Research supported by a grant from the Conselho Nacional de Desenvolvimento Cient&#237;fico e Tecnologico (480807/2011-6) and Funda&#231;&#227;o de Amparo &#224; Pesquisa de Minas Gerais (APQ-01237-11). This study was financed in part by the PROPP UESC (073.6764.2019.0021079-85). MGAG and URS thanks to the scholarship granted by Funda&#231;&#227;o de Amparo &#224; Pesquisa do Estado da Bahia (FAPESB), and Coordena&#231;&#227;o de Aperfei&#231;oamento de Pessoal de N&#237;vel Superior (CAPES), respectively.

All animal experiments were conducted according to international guidelines for animal ethics and were approved by institutional committees of care and use from the State University of Santa Cruz under protocol number 021/22. Swiss male mice (6-8 weeks) were acquired from the Animal Breeding, Maintenance and Experimentation Laboratory - State University of Santa Cruz (LaBIO-UESC) Animal Research Facility, maintained in specific pathogen-free conditions, receiving water and food ad libitum with 12 h light/dark cycles.
NOTE: Other mice lineage can be used; we recommend the use of adult mice (6-8 weeks) since they have more developed adipose tissue and cells with high proliferative activity.
1. Preparation
NOTE: Before proceeding, prepare the following reagents described below. See the Table of Materials for reagent and material supplier information. Personal protective equipment such as masks, caps, lab coats, and gloves must be worn in all practical procedures.
<ol>
	<li>Epididymal adipose tissue extraction
	<ol>
		<li>Reserve the surgery materials: three sets of sterile tweezers and scissors, five needles, and a beaker containing 200 mL of 70% ethanol.</li>
		<li>Prepare a terminal anesthetic, mixing ketamine (100 mg/kg) and xylazine (10 mg/kg).</li>
	</ol>
	</li>
	<li>ADSCs culture
	<ol>
		<li>Basal medium: Prepare Dulbecco&#39;s Modified Eagle Medium (DMEM) high glucose media supplemented with 10% fetal bovine serum (FBS), 50 &#181;g/mL gentamicin, 0.25 &#181;g/mL amphotericin B, 100 U/mL penicillin, and 100 mg/mL streptomycin.</li>
		<li>Digest solution: Prepare 0.15% of collagenase type II in PBS sterilized in a 0.25 &#181;m filter. 
		NOTE: It is not necessary to use the four antibiotics described in the basal medium. It will depend on the cell culture conditions of the laboratory where this is performed.</li>
	</ol>
	</li>
	<li>ADSCs phenotypic characterization
	<ol>
		<li>Prepare 1% bovine serum albumin (BSA) in PBS.</li>
		<li>Dilute the anti-mouse antibodies as mentioned in Table 1.</li>
		<li>Prepare 2% formaldehyde in PBS.</li>
	</ol>
	</li>
	<li>ADSCs osteogenic differentiation
	<ol>
		<li>Osteogenic differentiation medium: Prepare DMEM supplemented with 5.67 M ascorbic acid, 10 nM dexamethasone, 0.02 M &#946;-glycerophosphate, 10% FBS, and 1% penicillin/streptomycin.</li>
		<li>For Von Kossa staining, prepare the following solutions: 70% ethanol in water, 5% silver nitrate in water, distilled water, 5% sodium thiosulfate in water, and 1% eosin B in water.</li>
	</ol>
	</li>
	<li>Adipogenic differentiation:
	<ol>
		<li>Adipogenic differentiation medium: Prepare DMEM supplemented with 0.5 mM 3-Isobutyl-1-methylxanthine, 200 &#181;M indomethacin, 1 &#181;M dexamethasone, 10 &#181;M insulin, 10% FBS, and 1 % penicillin/streptomycin.</li>
		<li>For Oil-red staining, prepare the following solutions: 10% formalin in deionized water, 60% isopropanol in deionized water, lysochrome (fat-soluble dye) diazo dye (Oil-Red O solution) in 60% isopropanol, and 1% hematoxylin in deionized water.</li>
	</ol>
	</li>
	<li>Chondrogenic differentiation:
	<ol>
		<li>Chondrogenic differentiation medium: Prepare chondrogenic medium supplemented with 10% FBS and 1% penicillin/streptomycin.</li>
		<li>Prepare 10% formaldehyde in PBS.</li>
		<li>For proteoglycans and glycosaminoglycans staining, prepare the following solutions: Heteroglycan stain (Alcian Blue 1%) in acetic acid, pH 2.5, paraffin, hematoxylin, ethanol series dilution in water (100%, 96%, 80%, and 70%).</li>
	</ol>
	</li>
</ol>

<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Antibody/Fluorophore</td>
			<td>Dilution</td>
			<td>Clone</td>
			<td>Final concentration (&#181;g/mL)</td>
			<td colspan="3">Function and cell in which it is expressed</td>
		</tr>
		<tr>
			<td>CD34- PE</td>
			<td>1:100</td>
			<td>RAM34</td>
			<td>2</td>
			<td colspan="3">Cell adhesion factor. Hematopoietic stem cells.</td>
		</tr>
		<tr>
			<td>CD45- APC</td>
			<td>1:100</td>
			<td>30-F11</td>
			<td>2</td>
			<td colspan="3">Assistence in activation of leukocytes. Expressed in leukocytes.</td>
		</tr>
		<tr>
			<td>CD71- FITC</td>
			<td>1:100</td>
			<td>C2</td>
			<td>5</td>
			<td colspan="3">Controls iron uptake during cell proliferation. Proliferating cells, reticulocytes, and precursor cells.</td>
		</tr>
		<tr>
			<td>CD29- FITC</td>
			<td>1:100</td>
			<td>Ha2/5</td>
			<td>5</td>
			<td colspan="3">Adhesion and activation, embryogenesis, Leukocytes, dendritic cells, platelets, mast cells, fibroblasts, and endothelial cells.</td>
		</tr>
		<tr>
			<td>CD90- PerCP</td>
			<td>1:100</td>
			<td>OX-7</td>
			<td>2</td>
			<td colspan="3">Signaling, adhesion. T lymphocyte, NK, monocyte, Hemtopoietic Stem Cells, neuron, and fibroblast.</td>
		</tr>
	</tbody>
</table>
Table 1: Antibodies used for phenotypic characterization of ADSCs by flow cytometer. List of antibodies with their respective fluorochromes, dilutions, clone, and final concentration as well as their function in the cell which is expressed.
2. Methods
NOTE: The adipose tissue is distributed throughout the body in subcutaneous or intra-abdominal locations. In mice, the most common adipose tissues used for experiments include the subcutaneous epididymal, mesenteric, and retroperitoneal22. Here, the steps for obtaining epididymal adipose tissue are shown (Figure 1).
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/65722/65722fig01.jpg" /> 
Figure 1: Experimental design to obtain adipose tissue-derived stem cells from Swiss mice. (A) Using needles, place the animal on the cork or styrofoam board; (B) Lift the skin using tweezers, make a cut in the center of the abdominal region, and detach the skin from the peritoneum; (C) identify the white adipose tissue above the epididymis; (D) transfer the tissue to DMEM medium supplemented with 10% FBS and 1% antibiotics, wash the epididymal adipose tissue thoroughly with PBS, and transfer the tissue to digest solution; (E), fragment the tissue and (F) incubate at 37 &#176;C for 1 h vigorously shaking every 10 min; (G) after counting the cells, plate in 6-well plates and observe the cell morphology under an inverted microscope. (F) Cell morphology will change from round to fibroblast-like. Scale bar = 22.22 &#181;m. <a href="https://www.jove.com/files/ftp_upload/65722/65722fig01large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<ol>
	<li>Extraction of epididymal adipose tissue 
	NOTE: Be aware that all procedures must be carried out under sterile conditions in a laminar flow cabinet in order to ensure pure and contamination-free cell culture.
	<ol>
		<li>Euthanize the animals using ketamine and xylazine solution (100 and 10 mg/kg, as described in step 1.1.2) by intraperitoneal route. 
		NOTE: Other euthanizing methods can be used23. Make sure the animal is dead by confirming the absence of a heartbeat.</li>
		<li>Place the animal with the ventral side facing up on a cork or styrofoam board covered with aluminum foil and fix it using sterile needles (Figure 1A). 
		NOTE: To avoid contamination, spray 70% alcohol in the abdominal region. Alternatively, shave the hair with a scalpel.</li>
		<li>Lift the skin using tweezers in the center of the abdominal region and make a cut with sterile scissors. 
		NOTE: Two sets of sterile tweezers and scissors are necessary to avoid contamination. The first one is used to open the animal, cutting the skin and peritoneal layer; the second one is used to pick up the epididymal adipose tissue. Also, reserve 150 mL of 70% alcohol in a beaker to clean scissors and tweezers between steps.</li>
		<li>Introduce the scissors under the animal&#39;s skin and open it to detach it from the peritoneum (Figure 1B). Lift the peritoneal layer using tweezers and cut with sterile scissors.</li>
		<li>Use another set of sterile tweezers and scissors and identify the epididymis above the testes and the white adipose tissue above the epididymis. Pull the entire epididymal adipose tissue using sterile tweezers, approximately 2 cm in size, and cut very close to the epididymis (Figure 1C).</li>
		<li>Put the fat into a 50 mL sterile conical tube containing basal medium and place it on ice (Figure 1D). In the hood, proceed to the next steps as described below.</li>
	</ol>
	</li>
	<li>Adipose tissue-derived stem cells (ADSCs) isolation 
	NOTE: Process the samples in a biological class II laminar flow hood, and personnel should wear a lab coat, gloves, and surgical mask.
	<ol>
		<li>Wash the epididymal adipose tissue thoroughly with PBS. 
		NOTE: This step is essential to remove the blood and other particles from the sample. The blood can inhibit collagenase type II enzyme and compromise the experiment.</li>
		<li>Using a sterile tweezer, transfer the epididymal adipose tissue into a 50 mL tube containing 15-20 mL of digest solution, prepared as step 1.2.2. Fragment the tissue using sterile scissors and incubate the tissue at 37 &#176;C for 1 h (Figure 1E, F). 
		NOTE: A water bath or incubator at 37 &#176;C can be used in this step. Every 10 min, the suspension must be vigorously shaken to facilitate digestion. Do not extend the time of 1h incubation.</li>
		<li>Inactivate the collagenase by diluting the sample 1:1 in basal medium and centrifuge the suspension at 250 x g for 10 min at 4 &#176;C to obtain the vascular fraction of the stroma. Discard the supernatant and resuspend the pellet in 1 mL of basal medium.</li>
		<li>Check the viability and count the cells through the trypan blue dye exclusion method in a Neubauer chamber using a dilution of 1:10 or 1:100. 
		NOTE: The expected yield is around 0.5-1 million cells/g of processed adipose tissue and viability of 80%.</li>
		<li>Plate the isolated cells (0.3-0.5 million) in 3 mL of basal medium in one well of a 6-well plate. Incubate the cells overnight at 37 &#176;C with 5 % CO2.</li>
		<li>Next day: Remove the medium from the well and wash the cells with PBS. Add 3 mL of basal medium. Repeat this process every 2 days until the cells become 90% confluent. 
		NOTE: Always observe the morphology of the cells under the inverted microscope, changing from round to fibroblast-like (Figure 1H).</li>
	</ol>
	</li>
	<li>Adipose tissue-derived stem cells (ADSCs) expansion 
	NOTE: Once the cells grow ~90% confluent, proceed to subculture as described below.
	<ol>
		<li>Remove the medium from the well and wash the cells with PBS. Add 0.5 mL/well of trypsin/EDTA (0.05 % trypsin; 200 mg/L EDTA) and incubate the plate for 3-5 min at 37 &#176;C to detach the cells. 
		NOTE: Do not exceed 5 min in trypsin/EDTA. The complete detachment of the cells should be verified under the inverted microscope. The process can be accelerated by pipetting up and down carefully or tapping the side of the plate.</li>
		<li>Inactivate the enzyme by diluting the sample 1:1 in DMEM supplemented with 10% fetal bovine serum (FBS) and 1% antibiotics.</li>
		<li>Split the cell suspension into 2 wells and add 3 mL of basal medium (DMEM supplemented with 10 % FBS and 1 % antibiotics). Incubate overnight at 37 &#176;C with 5% CO2.</li>
		<li>Change medium the next day, then every 2 days until 90% confluence.</li>
		<li>Repeat the process until the third passage and proceed to phenotype and functional characterization. 
		NOTE: Always observe the morphology of the cells under the inverted microscope, changing from round to fibroblast-like.</li>
	</ol>
	</li>
	<li>Adipose tissue-derived stem cells (ADSCs) characterization
	<ol>
		<li>Phenotypic characterization by flow cytometry
		<ol>
			<li>Detach the cells using Trypsin/EDTA, as described in steps 2.3.1 to 2.3.2.</li>
			<li>Collect the cells in a conical tube (50 mL) and centrifuge at 250 x g for 10 min at 4 &#176;C. Discard the supernatant and resuspend the pellet in 1 mL of PBS.</li>
			<li>Count the cells as described in step 2.2.4 and seed 0.5-1 x 106 cells in 100 &#181;L of PBS in a 96 well-plate. 
			NOTE: The number of wells will depend on the color of the fluorochrome conjugate and the filters/lasers of the cytometer.</li>
			<li>Add antibodies (Table 1) diluted in 1% BSA in PBS. 
			NOTE: It is not necessary to use Fc block to avoid nonspecific binding because we already use BSA to dilute antibodies. Reserve a sample of cells without receiving antibodies that will be used as a control of staining. The antibodies can be combined in the same well according to the fluorochrome dye and cytometer available in the lab. All the antibodies described in Table 1 can be added in the same well, except the CD71 FITC and CD29 FITC, which must be in different wells because of the same fluorochrome.</li>
			<li>Incubate the plate for 30 min at 4 &#176;C in the dark.</li>
			<li>Wash cells, then complete the volume to 200 &#181;L using PBS, centrifuge the plate at 252 x g for 10 min at 4 &#176;C, and discard the supernatant. Repeat this step one more time.</li>
			<li>Fix the cells by adding 200 &#181;L per well of 2% formaldehyde in PBS. Store the cells in the dark at 4 &#176;C until analysis in the flow cytometer. 
			NOTE: For best results, acquire the cells on the flow cytometer as soon as possible. The brightness of fluorescence of markers decays significantly after 48 h for most fluorochromes. So, do not exceed 48 h to read the plate. Acquisition of 30,000 events is recommended.</li>
			<li>Use the gating strategy presented in Figure 2B to select the ASC population.</li>
		</ol>
		</li>
		<li>Functional characterization: Osteogenic differentiation
		<ol>
			<li>Detach the cells using Trypsin/EDTA (as described in steps 2.3.1 to 2.3.2), collect and centrifuge the cells (as described in steps 2.4.1.2 and 2.4.1.2), and count them (as described in steps 2.2.4).</li>
			<li>Plate, in triplicate, 2 x 105 cells per well in 6-well plates in basal medial (DMEM supplemented with 10 % FBS and 1 % antibiotics); incubate at 37 &#176;C in 5% CO2. 
			NOTE: Two 6-well plates will be needed, one for each differentiation time (14 and 21 days).</li>
			<li>Next day, change the medium to osteogenic medium (step 1.4.1). 
			NOTE: reserve 3 wells being cultured only with the basal medium, which will be the control for differentiation.</li>
			<li>Culture cells for 14 and 21 days in osteogenic media and the control cells, changing media every 3 days. Proceed to Von Kossa staining (step 1.4.2) to assess the mineralized nodules at the end of each culture period.</li>
			<li>Aspirate the medium from each well and wash the cells twice with PBS. Fix the cells with 2 mL of 70% ethanol overnight at room temperature (RT). Wash the cells carefully in running water.</li>
			<li>Add 2 mL of 5% silver nitrate solution and incubate the plate in ultraviolet light for 1 h. Wash the cells with distilled water. Add 2 mL of 5% sodium thiosulfate, and incubate for 5 min. Wash with distilled water.</li>
			<li>Counterstain with 2 mL of eosin for 40 s. Wash with distilled water until the staining solution is removed, and visualize the staining using an optical microscope.</li>
		</ol>
		</li>
		<li>Functional characterization: Adipogenic differentiation
		<ol>
			<li>Detach the cells using Trypsin/EDTA (as described in steps 2.3.1 to 2.3.2), collect and centrifuge the cells (as described in steps 2.4.1.2 and 2.4.1.2), and count them (as described in steps 2.2.4).</li>
			<li>Plate 2 x 105 cells per well in 6-well plates in basal medial (DMEM supplemented with 10 % FBS and 1 % antibiotics); incubate at 37 &#176;C in 5% CO2. 
			NOTE: Two 6-well plates will be needed, one for each differentiation time (14 and 21 days).</li>
			<li>The next day, change the medium to adipogenic medium (step 2.5.1). 
			NOTE: Reserve 3 wells being cultured only with the basal medium as control.</li>
			<li>Culture cells for 14 and 21 days in adipogenic medium, changing media every 3 days. At the end of each culture period, proceed to Oil-Red O staining (steps 2.4.3.5-2.4.3.7), an indicator of intracellular lipid accumulation.</li>
			<li>Aspirate the media from each well. Wash the cells twice with PBS. Fix cells in 2 mL of 10% formalin for 1 h. Wash once with PBS, and then one time with water.</li>
			<li>Stain with 2 mL of Oil-Red O solution in 60% isopropanol for 5 min. Wash once with distilled water.</li>
			<li>Counterstain with 2 mL of 1% hematoxylin diluted 1:2 in distilled water for 1 min. Wash with distilled water until the staining solution is removed, and visualize the stained samples using an optical microscope.</li>
		</ol>
		</li>
		<li>Functional characterization: Chondrogenic differentiation
		<ol>
			<li>Detach the cells using Trypsin/EDTA (as described in steps 2.3.1 to 2.3.2), collect and centrifuge the cells (as described in steps 2.4.1.2 and 2.4.1.2), and count them (as described in steps 2.2.4).</li>
			<li>Place 5 x 105 ADSCs in four polypropylene conical tubes and centrifuge at 450 x g for 5 min to form a pellet. Discard the supernatant.</li>
			<li>Culture the pellets in a conical tube in a chondrogenic medium (step 1.6.1) or only basal medium (control of differentiation) for 14 and 21 days at 37 &#176;C in 5% CO2. Change medium every 3 days and avoid removing pellets. 
			NOTE: Each cell pellet refers to each culture time, as well as their respective controls grown only with basal medium.</li>
			<li>At the end of each culture time point, collect pellets using fine-tip tweezers and place them in a 24-well plate. Proceed for histological sectioning and staining of proteoglycans and glycosaminoglycans (steps 2.4.4.5.-2.4.4.9). 
			NOTE: Each pellet is processed in a separate well.</li>
			<li>Fix pellets in 2 mL of 10% buffered formaldehyde for 30 min. Discard the formaldehyde solution, and add 2 mL of 70% ethanol. Remove the pellet from the conical tube using a tip and embed the pellets in paraffin.</li>
			<li>Using a rotating paraffin microtome, make 5 &#181;m histological sections. Incubate the sections for 15 min at 60 &#176;C, and immerse them twice in xylene (for 5 and 15 min).</li>
			<li>Rehydrate the samples by immersing the histological sections in alcohol baths at decreasing concentrations (100%, 96%, 80%, and 70%) for 2 min each, then rinse with deionized water for 5 min.</li>
			<li>Proceed to stain the samples with Alcian blue 1% in acetic acid, pH 2.5, for 30 min.</li>
			<li>Counterstain with hematoxylin for 1 min, and wash with distilled water. Mount with DPX (mountant for histology) or other mount solution and visualize samples using an optical microscope.</li>
		</ol>
		</li>
	</ol>
	</li>
</ol>

Primary Culture of Adipose Tissue Derived Stem Cells from Mouse Epididymis

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I. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Mesenchymal+stem+cells.">Mesenchymal stem cells.</a> J Orthop Res. 9 (5), 641-650 (1991).</li><li>Pittenger, M., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Mesenchymal+stem+cell+perspective:+cell+biology+to+clinical+progress.">Mesenchymal stem cell perspective: cell biology to clinical progress.</a> npj Regen Med. 4, 22 (2019).</li><li>Lin, W., 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=Mesenchymal+stem+cells+and+cancer:+Clinical+challenges+and+opportunities.">Mesenchymal stem cells and cancer: Clinical challenges and opportunities.</a> BioMed Res Int. 2820853, 1-12 (2019).</li><li>Mazini, L., 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=Hopes+and+limits+of+adipose-derived+stem+cells+(ADSCs)+and+mesenchymal+stem+cells+(MSCs)+in+wound+healing.">Hopes and limits of adipose-derived stem cells (ADSCs) and mesenchymal stem cells (MSCs) in wound healing.</a> Int J Mol Sci. 21 (4), 1306 (2020).</li><li>Shi, Y., 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=Immunoregulatory+mechanisms+of+mesenchymal+stem+and+stromal+cells+in+inflammatory+diseases.">Immunoregulatory mechanisms of mesenchymal stem and stromal cells in inflammatory diseases.</a> Nat Rev Nephrol. 14 (8), 493-507 (2018).</li><li>Uccelli, A., 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=Mesenchymal+stem+cells+in+health+and+disease.">Mesenchymal stem cells in health and disease.</a> Nat Rev Immunol. 8 (9), 726-736 (2008).</li><li>Dong, J., 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=Human+adipose+tissue-derived+small+extracellular+vesicles+promote+soft+tissue+repair+through+modulating+M1-to-M2+polarization+of+macrophages.">Human adipose tissue-derived small extracellular vesicles promote soft tissue repair through modulating M1-to-M2 polarization of macrophages.</a> Stem Cell Res Ther. 14 (1), 67 (2023).</li><li>Maffioli, E., 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=Proteomic+analysis+of+the+secretome+of+human+bone+marrow-derived+mesenchymal+stem+cells+primed+by+pro-inflammatory+cytokines.">Proteomic analysis of the secretome of human bone marrow-derived mesenchymal stem cells primed by pro-inflammatory cytokines.</a> J. 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M., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Stem+cell-based+therapy+for+human+diseases.">Stem cell-based therapy for human diseases.</a> Signal Transduct Target Ther. 7 (1), 272 (2022).</li><li>Lee, R. H., 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=Characterization+and+expression+analysis+of+mesenchymal+stem+cells+from+human+bone+marrow+and+adipose+tissue.">Characterization and expression analysis of mesenchymal stem cells from human bone marrow and adipose tissue.</a> Cell Physiol Biochem. 14 (4-6), 311-324 (2004).</li><li>Strem, B. M., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Multipotential+differentiation+of+adipose+tissue+derived+stem+cells.">Multipotential differentiation of adipose tissue derived stem cells.</a> Keio J Med. 54 (3), 132-141 (2005).</li><li>Kern, S., 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=Comparative+analysis+of+mesenchymal+stem+cells+from+bone+marrow,+umbilical+cord+blood,+or+adipose+tissue.">Comparative analysis of mesenchymal stem cells from bone marrow, umbilical cord blood, or adipose tissue.</a> Stem Cells. 24 (5), 1294-1301 (2006).</li><li>Dominici, M. D., 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=Minimal+criteria+for+defining+multipotent+mesenchymal+stromal+cells.+The+International+Society+for+Cellular+Therapy+position+statement.">Minimal criteria for defining multipotent mesenchymal stromal cells. The International Society for Cellular Therapy position statement.</a> Cytotherapy. 8 (4), 315-317 (2006).</li><li>Berryman, D. E., 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=Growth+hormone's+effect+on+adipose+tissue:+Quality+versus+quantity.">Growth hormone's effect on adipose tissue: Quality versus quantity.</a> International Journal of Molecular Sciences. 18 (8), 1621 (2017).</li><li>Shomer, N. H., 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=Review+of+rodent+euthanasia+methods.">Review of rodent euthanasia methods.</a> J Am Assoc Lab Anim Sci. 59 (3), 242-253 (2020).</li><li>Miranda, V. H. S., 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=Liver+damage+in+schistosomiasis+is+reduced+by+adipose+tissue-derived+stem+cell+therapy+after+praziquantel+treatment.">Liver damage in schistosomiasis is reduced by adipose tissue-derived stem cell therapy after praziquantel treatment.</a> PLoS Negl Trop Dis. 14 (8), e0008635 (2020).</li><li>Li, H., 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=Isolation+and+characterization+of+primary+bone+marrow+mesenchymal+stromal+cells.">Isolation and characterization of primary bone marrow mesenchymal stromal cells.</a> Ann N Y Acad Sci. 1370 (1), 109-118 (2016).</li><li>Boregowda, S. V., 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=Isolation+of+mouse+bone+marrow+mesenchymal+stem+cells.">Isolation of mouse bone marrow mesenchymal stem cells.</a> Methods Mol Biol. 1416, 205-223 (2016).</li><li>Sreejit, P., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Generation+of+mesenchymal+stem+cell+lines+from+murine+bone+marrow.">Generation of mesenchymal stem cell lines from murine bone marrow.</a> Cell Tissue Res. 350 (1), 55-68 (2012).</li><li>Bunnell, B. A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Adipose+tissue-derived+mesenchymal+stem+cells.">Adipose tissue-derived mesenchymal stem cells.</a> Cells. 10 (12), 3433 (2021).</li></ol>

The authors have nothing to disclose.

The MSCs can be extracted from different tissues. Despite bone marrow representing a common source of MSCs in both murine and humans25,26, we have chosen to work with adipose tissue in this study because of its richness in MSCs, distribution in the body, and ease of accessing it. As an alternative, adipose-derived stem cells can be used to generate MSCs-like immortalized cells27. 
Some points of the extraction d...

Mesenchymal stem cells (MSCs) are adult multipotential cells differentiating into cells such as osteoblast, chondroblast, and adipocyte1,2. These cells reside in several organs, and because of that, they can be extracted from adult tissues such as bone marrow, muscle, fat, hair follicle, tooth root, placenta, dermis, perichondrium, umbilical cord, lung, liver, and spleen3,4.
The effects of MSCs on physiology and the immune system have been reported5,6. These cells have been promising for treating several diseases, both in human and veterinary medicine. The MSCs can control inflammation and promote angiogenesis and tissue homeostasis through different mechanisms, such as cell-cell contact, soluble factors, and small extracellular vesicles7,8,9,10. Furthermore, the MSCs are immune-privileged cells capable of surviving in immunologically incompatible allogeneic transplant recipients because these cells show low expression of class I major histocompatibility complex (MHC) molecules and are used in cell-based therapy for allogeneic transplant11,12. The low immunogenicity combined with the regenerative potential makes MSCs ideal candidates for cell therapy, such as graft-versus-host disease (GvHD)13, systemic lupus erythematosus (SLE)14, and multiple sclerosis15, among others16,17.
Despite the fact that MSCs reside in several adult tissues, the adipose tissue offers advantages over other sources, such as accessibility for harvesting, with minimal surgical intervention; large number of available cells with high expansion rate; and easy in vitro expansion using an easy-to-perform protocol without the need for specific equipment and low-cost materials18,19,20. Once extracted, the adipose tissue-derived stem cells (ADSCs) must be characterized as established by the International Society for Cellular Therapy (ISCT)21. Thus, MSCs must show morphology fibroblast-like, adherence to plastic culture, expressing a high percentage (&#8805;95%) of mesenchymal markers such as endoglin (CD105), ecto-5&#39;-nucleotidase (CD73) and Thy-1 (CD90), and low percentage (&#8804;2%) of hematopoietic markers such as leukocyte common antigen (CD45), transmembrane phosphoglycoprotein (CD34), glycolipid-anchored membrane glycoprotein (CD14), integrin alpha M (CD11b), B-cell antigen receptor complex-associated protein alpha chain (CD79&#945;) or B-lymphocyte surface antigen B4 (CD19) and class II human leukocyte antigen (HLA-II). Furthermore, a functional characterization is required, and the cells should be able to differentiate into osteoblast, chondroblast, or adipoblast cells21.
Here, we show how to obtain the MSCs from epididymal adipose tissue using mechanical dissociation and enzymatic digestion for in vitro studies and the morphological characterization preconized by ISCT.

<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>140 &#176;C High Heat Sterilization CO2 Incubator</td>
			<td>RADOBIO SCIENTIFIC CO. LTD, China</td>
			<td>C180</td>
			<td></td>
		</tr>
		<tr>
			<td>3-Isobutyl-1-methylxanthine</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>I7018</td>
			<td></td>
		</tr>
		<tr>
			<td>Acetic acid glacial</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>PHR1748</td>
			<td></td>
		</tr>
		<tr>
			<td>Alcian Blue 8GX</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>A9186</td>
			<td>BioReagent, suitable for detection of glycoproteins. 1% in acetic acid, pH 2.5</td>
		</tr>
		<tr>
			<td>Alcohol 70%</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>65350-M</td>
			<td>70% in water</td>
		</tr>
		<tr>
			<td>Amphotericin B</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>PHR1662</td>
			<td></td>
		</tr>
		<tr>
			<td>Antibodies anti-mouse anti-CD29 FITC (Clone Ha2/5)</td>
			<td>BD Biosciences, San Diego, CA, USA</td>
			<td>555005</td>
			<td>Functions in the cell: Adhesion and activation, embryogenesis, Leukocytes, DC, platelets, mast cells, fibroblasts and endothelial cells</td>
		</tr>
		<tr>
			<td>Antibodies anti-mouse anti-CD34 PE (Clone RAM34)</td>
			<td>BD Biosciences, San Diego, CA, USA</td>
			<td>551387</td>
			<td>Functions in the cell: Cell adhesion factor. Hematopoietic stem cells</td>
		</tr>
		<tr>
			<td>Antibodies anti-mouse anti-CD45 APC (Clone 30-F11)</td>
			<td>BD Biosciences, San Diego, CA, USA</td>
			<td>559864</td>
			<td>Functions in the cell: Assists in the activation of leukocytes</td>
		</tr>
		<tr>
			<td>Antibodies anti-mouse anti-CD71 FITC (Clone C2)</td>
			<td>BD Biosciences, San Diego, CA, USA</td>
			<td>553266</td>
			<td>Functions in the cell: Controls iron uptake during cell proliferation. Proliferating cells, reticulocytes and precursors</td>
		</tr>
		<tr>
			<td>Antibodies anti-mouse anti-CD90 PerCP (Clone OX-7)</td>
			<td>BD Biosciences, San Diego, CA, USA</td>
			<td>557266</td>
			<td>Functions in the cell: Signaling, adhesion. T lymphocyte, NK, monocyte, HSC, neuron, fibroblast</td>
		</tr>
		<tr>
			<td>Ascorbic acid</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>PHR1008</td>
			<td></td>
		</tr>
		<tr>
			<td>Automatic pipettes</td>
			<td>Thermo Fisher Scientific, Waltham, Massachusetts, USA</td>
			<td>4700850N</td>
			<td>Finnpipette F1 Good Laboratory Pipetting (GLP) Kits</td>
		</tr>
		<tr>
			<td>Beaker</td>
			<td>Not applicable</td>
			<td></td>
			<td>1 unit</td>
		</tr>
		<tr>
			<td>Bovine serum albumin</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>A7906</td>
			<td></td>
		</tr>
		<tr>
			<td>Cell culture plates (6-well)</td>
			<td>Merck, Darmstadt, Germany</td>
			<td>Z707759</td>
			<td>07 units sterile. TPP tissue culture plates</td>
		</tr>
		<tr>
			<td>Cell culture plates (96-well. Round or V bottom)</td>
			<td>Merck, Darmstadt, Germany</td>
			<td>CLS353077</td>
			<td>01 unit sterile. Wells, 96, Tissue Culture (TC)-treated surface, round bottom clear wells, sterile</td>
		</tr>
		<tr>
			<td>Chondrogenic medium</td>
			<td>Stem Pro Chondrogenesis Differentiation&#8211;Life Technologies</td>
			<td>A1007101</td>
			<td>TGF-&#946;2, TGF-&#946;3, dexamethasone, insulin, transferrin, ITS, sodium-l - ascorbate, sodium pyruvate, ascorbate-2-phosphate</td>
		</tr>
		<tr>
			<td>Collagenase type II</td>
			<td>Life Technologies, California, USA</td>
			<td>17101015</td>
			<td></td>
		</tr>
		<tr>
			<td>cork or styrofoam board covered with aluminum</td>
			<td>Not applicable</td>
			<td></td>
			<td>1 unit</td>
		</tr>
		<tr>
			<td>cotton</td>
			<td>Not applicable</td>
			<td></td>
			<td>50 g</td>
		</tr>
		<tr>
			<td>Dexamethasone</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>D4902</td>
			<td></td>
		</tr>
		<tr>
			<td>Dissecting scissor</td>
			<td>Not applicable</td>
			<td></td>
			<td>03 units sterile</td>
		</tr>
		<tr>
			<td>DPX Mountant for histology</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>6522</td>
			<td></td>
		</tr>
		<tr>
			<td>Dulbecco&#8217;s modified Eagle&#8217;s medium (DMEM)</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>D5523</td>
			<td>With 1000 mg/L glucose and L-glutamine, without sodium bicarbonate, powder, suitable for cell culture</td>
		</tr>
		<tr>
			<td>Eosin B</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>861006</td>
			<td></td>
		</tr>
		<tr>
			<td>Fetal bovine serum (FBS)</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>F4135</td>
			<td></td>
		</tr>
		<tr>
			<td>Formaldehyde</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>47608</td>
			<td></td>
		</tr>
		<tr>
			<td>Formalin</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>HT501128</td>
			<td></td>
		</tr>
		<tr>
			<td>Gentamicin</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>G1397</td>
			<td></td>
		</tr>
		<tr>
			<td>Hematoxylin</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>H3136</td>
			<td></td>
		</tr>
		<tr>
			<td>Hypodermic Needle (0.3mm x 13mm)</td>
			<td>Not applicable</td>
			<td></td>
			<td>5 units</td>
		</tr>
		<tr>
			<td>Indomethacin</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>I0200000</td>
			<td></td>
		</tr>
		<tr>
			<td>Insulin</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>I3536</td>
			<td></td>
		</tr>
		<tr>
			<td>Isopropanol</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>563935</td>
			<td>70% in H2O</td>
		</tr>
		<tr>
			<td>Ketamine-D4 hydrochloride solution</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>K-006</td>
			<td>1.0 mg/mL in methanol (as free base), certified reference material, Cerilliant&#174;</td>
		</tr>
		<tr>
			<td>Neubauer chamber</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>BR718620</td>
			<td>BRAND counting chamber BLAUBRAND Neubauer pattern. With clips, double ruled</td>
		</tr>
		<tr>
			<td>Nichiryo pipette tips (0.1&#8211;10 &#956;L)</td>
			<td>Merck, Darmstadt, Germany</td>
			<td>Z645540</td>
			<td>Volume range 0.1&#8211;10 &#956;L, elongated, bulk pack. Sterile</td>
		</tr>
		<tr>
			<td>Nichiryo pipette tips (1&#8211;10 mL)</td>
			<td>Merck, Darmstadt, Germany</td>
			<td>Z717401</td>
			<td>Volume range 1&#8211;10 mL, universal, bulk pack. Sterile</td>
		</tr>
		<tr>
			<td>Nichiryo pipette tips (200 &#956;L)</td>
			<td>Merck, Darmstadt, Germany</td>
			<td>Z645516</td>
			<td>Maximum volume 200 &#956;L, graduated, ministack. Sterile</td>
		</tr>
		<tr>
			<td>Oil-Red O solution</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>O1391</td>
			<td>0.5% in isopropanol</td>
		</tr>
		<tr>
			<td>Paraffin</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>107.151</td>
			<td>46&#8211;48, in block form</td>
		</tr>
		<tr>
			<td>Penicillin/Streptomycin</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>P4333</td>
			<td>Solution stabilized, with 10,000 units penicillin and 10 mg streptomycin/mL, 0.1 &#956;m filtered, BioReagent, suitable for cell culture</td>
		</tr>
		<tr>
			<td>Phosphate-buffered saline solution 1x (PBS).</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>P3813</td>
			<td>Powder, pH 7.4, for preparing 1 L solutions. Balanced and sterile</td>
		</tr>
		<tr>
			<td>Polypropylene conical tubes (15 mL)</td>
			<td>Falcon, Fisher Scientific</td>
			<td>14-959-53A</td>
			<td>Sterile</td>
		</tr>
		<tr>
			<td>Polypropylene conical tubes (50 mL)</td>
			<td>Falcon, Fisher Scientific</td>
			<td>14-432-22</td>
			<td>2 units sterile</td>
		</tr>
		<tr>
			<td>scalpel (optional)</td>
			<td>Not applicable</td>
			<td></td>
			<td>1 unit</td>
		</tr>
		<tr>
			<td>Silver nitrate</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>85228</td>
			<td></td>
		</tr>
		<tr>
			<td>Sodium thiosulfate</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>72049</td>
			<td></td>
		</tr>
		<tr>
			<td>Surgical tweezer (15 cm)</td>
			<td>Not applicable</td>
			<td></td>
			<td>3 units sterile</td>
		</tr>
		<tr>
			<td>Swiss male mice (6&#8211;8 weeks)</td>
			<td>Bioterium, Santa Cruz State University</td>
			<td>021/22</td>
			<td></td>
		</tr>
		<tr>
			<td>syringe (1 mL)</td>
			<td>Not applicable</td>
			<td></td>
			<td>1 unit</td>
		</tr>
		<tr>
			<td>Trypan Blue Dye</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>T8154</td>
			<td>0.4%, liquid, sterile-filtered, suitable for cell culture</td>
		</tr>
		<tr>
			<td>Trypsin/EDTA (ethylenediaminetetraacetic acid)</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>T3924</td>
			<td></td>
		</tr>
		<tr>
			<td>Xylazine</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>PHR3263</td>
			<td></td>
		</tr>
		<tr>
			<td>&#946;-glycerophosphate disodium salt hydrate</td>
			<td>Sigma-Aldrich, San Luis, Missouri, USA</td>
			<td>G9422</td>
			<td>BioUltra, suitable for cell culture, suitable for plant cell culture, &#8805;99% (titration)</td>
		</tr>
	</tbody>
</table>

isolation, in vitro expansion, and characterization of mesenchymal stem cells from mouse epididymal adipose tissue

Mesenchymal stem cells (MSCs) have been extensively studied as a new therapeutic approach, mainly to stop exacerbated inflammation due to their potential to modulate the immune response. The MSCs are immune-privileged cells capable of surviving in immunologically incompatible allogeneic transplant recipients based on low expression of class I major histocompatibility complex (MHC) molecules and in the use of cell-based therapy for allogeneic transplant. These cells can be isolated from several tissues, the most commonly used being the bone marrow and adipose tissues. We provide an easy protocol to isolate, culture, and characterize MSCs from epididymal adipose tissue of mice. The epididymal adipose tissue is surgically excised, physically fragmented, and digested with 0.15% collagenase type II solution. Then, primary adipose tissue-derived stem (ADSCs) cells are cultured and expanded in vitro, and the phenotypic characterization is performed by flow cytometry. We also provide the steps to differentiate the ADSCs into osteogenic, adipogenic, and chondrogenic cells, followed by functional characterization of each cell lineage. The protocol provided here can be used for in vivo and ex vivo experiments, and as an alternative, the adipose-derived stem cells can be used to generate MSCs-like immortalized cells.

Cells extracted from adipose tissue according to the protocol presented here showed morphology matching the minimal criteria for MSCs proposed by ISCT. An overview of the protocol is shown in Figure 1. Phenotypically, ADSCs showed adherence to plastic and fibroblast-like morphology in the first days of cell culture (Figure 2A). In addition, they grew homogeneously and formed colonies. Furthermore, ADSCs showed low expression of CD34 (2.12%) and CD45 (1.81%), bot...

Read this Scientific Article Protocol about Author Spotlight: Advancing Treatment Approaches with Adipose-Derived Stem Cells at JoVE.com

Author Spotlight: Advancing Treatment Approaches with Adipose-Derived Stem Cells

The adipose tissue is an excellent source of mesenchymal stem cells. Here, we bring the step-by-step extraction, cultivation, and characterization of adipose tissue-derived stem cells (ADSCs) from Swiss mice epididymal adipose tissue.

Isolation, In Vitro Expansion, and Characterization of Mesenchymal Stem Cells from Mouse Epididymal Adipose Tissue

Mesenchymal stem cells (MSCs) have been extensively studied as a new therapeutic approach, mainly to stop exacerbated inflammation due to their potential ...

isolation-vitro-expansion-characterization-mesenchymal-stem-cells

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591 Views.  State University of Santa Cruz - UESC. The adipose tissue is an excellent source of mesenchymal stem cells. Here, we bring the step-by-step extraction, cultivation, and characterization of adipose tissue-derived stem cells (ADSCs) from Swiss mice epididymal adipose tissue. 

Video: Author Spotlight: Advancing Treatment Approaches with Adipose-Derived Stem Cells

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 &#38; Characterization of Hoechstlow CD45negative Mouse Lung Mesenchymal Stem Cells

Tissue resident mesenchymal stem cells (MSC) are important regulators of tissue repair or regeneration, fibrosis, inflammation, angiogenesis and tumor formation. Taken together these studies suggest that resident lung MSC play a role during pulmonary tissue homeostasis, injury and repair during diseases such as pulmonary fibrosis (PF) and arterial hypertension (PAH). Here we describe a technology to define a population of resident lung MSC. The definition of this population in vivo pulmonary tissue using a define set of markers facilitates the repeated isolation of a well-characterized stem cell population by flow cytometry and the study of a specific cell type and function.

Isolation & Characterization of Hoechstlow CD45negative Mouse Lung Mesenchymal Stem Cells

In this article we demonstrate the isolation of murine resident lung mesenchymal stem cells (lung MSC), their expansion, characterization and analysis of immunomodulatory properties.

Tissue resident mesenchymal stem cells (MSC) are important regulators of tissue repair or regeneration, fibrosis, inflammation, angiogenesis and tumor ...

Isolation of CD133+ Liver Stem Cells for Clonal Expansion

Liver stem cell, or oval cells, proliferate during chronic liver injury, and are proposed to differentiate into both hepatocytes and cholangiocytes. In addition, liver stem cells are hypothesized to be the precursors for a subset of liver cancer, Hepatocellular carcinoma. One of the primary challenges to stem cell work in any solid organ like the liver is the isolation of a rare population of cells for detailed analysis. For example, the vast majority of cells in the liver are hepatocytes (parenchymal fraction), which are significantly larger than non-parenchymal cells. By enriching the specific cellular compartments of the liver (i.e. parenchymal and non-parenchymal fractions), and selecting for CD45 negative cells, we are able to enrich the starting population of stem cells by over 600-fold.The proceduresdetailed in this report allow for a relatively rare population of cells from a solid organ to be sorted efficiently. This process can be utilized to isolateliver stem cells from normal murine liver as well as chronic liver injury models, which demonstrate increased liver stem cell proliferation. This method has clear advantages over standard immunohistochemistry of frozen or formalin fixed liver as functional studies using live cells can be performed after initial co-localization experiments. To accomplish the procedure outlined in this report, a working relationship with a research based flow-cytometry core is strongly encouraged as the details of FACS isolation are highly dependent on specialized instrumentation and a strong working knowledge of basic flow-cytometry procedures. The specific goal of this process is to isolate a population of liver stem cells that can be clonally expanded in vitro.

Here we describe the isolation of CD133 expressing liver stem cells and cancer stem cells from whole murine liver, a process that requires tissue digestion, cell enrichment, and flow cytometry isolation. We include methods for advanced single cell isolation and clonal expansion.

Liver stem cell, or oval cells, proliferate during chronic liver injury, and are proposed to differentiate into both hepatocytes and cholangiocytes. In ...

Generation of Mice Derived from Induced Pluripotent Stem Cells

The production of induced pluripotent stem cells (iPSCs) from somatic cells provides a means to create valuable tools for basic research and may also produce a source of patient-matched cells for regenerative therapies. iPSCs may be generated using multiple protocols and derived from multiple cell sources. Once generated, iPSCs are tested using a variety of assays including immunostaining for pluripotency markers, generation of three germ layers in embryoid bodies and teratomas, comparisons of gene expression with embryonic stem cells (ESCs) and production of chimeric mice with or without germline contribution2. Importantly, iPSC lines that pass these tests still vary in their capacity to produce different differentiated cell types2. This has made it difficult to establish which iPSC derivation protocols, donor cell sources or selection methods are most useful for different applications.
The most stringent test of whether a stem cell line has sufficient developmental potential to generate all tissues required for survival of an organism (termed full pluripotency) is tetraploid embryo complementation (TEC)3-5. Technically, TEC involves electrofusion of two-cell embryos to generate tetraploid (4n) one-cell embryos that can be cultured in vitro to the blastocyst stage6. Diploid (2n) pluripotent stem cells (e.g. ESCs or iPSCs) are then injected into the blastocoel cavity of the tetraploid blastocyst and transferred to a recipient female for gestation (see Figure 1). The tetraploid component of the complemented embryo contributes almost exclusively to the extraembryonic tissues (placenta, yolk sac), whereas the diploid cells constitute the embryo proper, resulting in a fetus derived entirely from the injected stem cell line.
Recently, we reported the derivation of iPSC lines that reproducibly generate adult mice via TEC1. These iPSC lines give rise to viable pups with efficiencies of 5-13%, which is comparable to ESCs3,4,7 and higher than that reported for most other iPSC lines8-12. These reports show that direct reprogramming can produce fully pluripotent iPSCs that match ESCs in their developmental potential and efficiency of generating pups in TEC tests. At present, it is not clear what distinguishes between fully pluripotent iPSCs and less potent lines13-15. Nor is it clear which reprogramming methods will produce these lines with the highest efficiency. Here we describe one method that produces fully pluripotent iPSCs and "all- iPSC" mice, which may be helpful for investigators wishing to compare the pluripotency of iPSC lines or establish the equivalence of different reprogramming methods.

Generating induced pluripotent stem cell (iPSC) lines produces lines of differing developmental potential even when they pass standard tests for pluripotency. Here we describe a protocol to produce mice derived entirely from iPSCs, which defines the iPSC lines as possessing full pluripotency1.

The production of induced pluripotent stem cells (iPSCs) from somatic cells provides a means to create valuable tools for basic research and may also ...

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 ...

Manual Isolation of Adipose-derived Stem Cells from Human Lipoaspirates

In 2001, researchers at the University of California, Los Angeles, described the isolation of a new population of adult stem cells from liposuctioned adipose tissue that they initially termed Processed Lipoaspirate Cells or PLA cells. Since then, these stem cells have been renamed as Adipose-derived Stem Cells or ASCs and have gone on to become one of the most popular adult stem cells populations in the fields of stem cell research and regenerative medicine. Thousands of articles now describe the use of ASCs in a variety of regenerative animal models, including bone regeneration, peripheral nerve repair and cardiovascular engineering. Recent articles have begun to describe the myriad of uses for ASCs in the clinic. The protocol shown in this article outlines the basic procedure for manually and enzymatically isolating ASCs from large amounts of lipoaspirates obtained from cosmetic procedures. This protocol can easily be scaled up or down to accommodate the volume of lipoaspirate and can be adapted to isolate ASCs from fat tissue obtained through abdominoplasties and other similar procedures.

In 2001, researchers at UCLA described the isolation of a population of adult stem cells, termed Adipose-derived Stem Cells or ASCs, from adipose tissue. This article outlines the isolation of ASCs from lipoaspirates using a manual, enzymatic digestion protocol using collagenase.

In 2001, researchers at the University of  California, Los Angeles, described the isolation of a new population of adult  stem cells from liposuctioned ...

Isolation and Culture of Dental Epithelial Stem Cells from the Adult Mouse Incisor

Understanding the cellular and molecular mechanisms that underlie tooth regeneration and renewal has become a topic of great interest1-4, and the mouse incisor provides a model for these processes. This remarkable organ grows continuously throughout the animal&#39;s life and generates all the necessary cell types from active pools of adult stem cells housed in the labial (toward the lip) and lingual (toward the tongue) cervical loop (CL) regions. Only the dental stem cells from the labial CL give rise to ameloblasts that generate enamel, the outer covering of teeth, on the labial surface. This asymmetric enamel formation allows abrasion at the incisor tip, and progenitors and stem cells in the proximal incisor ensure that the dental tissues are constantly replenished. The ability to isolate and grow these progenitor or stem cells in vitro allows their expansion and opens doors to numerous experiments not achievable in vivo, such as high throughput testing of potential stem cell regulatory factors. Here, we describe and demonstrate a reliable and consistent method to culture cells from the labial CL of the mouse incisor.

The continuously growing mouse incisor provides a model for studying renewal of dental tissues from dental epithelial stem cells (DESCs). A robust system for consistently and reliably obtaining these cells from the incisor and expanding them in vitro is reported here.

Understanding the cellular and molecular mechanisms that underlie tooth regeneration and renewal has become a topic of great interest1-4, and the mouse ...

Isolation, Characterization, and Differentiation of Cardiac Stem Cells from the Adult Mouse Heart

Myocardial infarction (MI) is a leading cause of morbidity and mortality around the world. A major goal of regenerative medicine is to replenish the dead myocardium after MI. Although several strategies have been used to regenerate myocardium, stem cell therapy remains a major approach to replenish the dead myocardium of an MI heart. Accumulating evidence suggests the presence of resident cardiac stem cells (CSCs) in the adult heart and their endocrine and/or paracrine effects on cardiac regeneration. However, CSC isolation and their characterization and differentiation toward myocardial cells, especially cardiomyocytes, remains a technical challenge. In the present study, we provided a simple method for the isolation, characterization, and differentiation of CSCs from the adult mouse heart. Here, we describe a density gradient method for the isolation of CSCs, where the heart is digested by a 0.2% collagenase II solution. To characterize the isolated CSCs, we evaluated the expression of CSCs/cardiac markers Sca-1, NKX2-5, and GATA4, and pluripotency/stemness markers OCT4, SOX2, and Nanog. We also determined the proliferation potential of isolated CSCs by culturing them in a Petri dish and assessing the expression of the proliferation marker Ki-67. For evaluating the differentiation potential of CSCs, we selected seven- to ten-days cultured CSCs. We transferred them to a new plate with a cardiomyocyte differentiation medium. They are incubated in a cell culture incubator for 12 days, while the differentiation medium is changed every three days. The differentiated CSCs express cardiomyocyte-specific markers: actinin and troponin I. Thus, CSCs isolated with this protocol have stemness and cardiac markers, and they have a potential for proliferation and differentiation toward cardiomyocyte lineage.

The overall goal of this article is to standardize the protocol for the isolation, characterization, and differentiation of cardiac stem cells (CSCs) from the adult mouse heart. Here, we describe a density gradient centrifugation method to isolate murine CSCs and elaborated methods for CSC culture, proliferation, and differentiation into cardiomyocytes.

Myocardial infarction (MI) is a leading cause of morbidity and mortality around the world. A major goal of regenerative medicine is to replenish the dead ...

Human Adipose Tissue Micro-fragmentation for Cell Phenotyping and Secretome Characterization

In the past decade, adipose tissue transplants have been widely used in plastic surgery and orthopaedics to enhance tissue repletion and/or regeneration. Accordingly, techniques for harvesting and processing human adipose tissue have evolved in order to quickly and efficiently obtain large amounts of tissue. Among these, the closed system technology represents an innovative and easy-to-use system to harvest, process, and re-inject refined fat tissue in a short time and in the same intervention (intra-operatively). Adipose tissue is collected by liposuction, washed, emulsified, rinsed and minced mechanically into cell clusters of 0.3 to 0.8 mm. Autologous transplantation of mechanically fragmented adipose tissue has shown remarkable efficacy in different therapeutic indications such as aesthetic medicine and surgery, orthopedic and general surgery. Characterization of micro-fragmented adipose tissue revealed the presence of intact small vessels within the adipocyte clusters; hence, the perivascular niche is left unperturbed. These clusters are enriched in perivascular cells (i.e., mesenchymal stem cell (MSC) ancestors) and in vitro analysis showed an increased release of growth factors and cytokines involved in tissue repair and regeneration, compared to enzymatically derived MSCs. This suggests that the superior therapeutic potential of microfragmented adipose tissue is explained by a higher frequency of presumptive MSCs and enhanced secretory activity. Whether these added pericytes directly contribute to higher growth factor and cytokine production is not known. This clinically approved procedure allows the transplantation of presumptive MSCs without the need for expansion and/or enzymatic treatment, thus bypassing the requirements of GMP guidelines, and reducing the costs for cell-based therapies.

Here, we present human adipose tissue enzyme-free micro-fragmentation using a closed system device. This new method allows the obtainment of sub-millimeter clusters of adipose tissue suitable for in vivo transplantation, in vitro culture, and further cell isolation and characterization.

In the past decade, adipose tissue transplants have been widely used in plastic surgery and orthopaedics to enhance tissue repletion and/or regeneration. ...