National Key R&#38;D Program of China (2018YFC1312504), National Natural Science Foundation of China (81970378, 81670360, 81870293), and Science and Technology Commission of Shanghai Municipality (17411971000, 17140902402) provided the funds for this study.

The animal protocol has been reviewed and approved by the Animal Care Committee of Shanghai Jiao Tong University.
1. Generation of Wnt-1 Cre+/-;Rosa26RFP/+ Mice
<ol>
	<li>Cross Wnt-1 Cre+/- mice16 with Rosa26RFP/+ mice18 to generate Wnt-1 Cre+/-;Rosa26RFP/+ mice. House mice under a 12 h light/dark cycle in a pathogen-free facility at 25 &#176;C and 45% humidity until they are 4&#8211;8 weeks old.</li>
</ol>
2. Dissection of the PAAT
NOTE: See Figure 1.
<ol>
	<li>Sterilize all surgical tools (e.g., surgical scissors, standard forceps, and microsurgical scissors and forceps) by autoclaving at 121 &#176;C for 30 min.</li>
	<li>Prepare the digestion medium (High glucose Dulbecco&#39;s Modified Eagle Medium [HDMEM] containing 2 mg/mL collagenase type I). Prepare the culture medium (HDMEM containing 10% fetal bovine serum [FBS] and 1% v/v penicillin-streptomycin [PS]). Sterilize using a 0.22 &#956;m syringe filter before use.</li>
	<li>Sterilize the cell culture reagents using UV, ethanol, filtration, or steam, as appropriate.</li>
	<li>Prepare a Petri dish with Hanks&#39; Balanced Saline Solution (HBSS) and a 15 mL conical tube with 10 mL of HBSS supplemented with 1% v/v of PS solution. Keep both on ice.</li>
	<li>Anesthetize the mice15 with isoflurane and sacrifice by cervical dislocation. Immerse the bodies in a beaker filled with 75% alcohol (200 mL) for 5 min to sterilize the skin surface.</li>
	<li>Snip and separate the skin on the abdomen and cut along the ventral midline from the pelvis to the neck. Open the abdomen and move the liver to expose the diaphragm19.</li>
	<li>Cut the diaphragm and the ribs on both sides of the midline and expose the heart and lungs by peeling back the ribs.</li>
	<li>Remove the lung and thymus and extract the PAAT along with the aorta and heart.</li>
	<li>Cut off the aorta at the aortic root to remove the heart. Make a cut between the aortic arch and descending aorta and carefully separate the adipose tissue surrounding both structures and the left and right common carotid arteries from the posterior chest wall. Transfer the tissue to the ice-cold HBSS buffer in the Petri dish.</li>
	<li>Using sterile forceps, remove as much of the vasculature (e.g., aorta, common carotid arteries, and other small vasculature) and fascia as possible, and transfer the adipose tissue into the 2 mL Eppendorf tubes contain 0.5 mL ice-cold HBSS buffer on ice.</li>
</ol>
3. Isolation of the SVF
Collect the PAAT of 5-6 mice into one 2 mL microcentrifuge tube containing 1 mL freshly prepared digestion medium and mince the tissue using surgical scissors in an Eppendorf tube at room temperature (RT).
<ol>
	<li>Transfer the mix into 50 mL tubes containing 9 mL of the digestion medium. Homogenize the tissues by pipetting up and down with a 1 mL pipette 10x.</li>
	<li>Incubate the tubes at 37 &#176;C with constant shaking at 100 rpm for 30&#8211;45 min and check every 5&#8211;10 min to prevent overdigestion. This is critical to improving cell viability and yield. 
	NOTE: Good tissue digestion will result in a homogenous, light yellow adipose tissue that is visible to the naked eye upon gently swirling the tube.</li>
	<li>Stop the digestion by adding 5 mL of HDMEM containing 10% FBS and 1% v/v PS at RT and mix well by pipetting.</li>
	<li>Centrifuge the cell suspension at 500 x g for 5 min at RT. The SVF will be visible as a brownish pellet. Carefully aspirate the floating adipocytes and decant the remaining supernatant without disturbing the SVF. Dissolve the SVF pellet in 10 mL of culture medium and filter through a 70 &#181;m cell strainer.</li>
	<li>Centrifuge the cell suspension at 500 x g for 5 min, remove the supernatant, and gently resuspend the pellet in 5 mL of erythrocyte lysis buffer in a 15 mL conical tube for 10 min at RT.</li>
	<li>Stop the reaction by adding 10 mL of 1x PBS containing 1% FBS. Centrifuge the cell suspension at 500 x g for 5 min at 4 &#176;C, remove the supernatant, and resuspend the pellet in 10 mL of 1x PBS containing 1% FBS.</li>
	<li>Centrifuge the cells again at 500 x g for 5 min at 4 &#176;C. Remove the supernatant and resuspend the pellet in 5 mL of culture medium in a 15 mL conical tube at 4 &#176;C.</li>
	<li>After a final round of centrifugation (500 x g for 5 min at 4 &#176;C), resuspend the pelleted cells in 5 mL of FACS buffer (PBS containing 10% FBS, 100 units/mL DNA I, and 1% v/v PS) on ice, and count the cells with a hemocytometer.</li>
</ol>
4. Isolation of NCADSCs by FACS
<ol>
	<li>Set up and optimize the cell sorter following the instruction manual. Select the 100 &#181;m nozzle, sterilize the collection tubes, install the required collection device, and set up the side streams20.</li>
	<li>A 561 nm yellow/green laser and optical filter 579/16 are recommended for sorting RFP+ cells. Perform the compensation using the negative control and the single-stained positive controls. See Figure 2A for the gating scheme.</li>
	<li>Filter the cells through a 40 &#181;m strainer, centrifuge at 500 x g for 5 min, and resuspend the cells in 2 mL of FACS buffer at a density of 0.5&#8211;1 x 107/mL. Transfer the cells to clearly labeled 5 mL round bottom polystyrene tubes, and load into the sorter.</li>
	<li>Run the experimental sample tube at 4 &#176;C, turn on the deflection plates, and sort into a 15 mL conical tube precoated with RPMI containing 1% FBS and 1% v/v PS. 
	NOTE: Protect the samples from strong light to minimize RFP quenching.</li>
</ol>
5. Culture of NCADSCs
<ol>
	<li>Plate the sorted cells at a density of 5,000 cells/cm2 in a 12 well culture plate in complete culture medium and incubate at 37 &#176;C in a humid atmosphere with 5% CO2 for 20&#8211;24 h.</li>
	<li>Remove the culture medium, wash the cells with prewarmed (37 &#176;C) PBS to remove cell debris and add fresh culture medium.</li>
	<li>Once the cells are 80&#8211;90% confluent, digest the monolayer using a 0.25% trypsin EDTA solution at 37 &#176;C in an incubator for 3&#8211;5 min, and neutralize with 2 mL of culture medium.</li>
	<li>Centrifuge the harvested cells for 15 min at 250 x g at RT, remove the supernatant, and resuspend the cells in 1 mL of culture medium. Count the cells with a hemocytometer.</li>
	<li>Seed the cells in a 12 well culture plate at the density of 5,000 cells/cm2.</li>
	<li>Resuspend the remaining cells in culture medium containing 10% DMSO, freeze, and store in liquid nitrogen.</li>
</ol>
6. Adipogenic Induction of NCADSCs
<ol>
	<li>Induce adipogenic differentiation of the NCADSCs at 80&#8211;90% confluency and standard culture conditions21.</li>
	<li>For brown adipogenic induction, first treat the cultured cells with brown adipogenic induction medium (HDMEM, 10% FBS, 1% v/v PS, 0.5 mM/L IBMX, 0.1&#956;M/L dexamethasone, 1 &#956;M/L rosiglitazone, 10 nmol/L triiodothyronine, and 1 &#956;g/mL insulin) for 2 days. Wash the cells with PBS 2x and replace with fresh medium (HDMEM, 10% FBS, 1% v/v PS, 1 &#956;M/L rosiglitazone, 10 nmol/L triiodothyronine, and 1 &#956;g/mL insulin). Change this medium every 2 days for a total of 3&#8211;5x.</li>
	<li>For white adipogenic induction, first treat the cells with white adipogenic induction medium (HDMEM, 10% FBS, 1% v/v PS, 0.5 mM/L IBMX, 0.1 &#956;M/L dexamethasone, and 1 &#956;g/mL insulin) for 2 days. Wash the cells with PBS 2x and replace with fresh medium (HDMEM, 10% FBS, 1% v/v PS, and 1 &#956;g/mL insulin). Change this medium every 2 days for a total of 3-5x.</li>
	<li>Analyze the adipogenic cells as appropriate. 
	NOTE: Be gentle when washing the cells with PBS. Differentiated adipocytes can easily wash away.</li>
</ol>

<ol>
	<li>Afshin, 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=Health+Effects+of+Overweight+and+Obesity+in+195+Countries+over+25+Years.">Health Effects of Overweight and Obesity in 195 Countries over 25 Years.</a> New England Journal of Medicine. 377 (1), 13-27 (2017).</li><li>Brown, N. K., 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=Perivascular+adipose+tissue+in+vascular+function+and+disease:+a+review+of+current+research+and+animal+models.">Perivascular adipose tissue in vascular function and disease: a review of current research and animal models.</a> Arteriosclerosis, Thrombosis, and Vascular Biology. 34 (8), 1621-1630 (2014).</li><li>Britton, K. 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=Prevalence,+distribution,+and+risk+factor+correlates+of+high+thoracic+periaortic+fat+in+the+Framingham+Heart+Study.">Prevalence, distribution, and risk factor correlates of high thoracic periaortic fat in the Framingham Heart Study.</a> Journal of the American Heart Association. 1 (6), 004200 (2012).</li><li>Police, S. B., Thatcher, S. E., Charnigo, R., Daugherty, A., Cassis, L. A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Obesity+promotes+inflammation+in+periaortic+adipose+tissue+and+angiotensin+II-induced+abdominal+aortic+aneurysm+formation.">Obesity promotes inflammation in periaortic adipose tissue and angiotensin II-induced abdominal aortic aneurysm formation.</a> Arteriosclerosis, Thrombosis, and Vascular Biology. 29 (10), 1458-1464 (2009).</li><li>Farmer, S. R. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Transcriptional+control+of+adipocyte+formation.">Transcriptional control of adipocyte formation.</a> Cell Metabolism. 4 (4), 263-273 (2006).</li><li>Aune, U. L., Ruiz, L., Kajimura, S. <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+differentiation+of+stromal+vascular+cells+to+beige/brite+cells.">Isolation and differentiation of stromal vascular cells to beige/brite cells.</a> Journal of Visualized Experiments. (73), e50191 (2013).</li><li>Ruan, H., Zarnowski, M. J., Cushman, S. W., Lodish, H. F. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Standard+isolation+of+primary+adipose+cells+from+mouse+epididymal+fat+pads+induces+inflammatory+mediators+and+down-regulates+adipocyte+genes.">Standard isolation of primary adipose cells from mouse epididymal fat pads induces inflammatory mediators and down-regulates adipocyte genes.</a> Journal of Biological Chemistry. 278 (48), 47585-47593 (2003).</li><li>Cinti, S. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Between+brown+and+white:+novel+aspects+of+adipocyte+differentiation.">Between brown and white: novel aspects of adipocyte differentiation.</a> Annals of Medicine. 43 (2), 104-115 (2011).</li><li>Van Harmelen, V., Rohrig, K., Hauner, H. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Comparison+of+proliferation+and+differentiation+capacity+of+human+adipocyte+precursor+cells+from+the+omental+and+subcutaneous+adipose+tissue+depot+of+obese+subjects.">Comparison of proliferation and differentiation capacity of human adipocyte precursor cells from the omental and subcutaneous adipose tissue depot of obese subjects.</a> Metabolism. 53 (5), 632-637 (2004).</li><li>Rodeheffer, M. S., Birsoy, K., Friedman, J. M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Identification+of+white+adipocyte+progenitor+cells+in+vivo.">Identification of white adipocyte progenitor cells in vivo.</a> Cell. 135 (2), 240-249 (2008).</li><li>Church, C. D., Berry, R., Rodeheffer, M. S. <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+study+of+adipocyte+precursors.">Isolation and study of adipocyte precursors.</a> Methods in Enzymology. 537, 31-46 (2014).</li><li>Chen, 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=Isolation+and+Differentiation+of+Adipose-Derived+Stem+Cells+from+Porcine+Subcutaneous+Adipose+Tissues.">Isolation and Differentiation of Adipose-Derived Stem Cells from Porcine Subcutaneous Adipose Tissues.</a> Journal of Visualized Experiments. (109), e53886 (2016).</li><li>Ye, 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=Developmental+and+functional+characteristics+of+the+thoracic+aorta+perivascular+adipocyte.">Developmental and functional characteristics of the thoracic aorta perivascular adipocyte.</a> Cellular and Molecular Life Sciences. 76 (4), 777-789 (2019).</li><li>Medeiros, D. M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=The+evolution+of+the+neural+crest:+new+perspectives+from+lamprey+and+invertebrate+neural+crest-like+cells.">The evolution of the neural crest: new perspectives from lamprey and invertebrate neural crest-like cells.</a> Wiley Interdisciplinary Reviews. Developmental Biology. 2 (1), 1-15 (2013).</li><li>Fu, 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=Neural+Crest+Cells+Differentiate+Into+Brown+Adipocytes+and+Contribute+to+Periaortic+Arch+Adipose+Tissue+Formation.">Neural Crest Cells Differentiate Into Brown Adipocytes and Contribute to Periaortic Arch Adipose Tissue Formation.</a> Arteriosclerosis, Thrombosis, and Vascular Biology. , (2019).</li><li>Danielian, P. S., Muccino, D., Rowitch, D. H., Michael, S. K., McMahon, A. P. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Modification+of+gene+activity+in+mouse+embryos+in+utero+by+a+tamoxifen-inducible+form+of+Cre+recombinase.">Modification of gene activity in mouse embryos in utero by a tamoxifen-inducible form of Cre recombinase.</a> Current Biology. 8 (24), 1323-1326 (1998).</li><li>Tamura, 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=Neural+crest-derived+stem+cells+migrate+and+differentiate+into+cardiomyocytes+after+myocardial+infarction.">Neural crest-derived stem cells migrate and differentiate into cardiomyocytes after myocardial infarction.</a> Arteriosclerosis, Thrombosis, and Vascular Biology. 31 (3), 582-589 (2011).</li><li>Madisen, 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=A+robust+and+high-throughput+Cre+reporting+and+characterization+system+for+the+whole+mouse+brain.">A robust and high-throughput Cre reporting and characterization system for the whole mouse brain.</a> Nature Neuroscience. 13 (1), 133-140 (2010).</li><li>Tan, P., Pepin, &. #. 2. 0. 1. ;., Lavoie, J. L. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Mouse+Adipose+Tissue+Collection+and+Processing+for+RNA+Analysis.">Mouse Adipose Tissue Collection and Processing for RNA Analysis.</a> Journal of Visualized Experiments. (131), e57026 (2018).</li><li>Basu, S., Campbell, H. M., Dittel, B. N., Ray, A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Purification+of+specific+cell+population+by+fluorescence+activated+cell+sorting+(FACS).">Purification of specific cell population by fluorescence activated cell sorting (FACS).</a> Journal of Visualized Experiments. (41), e1546 (2010).</li><li>Gupta, R. K., 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=Zfp423+expression+identifies+committed+preadipocytes+and+localizes+to+adipose+endothelial+and+perivascular+cells.">Zfp423 expression identifies committed preadipocytes and localizes to adipose endothelial and perivascular cells.</a> Cell Metabolism. 15 (2), 230-239 (2012).</li><li>Sowa, 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=Adipose+stromal+cells+contain+phenotypically+distinct+adipogenic+progenitors+derived+from+neural+crest.">Adipose stromal cells contain phenotypically distinct adipogenic progenitors derived from neural crest.</a> PLoS One. 8 (12), 84206 (2013).</li><li>Billo, N., 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=The+generation+of+adipocytes+by+the+neural+crest.">The generation of adipocytes by the neural crest.</a> Development. 134 (12), 2283-2292 (2007).</li><li>Thelen, K., Ayala-Lopez, N., Watts, S. W., Contreras, G. A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Expansion+and+Adipogenesis+Induction+of+Adipocyte+Progenitors+from+Perivascular+Adipose+Tissue+Isolated+by+Magnetic+Activated+Cell+Sorting.">Expansion and Adipogenesis Induction of Adipocyte Progenitors from Perivascular Adipose Tissue Isolated by Magnetic Activated Cell Sorting.</a> Journal of Visualized Experiments. (124), e55818 (2017).</li></ol>

The authors have nothing to disclose.

In this study, we present a reliable method for the isolation, culture, and adipogenic induction of NCADSCs extracted from the PVAT of Wnt-1 Cre+/-;Rosa26RFP/+ transgenic mice designed to produce RFP+ ADSCs. Previous reports show that there is no significant difference in the expression of general multipotent mesenchymal stem cells (MSCs) markers in NCADSCs and non NCADSCs22, and that NCADSCs have a strong potential to differentiate into adipocytes in vitro<sup cla...

The prevalence of obesity is increasing worldwide, which increases the risk of related chronic diseases, including cardiovascular disease and diabetes1. PVAT surrounds blood vessels and is a major source of endocrine and paracrine factors involved in vasculature function. Clinical studies show that high PVAT content is an independent risk factor of cardiovascular disease2,3, and its pathological function depends on the phenotype of the constituent adipose-derived stem cells (ADSCs)4.
Although ADSC cell lines like the murine 3T3-L1, 3T3-F442A, and OP9 are useful cellular models to study adipogenesis or lipogenesis5, regulatory mechanisms for adipogenesis differ between cell lines and primary cells. The ADSCs in the stromal vascular cell fraction (SVF) isolated directly from adipose tissues and induced to differentiate into adipocytes most likely recapitulate in vivo adipogenesis and lipogenesis6. However, the fragility, buoyancy, and the variations in size and immunophenotypes of the ADSCs make their direct isolation challenging. In addition, the different isolation procedures can also significantly affect the phenotype and adipogenic potential ability of these cells7, thus emphasizing the need for a protocol that maintains ADSC integrity.
Adipose tissue is typically classified as either the morphologically and functionally distinct white adipose tissue (WAT), or the brown adipose tissue (BAT)8, which harbors distinct ADSCs9. While ADSCs isolated from perigonadal and inguinal subcutaneous WATs have been characterized in previous studies9,10,11,12, less is known regarding the ADSCs from PVAT that is mainly composed of BAT13.
In a recent study, we found that a portion of the resident ADSCs in the periaortic arch adipose tissue (PAAT) are derived from neural crest cells (NCCs), a transient population of migratory progenitor cells that originate from the ectoderm14,15. Wnt1-Cre transgenic mice were used for tracing neural crest cell development16,17. We crossed Wnt1-Cre+ mice with Rosa26RFP/+ mice to generate Wnt-1 Cre+/-;Rosa26RFP/+ mice, in which NCCs and their descendants are labeled with red fluorescent protein (RFP) and are easily tracked in vivo and in vitro15. Here, we describe a method for isolating neural crest derived ADSCs (NC-derived ADSCs, or NCADSCs) from mouse PAAT and induce the NCADSCs to differentiate into white adipocytes or brown adipocytes.

<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>4% PFA</td>
			<td>BBI life sciences</td>
			<td>E672002-0500</td>
			<td>Lot #: EC11FA0001</td>
		</tr>
		<tr>
			<td>Agarose</td>
			<td>ABCONE (China)</td>
			<td>A47902</td>
			<td>1% working concentration</td>
		</tr>
		<tr>
			<td>Anti-cebp/&#945;</td>
			<td>ABclonal</td>
			<td>A0904</td>
			<td>1:1000 working concentration</td>
		</tr>
		<tr>
			<td>Anti-mouse IgG, HRP-linked</td>
			<td>CST</td>
			<td>7076</td>
			<td>1:5000 working concentration</td>
		</tr>
		<tr>
			<td>Anti-perilipin</td>
			<td>Abcam</td>
			<td>AB61682</td>
			<td>1 &#956;g/mL working concentration; lot #: GR66486-54</td>
		</tr>
		<tr>
			<td>Anti-PPARy</td>
			<td>SANTA CRUZ</td>
			<td>sc-7273</td>
			<td>0.2 &#956;g/mL working concentration</td>
		</tr>
		<tr>
			<td>Anti-rabbit IgG, HRP-linked</td>
			<td>CST</td>
			<td>7074</td>
			<td>1:5000 working concentration</td>
		</tr>
		<tr>
			<td>Anti-&#946;-Tubulin</td>
			<td>CST</td>
			<td>2146</td>
			<td>1:1000 working concentration</td>
		</tr>
		<tr>
			<td>BSA</td>
			<td>VWR life sciences</td>
			<td>0332-100G</td>
			<td>50 mg/mL working concentration; lot #: 0536C008</td>
		</tr>
		<tr>
			<td>Collagenase, Type I</td>
			<td>Gibco</td>
			<td>17018029</td>
			<td></td>
		</tr>
		<tr>
			<td>Dexamethasone</td>
			<td>Sigma-Aldrich</td>
			<td>D4902</td>
			<td>0.1 &#181;M working concentration</td>
		</tr>
		<tr>
			<td>Erythrocyte Lysis Buffer</td>
			<td>Invitrogen</td>
			<td>00-4333</td>
			<td></td>
		</tr>
		<tr>
			<td>FBS</td>
			<td>Corning</td>
			<td>R35-076-CV</td>
			<td>50 mg/mL working concentration; lot #: R2040212FBS</td>
		</tr>
		<tr>
			<td>HBSS</td>
			<td>Gibco</td>
			<td>14025092</td>
			<td></td>
		</tr>
		<tr>
			<td>HDMEM</td>
			<td>Gelifesciences</td>
			<td>SH30243.01</td>
			<td>Lot #: AD20813268</td>
		</tr>
		<tr>
			<td>IBMX</td>
			<td>Sigma-Aldrich</td>
			<td>I7018</td>
			<td>0.5 mM working concentration</td>
		</tr>
		<tr>
			<td>Insulin</td>
			<td>Sigma-Aldrich</td>
			<td>I3536</td>
			<td>1 &#956;g/mL working concentration</td>
		</tr>
		<tr>
			<td>Microsurgical forceps</td>
			<td>Suzhou Mingren Medical Equipment Co.,Ltd. (China)</td>
			<td>MR-F201A-1</td>
			<td></td>
		</tr>
		<tr>
			<td>Microsurgical scissor</td>
			<td>Suzhou Mingren Medical Equipment Co.,Ltd. (China)</td>
			<td>MR-H121A</td>
			<td></td>
		</tr>
		<tr>
			<td>Oil Red O solution</td>
			<td>Sigma-Aldrich</td>
			<td>O1516</td>
			<td>0.3% working concentration</td>
		</tr>
		<tr>
			<td>PBS (Phosphate buffered saline)</td>
			<td>ABCONE (China)</td>
			<td>P41970</td>
			<td></td>
		</tr>
		<tr>
			<td>Penicillin-Streptomycin</td>
			<td>Gibco</td>
			<td>15140122</td>
			<td></td>
		</tr>
		<tr>
			<td>PrimeScript RT reagent Kit</td>
			<td>TAKARA</td>
			<td>RR047A</td>
			<td>Lot #: AK4802</td>
		</tr>
		<tr>
			<td>RNeasy kit</td>
			<td>TAKARA</td>
			<td>9767</td>
			<td>Lot #: AHF1991D</td>
		</tr>
		<tr>
			<td>Rosa26RFP/+ mice</td>
			<td>JAX</td>
			<td>No.007909</td>
			<td>C57BL/6 backgroud; male and female</td>
		</tr>
		<tr>
			<td>Rosiglitazone</td>
			<td>Sigma-Aldrich</td>
			<td>R2408</td>
			<td>1 &#956;M working concentration</td>
		</tr>
		<tr>
			<td>Standard forceps</td>
			<td>Suzhou Mingren Medical Equipment Co.,Ltd. (China)</td>
			<td>MR-F424</td>
			<td></td>
		</tr>
		<tr>
			<td>Surgical scissor</td>
			<td>Suzhou Mingren Medical Equipment Co.,Ltd. (China)</td>
			<td>MR-S231</td>
			<td></td>
		</tr>
		<tr>
			<td>SYBR Premix Ex Taq</td>
			<td>TAKARA</td>
			<td>RR420A</td>
			<td>Lot #: AK9003</td>
		</tr>
		<tr>
			<td>Triiodothyronine</td>
			<td>Sigma-Aldrich</td>
			<td>T2877</td>
			<td>10 nM working concentration</td>
		</tr>
		<tr>
			<td>Wnt1-Cre+;PPAR&#947;flox/flox mice</td>
			<td>JAX</td>
			<td>No.009107</td>
			<td>C57BL/6 backgroud; male and female</td>
		</tr>
	</tbody>
</table>

isolation, culture, and adipogenic induction of neural crest original adipose-derived stem cells from periaortic adipose tissue

An excessive amount of adipose tissue surrounding the blood vessels (perivascular adipose tissue, also known as PVAT) is associated with a high risk of cardiovascular disease. ADSCs derived from different adipose tissues show distinct features, and those from the PVAT have not been well characterized. In a recent study, we reported that some ADSCs in the periaortic arch adipose tissue (PAAT) descend from the neural crest cells (NCCs), a transient population of migratory cells originating from the ectoderm.
In this paper, we describe a protocol for isolating red fluorescent protein (RFP)-labeled NCCs from the PAAT of Wnt-1 Cre+/-;Rosa26RFP/+ mice and inducing their adipogenic differentiation in vitro. Briefly, the stromal vascular fraction (SVF) is enzymatically dissociated from the PAAT, and the RFP+ neural crest derived ADSCs (NCADSCs) are isolated by fluorescence activated cell sorting (FACS). The NCADSCs differentiate into both brown and white adipocytes, can be cryopreserved, and retain their adipogenic potential for ~3&#8211;5 passages. Our protocol can generate abundant ADSCs from the PVAT for modeling PVAT adipogenesis or lipogenesis in vitro. Thus, these NCADSCs can provide a valuable system for studying the molecular switches involved in PVAT differentiation.

Using the protocol described above, we obtained ~0.5&#8211;1.0 x 106 ADSCs from 5&#8211;6 Wnt-1 Cre+/-;Rosa26RFP/+ mice (48 weeks old, male or female).
The flow chart of collection of PAAT from mice is presented in Figure 1. The morphology of the NCADSCs was similar to the ADSC from other mice adipose tissues. The cultured NCADSCs reached 80&#8211;90% confluency after 7&#8211;8 days of culture, and the NCADSCs had an expanded fibro...

Watch this Scientific Journal Video about Isolation, Culture, and Adipogenic Induction of Neural Crest Original Adipose-Derived Stem Cells from Periaortic Adipose Tissue at JoVE.com

Isolation, Culture, and Adipogenic Induction of Neural Crest Original Adipose-Derived Stem Cells from Periaortic Adipose Tissue

We present a protocol for the isolation, culture, and adipogenic induction of neural crest derived adipose-derived stem cells (NCADSCs) from the periaortic adipose tissue of Wnt-1 Cre+/-;Rosa26RFP/+ mice. The NCADSCs can be an easily accessible source of ADSCs for modeling adipogenesis or lipogenesis in vitro.

An excessive amount of adipose tissue surrounding the blood vessels (perivascular adipose tissue, also known as PVAT) is associated with a high risk of ...

isolation-culture-adipogenic-induction-neural-crest-original-adipose

Research

JoVE Journal

Developmental Biology

5.9K Views.  Shanghai Jiao Tong University. We present a protocol for the isolation, culture, and adipogenic induction of neural crest derived adipose-derived stem cells (NCADSCs) from the periaortic adipose tissue of Wnt-1 Cre+/-;Rosa26RFP/+ mice. The NCADSCs can be an easily accessible source of ADSCs for modeling adipogenesis or lipogenesis in vitro.

Video: Isolation, Culture, and Adipogenic Induction of Neural Crest Original Adipose-Derived Stem Cells from Periaortic Adipose Tissue

Isolation and Enrichment of Human Adipose-derived Stromal Cells for Enhanced Osteogenesis

Bone marrow-derived mesenchymal stromal cells (BM-MSCs) are considered the gold standard for stem cell-based tissue engineering applications. However, the process by which they must be harvested can be associated with significant donor site morbidity. In contrast, adipose-derived stromal cells (ASCs) are more readily abundant and more easily harvested, making them an appealing alternative to BM-MSCs. Like BM-MSCs, ASCs can differentiate into osteogenic lineage cells and can be used in tissue engineering applications, such as seeding onto scaffolds for use in craniofacial skeletal defects. ASCs are obtained from the stromal vascular fraction (SVF) of digested adipose tissue, which is a heterogeneous mixture of ASCs, vascular endothelial and mural cells, smooth muscle cells, pericytes, fibroblasts, and circulating cells. Flow cytometric analysis has shown that the surface marker profile for ASCs is similar to that for BM-MSCs. Despite several published reports establishing markers for the ASC phenotype, there is still a lack of consensus over profiles identifying osteoprogenitor cells in this heterogeneous population. This protocol describes how to isolate and use a subpopulation of ASCs with enhanced osteogenic capacity to repair critical-sized calvarial defects.

The transcriptional heterogeneity within human adipose-derived stromal cells can be defined on the single cell level using cell surface markers and osteogenic genes. We describe a protocol utilizing flow cytometry for the isolation of cell subpopulations with increased osteogenic potential, which may be used to enhance craniofacial skeletal reconstruction.

Bone marrow-derived mesenchymal stromal cells (BM-MSCs) are considered the gold standard for stem cell-based tissue engineering applications. However, the ...

Direct Induction of Human Neural Stem Cells from Peripheral Blood Hematopoietic Progenitor Cells

Human disease specific neuronal cultures are essential for generating in vitro models for human neurological diseases. However, the lack of access to primary human adult neural cultures raises unique challenges. Recent developments in induced pluripotent stem cells (iPSC) provides an alternative approach to derive neural cultures from skin fibroblasts through patient specific iPSC, but this process is labor intensive, requires special expertise and large amounts of resources, and can take several months. This prevents the wide application of this technology to the study of neurological diseases. To overcome some of these issues, we have developed a method to derive neural stem cells directly from human adult peripheral blood, bypassing the iPSC derivation process. Hematopoietic progenitor cells enriched from human adult peripheral blood were cultured in vitro and transfected with Sendai virus vectors containing transcriptional factors Sox2, Oct3/4, Klf4, and c-Myc. The transfection results in morphological changes in the cells which are further selected by using human neural progenitor medium containing basic fibroblast growth factor (bFGF) and vascular endothelial growth factor (VEGF). The resulting cells are characterized by the expression for neural stem cell markers, such as nestin and SOX2. These neural stem cells could be further differentiated to neurons, astroglia and oligodendrocytes in specified differentiation media. Using easily accessible human peripheral blood samples, this method could be used to derive neural stem cells for further differentiation to neural cells for in vitro modeling of neurological disorders and may advance studies related to the pathogenesis and treatment of those diseases.

A method was developed to directly derive human neural stem cells from hematopoietic progenitor cells enriched from peripheral blood cells.

Human disease specific neuronal cultures are essential for generating in vitro models for human neurological diseases. However, the lack of access to ...

Culturing Human Pluripotent and Neural Stem Cells in an Enclosed Cell Culture System for Basic and Preclinical Research

This paper describes how to use a custom manufactured, commercially available enclosed cell culture system for basic and preclinical research. Biosafety cabinets (BSCs) and incubators have long been the standard for culturing and expanding cell lines for basic and preclinical research. However, as the focus of many stem cell laboratories shifts from basic research to clinical translation, additional requirements are needed of the cell culturing system. All processes must be well documented and have exceptional requirements for sterility and reproducibility. In traditional incubators, gas concentrations and temperatures widely fluctuate anytime the cells are removed for feeding, passaging, or other manipulations. Such interruptions contribute to an environment that is not the standard for cGMP and GLP guidelines. These interruptions must be minimized especially when cells are utilized for therapeutic purposes. The motivation to move from the standard BSC and incubator system to a closed system is that such interruptions can be made negligible. Closed systems provide a work space to feed and manipulate cell cultures and maintain them in a controlled environment where temperature and gas concentrations are consistent. This way, pluripotent and multipotent stem cells can be maintained at optimum health from the moment of their derivation all the way to their eventual use in therapy.

Here is a protocol to grow pluripotent stem cells (PSC) and neural stem cells (NSC) in an enclosed cell culture system that permits maximum sterility and reproducibility, replacing the traditional biosafety cabinet and incubator. This equipment meets clinical good manufacturing practice (cGMP) and clinical good lab practice (cGLP) guidelines.

This paper describes how to use a custom manufactured, commercially available enclosed cell culture system for basic and preclinical research. Biosafety ...

Isolation and Differentiation of Adipose-Derived Stem Cells from Porcine Subcutaneous Adipose Tissues

Obesity is an unconstrained worldwide epidemic. Unraveling molecular controls in adipose tissue development holds promise to treat obesity or diabetes. Although numerous immortalized adipogenic cell lines have been established, adipose-derived stem cells from the stromal vascular fraction of subcutaneous white adipose tissues provide a reliable cellular system ex vivo much closer to adipose development in vivo. Pig adipose-derived stem cells (pADSC) are isolated from 7- to 9-day old piglets. The dorsal white fat depot of porcine subcutaneous adipose tissues is sliced, minced and collagenase digested. These pADSC exhibit strong potential to differentiate into adipocytes. Moreover, the pADSC also possess multipotency, assessed by selective stem cell markers, to differentiate into various mesenchymal cell types including adipocytes, osteocytes, and chondrocytes. These pADSC can be used for clarification of molecular switches in regulating classical adipocyte differentiation or in direction to other mesenchymal cell types of mesodermal origin. Furthermore, extended lineages into cells of ectodermal and endodermal origin have recently been achieved. Therefore, pADSC derived in this protocol provide an abundant and assessable source of adult mesenchymal stem cells with full multipotency for studying adipose development and application to tissue engineering of regenerative medicine.

This protocol describes the isolation of pig adipose-derived stem cells (pADSC) from subcutaneous adipose tissues with examination of multipotency. The multipotent pADSC are used to delineate processes of adipocyte differentiation and study transdifferentiation into multiple cell lineages of mesodermal mesenchyme or further lineages of ectoderm and endoderm for regenerative studies.

Obesity is an unconstrained worldwide epidemic. Unraveling molecular controls in adipose tissue development holds promise to treat obesity or diabetes. ...

Immunomagnetic Separation of Fat Depot-specific Sca1high Adipose-derived Stem Cells (ASCs)

The isolation of adipose-derived stem cells (ASCs) is an important method in the field of adipose tissue biology, adipogenesis, and extracellular matrix (ECM) remodeling. In vivo, ECM-rich environment consisting of fibrillar collagens provides a structural support to adipose tissues during the progression and regression of obesity. Physiological ECM remodeling mediated by matrix metalloproteinases (MMPs) plays a major role in regulating adipose tissue size and function1,2. The loss of physiological collagenolytic ECM remodeling may lead to excessive collagen accumulation (tissue fibrosis), macrophage infiltration, and ultimately, a loss of metabolic homeostasis including insulin resistance3,4. When a phenotypic change of the adipose tissue is observed in gene-targeted mouse models, isolating primary ASCs from fat depots for in vitro studies is an effective approach to define the role of the specific gene in regulating the function of ASCs. In the following, we define an immunomagnetic separation of Sca1high ASCs.

Immunomagnetic Separation of Fat Depot-specific Sca1high Adipose-derived Stem Cells ASCs

We present the techniques required to isolate the stromal vascular fraction (SVF) from mouse inguinal (subcutaneous) and perigonadal (visceral) adipose tissue depots to assess their gene expression and collagenolytic activity. This method includes the enrichment of Sca1high adipose-derived stem cells (ASCs) using immunomagnetic cell separation.

The isolation of adipose-derived stem cells (ASCs) is an important method in the field of adipose tissue biology, adipogenesis, and extracellular matrix ...

Isolation and Expansion of Mesenchymal Stem/Stromal Cells Derived from Human Placenta Tissue

Mesenchymal stem/stromal cells (MSC) are promising candidates for use in cell-based therapies. In most cases, therapeutic response appears to be cell-dose dependent. Human term placenta is rich in MSC and is a physically large tissue that is generally discarded following birth. Placenta is an ideal starting material for the large-scale manufacture of multiple cell doses of allogeneic MSC. The placenta is a fetomaternal organ from which either fetal or maternal tissue can be isolated. This article describes the placental anatomy and procedure to dissect apart the decidua (maternal), chorionic villi (fetal), and chorionic plate (fetal) tissue. The protocol then outlines how to isolate MSC from each dissected tissue region, and provides representative analysis of expanded MSC derived from the respective tissue types. These methods are intended for pre-clinical MSC isolation, but have also been adapted for clinical manufacture of placental MSC for human therapeutic use.

Herein we describe methods for the dissection of fetal and maternal tissues from human term placenta, followed by isolation and expansion of mesenchymal stem/stromal cells (MSC) from these tissues.

Mesenchymal stem/stromal cells (MSC) are promising candidates for use in cell-based therapies. In most cases, therapeutic response appears to be cell-dose ...

Large-Scale Production of Cardiomyocytes from Human Pluripotent Stem Cells Using a Highly Reproducible Small Molecule-Based Differentiation Protocol

Maximizing the benefit of human pluripotent stem cells (hPSCs) for research, disease modeling, pharmaceutical and clinical applications requires robust methods for the large-scale production of functional cell types, including cardiomyocytes. Here we demonstrate that the temporal manipulation of WNT, TGF-&#946;, and SHH signaling pathways leads to highly efficient cardiomyocyte differentiation of single-cell passaged hPSC lines in both static suspension and stirred suspension bioreactor systems. Employing this strategy resulted in ~ 100% beating spheroids, consistently containing &#62; 80% cardiac troponin T-positive cells after 15 days of culture, validated in multiple hPSC lines. We also report on a variation of this protocol for use with cell lines not currently adapted to single-cell passaging, the success of which has been verified in 42 hPSC lines. Cardiomyocytes generated using these protocols express lineage-specific markers and show expected electrophysiological functionalities. Our protocol presents a simple, efficient and robust platform for the large-scale production of human cardiomyocytes.

Here, we present a robust, fast and scalable cardiomyocyte differentiation protocol for human pluripotent stem cells (hPSCs). Cardiomyocytes derived using this large-scale method can provide sufficient cell numbers for their effective use in human cardiovascular disease modeling, high-throughput drug screening, and potentially clinical applications.

Maximizing the benefit of human pluripotent stem cells (hPSCs) for research, disease modeling, pharmaceutical and clinical applications requires robust ...

Chondrogenic Differentiation Induction of Adipose-derived Stem Cells by Centrifugal Gravity

Impaired cartilage cannot heal naturally. Currently, the most advanced therapy for defects in cartilage is the transplantation of chondrocytes differentiated from stem cells using cytokines. Unfortunately, cytokine-induced chondrogenic differentiation is costly, time-consuming, and associated with a high risk of contamination during in vitro differentiation. However, biomechanical stimuli also serve as crucial regulatory factors for chondrogenesis. For example, mechanical stress can induce chondrogenic differentiation of stem cells, suggesting a potential therapeutic approach for the repair of impaired cartilage. In this study, we demonstrated that centrifugal gravity (CG, 2,400 &#215; g), a mechanical stress easily applied by centrifugation, induced the upregulation of sex determining region Y (SRY)-box 9 (SOX9) in adipose-derived stem cells (ASCs), causing them to express chondrogenic phenotypes. The centrifuged ASCs expressed higher levels of chondrogenic differentiation markers, such as aggrecan (ACAN), collagen type 2 alpha 1 (COL2A1), and collagen type 1 (COL1), but lower levels of collagen type 10 (COL10), a marker of hypertrophic chondrocytes. In addition, chondrogenic aggregate formation, a prerequisite for chondrogenesis, was observed in centrifuged ASCs.

Mechanical stress can induce the chondrogenic differentiation of stem cells, providing a potential therapeutic approach for the repair of impaired cartilage. We present a protocol to induce the chondrogenic differentiation of adipose-derived stem cells (ASCs) using centrifugal gravity (CG). CG-induced upregulation of SOX9 results in the development of chondrogenic phenotypes.

Impaired cartilage cannot heal naturally. Currently, the most advanced therapy for defects in cartilage is the transplantation of chondrocytes ...

Rapid Isolation of BMPR-IB+ Adipose-Derived Stromal Cells for Use in a Calvarial Defect Healing Model

Invasive cancers, major injuries, and infection can cause bone defects that are too large to be reconstructed with preexisting bone from the patient's own body. The ability to grow bone de novo using a patient's own cells would allow bony defects to be filled with adequate tissue without the morbidity of harvesting native bone. There is interest in the use of adipose-derived stromal cells (ASCs) as a source for tissue engineering because these are obtained from an abundant source: the patient's own adipose tissue. However, ASCs are a heterogeneous population and some subpopulations may be more effective in this application than others. Isolation of the most osteogenic population of ASCs could improve the efficiency and effectiveness of a bone engineering process. In this protocol, ASCs are obtained from subcutaneous fat tissue from a human donor. The subpopulation of ASCs expressing the marker BMPR-IB is isolated using FACS. These cells are then applied to an in vivo calvarial defect healing assay and are found to have improved osteogenic regenerative potential compared with unsorted cells.

Adipose-derived stromal cells may be useful for engineering new tissue from a patient's own cells. We present a protocol for the isolation of a subpopulation of human adipose-derived stromal cells (ASCs) with increased osteogenic potential, followed by application of the cells in an in vivo calvarial healing assay.

Invasive cancers, major injuries, and infection can cause bone defects that are too large to be reconstructed with preexisting bone from the patient's own ...

In Vivo Tracking of Human Adipose-derived Mesenchymal Stem Cells in a Rat Knee Osteoarthritis Model with Fluorescent Lipophilic Membrane Dye

In order to support the clinical application of human adipose-derived mesenchymal stem cell (haMSC) therapy for knee osteoarthritis (KOA), we examined the efficacy of cell persistence and biodistribution of haMSCs in animal models. We demonstrated a method to label the cell membrane of haMSCs with lipophilic fluorescent dye. Subsequently, intra-articular injection of the labeled cells in rats with surgically induced KOA was monitored dynamically by an in vivo imaging system. We employed the lipophilic carbocyanines DiD (DilC18 (5)), a far-red fluorescent Dil (dialkylcarbocyanines) analog, which utilized a red laser to avoid excitation of the natural green autofluorescence from surrounding tissues. Furthermore, the red-shifted emission spectra of DiD allowed deep-tissue imaging in live animals and the labeling procedure caused no cytotoxic effects or functional damage to haMSCs. This approach has been shown to be an efficient tracking method for haMSCs in a rat KOA model. The application of this method could also be used to determine the optimal administration route and dosage of MSCs from other sources in pre-clinical studies.

In Vivo Tracking of Human Adipose-derived Mesenchymal Stem Cells in a Rat Knee Osteoarthritis Model with Fluorescent Lipophilic Membrane Dye

This protocol describes an efficient way to monitor the cell persistence and biodistribution of human adipose-derived mesenchymal stem cells (haMSCs) by far-red fluorescence labeling in a rat knee osteoarthritis (KOA) model via intra-articular (IA) injection.

In order to support the clinical application of human adipose-derived mesenchymal stem cell (haMSC) therapy for knee osteoarthritis (KOA), we examined the ...