For the same amount of tissue used, we have observed that subcutaneous adipose tissue is more dense, tougher and yields less cells from digestion compared to omental adipose tissue. This protocol has also been used to isolate ADSCs from human adipose samples16.

<table>
	<tbody>
		<tr>
			<td>0.4 % trypan blue</td>
			<td>Thermo-Fisher</td>
			<td>15250061</td>
			<td></td>
		</tr>
		<tr>
			<td>1.5-ml microcentrifuge tube</td>
			<td>Dot Scientific</td>
			<td>707-FTG</td>
			<td></td>
		</tr>
		<tr>
			<td>100 % isopropanol</td>
			<td>Sigma-Aldrich</td>
			<td>PX1838-P</td>
			<td></td>
		</tr>
		<tr>
			<td>100-mm cell culture dish</td>
			<td>Corning</td>
			<td>430167</td>
			<td></td>
		</tr>
		<tr>
			<td>3-Isobutyl-1-methylxanthine</td>
			<td>Sigma-Aldrich</td>
			<td>I7018</td>
			<td></td>
		</tr>
		<tr>
			<td>50-mL plastic conical tube</td>
			<td>Fisher Scientific</td>
			<td>50-465-232</td>
			<td></td>
		</tr>
		<tr>
			<td>70-&#181;m cell strainer</td>
			<td>Corning</td>
			<td>CLS431751</td>
			<td></td>
		</tr>
		<tr>
			<td>a-MEM</td>
			<td>Thermo-Fisher</td>
			<td>12561056</td>
			<td></td>
		</tr>
		<tr>
			<td>Aluminum foil</td>
			<td>Reynolds Wrap</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>BODIPY</td>
			<td>Thermo-Fisher</td>
			<td>D3922</td>
			<td></td>
		</tr>
		<tr>
			<td>Bovine serum albumin (BSA)</td>
			<td>Sigma-Aldrich</td>
			<td>05470</td>
			<td></td>
		</tr>
		<tr>
			<td>Centrifuge</td>
			<td>Eppendorf</td>
			<td>5810 R</td>
			<td></td>
		</tr>
		<tr>
			<td>Collagenase, Type I</td>
			<td>Thermo-Fisher</td>
			<td>17100017</td>
			<td></td>
		</tr>
		<tr>
			<td>Dexamethasone-Water Soluble</td>
			<td>Sigma-Aldrich</td>
			<td>D2915</td>
			<td></td>
		</tr>
		<tr>
			<td>Dimethyl sulfoxide, DMSO</td>
			<td>Sigma-Aldrich</td>
			<td>D2650</td>
			<td></td>
		</tr>
		<tr>
			<td>Distilled water</td>
			<td>Thermo-Fisher</td>
			<td>15230162</td>
			<td></td>
		</tr>
		<tr>
			<td>Fetal Bovine Serum, USDA-approved</td>
			<td>Sigma-Aldrich</td>
			<td>F0926</td>
			<td></td>
		</tr>
		<tr>
			<td>Fungizone/Amphotericin B (250 ug/mL)</td>
			<td>Thermo-Fisher</td>
			<td>15290018</td>
			<td></td>
		</tr>
		<tr>
			<td>Hanks&#39; Balanced Salt Solution (HBSS)</td>
			<td>Thermo-Fisher</td>
			<td>14175095</td>
			<td></td>
		</tr>
		<tr>
			<td>Hemacytometer with cover slip</td>
			<td>Sigma-Aldrich</td>
			<td>Z359629</td>
			<td></td>
		</tr>
		<tr>
			<td>Indomethacin</td>
			<td>Sigma-Aldrich</td>
			<td>I7378</td>
			<td></td>
		</tr>
		<tr>
			<td>Inverted light microscope</td>
			<td>Nikon</td>
			<td>DIAPHOT-TMD</td>
			<td></td>
		</tr>
		<tr>
			<td>L-glutamine (200 mM)</td>
			<td>Thermo-Fisher</td>
			<td>25030081</td>
			<td></td>
		</tr>
		<tr>
			<td>Laboratory rocker, 0.5 to 1.0 Hz</td>
			<td>Reliable Scientific</td>
			<td>Model 55 Rocking</td>
			<td></td>
		</tr>
		<tr>
			<td>Neutral buffered formalin (10 %)</td>
			<td>Pharmco</td>
			<td>8BUFF-FORM</td>
			<td></td>
		</tr>
		<tr>
			<td>Oil Red O</td>
			<td>Sigma-Aldrich</td>
			<td>O0625</td>
			<td></td>
		</tr>
		<tr>
			<td>Paraformeldehyde</td>
			<td>Sigma-Aldrich</td>
			<td>P6148</td>
			<td></td>
		</tr>
		<tr>
			<td>Penicillin-Streptomycin (10,000 U/mL)</td>
			<td>Thermo-Fisher</td>
			<td>15140122</td>
			<td></td>
		</tr>
		<tr>
			<td>Phosphate buffered saline (PBS), pH 7.4</td>
			<td>Thermo-Fisher</td>
			<td>10010023</td>
			<td></td>
		</tr>
		<tr>
			<td>Red blood cell (RBC) lysis buffer</td>
			<td>Qiagen</td>
			<td>158904</td>
			<td></td>
		</tr>
		<tr>
			<td>Serological pipettes, 2 to 25 mL</td>
			<td>Costar Stripettes</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Standard humidified cell culture incubator, 37 &#176;C, 5 % CO2</td>
			<td>Sanyo</td>
			<td>MCO-17AIC</td>
			<td></td>
		</tr>
		<tr>
			<td>Trypsin-EDTA (0.25%)</td>
			<td>Thermo-Fisher</td>
			<td>25200056</td>
			<td></td>
		</tr>
	</tbody>
</table>

isolation, proliferation and differentiation of rhesus macaque adipose-derived stem cells

Adipose tissue provides a rich and accessible source of multipotent stem cells, which are able to self-renew. These adipose-derived stem cells (ADSCs) provide a consistent ex vivo cellular system that are functionally like that of in vivo adipocytes. Use of ADSCs in biomedical research allows for cellular investigation of adipose tissue metabolic regulation and function. ADSC differentiation is necessary for adequate adipocyte expansion, and suboptimal differentiation is a major mechanism of adipose dysfunction. Understanding changes in ADSC differentiation is crucial to understanding the development of metabolic dysfunction and disease. The protocols described in this manuscript, when followed, will yield mature adipocytes that can be used for several in vitro functional tests to assess ADSC metabolic function, including but not limited to assays measuring glucose uptake, lipolysis, lipogenesis, and secretion. Rhesus macaques (Macaca mulatta) are physiologically, anatomically, and evolutionarily similar to humans and as such, their tissues and cells have been used extensively in biomedical research and for development of treatments. Here, we describe ADSC isolation using fresh subcutaneous and omental adipose tissue obtained from 4&#8211;9-year old rhesus macaques. Adipose tissue samples are enzymatically digested in collagenase followed by filtration and centrifugation to isolate ADSCs from the stromal vascular fraction. Isolated ADSCs are proliferated in stromal media followed by approximately 14&#8211;21 days of differentiation using a cocktail of 0.5 &#956;g/mL dexamethasone, 0.5 mM isobutyl methylxanthine, and 50 &#956;M indomethacin in stromal media. Mature adipocytes are observed at approximately 14 days of differentiation. In this manuscript, we describe protocols for ADSC isolation, proliferation, and differentiation in vitro. Although, we have focused on ADSCs from rhesus macaque adipose tissue, these protocols can be utilized for adipose tissue obtained from other animals with minimal adjustments.

The ADSCs isolated from rhesus macaque adipose tissue samples were seeded on culture plates and is shown in Figure 1. On the day of plating, cells are non-adherent and float in the culture dish as shown in Figure 1A. Within 72 h, ADSCs will become 80% confluent and are ready for adipocyte differentiation (Figure 1B). ADSCs exhibit strong adipogenic characteristics after chemical induction. After 14 days of differentiation, mature ad...

Watch this Scientific Journal Video about Isolation, Proliferation and Differentiation of Rhesus Macaque Adipose-Derived Stem Cells at JoVE.com

Isolation, Proliferation and Differentiation of Rhesus Macaque Adipose-Derived Stem Cells

In this article, we describe isolation of rhesus macaque derived adipose-derived stem cells (ADSCs) using an enzymatic tissue digestion protocol. Next, we describe ADSC proliferation which includes cell detachment, counting and plating. Lastly, ADSC differentiation is described using specific adipogenic inducing agents. Additionally, we describe staining techniques to confirm differentiation.

Adipose tissue provides a rich and accessible source of multipotent stem cells, which are able to self-renew. These adipose-derived stem cells (ADSCs) ...

isolation-proliferation-differentiation-rhesus-macaque-adipose

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2.0K Views.  Louisiana State University Health Sciences Center - New Orleans. In this article, we describe isolation of rhesus macaque derived adipose-derived stem cells (ADSCs) using an enzymatic tissue digestion protocol. Next, we describe ADSC proliferation which includes cell detachment, counting and plating. Lastly, ADSC differentiation is described using specific adipogenic inducing agents. Additionally, we describe staining techniques to confirm differentiation.

Video: Isolation, Proliferation and Differentiation of Rhesus Macaque Adipose-Derived Stem Cells

Isolation and Transplantation of Hematopoietic Stem Cells (HSCs)

Isolation and Transplantation of Hematopoietic Stem Cells HSCs

I am Christina Ceso. I am a postdoc in David's Den lab and I work on the hematopoietic stem cells. Today we are going to purify long-term recuperating hematopoietic stem cells and we'll transplant them into a mouse.We start by spraying the mice with alcohol so that first of all, the mind starts sterilized and also the hair doesn't interfere with the dissection. We use PBS with 2%serum for the dissection. I cut the back skin and I pull the skin apart in order to expose the tissue.In order to isolate the tibia, I hold the tibia with tweezers. I cut the tendon on top of the knee and I cut the muscles below the knee and after that I cut through the knee so that the TBI is not connected to the rest of the limb anymore and I pull in order to isolate it. I then hold the TB upside down and with the scissors I separate the foot from the tibia In order to obtain the femur.I cut the muscles around the femur and then I dislocate the femur from the hip. In order to isolate the hip, I cut the muscle around the hip bone on the side of the tail of the mouse and then I pull the hip away from the body of the mouth In order to isolate the spine. I cut through the tail as close as I can to the beginning of the back and then I cut on the two sides of the spine and below the spine, trying to stay as close as possible to the spine so that the peritoneum is not cut and the intestine is left untouched.A first round of cleaning of the bones is done with a scalpel, which is used to scrape the bone, the muscles away from the bone. The scalpel is good to clean the femurs, the hip and the spine. In order to clean the tibia, I hold them with forceps and I use the forceps to remove as much tissue as possible.A second round of cleaning is done using clean wipe to completely clean the bones outta the muscle, and I use the F wipe to clean the tibia, the femurs and the hips. So this is how bones look. After cleaning, I prefer 50 amount tubes with filters on top and I transfer the bones into the mortar.I add the section media and I crush the bones ask of the first round of crashing of the bones. I piped the mixture in order to release as many styles as possible into solution and reduce clumps. I transferred the mixture on the tubes through the filters and this is what the bone fragments look like after the first round of crushing.So I add more dissection medium to the bone fragments and I flash them again. I transferred the seline mixture to the tubes through the filters and at this point the remaining bone fragments are white and there is no bone marrow left. The tubes are filled with PBS 2%serum and in order to have them all with the same weight so that they're balanced in the centrifuge, but also in order to wash the filters so that we obtain as many cells as possible, I then centrifuge the cell mixture and after centrifugation, the palt includes the bone marrow cells.I aspirate the medium and I move back and forward the tube on the rack so that the pelle is becomes loose and fewer clamps are formed. When I add medium, at this point I add one ml of medium per tube and I ics since I'm sorting hematopoietic stem cells. Later on, I'm going to store an ALI output of total bone marrow sizes at this point, which I will use later for the fact single color control.I add lineage antibody cocktail. I ordered the samples to mix them well and I invaded four degrees for 15 minutes. In the meantime, I start preparing the columns for the lineage division.I put the columns on the magnet and I prepare Ian tubes under the columns. I also prepared the gas PBS using aster flip filter and attaching it to the vacuum so that all the bubbles of air move in the top part of the filter. I then add three ml of the gas DBS to each column in order for the column to become wet.After the incubation with the antibodies, I add medium to the cell samples and I centrifuge them in order to remove the excess of antibodies. After the centrifugation, the stain cells are in the pallet. I aspirate the medium and I suspend the pallet in one mile of the gas PBSI Add the strip tab beans, I mix the cells and I incubate for 15 minutes at four degrees.After the incubation, I put new elucian tubes under the columns. I add two ml of PBS to each tube with the cells and I transferred the cell mixture to the column through a 40 micron filter. I wash the tubes with more medium in order to collect all the cells remaining and I apply the remaining medium through the filters to the columns.The progenitor cells lineage low are alluded into the collection views. I pulled the luted samples and I sent tofu them. So after the centrifugation, the depleted cells are in a white pate.I aspirate the medium and re suspend the cells. I store an adequate of the depleted cells and I add the antibodies to the cell mixture for the sorting and also to all the single color controls. The antibodies are incubated in that with the size for 15 minutes in the fridge.After the ation, I add medium to the cells and and centrifuge them to remove the ex excess of antibodies. After the centrifugation, the cells are in the pt, I aspirate the media that I suspend the cells and I transfer the cells into fox tubes with a blue filter. At this point, the cells are ready to be sorted.I place, I place the mouse under a heating lamp for a few minutes so that the veins dilate and they are more easily seen. When preparing the syringe, you have to be careful to eliminate all the bubbles from the, the mixture that is in the syringe and then you bend the needle at 90 degrees. I put the mouse under a glass cup with a weight on top so that it can run away.I sterilize the tail with the alcohol pad so that the site of injection is sterile, but also it's easier to identify the vein. If you look at the tail of the mouse from the top in the middle and top of the tail, there is an artery while on the two sides there are the two veins and we inject the cells in one of the two veins. I insert the needle into the vein and I inject following injection.It is to wait for a couple of seconds before removing the needle, the needle, and after that I clean the side of injection. This is a representation of the syringe with the ben needle bent at 90 degrees with the knee, the at this ankle compared to the tail, which makes the injection the easiest. When you injecting the tail of the mouse, you have to keep in mind that the tail vein is extremely superficial, so really this is the orientation of the needle compared to the tail.And it looks like you will just keep sliding on top of the tail, but actually you will get into the tail then. I am Christina Ceso. I am a post in David Kaden lab, and I work on the hematopoietic stem cells.I usually use for animals to start with, and I had more variability at the beginning, but once you become consistent with your methods, I consistently get about 50, 000 to 60, 000 stem cells out for mice. I did my PhD in London with Dr.Fiona Wat working on derma stem cells. After that, I just wanted to have a wider knowledge of adult stem cells in various tissues, and so I decided to move to David Kaden lab to work on hematopoietic stem cells, mainly because the things that are known about hematopoietic stem cells are the things that are not known for the epidermic stem cells and a number of assays that can be done with epi.Epidermal stem cells are not really done yet with the hematopoietic stem cells, and so at this point I'm trying to put together the, the knowledge from the two different fields and ultimately I'm interested in the study of the mechanism to regulate adult tissue sensors in general, so not just the epidermis or the stem cells, but also different tissues because there are, there are similar mechanism that is, it's always the same genes that are involved in the regulation that just interact with each other in different ways, and it's just interesting to understand what makes each stem cell be a stem, but then ultimately a stem cell in a different tissue. So giving rise to a different protein.

Isolation and Analysis of Hematopoietic Stem Cells from the Placenta

Hematopoietic stem cells (HSCs) have the ability to self-renew and generate all cell types of the blood lineages throughout the lifetime of an individual. All HSCs emerge during embryonic development, after which their pool size is maintained by self-renewing cell divisions. Identifying the anatomical origin of HSCs and the critical developmental events regulating the process of HSC development has been complicated as many anatomical sites participate during fetal hematopoiesis. Recently, we identified the placenta as a major hematopoietic organ where HSCs are generated and expanded in unique microenvironmental niches (Gekas, et al 2005, Rhodes, et al 2008). Consequently, the placenta is an important source of HSCs during their emergence and initial expansion.
In this article, we show dissection techniques for the isolation of murine placenta from E10.5 and E12.5 embryos, corresponding to the developmental stages of initiation of HSCs and the peak in the size of the HSC pool in the placenta, respectively. In addition, we present an optimized protocol for enzymatic and mechanical dissociation of placental tissue into single-cell suspension for use in flow cytometry or functional assays. We have found that use of collagenase for single-cell suspension of placenta gives sufficient yields of HSCs. An important factor affecting HSC yield from the placenta is the degree of mechanical dissociation prior to, and duration of, enzymatic treatment.
We also provide a protocol for the preparation of fixed-frozen placental tissue sections for the visualization of developing HSCs by immunohistochemistry in their precise cellular niches. As hematopoietic specific antigens are not preserved during preparation of paraffin embedded sections, we routinely use fixed frozen sections for localizing placental HSCs and progenitors.

We have identified the placenta as a major hematopoietic organ during development. We found that hematopoietic stem cells (HSCs) are both generated and expanded in the placenta in unique microenvironmental niches. Here, we describe experimental techniques required for isolation and visualization of HSCs in the mouse placenta.

Hematopoietic stem cells (HSCs) have the ability to self-renew and generate all cell types of the blood lineages throughout the lifetime of an individual. ...

Isolation and Large Scale Expansion of Adult Human Endothelial Colony Forming Progenitor Cells

This paper introduces a novel recovery strategy for endothelial colony forming progenitor cells (ECFCs) from heparinized but otherwise unmanipulated adult human peripheral blood within a mean of 12 days. After large scale expansion &gt;1x108 ECFCs can be obtained for further tests. Advantageously by using pHPL the contact of human cells with bovine serum antigens can be excluded. By flow cytometry and immunohistochemistry the isolated cells can be characterized as ECFC and their in vitro functionality to form vascular like structures can be tested in a matrigel assay. Further these cells can be subcutaneously injected in a mouse model to form functional, perfused vessels in vivo. After long term expansion and cryopreservation proliferation, function and genomic stability appear to be preserved. 3,4
This animal-protein free isolation and expansion method is easily applicable to generate a large quantity of ECFCs.

Endothelial colony forming progenitor cells (ECFCs) are a promising tool to study vascular homeostasis and repair.1,2 This paper introduces a novel animal-serum free method for isolation and expansion of ECFC from heparinised adult human peripheral blood with pooled human platelet lysate (pHPL) diminishing the risk of anti-bovine immunisation.

This paper introduces a novel recovery strategy for endothelial colony forming progenitor cells (ECFCs) from heparinized but otherwise unmanipulated adult ...

Isolation and Animal Serum Free Expansion of Human Umbilical Cord Derived Mesenchymal Stromal Cells (MSCs) and Endothelial Colony Forming Progenitor Cells (ECFCs)

The umbilical cord is a rich source for progenitor cells with high proliferative potential including mesenchymal stromal cells (also termed mesenchymal stem cells, MSCs) and endothelial colony forming progenitor cells (ECFCs). Both cell types are key players in maintaining the integrity of tissue and are probably also involved in regenerative processes and tumor formation.
To study their biology and function in a comparative manner it is important to have both cells types available from the same donor. It may also be beneficial for regenerative purposes to derive MSCs and ECFCs from the same tissue.
Because cellular therapeutics should eventually find their way from bench to bedside we established a new method to isolate and further expand progenitor cells without the use of animal protein. Pooled human platelet lysate (pHPL) replaced fetal bovine serum in all steps of our protocol to completely avoid contact of the cells to xenogeneic proteins.
This video demonstrates a methodology for the isolation and expansion of progenitor cells from one umbilical cord.
All materials and procedures will be described.

Isolation and Animal Serum Free Expansion of Human Umbilical Cord Derived Mesenchymal Stromal Cells MSCs and Endothelial Colony Forming Progenitor Cells ECFCs

This protocol describes the isolation and subsequent expansion of mesenchymal stromal cells and endothelial colony forming cells without the use of animal serum to generate autologous pairs for experimental transplantation purposes.

The umbilical cord is a rich source for progenitor cells with high proliferative potential including mesenchymal stromal cells (also termed mesenchymal ...

Isolation and Derivation of Mouse Embryonic Germinal Cells

The ability of embryonic germinal cells (EG) to differentiate into primordial germinal cells (PGCs) and later into gametes during early developmental stages is a perfect model to address our hypothesis about cancer and infertility. This protocol shows how to isolate primordial germinal cells from developing gonads in 10.5-11.5 days post coitum (dpc) mouse embryos.  Developing gonadal ridges from mouse embryos (C57BL6J) were dissociated by mechanical disruption with collagenase, then plated in a mouse embryo fibroblast feeder layer (MEF-CF1) that was previously mitotically inactivated with mitomycin C in the presence of knockout media and supplemented with Leukemia Inhibitor Factor (LIF), basic Fibroblast Growth Factor (bFGF), and Stem Cell Factor (SCF).  Using these optimized methods for PCG identification, isolation, and establishment of culture conditions permits long term cultures of EG cells for more than 40 days.  The embryonic germinal cell lines showed embryonic phenotype and expression of common used markers of the pluripotent state.  Isolation and derivation of germinal cells in culture provide a tool to understand their development in vitro and offer the opportunity to monitor cumulative damage at genetic and epigenetic levels after exposure to oxidative stress.

The ability of embryonic germinal cells to differentiate into primordial germinal cells during early development stages is a perfect model to address our hypothesis about cancer and infertility. This protocol shows how to isolate primordial germinal cells from developing gonads in 10.5-11.5 days post coitum mouse embryos.

The ability of embryonic germinal cells (EG) to differentiate into primordial germinal cells (PGCs) and later into gametes during early developmental ...

Differentiation of Embryonic Stem Cells into Oligodendrocyte Precursors

Oligodendrocytes are the myelinating cells of the central nervous system. For regenerative cell therapy in demyelinating diseases, there is significant interest in deriving a pure population of lineage-committed oligodendrocyte precursor cells (OPCs) for transplantation. OPCs are characterized by the activity of the transcription factor Olig2 and surface expression of a proteoglycan NG2. Using the GFP-Olig2 (G-Olig2) mouse embryonic stem cell (mESC) reporter line, we optimized conditions for the differentiation of mESCs into GFP+Olig2+NG2+ OPCs. In our protocol, we first describe the generation of embryoid bodies (EBs) from mESCs. Second, we describe treatment of mESC-derived EBs with small molecules: (1) retinoic acid (RA) and (2) a sonic hedgehog (Shh) agonist purmorphamine (Pur) under defined culture conditions to direct EB differentiation into the oligodendroglial lineage. By this approach, OPCs can be obtained with high efficiency (&gt;80%) in a time period of 30 days. Cells derived from mESCs in this protocol are phenotypically similar to OPCs derived from primary tissue culture. The mESC-derived OPCs do not show the spiking property described for a subpopulation of brain OPCs in situ. To study this electrophysiological property, we describe the generation of spiking mESC-derived OPCs by ectopically expressing NaV1.2 subunit. The spiking and nonspiking cells obtained from this protocol will help advance functional studies on the two subpopulations of OPCs.

We describe a small molecule-based protocol for differentiation of mouse embryonic stem cells into oligodendrocyte precursor cells (OPCs). This protocol generates Olig2+NG2+ OPCs with high efficiency by 30 days of differentiation. We also describe a method to generate "spiking" OPCs that can fire action potentials.

Oligodendrocytes are the myelinating cells of the central nervous system. For regenerative cell therapy in demyelinating diseases, there is significant ...

Isolation of Mouse Salivary Gland Stem Cells

Mature salivary glands of both human and mouse origin comprise a minimum of five cell types, each of which facilitates the production and excretion of saliva into the oral cavity. Serous and mucous acinar cells are the protein and mucous producing factories of the gland respectively, and represent the origin of saliva production. Once synthesised, the various enzymatic and other proteinaceous components of saliva are secreted through a series of ductal cells bearing epithelial-type morphology, until the eventual expulsion of the saliva through one major duct into the cavity of the mouth. The composition of saliva is also modified by the ductal cells during this process.
In the manifestation of diseases such as Sj&ouml;gren's syndrome, and in some clinical situations such as radiotherapy treatment for head and neck cancers, saliva production by the glands is dramatically reduced 1,2. The resulting xerostomia, a subjective feeling of dry mouth, affects not only the ability of the patient to swallow and speak, but also encourages the development of dental caries and can be socially debilitating for the sufferer.
The restoration of saliva production in the above-mentioned clinical conditions therefore represents an unmet clinical need, and as such several studies have demonstrated the regenerative capacity of the salivary glands 3-5. Further to the isolation of stem cell-like populations of cells from various tissues within the mouse and human bodies 6-8, we have shown using the described method that stem cells isolated from mouse salivary glands can be used to rescue saliva production in irradiated salivary glands 9,10. This discovery paves the way for the development of stem cell-based therapies for the treatment of xerostomic conditions in humans, and also for the exploration of the salivary gland as a microenvironment containing cells with multipotent self-renewing capabilities.

An optimized protocol for the isolation of stem cells from the mouse salivary gland is described. The method employs enzymatic and mechanical digestion, and permits isolation of salispheres containing cells with characteristics of stem cells.

Mature salivary glands of both human and mouse origin comprise a minimum of five cell types, each of which facilitates the production and excretion of ...

Isolation and Differentiation of Stromal Vascular Cells to Beige/Brite Cells

Brown adipocytes have the ability to uncouple the respiratory chain in mitochondria and dissipate chemical energy as heat. Development of UCP1-positive brown adipocytes in white adipose tissues (so called beige or brite cells) is highly induced by a variety of environmental cues such as chronic cold exposure or by PPAR&gamma; agonists, therefore, this cell type has potential as a therapeutic target for obesity treatment. Although most immortalized adipocyte lines cannot recapitulate the process of "browning" of white fat in culture, primary adipocytes isolated from stromal vascular fraction in subcutaneous white adipose tissue (WAT) provide a reliable cellular system to study the molecular control of beige/brite cell development. Here we describe a protocol for effective isolation of primary preadipocytes and for inducing differentiation to beige/brite cells in culture. The browning effect can be assessed by the expression of brown fat-selective markers such as UCP1.

Primary white preadipocytes isolated from white adipose tissues in mice can be differentiated into beige/brite cells. Presented here is a reliable cellular model system to study the molecular regulation of "browning" of white fat.

Brown adipocytes have the ability to uncouple the  respiratory chain in mitochondria and dissipate chemical energy as heat.  Development of UCP1-positive ...

Induction and Analysis of Epithelial to Mesenchymal Transition

Epithelial to mesenchymal transition (EMT) is essential for proper morphogenesis during development. Misregulation of this process has been implicated as a key event in fibrosis and the progression of carcinomas to a metastatic state. Understanding the processes that underlie EMT is imperative for the early diagnosis and clinical control of these disease states. Reliable induction of EMT in vitro is a useful tool for drug discovery as well as to identify common gene expression signatures for diagnostic purposes. Here we demonstrate a straightforward method for the induction of EMT in a variety of cell types. Methods for the analysis of cells pre- and post-EMT induction by immunocytochemistry are also included. Additionally, we demonstrate the effectiveness of this method through antibody-based array analysis and migration/invasion assays.

A straightforward method is described for the induction of epithelial to mesenchymal transition (EMT) in a variety of cell types. Methods for the analysis of cells in EMT states by immunocytochemistry are included.

Epithelial  to mesenchymal transition (EMT) is essential for proper morphogenesis during  development. Misregulation of this  process has been implicated ...

Differentiation of Newborn Mouse Skin Derived Stem Cells into Germ-like Cells In vitro

Studying germ cell formation and differentiation has traditionally been very difficult due to low cell numbers and their location deep within developing embryos. The availability of a "closed" in vitro based system could prove invaluable for our understanding of gametogenesis. The formation of oocyte-like cells (OLCs) from somatic stem cells, isolated from newborn mouse skin, has been demonstrated and can be visualized in this video protocol. The resulting OLCs express various markers consistent with oocytes such as Oct4 , Vasa , Bmp15, and Scp3. However, they remain unable to undergo maturation or fertilization due to a failure to complete meiosis. This protocol will provide a system that is useful for studying the early stage formation and differentiation of germ cells into more mature gametes. During early differentiation the number of cells expressing Oct4 (potential germ-like cells) reaches ~5%, however currently the formation of OLCs remains relatively inefficient. The protocol is relatively straight forward though special care should be taken to ensure the starting cell population is healthy and at an early passage.

Differentiation of Newborn Mouse Skin Derived Stem Cells into Germ-like Cells In vitro

In recent years the formation of germ cells using in vitro culture methods has been demonstrated using several different types of somatic stem cells. This article will visually present the differentiation of newborn mouse derived stem cells to early oocyte-like cells.

Studying  germ cell formation and differentiation has traditionally been very difficult  due to low cell numbers and their location deep within developing ...

Isolation, Proliferation and Differentiation of Rhesus Macaque Adipose-Derived Stem Cells

Summary

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Chapters in this video

Isolation and Transplantation of Hematopoietic Stem Cells (HSCs)

Isolation and Analysis of Hematopoietic Stem Cells from the Placenta

Isolation and Large Scale Expansion of Adult Human Endothelial Colony Forming Progenitor Cells

Isolation and Animal Serum Free Expansion of Human Umbilical Cord Derived Mesenchymal Stromal Cells (MSCs) and Endothelial Colony Forming Progenitor Cells (ECFCs)

Isolation and Derivation of Mouse Embryonic Germinal Cells

Differentiation of Embryonic Stem Cells into Oligodendrocyte Precursors

Isolation of Mouse Salivary Gland Stem Cells

Isolation and Differentiation of Stromal Vascular Cells to Beige/Brite Cells

Induction and Analysis of Epithelial to Mesenchymal Transition

Differentiation of Newborn Mouse Skin Derived Stem Cells into Germ-like Cells In vitro