Dr. Rountree acknowledges current support from the Children's Miracle Network, National Institute of Health, K08DK080928 and R03DK088013, and the American Cancer Society Research Scholar Award, MGO-11651. Dr. Rountree acknowledges that this procedure was initially developed and refined while funded by the Pediatric Scientist Development Program (NICHD Grant Award K12-HD00850).

All solutions, media, instruments, filters, and tubes should be sterile and handled with sterile technique to reduce the risk of contamination. Prepare all buffers and media 24 hours in advance and store at 4&deg;C.
1. Parenchymal and non-parenchymal separation from whole liver
<ol>
<li>Prepare the enzyme solution for digestion using a 15 cc tube with screw top in 10 ml sterile PBS containing 5 mg collagenase, 5 mg pronase, and 1 mg DNAse.</li>
<li>Euthanize mouse using institution approved (Institutional Animal Care and Use Committee) method such as CO2 asphyxiation. Wipe abdominal area of euthanized animals with 70% ethanol solution. Using sterile instruments, open abdominal cavity and explant liver en-block. Remove gall-bladder from explanted liver. Transfer whole liver to laminar flow hood in closed sterile dish.</li>
<li>This procedure is completed in a laminar flow hood. Using a sterile razor blade, mince liver with combination of multiple horizontal and vertical cuts for 1 minute in sterile dish. Place &frac14; of minced liver pulp in 15 cc tube with 10 cc PBS with collagenase, pronase, and DNAse from step 1.1 above. Repeat with each &frac14; minced liver.</li>
<li>Place tubes with &frac14; minced liver pulp and enzymes into water bath at 37&deg;C for 45 minutes, with shaker at 1-2 cycles/second. Wipe tubes with 70% ethanol after removal from water bath prior to transfer to laminar flow hood.</li>
<li>This procedure is completed in a laminar flow hood. Strain digested liver pulp through 70 micron mesh filter to collect into a sterile dish. Using 2 ml aliquots of sterile DMEM:F12 media with 10% heat inactivated fetal bovine serum, rinse the filter and use the rubber end of a syringe plunger to mash the digested pulp through the filter. Repeat 5 times to make total volume of filtrate approximately 20 mL. Divide the filtrate into 2 equal 15 mL tubes.</li>
<li>All transfers should be completed in laminar flow hood, and use refrigerated centrifuge at 4&deg;C if available. Centrifuge at 50 x g for 1 minute. Save supernatant #1 and discard parenchymal pellet. Centrifuge supernatant #1 at 50 x g for 1 minute. Save supernatant #2 and discard pellet. Centrifuge supernatant #2 at 50 x g for 1 minute. Save supernatant #3 and discard pellet. Centrifuge final supernatant #3 for 180 x g for 8 minute to obtain non-parenchymal fraction.</li>
</ol>
2. Red cell lysis 
Work in laminar flow hood, keep cells cold, and use solutions cooled to 4&deg;C.

<ol>
<li>The night before the procedure, prepare red cell lysis buffer by diluting 10X concentration stock BD Pharm Lyse buffer with a 1:10 dilution with sterile distilled water. 1X solutionshould be stored for 30 days at 4&deg;C.</li>
<li>The night before the procedure, prepare Miltenyi buffer using sterile PBS, 0.5% bovine serum Albumin, and 2mM EDTA. Filter solution using vacuum filter unit with 0.45 micron filter. Cover top of tilter unit with original plastic lid and secure with plastic wrap. Storeentire filter unit at 4&deg;C for 12 hours to degas EDTA. Filter unit can be replaced with standard sterile cap after 12 hours.</li>
<li>This procedure is completed in a laminar flow hood. Using a 5 ml sterile tube, re-suspend non-parenchymal pellet from step 1.6 above into 1 mL of 1X diluted red blood cell lysis buffer from 2.1 above. Cap the tube for transfer out of the laminar flow hood. </li>
<li>Gently vortex for 5seconds and incubate for 15 minutes at 4&deg;C protected from light.</li>
<li>Centrifuge at 200 x g for 5 minutes. </li>
<li>This procedure is completed in a laminar flow hood. Discard lysed RBCs in supernatant, and re-suspend pellet in 1 ml ice-cold and sterile Miltenyi buffer. </li>
<li>Centrifuge at 200 x g for 5 minutes.</li>
<li>This procedure is completed in a laminar flow hood. Discard supernatant and re-suspend pellet in 1 ml ice-cold and sterile Miltenyi buffer.</li>
<li>Remove 10 &mu;l of PBS cell suspension and add 10 &mu;l tryan blue. Count remainingnon-parenchymal cells using hemocytometer.</li>
</ol>
3. CD45 hematopoietic cell depletion from non-parenchymal fraction
Work in laminar flow hood, keep cells cold, and use solutions cooled to 4&deg;C.
<ol>
<li>Suspend cells in 100 &mu;L of Miltenyi buffer per 107 cells up to 108 total cells.</li>
<li>Apply 20 &mu;L Miltenyi CD45 microbead antibody for each 107 cells and incubate at 4&deg;C for 15 minutes.</li>
<li>Add additional 2 ml Miltenyi buffer and centrifuge at 200 x g for 5 minutes. Remove supernatant. Re-suspend cell pellet (up to 108 total cells) in 1 ml Miltenyi buffer.</li>
<li>In laminar flow hood, filter cells using Miltenyi LD magnetic column. Start by placing column in magnetic holder (Miltenyi MidiMACS or QuadroMACS). Place sterile 5 ml tube below filter to catch filtrate. Prepare column by loading 2 ml Miltenyi buffer.</li>
<li>Once pre-filter wash is complete, load cells onto LD column. Once the cell suspension is within the column, add 1 ml Miltenyi buffer and repeat 1 ml Miltenyi buffer wash 2 additional times. Do NOT use plunger provided with column to increase speed of filtration. ONLY collect filtrate when the filter in placed in the magnetic holder. </li>
<li>Centrifuge the collected filtrate of approximately 5 ml (the column holds the remaining 1 ml) of CD45-depleted non-parenchymal cells at 200 x g for 5 minutes. Discard the column with the retained CD45 positive cells.</li>
</ol>
4. Flow cytometry isolation of CD133 positive cells
<ol>
<li>Prepare oval cell media. Use 1:1 DMEM:F12 medium with 10 % heat inactivated fetal calf serum as base, and add insulin (1 &mu;g/ml), HEPES (5 mol/L), and Penicillin/Streptomycin (1% volume/volume). Filter solution using vacuum filter unit with 0.45 micron filter.</li>
<li>Re-suspend cells in Miltenyi buffer at 100 &mu;L per 107 cells. Add 2 &mu;L of CD133-PE conjugated antibody. Using a second group of cells, incubate with IgG-PE conjugated antibody as a control. Retain a third group of cells without staining as an unstained control for FACS.</li>
<li>Incubate at 4&deg;C for 15 minutes in the dark. Re-suspend in 2 ml staining buffer. Centrifuge at 200 x g for 5 minutes. Discard supernatant and re-suspend pellet in 1 ml Miltenyi buffer.</li>
<li>This step is conducted using standard flow cytometry cell sorting procedures, which may be institution specific. Using unstained cells and IgG PE stained cells, adjust sorting parameters for optimized gating of CD133+ cell population. PE (R-Phytoerythrin) can generally be used with any flow cytometer that has a laser that emits at 488 nm. The peak emission for PE is 575 nm and is detected in the FL-2 channel. 
Note: Using a BD FACS Calibur or BD FACS Vantage machines, with the Cell Quest program for data collection, we use Forward Scatter and Side Scatter view in the log scale to identify cell populations, with side scatter set to 250. FL1 and FL2 are both in log scale and set to 550. These parameters provide an initial starting place to view liver non-parenchymal cells, and are adjusted as needed based on staining intensity of positive and negative populations.</li> 
<li>Isolate the CD133+ cell population using CD133+ gate and collect the cells in sterile filtered cell media.</li>
</ol>
5. Cell culture methods
<ol>
<li>Centrifuge FACS collected cells at 200 x g for 5 minutes. Re-suspend cell pellet in oval cell media with approximately 5000 cells per ml. May start with higher concentrations, up to 50,000 cells/ml for initial experiments, and reduce as technique improves and overall cell viability and yield improves.</li>
<li>Plate cells onto BD Biocoat Laminin coated 96 well plates using 1000 cells/cm2. Place in humidified cell culture incubator at 37&deg;C, with 5% CO2. After 24 hours, add Hepatocyte Growth Factor (50 ng/nl) and Epidermal Growth Factor (20 ng/ml).</li>
<li>For single cells, isolate cells directly into 50 &mu;l of oval cell media in each well of a 96 well Laminin coated plate. Use single cell FACS settings for strict selection of one positive cell only. After 24 hours, add 50 &mu;l of oval cell media with HGF and EGF as above in step 5.2. Change media fully after 5-7 days.</li>
<li>Once the expanding colonies are greater than 50% confluent, which typically occurs after 2 weeks, depending on total number of cells plated and cell viability, the cells may be split 1:3 as below.</li>
<li>Split cells using Trypsin 0.05%-EDTA. Apply just enough to cover well bottom, 50-100 &mu;L/well on 96 well plate. Place in incubator at 37&deg;C for 3-5 minutes.</li>
<li>Add 100 &mu;L of media to each well and transfer all liquid to 5 ml tube. Add 1 mL media to each tube and centrifuge at 200 x g for 5 minutes.</li>
<li>Re-suspend cells in media plate in laminin coated dish, using cells from 1 well to plate into 3 new wells (1:3 ratio).</li>
</ol>
6. Confirmation of bi-potential status using RT-PCR
This procedure is detailed in the RNeasy protocol handbook, which is supplied with the RNeasy Kit.
<ol>
<li>Use RNeasy micro columns for 96 well plate colonies. Aspirate culture media from each well. Add 75 &mu;l Buffer RLT (from RNeasy Kit) directly to each well. Scrape plate bottom with sterile rubber policeman. Pipettelysate into micro-centrifuge tube and vortex mixture for 1 minute. Add 70% ethanol to lysates and mix by pipetting.</li>
<li>Transfer the solution to RNeasy column placed in a 2 ml collection tube (as supplied in RNeasy Kit) and centrifuge in micro-centrifuge for 15 seconds at 10,000 rpm. Discard eluted filtrate.</li>
<li>Re-use the collection tube. Add 350 &mu;L Buffer RW1 (RNeasy Kit) to the RNeasy column and centrifuge for 15 seconds at 10,000 rpm to wash the column membrane. Discard eluted wash.</li>
<li>Add 10 &mu;L DNase I stock solution to 70 &mu;L Buffer RDD (both supplied in RNeasy Kit).Add the 80 &mu;L DNase I Buffer RDD incubation mix to the RNeasy column membrane and incubate for 15 minutes at room temperature.</li>
<li>Add 350 &mu;L Buffer RW1 (RNeasy kit) to the RNeasy column and centrifuge for 15 seconds at 10,000 rpm to wash the membrane. Discard eluted wash and collection tube.</li>
<li>Place the RNeasy column in a new 2 ml collection tube (supplied in RNeasy kit).
Add 500 &mu;L Buffer RPE(RNeasy Kit) to the RNeasy column and centrifuge for
15 seconds at 10,000 rpm to wash the membrane. Discard eluted wash.</li>
<li>Prepare 80% ethanol using RNase-free water (RNeasy Kit). Add 500 &mu;L of 80% ethanol to the RNeasy columnand centrifuge for 2 minutes at 10,000 rpm. Discard eluted wash.</li>
<li>Place the RNeasy column in a new 2 ml collection tube (RNeasy Kit) and centrifuge at full speed for 5 minutes. Discard any eluted wash and collection tube.</li>
<li>Place the RNeasy column in a new 1.5 ml collection tube (RNeasy kit). Add 14 &mu;L RNase-free water (RNeasy Kit) to the center of the column membrane and centrifuge for 1 minute at full speed. Collect filtrate with purified RNA and transfer to ice if creating cDNA immediately or store at minus 80&deg;C for future use.</li>
<li>Reverse transcription using Omniscript.Dilute RNase inhibitor to a final concentration of 10 units/ &mu;L in ice-cold 1x Buffer RT. Vortex for 5 seconds, and pulse centrifuge for 5 seconds. Prepare a fresh master mix on ice according to page 13 of Omniscript protocol. Vortex for 5 seconds, and pulse centrifuge for 5 seconds. Recommend to prepare a volume of mastermix 10% greater than that required for the total required for all reactions.</li>
<li>Add template RNA to the individual tubes containing master mix. Vortex for 5 seconds, and pulse centrifuge for 5 seconds. Incubate for 60 min at 37&deg;C.</li>
<li>PCR amplification of hepatocyte (Albumin) and cholangiocyte specific genes using HotStarTaq DNA polymerase. Prepare reaction mix per page 15 of HotStarTaq protocol book. Recommend diluting stock primers to concentration of 20 pm/&mu;l, and with 1 &mu;L/reaction tube used for forward and reverse primers. Depending on number of cells initially used for RNA extraction, we recommend dividing final cDNA among 3 reaction tubes (&beta;-actin for loading control, Albumin, and KRT19) to start.</li>
<li>PCR primer design is listed in Table 1.</li>
<li>Place reaction tubes into thermocycler. Recommend following program for initial experiments: 95&deg;Cfor 15 minutes x 1 cycle followed by 95&deg;C for 30 seconds, 55&deg;C for 30 seconds, 72&deg;C for 30 seconds x 35 cycles, followed by 72&deg;C for 10 minutes.</li>
<li>PCR products are analyzed using ethidium bromide impregnated agarose gel.</li>
</ol>
7. Confirmation of tumor potential of CD133+ stem cells
<ol>
<li>This procedure can be done with freshly isolated cells from step 4 or using cells that have been cultured from step 5. We recommend performing initial experiments with cultured cells, as freshly isolated cells will have reduced viability and reduced yield.</li>
<li>Trypsinize cells using Trypsin 0.05%-EDTA from step 5.5 above. After 3-5 minute incubation at 37&deg;C, add 100 &mu;L of media to each well and transfer all liquid from each well to individual 5 ml tubes (1 well = 1 tube). Add 1 ml media to each tube and centrifuge at 200 x g for 5 minutes.</li>
<li>Re-suspend cells in 1 ml ice cold PBS. Remove 10 &mu;l of PBS cell suspension and add 10 &mu;l trypan blue. Using trypan blue exclusion, determine numbers of live cells. If using FACS isolated cells, cell number will be determined by FACS isolation count.</li>
<li>Centrifuge cells at 200 x g for 5 minutes and re-suspended in PBS at a concentration of 1 x 106 live cells/100 &mu;l. Add 100 &mu;l Matrigel. Six-week-old immune-deficient Nude mice were injected subcutaneously using 28 gague needle. Inject 1 x 106 cells in 200 &mu;l per site.</li>
<li>Mice are monitored for tumor growth daily. Once tumors form, typically after 3-4 weeks incubation, tumor volume is measured using calipers (height x length x width).</li>
</ol>
8. Representative Results: 
From normal, healthy murine liver, the expected cellular yield of CD133+liver stem cells is 1,000 to 5,000 per liver. These cells are relatively rare in quiescent liver and will not expand well in culture. We do not recommend using single cell analysis on normal liver and the yield of viable cells that will expand is extremely low.
For livers with significant chronic injury, such as the DDC 0.1% diet for 6 weeks1 or genetic modification resulting in chronic injury, such as the MAT1a-/- or liver specific Pten-/-mice,2-4the expected number of cells isolated increases, with up to 100,000 cells isolated/liver (Figure 2). If using genetic models, knowledge of spontaneous tumor rate is critical, as these procedures for liver stem cell isolation should be conducted in tumor free animals. For example, if the MAT1a-/- model forms spontaneous tumors at 18 months, we recommend using animals no later than 15-16 months, prior to any reported spontaneous tumors. 
Isolation of single cells from chronic injury models will yield several (3-9 colonies/96 well plate) colonies that expand from single cells once the procedure is mastered, and cell viability is ensured. Figure 3 present representative phase contrast images of colonies derived from single CD133+ cells expanded after 7 days. 
Confirmation of bi-potential status is conducted using Albumin and Krt19 RT-PCR. Colonies from expanded single cells will demonstrate both expression for markers of hepatocytes (Albumin) and cholangiocytes (Krt19). Figure 4 demonstrates bi-potential expression from three isolated colonies, with approximately 25 cells/colony at 7 days.
CD133+ stem cells from normal liver and chemically induced liver injury (e.g. DDC 0.1% diet for 6 weeks) will not form tumors in nude mice. CD133+ stem cells from specific genetic models (MAT1a-/- or liver specific Pten-/- mice) will form tumors in nude mice if isolated late in late pre-tumor chronic injury phase. This tumor forming phenotype is currently identified as a cancer stem cell.2-4For example, the MAT1a-/- mice form spontaneous liver tumors at 18 weeks of age. CD133+ liver stem cells isolated at 15-16 weeks, during a late chronic injury phase of liver disease, will form tumors in nude mice. Figure 5 demonstrates representative tumors from bilateral injection of 1 x 106 cells expanded in vitro from single CD133+ liver stem cells.
<table border="1">
 <tbody>
 <tr>
 <td>Gene</td>
 <td>Forward Primer </td>
 <td>Reverse Primer</td>
 </tr>
 <tr>
 <td>&beta;-Actin</td>
 <td>5'-TGTTACCAACTGGGACGACA-3'</td>
 <td>5'-GGGGTGTTGAAGGTCTCAAA-3'</td>
 </tr>
 <tr>
 <td>Albumin</td>
 <td>5'-CATGCCAAATTAGTGCAGGA-3'</td>
 <td>5'-GCTGGGGTTGTCATCTTTGT-3'</td>
 </tr>
 <tr>
 <td>Keratin 19</td>
 <td>5'-TGCTGGATGAGCTGACTCTG-3'</td>
 <td>5'-AATCCACCTCCACACTGACC-3'</td>
 </tr>
 </tbody>
</table>
Table 1: Primer design for RT-PCR
<img src="/files/ftp_upload/3183/3183fig1.jpg" alt="Figure 1"/> Figure 1: Overall schematic of methods.
<img src="/files/ftp_upload/3183/3183fig2.jpg" alt="Figure 2"/> Figure 2: CD133+ liver stem cells identified in highly enriched CD45 depleted non-parenchymal fraction. Control uninjured liver from wild-type mice demonstrates 0.4% CD133+ cells within the highly enriched CD45 depleted non-parenchymal fraction. In the genetic knock-out MAT1a-/-, which is a model of chronic liver injury, the CD133 population expands 10 fold or more in the same highly enriched fraction.
<img src="/files/ftp_upload/3183/3183fig3.jpg" alt="Figure 3"/> Figure 3: Expanding colonies from single CD133+ clones. Phase-contrast images of four colonies derived from single CD133+ cells expanded on laminin coated 96 well plates. 
<img src="/files/ftp_upload/3183/3183fig4.jpg" alt="Figure 4"/> Figure 4: Bi-potential gene expression from CD133+ liver stem cell clonally expanded colonies. At Day 7, colonies are approximately 25 cells. Gene expression demonstrates expression of hepatocyte marker Albumin and cholangiocyte marker Krt19, confirming bi-potential status of CD133+ cells.
<img src="/files/ftp_upload/3183/3183fig5.jpg" alt="Figure 5"/> Figure 5: CD133+ liver stem cells form tumors in nude mice.Arrows indicate tumors growing 4 weeks after 1x106 CD133+ cells injected from MAT1a-/- model. CD133+ cells from toxin induced chronic liver injury, such as CCl4 or 0.1% DDC diet, do not form tumors. Tumor formation is used to identify malignant potential, or cancer stem cell phenotype within the stem cell population.

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W. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Activation+of+hepatic+stem+cell+marker+EpCAM+by+Wnt-beta-catenin+signaling+in+hepatocellular+carcinoma.">Activation of hepatic stem cell marker EpCAM by Wnt-beta-catenin signaling in hepatocellular carcinoma.</a> Cancer Res. 67, 10831-10839 (2007).</li><li>Furuyama, K. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Continuous+cell+supply+from+a+Sox9-expressing+progenitor+zone+in+adult+liver,+exocrine+pancreas+and+intestine.">Continuous cell supply from a Sox9-expressing progenitor zone in adult liver, exocrine pancreas and intestine.</a> Nat Genet. 43, 34-41 (2011).</li><li>Kordes, C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=CD133++hepatic+stellate+cells+are+progenitor+cells.">CD133+ hepatic stellate cells are progenitor cells.</a> Biochem Biophys Res Commun. 352, 410-417 (2007).</li><li>Berg, T. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Fibroblast+Growth+Factor+10+is+critical+for+liver+growth+during+embryogenesis+and+controls+of+hepatoblast+survival+via+b-catenin+activation.">Fibroblast Growth Factor 10 is critical for liver growth during embryogenesis and controls of hepatoblast survival via b-catenin activation.</a> Hepatology. , (2007).</li><li>Turner, R. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Human+hepatic+stem+cell+and+maturational+liver+lineage+biology.">Human hepatic stem cell and maturational liver lineage biology.</a> Hepatology. 53, 1035-1045 (2011).</li><li>Wang, Y. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Lineage+restriction+of+human+hepatic+stem+cells+to+mature+fates+is+made+efficient+by+tissue-specific+biomatrix+scaffolds.">Lineage restriction of human hepatic stem cells to mature fates is made efficient by tissue-specific biomatrix scaffolds.</a> Hepatology. 53, 293-305 (2011).</li><li>Galicia, V. 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+of+hepatic+tumor+progenitor+cells+in+Pten-null+mice+requires+liver+injury+and+is+reversed+by+loss+of+AKT2.">Expansion of hepatic tumor progenitor cells in Pten-null mice requires liver injury and is reversed by loss of AKT2.</a> Gastroenterology. 139, 2170-2182 (2010).</li><li>Ding, W. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Epithelial-to-mesenchymal+transition+of+murine+liver+tumor+cells+promotes+invasion.">Epithelial-to-mesenchymal transition of murine liver tumor cells promotes invasion.</a> Hepatology. 52, 945-953 (2010).</li></ol>

Dr. Rountree receives research support from Bayer Pharmaceutics. Drs. Ding and Crooks and Ms. Dang and Ms. VanKirk have no disclosures to report.

Unlike the hematopoietic system, in which hematopoietic stem cells are responsible for maintaining a cellular differentiation system that replacesnormal physiologic turn-over of leukocytes, red blood cells, and platelets, liver stem cell, or adult liver progenitor cells, do not participate in normal liver homeostasis.5,6 After acute liver injury or partial hepatectomy, hepatocytes, as differentiated liver epithelium, undergo several rounds of proliferation to replace the lost liver mass.5,6Only during chronic injury are liver stem cells observed to proliferate.1,5-11 These adult, organ specific stem cells are proposed to differentiate into both hepatocytes and cholangiocytes.1,5-8Interestingly, the vast majority of liver cancer develops on the background of chronic injury, and thus liver stem cells are also hypothesized to be the precursors for a subset of liver cancer.2-4,12-17
One of the major challenges to stem cell work in the liver is isolation of rare populations of cells for functional analysis. For example, the vast majority of cells in the liver are hepatocytes, which are significantly larger than cholangiocytes and other smaller non-parenchymal cells. By breaking the whole liver into cell compartments (large hepatocytes - parenchymal fraction and smaller cells - non-parenchymal fraction), and further selecting for CD45 negative cells (non-hematopoietic cells), we are able to enrich the starting population of stem cells by over 600-fold.1,18-21Of note, we are by no means indicating that the CD133+ population is a 100% pure stem cell population, but clearly represents a heterogeneous population of cells, with different lineage and repopulation potential. One of the major limitations of the field is definitions of stem cells and progenitor cells. We use the term "stem cell" more broadly in this work, but in strict definition, CD133+ non-parenchymal cells represent a bi-lineage progenitor population. Given the state of current stem and progenitor research in the liver, this report does provide a starting place for investigators who are interested in this field. As new markers emerge, such as EpCAM,22,23 or transcription factors, such as Sox9,24 they can be incorporated. For example, we have found a fairly high rate of overlap between EpCAM+ cells and CD133+ cells.
In this report, we detail a process for stem cell isolation 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 isolation.1,3,4 The specific goal of this process is to isolate a relatively pure population of liver stem cells that can be clonally expanded in vitro. 
The primary limitation to this procedure is that the majority of cells isolated will not be viable after flow cytometry (see Trouble Shooting section). This is the result of the hours required to prepare the cells, and the numerous procedures required to refine the population prior to isolation. If the liver is digested in single cell suspension for immediate FACS analysis, the size difference between hepatocytes and other non-parenchymal cells will make effective FACS gate creation impossible. If the liver non-parenchymal cells are utilized, without elimination of hematopoietic cells, there is a risk that a significant number of CD133+ cells may be of hematopoietic origin may contaminate the fraction. Furthermore, by processing the cells through the Miltenyi filter, only single cells and very small clusters of cells are collected. This ensures that the sample will not clog the FACS intake needle.
Alternatives for this procedure include modification for any alternative cell surface marker, such as CD49f, EpCAM, or combination of markers, such as CD133+EpCAM+A second published report utilizes a density gradient to isolate liver stem cells from a non-parenchymal fraction. This procedure requires an Ultra-centrifuge (8000 x g), adds significant time to the procedure, and in our experience, significantly reduced pre-FACS cellular yield and post-FACS viability.8
Future experiments include a broader range of gene expression analysis, including fetal liver genes, such as HNF3, HNF4&alpha;, and &alpha;fp.In addition, Western blot analysis and immunocytochemistry of expressed proteins can be utilized to confirm RT-PCR results of cells in culture.
One issue to note is recent work that identified CD133 expression on hepatic stellate cells.25 We now routinely screen our samples for markers of stellate cells (see Trouble Shooting section), and have not identified significant contamination in our fractions. This may be related to different techniques of liver digestion and cell isolation.2,3,26
Based on the fact that the majority of cells will not be viable immediately after FACS isolation, we recommend that the cells be plated, either as bulk CD133+ cells or single cells, prior to use in animals. 5-7 days in vitro will significantly improve results of tumor analysis. In addition, given the rigors of single cell isolation, this should only be conducted once colonies can be expanded from bulk CD133+ isolated cells. A more thorough discussion of the various culture conditions and scaffold proteins which may be utilized to culture liver stem and progenitor cells has been well characterized by Lola Reid. This work provides alternative conditions and modifications, which investigators may incorporate into their research program once basic isolation techniques are mastered.27,28 Dr. Reid's work also provides a more detailed analysis of the lineage biology and maturation between hepatic stem cells and committed progenitors. 
In terms of in vivo tumor analysis, we have had success using freshly isolated cells and cells from clonally expanded CD133+ cells in vitro, primarily using 1x106 cells. We have focused ontwo genetic strains of chronic liver injury, the MAT1a-/- and liver specific Pten-/- mice, and we have utilized both nude mice and wild-type mice as hosts for tumor growth. In our experience, CD133+ liver stem cells will only form tumors if they are isolated from significant liver injury models that are pre-malignant. Note that the tumors formed from CD133+ cells general have both hepatocellular carcinoma and cholangiocarcinoma features, suggesting a stem cell or progenitor cell origin to the tumors.2-4,29
Follow-up work after tumors are documented includes standard pathologic analysis of tumor tissue (H&amp;E staining) and immunohistochemical staining. In addition, tumors can be minced and digested for FACS analysis or re-culture.2-4,30
In conclusion, we have detailed a procedure for the isolation, expansion, and basic characterization of CD133+ liver stem cells and CD133+ cancer stem cells.
Trouble Shooting: 
CD45 contamination: 
For Step 3, if there is contamination of CD45+ cells, which can be assessed by adding a CD45-FITC Ab prior to FACS analysis and isolation, check to ensure that the CD45 microbead antibody is not expired and that the filtrate was collected only while the filter was in the magnetic holder. Any filtrate collected while the filter is not in the magnetic holder will contain CD45+ cells. 
Low cell number: 
For the uninjured liver, the total number of CD133+ non-parenchymal isolated may be less than 10,000. These cells are rare in the quiescent liver. For a chronic injury model, such as the DDC 0.1% diet, the number will increase greatly to 100,000 cells. If the total cell number is significantly below these numbers, one issue to consider is the FACS Ab staining. Check to ensure that the CD133 Ab is not expired, as poor staining will result in a poor yield. Also, we recommend performing a FACS analysis of liver non-parenchymal cells to determine the relative population prior to attempting FACS isolation. 
Low cell viability after FACS: 
One of the issues of viability may be related to how the cells are processed and over what time. Ideally, the entire cell isolation procedure, steps 1-4, should be conducted without any delays between steps and completed in the same day. Any significant delay between steps 1-4 will greatly reduce the cell viability. A second issue related to cell viability may be related to the sheath pressure used for FACS isolation. We recommend using a lower sheath pressure. Lastly, once the cells are isolated, they should be immediately plated, as any significant storage on ice after sorting will also reduce viability. 
CD133+ non-parenchymal heterogeneity: 
Recent reports indicate that hepatic stellate cells may also have CD133 expression and have some plasticity.25 Therefore, in addition to verifying bi-potency genes with Albumin and Krt19, additional verification can include genes associated with stellate cells, such as glial fibrillary acidic protein in quiescent stellate cells and alpha-smooth muscle actin and desmin in activated stellate cells.3,4,26 In addition, the CD133+ population represents a broader progenitor population. The addition of a second marker, such as EpCAM, may help to refine the population further, and limit heterogeneity.

<table border="1">
	<tbody>
		<tr>
			<th>Name of the reagent</th>
			<th>Company</th>
			<th>Catalogue number</th>
			<th>Comments (optional)</th>
		</tr>
		<tr>
			<td>DMEM:F12</td>
			<td>Invitrogen</td>
			<td>10565-018</td>
			<td>With phenol red</td>
		</tr>
		<tr>
			<td>CD45 microbeads</td>
			<td>Miltenyi</td>
			<td>130-052-301</td>
			<td>&nbsp;</td>
		</tr>
		<tr>
			<td>Hepatocyte Growth Factor	</td>
			<td>Sigma</td>
			<td>	H1404</td>
			<td>&nbsp;</td>
		</tr>
		<tr>
			<td>Epidermal Growth Factor		</td>
			<td>Sigma</td>
			<td>E4127</td>
			<td>&nbsp;</td>
		</tr>
		<tr>
			<td>DNase			</td>
			<td>Sigma</td>
			<td>DN25</td>
			<td>1 gram</td>
		</tr>
		<tr>
			<td>Collagenase D		</td>
			<td>Roche</td>
			<td>1088874</td>
			<td>&nbsp;</td>
		</tr>
		<tr>
			<td>Pronase		</td>
			<td>Roche</td>
			<td>0165921</td>
			<td>&nbsp;</td>
		</tr>
		<tr>
			<td>70 micron mesh strainer		</td>
			<td>Fisher</td>
			<td>352350</td>
			<td>&nbsp;</td>
		</tr>
		<tr>
			<td>Omniscript RT			</td>
			<td>Quaigen</td>
			<td>205111</td>
			<td>50 reactions</td>
		</tr>
		<tr>
			<td>HotStarTaq</td>
			<td>Quaigen</td>
			<td>203203</td>
			<td>&nbsp;</td>
		</tr>
		<tr>
			<td>Miltenyi LD column</td>
			<td>Miltenyi</td>
			<td>130-042-901</td>
			<td>&nbsp;</td>
		</tr>
		<tr>
			<td>CD133-PE FACS Ab		</td>
			<td>eBioscience</td>
			<td>12-1331-82</td>
			<td>&nbsp;</td>
		</tr>
		<tr>
			<td>Laminin coated plates			</td>
			<td>BD</td>
			<td>354410</td>
			<td>96 well</td>
		</tr>
		<tr>
			<td>Trypsin 0.05% EDTA			</td>
			<td>Invitrogen</td>
			<td>25300-354</td>
			<td>100 mL</td>
		</tr>
		<tr>
			<td>RNeasy Micro Kit	</td>
			<td>Quaigen	</td>
			<td>74004	</td>
			<td>50 columns for 5x105 cells or less</td>
		</tr>
		<tr>
			<td>Pharm Lyse			</td>
			<td>BD</td>
			<td>555899</td>
			<td>10X concentration</td>
		</tr>
	</tbody>
</table>

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.

Watch this Scientific Journal Video about Isolation of CD133+ Liver Stem Cells for Clonal Expansion at JoVE.com

Isolation of CD133+ Liver Stem Cells for Clonal Expansion

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 ...

isolation-of-cd133-liver-stem-cells-for-clonal-expansion

Research

JoVE Journal

Biology

22.3K 次观看.  Pennsylvania State College of Medicine. 在这里，我们描述CD133的表达肝干细胞和整体的小鼠肝，一个过程，需要组织消化，细胞富集和流式细胞仪分离肿瘤干细胞的分离。包括先进的单细胞的分离和克隆扩增的方法。

视频: Isolation of CD133+ Liver Stem Cells for Clonal Expansion

Isolation and Transplantation of Hematopoietic Stem Cells (HSCs)

Isolation and Transplantation of Hematopoietic Stem Cells HSCs

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

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

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

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

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

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

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

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

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

Isolation and Derivation of Mouse Embryonic Germinal Cells

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

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

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

Isolation of Mouse Salivary Gland Stem Cells

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

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

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

Isolation and Culture of Individual Myofibers and their Satellite Cells from Adult Skeletal Muscle

Muscle regeneration in the adult is performed by resident stem cells called satellite cells. Satellite cells are defined by their position between the basal lamina and the sarcolemma of each myofiber. Current knowledge of their behavior heavily relies on the use of the single myofiber isolation protocol. In 1985, Bischoff described a protocol to isolate single live fibers from the Flexor Digitorum Brevis (FDB) of adult rats with the goal to create an in vitro system in which the physical association between the myofiber and its stem cells is preserved 1. In 1995, Rosenblattmodified the Bischoff protocol such that myofibers are singly picked and handled separately after collagenase digestion instead of being isolated by gravity sedimentation 2, 3. The Rosenblatt or Bischoff protocol has since been adapted to different muscles, age or conditions 3-6. The single myofiber isolation technique is an indispensable tool due its unique advantages. First, in the single myofiber protocol, satellite cells are maintained beneath the basal lamina. This is a unique feature of the protocol as other techniques such as Fluorescence Activated Cell Sorting require chemical and mechanical tissue dissociation 7. Although the myofiber culture system cannot substitute for in vivo studies, it does offer an excellent platform to address relevant biological properties of muscle stem cells. Single myofibers can be cultured in standard plating conditions or in floating conditions. Satellite cells on floating myofibers are subjected to virtually no other influence than the myofiber environment. Substrate stiffness and coating have been shown to influence satellite cells' ability to regenerate muscles 8, 9 so being able to control each of these factors independently allows discrimination between niche-dependent and -independent responses. Different concentrations of serum have also been shown to have an effect on the transition from quiescence to activation. To preserve the quiescence state of its associated satellite cells, fibers should be kept in low serum medium 1-3. This is particularly useful when studying genes involved in the quiescence state. In serum rich medium, satellite cells quickly activate, proliferate, migrate and differentiate, thus mimicking the in vivo regenerative process 1-3. The system can be used to perform a variety of assays such as the testing of chemical inhibitors; ectopic expression of genes by virus delivery; oligonucleotide based gene knock-down or live imaging. This video article describes the protocol currently used in our laboratory to isolate single myofibers from the Extensor Digitorum Longus (EDL) muscle of adult mice (6-8 weeks old).

Isolation and culture of myofibers is the gold standard in vitro system to study the transition of satellite cells through quiescence, activation and differentiation. Importantly, the single myofiber culture system preserves the myofiber/stem cell association, which is an essential component of the muscle stem cell niche.

Muscle  regeneration in the adult is performed by resident stem cells called satellite  cells. Satellite cells are defined by  their position between the ...

Na&iuml;ve Adult Stem Cells Isolation from Primary Human Fibroblast Cultures

Over the last decade, several adult stem cell populations have been identified in human skin 1-4. The isolation of multipotent adult dermal precursors was first reported by Miller F. D laboratory 5, 6. These early studies described a multipotent precursor cell population from adult mammalian dermis 5. These cells--termed SKPs, for skin-derived precursors-- were isolated and expanded from rodent and human skin and differentiated into both neural and mesodermal progeny, including cell types never found in skin, such as neurons 5. Immunocytochemical studies on cultured SKPs revealed that cells expressed vimentin and nestin, an intermediate filament protein expressed in neural and skeletal muscle precursors, in addition to fibronectin and multipotent stem cell markers 6. Until now, the adult stem cells population SKPs have been isolated from freshly collected mammalian skin biopsies.
Recently, we have established and reported that a population of skin derived precursor cells could remain present in primary fibroblast cultures established from skin biopsies 7. The assumption that a few somatic stem cells might reside in primary fibroblast cultures at early population doublings was based upon the following observations: (1) SKPs and primary fibroblast cultures are derived from the dermis, and therefore a small number of SKP cells could remain present in primary dermal fibroblast cultures and (2) primary fibroblast cultures grown from frozen aliquots that have been subjected to unfavorable temperature during storage or transfer contained a small number of cells that remained viable 7. These rare cells were able to expand and could be passaged several times. This observation suggested that a small number of cells with high proliferation potency and resistance to stress were present in human fibroblast cultures 7.
We took advantage of these findings to establish a protocol for rapid isolation of adult stem cells from primary fibroblast cultures that are readily available from tissue banks around the world (Figure 1). This method has important significance as it allows the isolation of precursor cells when skin samples are not accessible while fibroblast cultures may be available from tissue banks, thus, opening new opportunities to dissect the molecular mechanisms underlying rare genetic diseases as well as modeling diseases in a dish.

Na&amp;#239;ve Adult Stem Cells Isolation from Primary Human Fibroblast Cultures

We report a method to isolate na&#239;ve multipotent skin-derived precursor (SKP) cells from primary human fibroblast cultures. We show that these SKPs derived from fibroblast cultures share similar stem cell properties to the ones derived directly from human skin biopsies. These cells express the neural crest marker, nestin, in addition to the multipotent markers such as OCT4 and Nanog.

Over the last decade, several adult stem cell  populations have been identified in human skin 1-4.  The isolation of multipotent adult dermal precursors ...

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 ...

Isolation, Culture, and Transplantation of Muscle Satellite Cells

Muscle satellite cells are a stem cell population required for postnatal skeletal muscle development and regeneration, accounting for 2-5% of sublaminal nuclei in muscle fibers. In adult muscle, satellite cells are normally mitotically quiescent. Following injury, however, satellite cells initiate cellular proliferation to produce myoblasts, their progenies, to mediate the regeneration of muscle. Transplantation of satellite cell-derived myoblasts has been widely studied as a possible therapy for several regenerative diseases including muscular dystrophy, heart failure, and urological dysfunction. Myoblast transplantation into dystrophic skeletal muscle, infarcted heart, and dysfunctioning urinary ducts has shown that engrafted myoblasts can differentiate into muscle fibers in the host tissues and display partial functional improvement in these diseases. Therefore, the development of efficient purification methods of quiescent satellite cells from skeletal muscle, as well as the establishment of satellite cell-derived myoblast cultures and transplantation methods for myoblasts, are essential for understanding the molecular mechanisms behind satellite cell self-renewal, activation, and differentiation. Additionally, the development of cell-based therapies for muscular dystrophy and other regenerative diseases are also dependent upon these factors.

However, current prospective purification methods of quiescent satellite cells require the use of expensive fluorescence-activated cell sorting (FACS) machines. Here, we present a new method for the rapid, economical, and reliable purification of quiescent satellite cells from adult mouse skeletal muscle by enzymatic dissociation followed by magnetic-activated cell sorting (MACS). Following isolation of pure quiescent satellite cells, these cells can be cultured to obtain large numbers of myoblasts after several passages. These freshly isolated quiescent satellite cells or ex vivo expanded myoblasts can be transplanted into cardiotoxin (CTX)-induced regenerating mouse skeletal muscle to examine the contribution of donor-derived cells to regenerating muscle fibers, as well as to satellite cell compartments for the examination of self-renewal activities.

The isolation and culture of a pure population of quiescent satellite cells, a muscle stem cell population, is essential to the understanding of muscle stem cell biology and regeneration, as well as stem cell transplantation for therapies in muscular dystrophy and other degenerative diseases.&#160;

Muscle satellite cells are a stem cell population required for postnatal skeletal muscle development and regeneration, accounting for 2-5% of sublaminal ...

Protocol for Isolation of Primary Human Hepatocytes and Corresponding Major Populations of Non-parenchymal Liver Cells

Beside parenchymal hepatocytes, the liver consists of non-parenchymal cells (NPC) namely Kupffer cells (KC), liver endothelial cells (LEC) and hepatic Stellate cells (HSC). Two-dimensional (2D) culture of primary human hepatocyte (PHH) is still considered as the &#34;gold standard&#34; for in vitro testing of drug metabolism and hepatotoxicity. It is well-known that the 2D monoculture of PHH suffers from dedifferentiation and loss of function. Recently it was shown that hepatic NPC play a central role in liver (patho-) physiology and the maintenance of PHH functions. Current research focuses on the reconstruction of in vivo tissue architecture by 3D- and co-culture models to overcome the limitations of 2D monocultures. Previously we published a method to isolate human liver cells and investigated the suitability of these cells for their use in cell cultures in Experimental Biology and Medicine1. Based on the broad interest in this technique the aim of this article was to provide a more detailed protocol for the liver cell isolation process including a video, which will allow an easy reproduction of this technique.
Human liver cells were isolated from human liver tissue samples of surgical interventions by a two-step EGTA/collagenase P perfusion technique. PHH were separated from the NPC by an initial centrifugation at 50 x g. Density gradient centrifugation steps were used for removal of dead cells. Individual liver cell populations were isolated from the enriched NPC fraction using specific cell properties and cell sorting procedures. Beside the PHH isolation we were able to separate KC, LEC and HSC for further cultivation.
Taken together, the presented protocol allows the isolation of PHH and NPC in high quality and quantity from one donor tissue sample. The access to purified liver cell populations could allow the creation of in vivo like human liver models.

A technique to isolate human hepatocytes and non-parenchymal liver cells from the same donor is described. The different liver cell types build the basis for functional liver models and tissue engineering. This new method aims to isolate liver cells in a high yield and viability.

Beside parenchymal hepatocytes, the liver consists of non-parenchymal cells (NPC) namely Kupffer cells (KC), liver endothelial cells (LEC) and hepatic ...