Division of Gastrointestinal and Liver Diseases, USC Research Center for Liver Diseases, USC-UCLA Research Center for Alcoholic Liver and Pancreatic Diseases, Keck School of Medicine, USC, Los Angeles, CA
Division of Gastrointestinal and Liver Diseases, Keck School of Medicine, USC, HMR 415, 2011 Zonal Avenue, Los Angeles, CA 90033
Potential conflict of interest: Nothing to report.
Methionine adenosyltransferase (MAT) is an essential enzyme that catalyzes the biosynthesis of S-adenosylmethionine. Hepatic MAT activity falls in chronic liver diseases, and mice lacking Mat1a are predisposed to liver injury and develop hepatocellular carcinoma (HCC) spontaneously by 18 months. The current work examined the hypothesis that liver cancer stem cells contribute to HCC in this model. Livers from 6- and 18-month-old Mat1a-knockout (KO) mice and their wild-type (WT) littermates were fractionated and isolated by flow cytometry. CD45− nonparenchymal (NP) cells were cultured using liver stem cell conditions. Cells were analyzed by real-time PCR and fluorescent immunohistochemistry (FIHC). Tumor formation was assessed by injecting 1 × 106 CD133+CD49f+ cells intraperitoneally into immune-deficient mice. The proportion of CD49f+ and CD133+ cells in the CD45-NP fraction increased 4.5- to 5.5-fold from 6 to 18 months in KO mice but not in their WT littermates. Compared to CD49f− cells from old KO mice, CD49f+ cells from the same animals had a markedly increased expression of several oncogenes. CD133+ cells with CD49f coexpression were selected in vitro and exhibited rapid growth, with the expression of biliary cytokeratins, α-fetoprotein, and c-Met by FIHC. Clonal expansion of single CD133+CD49f+ cells revealed maintenance of bipotency. After CD133+CD49f+ cells were injected into immune-deficient mice, 3 of the 8 mice developed tumors of liver epithelial cells after 6–8 weeks. Conclusion: Mat1a−/− mice have expansion of liver stem cells as they age. These cells have increased expression of several oncogenes and are tumorigenic in vivo. This is the first demonstration of adult liver stem cells possessing tumorigenic potential without the use of a carcinogen or manipulation of tumor-suppressor or oncogene expression. (HEPATOLOGY 2008.)
If you can't find a tool you're looking for, please click the link at the top of the page to "Go to old article view". Alternatively, view our Knowledge Base articles for additional help. Your feedback is important to us, so please let us know if you have comments or ideas for improvement.
S-adenosylmethionine (SAMe) is the principal biological methyl donor and a key metabolite that regulates hepatocyte growth, differentiation, and death.1 The biosynthesis of SAMe occurs as the first step in methionine catabolism in a reaction catalyzed by methionine adenosyltransferase (MAT).2 Three distinct enzymes synthesize SAMe: MATI, MATII, and MATIII. MATI and MATIII are the gene products of MAT1A, whereas MATII is the gene product of MAT2A.3 In adult mammals, MAT1A is expressed predominantly in the liver, and MAT2A is expressed in all tissues.3
The liver plays a central role in the homeostasis of SAMe as the major site of its biosynthesis and degradation.1 SAMe is the link to 3 key metabolic pathways: polyamine synthesis, transmethylation, and transsulfuration, which converts homocysteine to cysteine, the rate-limiting precursor of GSH.1 Patients with cirrhosis have decreased SAMe biosynthesis because of lower hepatic MAT activity.4 This may contribute to a decreased hepatic GSH level in these patients as SAMe administration normalizes GSH levels.5
The Mat1a−/− mouse model allows us to study the consequences of chronic hepatic SAMe deficiency. Mat1a−/− mice have markedly increased serum methionine levels and reduced hepatic SAMe and GSH levels.6Mat1a−/− mice are more prone to develop choline-deficient diet-induced fatty liver and develop spontaneous nonalcoholic steatohepatitis by 8 months and hepatocellular carcinoma (HCC) by 18 to 20 months.1, 6 Because mice fed a diet deficient in methionine also develop steatohepatitis and are more susceptible to developing HCC, it raises the possibility that SAMe deficiency may have been responsible for these pathological changes.7 The mechanism for HCC formation in Mat1a−/− mice is unknown.
Methyl-deficient diets have been used to induce oval cell proliferation and HCC formation in susceptible models such as p53−/− mice.8 Oval cells (OCs) are liver stem cells found in the nonparenchymal (NP) fraction of the liver and reside near the terminal bile ducts, at the hepatocyte–cholangiocyte interface.9 In normal adult liver, OCs are quiescent and few in number and proliferate only during severe, prolonged liver injury and in various models of experimental carcinogenesis.10 OCs isolated from p53-null mice treated with a choline-deficient ethionine-supplemented diet induced tumors in athymic mice.8 There are no reports of tumorigenic progenitor cells isolated from adult mouse liver not involving the use of a carcinogen or manipulation of tumor-suppressor/oncogene expression.
Various markers have been used to characterize murine OCs. In this work, we focused on CD49f and CD133 as cell surface markers of OCs. CD49f has been used as a cell surface marker of fetal hepatoblasts.11 CD49f represents α-6 integrin on epithelial cells, binding to laminins in the basement membrane.12 CD133, or Prominin1, is a membrane protein found on several types of adult stem cells13 and cancer stem cells.14 Single-cell analysis confirmed the bilineage potential of CD133+CD45− OCs isolated from the 3,5-diethoxycarbonyl-1,4-dihydro-collidine (DDC)–induced chronic liver damage model.15
Our hypothesis is that liver cancer stem cells contribute to carcinoma formation in the Mat1a−/− mouse, a model of chronic liver injury. We used cell surface markers and flow cytometry to identify and isolate a novel population in an OC-enriched fraction. These populations were characterized by gene expression and fluorescent immunohistochemistry. In vitro analysis confirmed an OC phenotype, and an in vivo tumorigenic assay demonstrated that these cells are capable of forming epithelial tumors.
Mice were fed ad libitum a standard diet (Harlan Teklad irradiated mouse diet 7912, Madison, WI) and housed in a temperature-controlled animal facility with a 12-hour light/12-hour dark cycle. Animals were treated humanely, and all procedures were in compliance with our institution's guidelines for the use of laboratory animals and were approved by the Institutional Animal Care and Use Committee. Six- month-old and 18-month-old Mat1a−/− mice and their wild-type (WT) littermates were used for all experiments as described.6 Six-week-old NOD/SCID/Gamma-chain-null mice (The Jackson Laboratory, Bar Harbor, ME) were used for tumor formation analysis.
Parenchymal and Nonparenchymal Cell Separation.
The protocol for the digestion and centrifugation of the liver cells was modified from Shimano,16 as described.17 Liver was minced and digested with collagenase, pronase, and DNAse (Sigma, St. Louis, MO) and filtered using a 70-μm pore filter (BD Biosciences, Franklin Lakes, NJ). After suspension in 10% fetal bovine serum (Omega Scientific, Tarzana, CA) in phosphate-buffered saline (PBS; Mediatech, Herdon, VA), cells were centrifuged using a BD GS-6R centrifuge.17 The final NP cell pellet was resuspended in a 1× ammonium chloride red blood cell (RBC) lysis buffer (PharMLyse, BD Pharmingen, San Diego, CA) and washed, and the NP cells were counted and subjected to CD45 depletion using Miltenyi magnetic bead depletion per the manufacturer's protocol (Miltenyi Biotech, Auburn, CA).
FACS Analysis of the Oval Cell–Enriched NP Fraction.
Freshly isolated liver NP cells (1 × 106) that were RBC and CD45 depleted were resuspended in PBS. Alternatively, cells in culture were trypsinized for 3 minutes and then washed once in culture medium and a second time in PBS. Following Fc blocking, combinations of the following flow cytometry (FACS) antibodies were added: CD45 fluorescein isothiocyanate (FITC), phycoerythrin (PE), and allophycocyanin (APC); CD34 FITC and PE; Thy 1.2 FITC and PE; c-Kit FITC; Sca-1 FITC and PE; CD49f PE (BD Pharmingen); and CD133 FITC and PE (eBioscience, San Diego, CA), incubated at 4°C for 30 minutes. Cells were washed with PBS prior to analysis using a FACSCalibur (BD Bioscience). Cells isolation was conducted on a FACS Vantage (BD Bioscience). Compensation for FITC, PE, and APC was performed using compensation beads (BD Pharmingen). Analysis was done using the Flow-Jo program (Tree Star, Ashland, OR). Positive and negative gates were determined using IgG stained and unstained controls.
Real-Time Polymerase Chain Reaction of FACS Isolated Cells.
CD49f+CD45− and CD49f−CD45− NP liver cells were isolated on a BD FACS-Vantage. Cells were pelleted at 200g for 5 minutes, and total RNA was extracted using an RNA Easy Kit (Qiagen, Valencia, CA) per the manufacturer's protocol. RNA was quantified using an ND-1000 spectrophotometer (Nanodrop Technologies, Wilmington, DE). Then 200 ng of purified mRNA per 20-μL reaction volume was used to construct first-strand cDNA using an oligo (dT) reverse-transcriptase kit at 37°C for 60 minutes (Invitrogen, Carlsbad, CA). Real-time experiments were conducted using an ABI-Prism 7700 Thermal Cycler and TaqMan Universal PCR Master Mix (Applied Biosystems, Foster City, CA). Housekeeping genes included β-actin, hypoxanthine phosphoribosyl-transferase 1, and ubiquitin C; and a geometric mean of housekeeping Ct values was used for all ΔΔCt calculations.18 Relative expression was calculated for the genes albumin, Ck19, Hnf4α, c-Met, epidermal growth factor receptor (Egfr), cyclin D1, Kras, Nras, Survivin, c-Myc, Mat2a, and Abcg2, which were assessed using real-time PCR primer/probe sets (Applied Biosystems). Amplification efficiency of the amplification plots was determined by the ΔΔCt method.19
CD45− cells were isolated from the NP fraction using magnetic bead separation as described in the Parenchymal and Nonparenchymal Cell Separation section. This CD45− NP cell fraction was labeled with CD133 magnetic bead antibodies (Miltenyi), and CD133+CD45− cells were isolated using positive cell selection per the manufacturer's protocol. This enriched population of CD133+CD45− cells was plated in BioCoat 6-well laminin-coated culture plates (BD Bioscience) at a density of 1 × 104 cells/cm2. The culture medium was modified from Suzuki.12 The medium contained DMEM:F12 at 1:1 (Sigma) with 10% fetal bovine serum, was heat inactivated (Omega Scientific, Tarzana, CA), and had the following additives: insulin (1 mg/mL), dexamethasone (1 × 10−7 mol/L), nicotinamide (10 mmol/L), Hepes (5 mmol/L), and penicillin/streptomycin (1% [vol/vol]), all from Sigma. Recombinant hepatocyte growth factor (HGF; 50 ng/mL) and epidermal growth factor (EGF; 20 ng/mL), both from Sigma, were added on day 1. The medium was changed every 3 days. For alkaline phosphatase analysis, cells were fixed in 90% methanol/10% formalin (Sigma) for 1 minute and stained using an Alkaline Phosphatase Detection Kit (Chemicon International, Temecula, CA).
Gene Expression of CD133+CD49f+CD45− Cells.
RNA was extracted directly from the culture well using an RNA Easy Kit (Qiagen). Two hundred nanograms of purified RNA per 20-μL reaction volume was used in the synthesis of first-strand cDNA as described previously. PCR was conducted using the primers listed in Table 1. All primers were selected in 2 separate exons to distinguish cDNA from possible contaminating genomic DNA, and PCR conditions were used as described.17
Table 1. Primers Used for Real-Time PCR
Abcg2 transmembrane pump
α-Smooth muscle actin
For single-cell experiments, DAPI was used as a marker of cell viability. Single CD133+CD49f+CD45−DAPI− OCs (n = 192) were isolated using a FACS Vantage set for Single Cell Purity, and single cells were each robotically plated directly in a 96-well flat-bottomed, laminin-coated plate (BD Bioscience) with 100 μL of medium/well as described.20 After 24 hours, an additional 100 μL of medium was added to each well. Approximately half the medium was replaced after 1 week. After 3 week in culture, single-cell-derived colonies that filled more than 50% of the well area had RNA extracted for RT-PCR analysis (n = 4 for PCR analysis).
Tumor Formation Assay.
CD133+CD49f+CD45− cells and CD133-CD49f+CD45− cells were isolated from bulk culture as already described and counted with trypan blue exclusion to determine numbers of live cells. Cells were resuspended in PBS for transplant at a concentration of 1 × 106 live cells/50 μL. Six-week-old immune-deficient NOD/SCID/Gama-chain-null mice were injected intraperitoneally as described.14 Mice were sacrificed after 6 to 8 weeks, and liver, spleen, and tumors were isolated for immunohistochemistry.
Fluorescent immunohistochemistry (FIHC) was performed on perpendicular wedges of liver, spleen, and tumor after injection with CD133+CD49f+CD45− and CD133-CD49f+CD45− cells. Tissues were fixed and paraffin embedded as described.21 After antigen retrieval (Vector Unmasking Solution, Vector Labs, Burlingame, CA), the slides were incubated with Tris-buffered saline (TBS; pH 7.5, 100 mM Tris, 150 mM NaCl) + 0.1% Triton X solution. Slides were blocked for nonspecific binding using TBS + 0.1% Tween 20 (TBST; Sigma) with 1% bovine albumin (Sigma) and 5% normal donkey serum (Jackson ImmunoResearch, West Grove, PA). Slides were incubated with primary antibody overnight at 4°C (concentration in TBST 1% BSA): rabbit anti-cow pancytokeratin (pan-CK; 1:400; DAKO, Carpintera, www.dako.com),22 rabbit antimouse albumin (1:200; Accurate Chemical and Scientific, Westburry, NY), rat antimouse A6 (1:10; generous gift of Dr. V. Factor), mouse antimouse alpha-fetoprotein (AFP; 1:100; R&D Systems, Minneapolis, MN), and rat antimouse CD45 (1:100; AbCam, Cambridge, MA). Slides were washed twice and incubated with secondary antibodies at room temperature for 2 hours. Secondary antibodies (concentration in TBST 1% BSA) included: donkey antirabbit FITC or Cy3, donkey antirat Cy3, and donkey antimouse Cy3 (all 1:200; AbCam). The slides were washed and mounted with coverslips using Vectashield with DAPI (Vector). All FIHC experiments were conducted with negative and positive controls.
Images were viewed with a Leica DMRA microscope using a Plan Apo 40×/1.25 NA phase 3 DIC or Plan Apo 63 X/1.32 oil immersion objective lens (Leica Microsystems, Wetzlar, Germany). The microscope was equipped with a Shutter LS175W ozone-free xenon arc lamp (Shutter Instrument, Novato, CA). Images were acquired with an Applied Spectral Imaging Sky Vision-2/VDS camera from EasyFISH software (Applied Spectral Imaging, Vista, CA) and printed using Adobe Photoshop (Adobe Systems, San Jose, CA).
The paired 2-tailed Student t test was used when comparing 2 groups. A P value less than 0.05 was considered significant. ANOVA analysis was used for comparison of multiple groups, followed by pairwise multiple comparison procedures (Systat Software, Richmond, CA).
Expansion of Oval Cells with Age in Mat1a−/− Mice.
Six- and 18-month-old Mat1a−/− mice were analyzed for degree of injury and OC proliferation using hematoxyin and eosin (H&E) staining and pan-CK FIHC as an OC marker.10 In 6- and 18-month-old WT animals, H&E staining revealed no injury, steatosis, or OC proliferation (Fig. 1A). In the Mat1a−/− mice, H&E staining revealed significant injury and steatosis, with OCs expanding from portal zones in the 18-month-old mice (Fig. 1B). This injury and morphological OCs in old Mat1a−/− mice correlated with increased panCK staining in the same animals (Fig. 1E). This degree of OC proliferation was consistent with DDC-induced injury, a common method of inducing OC proliferation (Fig. 1C,F).23 There was no evidence of gross or microscopic tumor in any of the animals assessed.
For FACS analysis, CD45 depletion removed all CD45+ hematopoietic cells prior to analysis. FACS analysis of the NP OC-enriched fraction has been previously described in isolating CD133+CD45− OCs.15 Using FACS analysis, a comparison of 6- and 18-month-old mice demonstrated a significant increase in CD133+CD45− and CD49f+CD45− NP cells (6-month WT CD133+, 4% ± 2%, and CD49f+, 3.5% ± 2%; 6-month knockout [KO] CD133+, 6.5% ± 3%, and CD49f+, 6% ± 3%; 18-month WT CD133+, 5.5% ± 2%, and CD49f+, 5% ± 3%; and 18-month KO CD133+, 26% ± 7%, and CD49f+, 23% ± 5%; P < 0.05 for 18-month KO group compared with other groups using ANOVA, n = 4 mice/group; Fig. 2A –E). When CD133 and CD49f were analyzed simultaneously, 9% ± 4% cells coexpressed both CD133 and CD49f in old KO mice.
Increase in Oncogene Expression in CD49f+CD45− Cells Isolated from Old Mat1a−/− Mice.
CD49f+CD45− and CD49f−CD45− cells were FACS isolated from young and old WT and Mat1a−/− mice (n = 3/group). CD49f+CD45− NP cells from 18 month-old Mat1a−/− mice demonstrated the highest relative levels of Kras, Nras, Survivin, and Egfr compared with any other group. When isolated from the same old Mat1a−/− mouse, CD49f+CD45− NP cells demonstrated a marked increase in the expression of Kras (8-fold) and Survivin (8-fold) mRNA compared with CD49f−CD45− NP cells (Fig. 3B). The same population of CD49f+CD45− NP cells from 18-month-old Mat1a−/− mice demonstrated increased expression of oncogenes and cyclin D (5.4-fold) when compared with CD49f+CD45− NP cells isolated from 6-month-old Mat1a−/− mice (Fig. 3C), indicating a mechanism of proliferation during the aging process. CD49f+CD45− cells from 18-month-old Mat1a−/− mice demonstrated an increase in Mat2a expression (4.5-fold) compared with that in the same population isolated from WT animals (Fig. 3D).
Enrichment of CD133+CD49f+ Oval Cells.
To further characterize lineage potential, CD133+CD45− OCs were isolated from 18-month-old Mat1a−/− mice using a 2-step enrichment process of magnetic filtration. After enrichment, CD133+CD45− OCs (85% with CD49f coexpression) were plated in 6-well, laminin-coated tissue culture plates using a fetal hepatoblast-derived medium.12 Laminin-coated plates allow for further selection of CD49f+ cells. On day 1, small, round cells were observed adhering to the plate (Fig. 4A). After 1 week in culture, clusters of cells were observed growing, with most cells having a morphology that ranged from flat, cuboidal cells in sheets to more elongated cells with projections (Fig. 4D). After 1 week in culture, the cells were 90% confluent, and were trypsinized and replated 1:3. Early-passage cells (passages 1–4) cultured in identical conditions without HGF and EGF failed to form colonies.
Characteristics of Plated CD133+CD49f+ Cells.
After 6 months of replating, the basic morphology of the cells was maintained. In terms of CD49f, 90.3% ± 2.8% of cells expressed CD49f+ in passages 20–24, indicating stable expression from early to late passage (Fig. 4J,K). In contrast, C133 expression was not stable in vitro. In early-passage cells (passages 1–4), the expression of CD133 decreased after positive selection, to a stable baseline of 15% after 1 week. Using a process of positive selection to isolate CD133+ cells from later-passage (passages 20–24) cultures revealed a similar loss of CD133 expression over time, with a starting population of 71% ± 12% CD133+ cells immediately postisolation and a gradual decline in CD133 expression to 15% after 7–10 days (Fig. 4K). Of the CD133+ cells in these later-passage cultures, 99.0% ± 0.4% coexpressed CD49f+ (Fig. 4K).
In terms of functional analysis of later-passage cells, alkaline phosphatase staining demonstrated single cells and clusters of cells with alkaline phosphatase activity (Fig. 4I). Alkaline phosphatase staining has been used to identify primitive embryonic stem cells as well as biliary epithelium.24, 25 These same cells also demonstrated AFP and A6 staining, both markers of OCs (Fig. 4E,G).
Costaining of hepatocyte (AFP) and cholangiocyte (CK) markers was conducted to confirm the oval cell phenotype in vitro. Of the 1000 cells counted, 74% ± 8% were positive for CK, 49% ± 10% were positive for AFP, and 33% ± 4% were double positive for both markers (Fig. 5). This analysis confirms maintenance of a bipotent population of oval cells in later-passage cells. Because later-passage cultures had selected for CD49f and 99% of the CD133+ cells coexpresssed CD49f, we elected to further analyze the specific fraction of CD133+CD49f+ cells from later-passage cultures (passages 20–24).
Single-Cell Isolation Defines Bipotency in CD133+CD49f+CD45− OCs.
Single cells were isolated by FACS using automated plating robotics. CD133+CD49f+CD45−DAPI− cells were selected from late-passage cultures (passages 20–24, Fig. 6A). Of 192 individual cells plated, 28 (14.5%) demonstrated colonies growing over more than 50% of the well bottom after 2 weeks. These colonies were replated into 6-well plates, and the basic cell morphology matched that of the original culture, with flat, cuboidal cells (Fig. 6B,C). After 2 weeks, 100% of analyzed colonies demonstrated expression of both hepatocyte (Albumin and α1-Antitrypsin) and cholangiocyte (Ck19, γGt, and aquaporin 1) markers, as well as strong expression of oval cell–associated genes (Hnf4α, Hnf1β, and Abcg2).26 All CD133+CD49f+CD45− clones demonstrated strong expression of both c-Met and Egfr. Last, no expression of hematopoietic (Cd45) or stellate cell (α-smooth muscle actin and desmin) markers were demonstrated in CD133+CD49f+CD45− clones (n = 4 clones analyzed, Fig. 6D).
Tumor Formation from CD133+CD49f+CD45− Cells.
To assess the tumor-forming ability of CD133+CD49f+CD45− versus CD133−CD49f+CD45− cells isolated from late-passage cultures, a tumor model with immune-deficient mice was used.14 One million CD133+CD49f+CD45− or CD133−CD49f+CD45− cells isolated from late-passage cultures were injected intraperitoneally into immune-deficient mice (n = 8/group). No CD133−CD49f+CD45− cells formed tumors after 6–8 weeks. Three (37.5%) of the CD133+CD49f+CD45− cell injections resulted in tumor formation. Two of the tumors detected after 6 weeks were single 4-mm tan, round nodules growing on the mesentery, and the third tumor was a 15-mm tan growth on the liver detected 8 weeks after injection (Fig. 7A). Histology and FIHC of the mesenteric tumors demonstrated immature, small, round cells with cytokeratin staining (Fig. 7D,E). Very little CD45 was demonstrated in these tumors (Fig. 7F). The larger liver tumor consisted of poorly organized hepatocyte-like cells with albumin staining (Fig. 7B,C). Positive control staining included normal liver for cytokeratin and spleen for CD45. FACS analysis of the largest tumor demonstrated that most cells were both CD133+ (60.4%) and CD49f+ (77.2%). No gross lung tumors or nodules were observed in any animals.
The relationship between OCs and liver cancer stem cells is poorly understood. In his review, Sell proposed 2 main cellular origins of hepatocellular carcinomas: the mature hepatocyte causing HCC and the bipotent cancer stem cell causing HCC or mixed tumors.27 Progenitor or OC-derived carcinomas tend to have a more aggressive phenotype, with as many as 50% of HCCs defined as having a progenitor cell phenotype, expressing makers of both hepatocytes and cholangiocytes.28 Although this model of aggressive HCC with a stem cell phenotype has been validated in murine models and human patients, a defined population of liver cancer stem cells remains elusive.29
The ability to identify and isolate adult liver stem cells is an essential first step in studying their potential for cancer formation.30 In the past, investigators identified OCs based on their histological location, risking the inclusion of hematopoietic cells in the analysis. In models of liver damage, such as Mat1a−/− mice, which have hepatic infiltration of inflammatory cells, separation of hematopoietic cells from liver cells is critical prior to analysis.17 In defining a reliable OC immunophenotype, the surface markers previously attributed to OCs, such as c-kit and CD34, are traditionally assigned to hematopoietic stem cells.31 Single-cell gene expression analysis has recently confirmed the bilineage potential of CD133+CD45− OCs isolated from the DDC toxic injury model.15 Single-cell clonal studies in fetal liver have identified fetal hepatoblasts with CD49f expression that are capable of both cholangiocyte and hepatocyte differentiation in vivo.11 Our current work is the first to use single-cell FACS isolation and clonal expansion to demonstrate bilineage potential in liver cells isolated from adult animals. CD133+CD49f+CD45− cells consistently demonstrated both hepatocyte and cholangiocyte markers, and 100% of CD133+CD49f+CD45− single-cell clones demonstrated bilineage potential.
The cell surface marker CD133 has been associated with both multipotent stem cells and cancer stem cells of epithelial origin.32 CD133, or Prominin 1, was originally described in 1997 as being localized to the apical membrane protrusions of murine neuroepithelial cells.33 A marker with similar homology was described later on the surface of human hematopoietic stem cells.13 Both human and mouse CD133 have 5 membrane-spanning domains and share 60% homology at the protein level.34CD133 mRNA was detected in rat OCs, isolated by size, as part of a microarray screen.35
In our in vitro analysis, we initially plated CD133+CD45− OCs on laminin-coated culture dishes to further select for CD49f+ cells. Freshly isolated CD49f+CD45− cells from old Mat1a−/− mice demonstrated the highest levels of HCC-associated oncogenes such as Kras and Survivin. We also demonstrate that CD133 identifies a subpopulation of CD49f+ NP cells isolated from adult liver, with the traditionally accepted morphology and size of OCs. CD133+CD49f+CD45− OCs proliferated and significantly expanded in number in vitro. Furthermore, these cells have tumorigenic potential when injected into immunodeficient mice. The histology of tumors that formed was mixed; the smaller mesenteric tumors were undifferentiated epithelial carcinomas, whereas the largest tumor was more consistent with a hepatocellular carcinoma. FACS analysis of the largest tumor showed that most cells were both CD133+ and CD49f+, confirming the origin of the tumor from CD133+/CD49f+ cells. This is the first report of tumorgenic OCs without manipulation of oncogenes or use of a carcinogenic regimen.8
Expansion of OCs with age in Mat1a−/− mice is consistent with the known effects of a methyl-deficient diet's ability to induce OC proliferation.10, 36 These diets would be expected to also lower hepatic SAMe level. Whether expansion of the OCs occurred because of increased oxidative stress or liver injury or because of chronic SAMe deficiency is unknown. The possibility that SAMe can directly influence the growth of OCs is real, as SAMe is an important regulator of hepatocyte growth.1 In hepatocytes, SAMe level is related to differentiation status, being high in quiescent and low in proliferating hepatocytes. A fall in SAMe level occurs early after partial hepatectomy,37 and if prevented, liver regeneration is impaired.38 We have shown recently that SAMe inhibits hepatocyte growth by blocking the effect of HGF.39 Thus, in chronic hepatic SAMe deficiency such as that in Mat1a−/− mice, there is increased baseline cyclin D expression and other growth markers.38 The exact molecular mechanisms and signaling pathways responsible for the expansion of OCs in this mouse model will require further investigations.
In summary, we have demonstrated expansion of liver progenitor cells in the Mat1a−/− mice during aging. These cells have been singly isolated, analyzed, and clonally expanded. The CD133+ fraction of CD49f+ cells exhibited in vivo tumorigenic potential. These findings are highly relevant to patients with cirrhosis in whom MAT1A expression is often low or absent and the risk of HCC is high. Our results suggest that expansion of liver cancer stem cells can occur in the setting of chronic hepatic SAMe deficiency, and this can contribute to HCC formation.