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Oral Methylthioadenosine Administration Attenuates Fibrosis and Chronic Liver Disease Progression in Mdr2−/− Mice

  • M. Ujue Latasa ,

    Contributed equally to this work with: M. Ujue Latasa, Carmen Gil-Puig

    Affiliation Division of Hepatology and Gene Therapy, CIMA, University of Navarra, Pamplona, Spain

  • Carmen Gil-Puig ,

    Contributed equally to this work with: M. Ujue Latasa, Carmen Gil-Puig

    Affiliations Division of Hepatology and Gene Therapy, CIMA, University of Navarra, Pamplona, Spain, Digna Biotech, Madrid, Spain

  • Maite G. Fernández-Barrena,

    Affiliations Division of Hepatology and Gene Therapy, CIMA, University of Navarra, Pamplona, Spain, CIBERehd, University Clinic, University of Navarra, Pamplona, Spain

  • Carlos M. Rodríguez-Ortigosa,

    Affiliations Division of Hepatology and Gene Therapy, CIMA, University of Navarra, Pamplona, Spain, CIBERehd, University Clinic, University of Navarra, Pamplona, Spain

  • Jesús M. Banales,

    Affiliations Division of Hepatology and Gene Therapy, CIMA, University of Navarra, Pamplona, Spain, CIBERehd, University Clinic, University of Navarra, Pamplona, Spain

  • Raquel Urtasun,

    Affiliation Division of Hepatology and Gene Therapy, CIMA, University of Navarra, Pamplona, Spain

  • Saioa Goñi,

    Affiliation Division of Hepatology and Gene Therapy, CIMA, University of Navarra, Pamplona, Spain

  • Miriam Méndez,

    Affiliation Division of Hepatology and Gene Therapy, CIMA, University of Navarra, Pamplona, Spain

  • Sara Arcelus,

    Affiliation CIBERehd, University Clinic, University of Navarra, Pamplona, Spain

  • Nerea Juanarena,

    Affiliation Division of Hepatology and Gene Therapy, CIMA, University of Navarra, Pamplona, Spain

  • Juan A. Recio,

    Affiliation Vall d'Hebron Research Institute, Institute of Oncology and Hospital, Barcelona, Spain

  • Sophie Lotersztajn,

    Affiliations Inserm, U955, Créteil, France, Université Paris-Est, Faculté de Médecine, UMR-S955, Créteil, France

  • Jesús Prieto,

    Affiliations Division of Hepatology and Gene Therapy, CIMA, University of Navarra, Pamplona, Spain, CIBERehd, University Clinic, University of Navarra, Pamplona, Spain

  • Carmen Berasain,

    Affiliation Division of Hepatology and Gene Therapy, CIMA, University of Navarra, Pamplona, Spain

  • Fernando J. Corrales,

    Affiliation Division of Hepatology and Gene Therapy, CIMA, University of Navarra, Pamplona, Spain

  • Jon Lecanda ,

    These authors also contributed equally to this work.

    Affiliations Division of Hepatology and Gene Therapy, CIMA, University of Navarra, Pamplona, Spain, Digna Biotech, Madrid, Spain

  •  [ ... ],
  • Matías A. Ávila

    These authors also contributed equally to this work.

    Affiliation Division of Hepatology and Gene Therapy, CIMA, University of Navarra, Pamplona, Spain

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Oral Methylthioadenosine Administration Attenuates Fibrosis and Chronic Liver Disease Progression in Mdr2−/− Mice

  • M. Ujue Latasa, 
  • Carmen Gil-Puig, 
  • Maite G. Fernández-Barrena, 
  • Carlos M. Rodríguez-Ortigosa, 
  • Jesús M. Banales, 
  • Raquel Urtasun, 
  • Saioa Goñi, 
  • Miriam Méndez, 
  • Sara Arcelus, 
  • Nerea Juanarena



Inflammation and fibrogenesis are directly related to chronic liver disease progression, including hepatocellular carcinoma (HCC) development. Currently there are few therapeutic options available to inhibit liver fibrosis. We have evaluated the hepatoprotective and anti-fibrotic potential of orally-administered 5′-methylthioadenosine (MTA) in Mdr2−/− mice, a clinically relevant model of sclerosing cholangitis and spontaneous biliary fibrosis, followed at later stages by HCC development.


MTA was administered daily by gavage to wild type and Mdr2−/− mice for three weeks. MTA anti-inflammatory and anti-fibrotic effects and potential mechanisms of action were examined in the liver of Mdr2−/− mice with ongoing fibrogenesis and in cultured liver fibrogenic cells (myofibroblasts).

Principal Findings

MTA treatment reduced hepatomegaly and liver injury. α-Smooth muscle actin immunoreactivity and collagen deposition were also significantly decreased. Inflammatory infiltrate, the expression of the cytokines IL6 and Mcp-1, pro-fibrogenic factors like TGFβ2 and tenascin-C, as well as pro-fibrogenic intracellular signalling pathways were reduced by MTA in vivo. MTA inhibited the activation and proliferation of isolated myofibroblasts and down-regulated cyclin D1 gene expression at the transcriptional level. The expression of JunD, a key transcription factor in liver fibrogenesis, was also reduced by MTA in activated myofibroblasts.


Oral MTA administration was well tolerated and proved its efficacy in reducing liver inflammation and fibrosis. MTA may have multiple molecular and cellular targets. These include the inhibition of inflammatory and pro-fibrogenic cytokines, as well as the attenuation of myofibroblast activation and proliferation. Downregulation of JunD and cyclin D1 expression in myofibroblasts may be important regarding the mechanism of action of MTA. This compound could be a good candidate to be tested for the treatment of (biliary) liver fibrosis.


Liver diseases are currently the fifth cause of mortality in the Western world, and as opposed to other major causes of mortality their incidence is increasing [1], [2]. The principal causes of the most common liver ailments are well known, and include chronic alcohol consumption, infection by hepatitis viruses, genetic conditions such as hemochromatosis or α1-antitrypsin deficiency, autoimmune hepatitis and metabolic disorders [1], [2]. Regardless of the etiology, chronic tissue injury and inflammation are increasingly recognized as driver mechanisms in liver disease progression from fibrosis, characterized by the excessive accumulation of extracellular matrix (ECM), to hepatocellular carcinoma (HCC) [1][3]. The molecular links in the so-called inflammation-fibrosis-cancer axis in the liver are currently being elucidated in experimental models of acute and chronic injury. These links include a variety of intracellular pathways triggered by extracellular mediators like the cytokines interleukin 1 (IL1), IL6 and tumour necrosis factor alpha (TNFα), platelet-derived growth factors and transforming growth factor beta (TGFβ), among others [3][5]. These growth factors and cytokines stimulate ECM synthesis by the activation of hepatic stellate cells and myofibroblasts in the hepatic parenchyma [3][5]. Targeted interference with these and other mediators has clearly shown a beneficial effect on the course of the experimental disease, lending support to their pathological role [6], [7]. However, in spite of these remarkable advances the availability of safe and efficacious therapies to halt the progression of fibrosis and liver disease in humans is still limited [8], [9]. The use of experimental models of chronic liver injury resembling the human pathology is important to evaluate candidate drugs with chances of succeeding in the clinical setting. One such experimental model are the Mdr2/Abcb4-deficient mice (Mdr2−/−), which lack the canalicular phosphatidylcholine flippase [10]. The absence of phosphatidylcholine from bile occurring in these mice leads to bile regurgitation into the portal tracts, causing periportal inflammation and injury early in life (2–3 weeks), periportal fibrosis (4 weeks), and the appearance of preneoplastic lesions (at 4–6 months) [10][12]. These pathogenic characteristics resemble what occurs in human primary sclerosing cholangitis and biliary fibrosis, making these mice an excellent model to study disease mechanisms, and a test ground for hepatoprotective and antifibrotic therapies [10][13]. In analogy to the situation found in humans, protracted injury and inflammation lead to HCC development in virtually 100% of Mdr2−/− mice by 16 months [14].

We and others have previously demonstrated the in vivo anti-inflammatory effects of 5′-methylthioadenosine (MTA), a sulphur-containing adenine nucleoside produced from S-adenosylmethionine (SAMe) during polyamine biosynthesis [15]. Parenteral MTA administration reduces the production of inflammatory mediators triggered by bacterial lipopolysaccharide or pro-inflammatory peptides in mice [16][18], and protects from liver injury in rats treated with CCl4 or with the carcinogen diethylnitrosamine [19], [20]. MTA is therefore a compound with an attractive pharmacological profile for the treatment of chronic liver disease. Using the Mdr2−/− mice as a model, here we show for the first time that orally administered MTA attenuates liver injury and inflammation, and inhibits the progression of hepatic fibrosis. The mechanism of action of MTA is likely to be multifaceted. MTA reduced the production of inflammatory and pro-fibrogenic mediators and inhibited the proliferation and activation of fibrogenic cells. These observations gathered in the Mdr2−/− mouse model indicate that MTA could be useful for the treatment of biliary fibrosis and conditions such as primary sclerosing cholangitis, a severe disease frequently associated with hepatobiliary cancer and with limited therapeutic options.


Ethics statement

Animals received humane care and study protocols complied with our institution's guidelines and the recommendations of the European Accreditation of Laboratory Animal Care. The protocol was approved by the Committee on the Ethics of Animal Experiments of the University of Navarra (protocol number: 025-10).

Animal studies

Male Mdr2−/− and Mdr2+/+ mice (The Jackson Laboratory, Bar Harbor, ME) were fed standard laboratory diet. Two groups of mice per genotype were established (2 months old, n = 8 per group). One group received a daily oral dose of 30 mg/Kg body weight of MTA dissolved in 0.2% dimethylsulfoxide by gavage for three weeks, the control group received the same volume of vehicle (0.2% dimethylsulfoxide). MTA was from Enantia S.L. (Barcelona, Spain). This dose of MTA has been used previously, but was administered intraperitoneally [16], [17]. Liver enzymes and bilirrubin levels were analyzed in serum (Cobas® analyzer, Roche). Livers were excised, weighted, and were either snap frozen or fixed in formalin and paraffin-embedded.

Metabolite measurement in liver tissues

Glutathione (GSH) was measured using the Gluthatione Assay Kit (Sigma, St. Louis, USA). Tissue samples were processed as recommended by the manufacturer. SAMe was measured as previously described [21].

Tissue staining and immunohistochemistry

Tissue sections were stained with Picro-Sirius Red to visualize collagen deposition as reported [22]. For morphometric analysis images were captured at 100X magnification (Nikon Eclipse 1000), and percentage of collagen cover per field was estimated with an Arkon software (Arkon Resources Inc. Arcadia, CA) as described [22]. Values are the means of five fields taken from different tissue sections per mouse. Immunodetection of α-smooth muscle actin (αSMA) on liver sections was carried out as described using a monoclonal anti-αSMA antibody (#A2547) from Sigma (St. Louis, MO) [22]. Tenascin-C and Ki-67 immunostainings were performed using rabbit polyclonal antibodies from Millipore (#AB1951) (Millipore Iberica, Madrid, Spain) and Abcam (#ab833) (Cambridge, UK) respectively. Immunostaining for CD45 was performed with a rat-anti-mouse CD45 antibody (clone 30-F11, #103101) from BioLegend (San Diego, CA).

Cell culture and treatments

Liver myofibroblasts were isolated from wild type and Mdr2−/− mice by collagenase perfusion and density-gradient purification in Nycodenz, and cultured in Dulbecco's Modified Eagle's medium (DMEM) containing 10% fetal calf serum (FCS) as described [23]. For [3H]thymidine incorporation myofibroblasts were incubated under the specified conditions for 24 h with 2 µCi/ml [3H]thymidine. Cells were lysed and radioactivity measured as described [22]. Human recombinant platelet derived growth factor BB (PDGF) was from Calbiochem (#521225) (Merck KGaA, Darmstadt, Germany). MTA showed no cytotoxic effects, as determined by measuring lactate-dehydrogenase in culture media using the Cytotox assay (Promega, Madison, WI). Apoptosis was measured in cultured myofibroblasts using the Cell Death Detection Assay from Roche (Barcelona, Spain) as previously described [22].

The murine monocyte/macrophage RAW 264.7 cells (American Type Culture Collection, ATCC) were cultured in DMEM supplemented with 10% FCS. Where indicated cells were treated with Salmonella typhymurium lipopolysaccharide (LPS) (50 mg/mL) from Sigma (#L6511, Lot#3944110). The adenosine receptor agonist 5′-(N-Ethylcarboxamido) adenosine (NECA) and the adenosine A2B receptor antagonist MRS 1754 were from Sigma, the adenosine A2A receptor antagonist ZM 241385 was purchased from Tocris Bioscience (Bristol, UK). TNFα concentration in conditioned media was measured using an enzyme-linked immunosorbent assay (ELISA) kit from BD Biosciences (San Diego, CA).

RNA isolation and quantitative real-time RT-PCR

Total RNA was extracted using the TRI Reagent (Sigma). Real time PCR was performed using an iCycler (BioRad, Hercules, CA) and the iQ SYBR Green Supermix (BioRad) as reported [22]. Gene expression was determined using the ΔΔCT calculation as described [21], [22]. We designed all primers to distinguish between genomic and cDNA amplification and sequenced all PCR products to confirm the specificity. Primers for α1(I)-procollagen, matrix metalloprotease-13 (MMP13) and TIMP1 determination were described previously [22]. αSMA, TGFβ1 and TGFβ2 primers were as reported [11], TNFα, IL6 and inducible NO synthase (iNOS) primers were as described [17], tenascin-C primers were as reported [24]. Monocyte chemotactic protein-1 (Mcp-1) primers were: sense 5′-CCACTCACCTGCTGCTACTC-3′, antisense 5′-TTCACATTCAAAGGTGCTGAAG-3′. JunD primers were: sense 5′-CGCCCATCGACATGGACAC-3′, antisense 5′-GTTGACGTGGCTGAGGACTT-3′. Adenosine A2B receptor primers were: sense 5′-TGGCGCTGGAGCTGGTTA-3′, antisense 5′-GCAAAGGGGATGGCGAAG-3′.

Western blot analysis

Tissues and cells were homogenized and analyzed by Western blotting as described [22]. The antibodies used were: anti-cyclin-D1 (#sc-450), anti-c-Jun N-terminal kinase (JNK) (#sc-571), anti-phospho-extracellular signal-regulated kinase (Tyr204) (pErk1/2) (#sc7383), anti-Smad1/5/8 (#sc-6031-R), anti-JunD (#sc-74) from Santa Cruz Biotechnology (Santa Cruz, CA); anti-phospho-JNK(Thr183/Tyr185) (#9251), anti-c-Jun (#9165), anti-phospho-c-Jun (Ser63) (#9261), and anti-phospho-S6 ribosomal protein (Ser235/Ser236)(#4857) were from Cell Signaling Technology (Danvers, MA); anti-phospho-Smad2 (Ser465/467) (#AB3849), anti-Smad2/3 (#05-914), anti-phospho-Smad1/5/8(Ser463/465) (#AB3848), anti-Erk1/2 (#06-182) were from Millipore (Billerica, MA). GAPDH antibodies (#MCA4739) were from AbD-Serotec (Dusseldorf, Germany).

Chromatin immunoprecipitation (ChIP)

ChIP assay was performed in mouse myofibroblasts essentially as described [18], using anti-JunD (#sc-74x) (Santa Cruz Biotechnology) or anti-tri-methyl-H3K4 (#ab8580) (Abcam) antibodies, or a control rabbit IgG (Santa Cruz Biotechnology). The promoter region −905 to −725 of the murine cyclin D1 gene, which includes a growth factor-responsive binding site for activator protein 1 (AP1) factors [25], was analyzed by RT-PCR with the following primers: 5′-AACGAAGCCAATCAAGAAGC-3′, 5′-CAGTATCCCCCTCCTCCACT-3′. Values were normalized to average values of inputs.

Statistical analysis

Data are means ±SEM. Analyses were performed using GraphPad Prism version 5.00 (GraphPad Software, San Diego, USA). Data were compared among groups using the Student t test. A P value of <0.05 was considered significant.


MTA treatment reduces liver injury in Mdr2−/− mice

By three months of age Mdr2−/− mice typically display hepatomegaly and elevated serum levels of hepatic enzymes [10], [11], [14]. MTA administration was well tolerated, and treated animals gained similar weight as controls. MTA reduced the liver to body weight ratio (Fig. 1A), and improved aspartate aminotransferase (AST) and alanino aminotransferase (ALT) serum levels (Fig. 1B). Circulating levels of alkaline phosphatase (AP) and bilirubin were also lowered by MTA (Fig. 1C and 1D).

Figure 1. Oral administration of MTA to Mdr2−/− mice reduces hepatomegaly and serum parameters of liver injury.

Mdr2+/+ and Mdr2−/− mice were treated with MTA during three weeks. Increased liver-to-body weight ratio (%) in Mdr2−/− mice was reduced by MTA (A). Serum transaminases (B), alkaline phosphatase (C) and bilirubin (D), levels that are increased in Mdr2−/− mice were attenuated by MTA. *P<0.05 vs untreated Mdr2+/+ mice, #P<0.05 vs untreated Mdr2−/− mice.

MTA treatment attenuates liver fibrosis in Mdr2−/− mice

MTA significantly reduced the periductal fibrosis that spontaneously develops in these mice [11], as determined by Sirius Red staining of crosslinked collagen in liver sections and morphometric quantitation of stained areas (Fig. 2A and B). MTA administration to Mdr2+/+ mice had no effect on collagen levels (not shown). As previously described [11], we found an increase in periductal αSMA-positive cells and αSMA mRNA levels, which were also reduced by MTA treatment (Fig. 3A and B). In accordance with the histology, the expression of α1(I)procollagen mRNA was reduced in MTA treated mice (Fig. 4A). As reported [11], the expression of the interstitial collagenase MMP13, and that of its inhibitor TIMP1, was significantly increased in Mdr2−/− mice (Fig. 4B and C). MTA reduced MMP13 expression, and although not statistically significant there was a tendency towards decreased TIMP1 mRNA levels (Fig. 4B and C).

Figure 2. MTA administration reduces the spontaneous fibrosis that develops in Mdr2−/− mice.

Representative Sirius Red-stained liver sections from Mdr2+/+, control Mdr2−/− and MTA-treated Mdr2−/− mice (Mdr2−/− + MTA) (A). Fibrosis was quantified as function of mean percentage of stained area (B). *P<0.05 vs Mdr2+/+ mice, #P<0.05 vs untreated Mdr2−/− mice.

Figure 3. MTA administration reduces αSMA expression in Mdr2−/− mice.

Immunohistochemical staining of αSMA in representative liver sections from wild type, control Mdr2−/− mice, and MTA-treated Mdr2−/− mice (Mdr2−/− + MTA). The increased number of positive periductal myofibroblasts was reduced upon MTA administration (A). αSMA mRNA levels in Mdr2+/+, control Mdr2−/−, and MTA-treated Mdr2−/− mice (B). AU: arbitrary units. *P<0.05 vs untreated Mdr2−/− mice.

Figure 4. Fibrosis-related gene expression in Mdr2−/− mouse liver is attenuated by MTA treatment.

mRNA levels of α1(I) procollagen (A), MMP13 (B) and TIMP1 (C), were measured in the liver of Mdr2+/+, control Mdr2−/−, and MTA-treated Mdr2−/− mice. AU: arbitrary units. *P<0.05 vs Mdr2+/+ mice, #P<0.05 vs untreated Mdr2−/− mice.

MTA reduces hepatic levels of inflammatory and pro-fibrogenic mediators in Mdr2−/− mice

Although the expression of inflammatory cytokines in the liver of Mdr2−/− mice is maximal between 2–8 weeks [10], [11], we still detected elevated TNFα and IL6 mRNA levels (Fig. 5A and B). MTA tended to reduce TNFα mRNA, and significantly lowered IL6 expression (Fig. 5A and B). Consistently, the expression of iNOS gene, a transcriptional target of pro-inflammatory cytokines, was decreased by MTA (Fig. 5C). Importantly, upon MTA administration we observed reduced Mcp-1 expression (Fig. 5D), a pro-fibrogenic chemokine up-regulated in Mdr2−/− mice [12]. TGFβ1 and TGFβ2 expression is elevated in the liver of these animals, particularly during the first 8 weeks of life [10][12]. Accordingly we found that by 11 weeks TGFβ1 expression in Mdr2−/− mice was similar to wild types, while TGFβ2 levels were still high, and were attenuated by MTA (Fig. 5E and F). These findings were accompanied by a significant decrease in inflammatory infiltrate, as assessed by staining for the leukocyte marker CD45 (Fig. 6).

Figure 5. Effect of MTA on the expression of inflammatory cytokines and iNOS in Mdr2−/− mouse liver.

mRNA levels of TNFα (A), IL6 (B), iNOS (C), Mcp-1 (D), TGFβ1 (E) and TGFβ2 (F) were measured in the liver of Mdr2+/+, control Mdr2−/−, and MTA-treated Mdr2−/− mice. *P<0.05 vs Mdr2+/+ mice, #P<0.05 vs untreated Mdr2−/− mice.

Figure 6. MTA reduces the recruitment of leukocytes to the portal fields of Mdr2−/− mice.

Representative staining for the pan-leukocyte marker CD45 showing increased accumulation of CD45 positive cells in the portal field of Mdr2−/− mice compared to WT animals. Treatment with MTA reduced CD45 positive leukocyte accumulation. Representative images are shown.

Tenascin-C is a TGFβ-inducible extracellular protein expressed in liver fibrogenic cells that participates in inflammation and fibrogenesis [24], [26]. As described in other models of chronic liver injury [24], we found increased tenascin-C staining around portal areas in Mdr2−/− mice (Fig. 7A). MTA treatment reduced tenascin-C immunostaining and mRNA levels (Fig. 7A and B). However, the expression of αvβ6 integrin, which is induced in Mdr2−/− mice biliary epithelia and binds tenascin-C [13], was unaffected by MTA (not shown).

Figure 7. Expression of the fibrosis-associated protein tenascin-C, up-regulated in Mdr2−/− mice, is attenuated by MTA administration.

Immunohistochemistry of tenascin-C in representative liver sections shows increased staining around portal areas in Mdr2−/− mice and its downregulation by MTA (A). Tenascin-C mRNA levels in the liver of Mdr2+/+, control Mdr2−/−, and MTA-treated Mdr2−/− mice (B). *P<0.05 vs Mdr2+/+ mice, #P<0.05 vs untreated Mdr2−/− mice.

Effect of MTA on signalling pathways involved in fibrosis and hepatocellular proliferation in the Mdr2−/− mouse liver

To further explore the mechanism of action of MTA we examined the activation of signalling pathways associated with fibrogenesis and disease progression, including the Smad and mitogen-activated protein kinase (MAPK) pathways [3], [6], [9], [27][30]. We found that total and phosphorylated Smad1/5/8 and Smad2 levels were increased in Mdr2−/− mouse liver extracts, and that MTA treatment reduced Smad2 and p-Smad2 contents (Fig. 8A and B). We also observed increased MAPK pathway activity in Mdr2−/− mice, as evidenced by elevated levels of p-Erk1/2, p-JNK and p-c-Jun. These pathways were also inhibited by MTA (Fig. 8C and D). No changes were observed in MTA-treated Mdr2+/+ mice (not shown).

Figure 8. MTA modulates intracellular signalling pathways activated in Mdr2−/− mouse liver.

Phosphorylation levels of Smad1/5/8 (A), Smad2 (B), JNK and c-Jun (C) and Erk1/2 (D) were analyzed by western blotting in liver extracts from Mdr2+/+, control Mdr2−/−, and MTA-treated Mdr2−/− mice. *P<0.05 vs Mdr2+/+ mice, #P<0.05 vs untreated Mdr2−/− mice.

In agreement with the hyperactivation of pro-mitogenic signalling pathways, and confirming previous reports [6], [30], we found enhanced hepatocellular proliferation in Mdr2−/− mice, as evidenced by increased hepatocyte staining with the proliferation marker Ki-67 (Fig. 9A and B). MTA reduced hepatocellular proliferation (Fig. 9A and B) and cyclin D1 protein levels (Fig. 9C), markedly elevated in the liver parenchymal cells of these animals [14].

Figure 9. Increased hepatocellular proliferation in Mdr2−/− mice is attenuated by MTA administration.

Immunohistochemical staining of Ki-67 in liver sections from Mdr2+/+, control Mdr2−/−, and MTA-treated Mdr2−/− mice (Mdr2−/−+MTA)(A). Ki-67 positive hepatocytes were counted in 30 high-power fields per mouse, n = 5 per group (B). *P<0.01 vs Mdr2+/+ mice, #P<0.05 vs untreated Mdr2−/− mice. Western blot analysis of cyclin-D1 protein in liver extracts from Mdr2+/+ mice, untreated Mdr2/ and MTA-treated Mdr2−/− mice (C).

MTA effects on liver SAMe and GSH levels in Mdr2−/− mice

In vivo MTA is produced from SAMe during polyamine metabolism, and subsequently MTA can be metabolically recycled back to methionine [15], [31]. Methionine metabolism in turn is necessary for the production of SAMe and GSH, and it is impaired in liver injury [31]. The expression of key genes in methionine metabolism is down-regulated in Mdr2−/− mice [32]. In view of this we measured MTA effects on liver SAMe levels. We observed that SAMe was not reduced in Mdr2−/− mice, and was unaffected by MTA treatment (82.9±10.6 in Mdr2+/+; 110.6±9.7 in Mdr2−/− and 103.2±12.3 in MTA-treated Mdr2−/−, values are nmol/g tissue). GSH levels were not altered either in Mdr2−/− mice compared to Mdr2+/+, and were not affected by MTA (6.49±0.57 in Mdr2+/+; 5.92±0.68 in Mdr2−/− and 5.61±0.51 in MTA-treated Mdr2−/−, values are µmol/g tissue).

Effects of MTA on inflammatory cells

Our current in vivo observations indicate that MTA administration significantly attenuated the inflammatory response found in the liver of Mdr2−/− mice. MTA is structurally very close to adenosine, a potent endogenous immune regulatory molecule produced mainly by cells of the immune system during tissue injury and inflammation [33]. Adenosine mediates its cellular effects through the interaction with cell surface receptors such as A2A and A2B, which are expressed in monocytes/macrophages and play a major role in the anti-inflammatory and immunomodulatory actions of this nucleoside [33], [34]. In view of this and considering the ability of MTA to interact with adenosine receptors [35], we decided to explore the potential implication of A2A and A2B receptors in MTA anti-inflammatory effects. To directly address this issue we took advantage of the murine monocyte/macrophage cell line RAW 264.7, which has been widely used in mechanistic studies on the anti-inflammatory effects of adenosine upon bacterial lipopolysaccharide (LPS) challenge [36], [37]. First we evaluated the expression and release of TNFα in LPS-stimulated RAW 264.7 cells in the presence of MTA. As shown in Fig. 10A, and in agreement with our previous findings [16], we found a potent inhibitory effect of MTA on TNFα expression. We also observed that the inhibitory effect of MTA was preserved when RAW 264.7 cells were incubated in the presence of the A2A or A2B specific antagonists ZM 241385 and MRS 1754 respectively (Fig. 10A and B). On the other hand, and in accordance with the literature [38], [39], the inhibition of LPS-elicited TNFα production by the stable adenosine analogue NECA was attenuated by the A2A antagonist ZM 241385 (Fig. 10A). These observations suggested that the effect of MTA on the activation of inflammatory cells was not dependent on its potential direct interaction with adenosine receptors. However, although apparently MTA was not acting as an A2B receptor agonist we found that this molecule dramatically synergized with LPS in the up-regulation of A2B mRNA levels (Fig. 10C). Increased A2B expression has been linked to the activation of anti-inflammatory responses [37], [39], [40]. Interestingly this effect of MTA was not reproduced by the adenosine analogue NECA (Fig. 10C).

Figure 10. Effect of MTA on the activation of inflammatory cells: interaction with adenosine receptors.

As indicated in the figure serum-starved murine monocyte/macrophages RAW 264.7 cells were pre-treated for 30 min with the A2A receptor antagonist ZM 241385 (10 µM) or the A2B receptor antagonist MRS 1754 (1 µM), then MTA or the adenosine receptor agonist NECA (20 µM) where added to the cultures for another 30 min. Subsequently and where indicated cells were treated with LPS (50 ng/ml) for up to 5 h. TNFα mRNA levels in cell lysates (A) and TNFα protein contents in conditioned media (B) were measured. *P<0.01 vs control, **P<0.01 vs LPS, #P<0.05 vs LPS. The expression of the adenosine A2B receptor was measured in RAW 264.7 cells pre-treated with MTA or the adenosine agonist NECA (20 µM) for 30 min and then where indicated with LPS (50 ng/ml) for up to 5 h (C). *P<0.01 vs control, **P<0.01 vs LPS.

Effect of MTA on cultured liver myofibroblasts

Next we tested whether MTA had a direct effect on liver myofibroblasts, which participate in biliary fibrosis and represent a relevant source of extracellular matrix in Mdr2/ mice [9], [30], [41]. Given that isolated myofibroblasts display high proliferation and activity upon in vitro culture, we pre-incubated the cells in serum free medium for 12 h to attenuate activation and proliferation, and subsequently cultures were stimulated with 10% FCS to promote myofibroblast activation in the presence or absence of MTA. We observed that the expression of the fibrogenic markers α1(I)procollagen and αSMA elicited by FCS treatment was inhibited by MTA (Fig. 11A and B). Similar observations were made when myofibroblasts were challenged with TGFβ (not shown). Additionally, TGFβ1 and TGFβ2 expression triggered by FCS was also attenuated by MTA (Fig. 11C and D). In agreement with previous reports [30] we found that FCS treatment increased Mcp-1 expression, and this response was also reduced by MTA (Fig. 11E), while IL6 expression was unaltered (Fig. 11F).

Figure 11. Effects of MTA on liver myofibroblast activation and cytokine expression.

Primary myofibroblasts were serum starved (12 h) and then treated (12 h) with 10% FCS and MTA as indicated. mRNA levels of α1(I)procollagen (A), αSMA (B), TGFβ1 (C), TGFβ2 (D), Mcp-1 (E) and IL6 (F) were measured at the end of treatments. *P<0.05 vs FCS, #P<0.05 vs FCS+MTA 200 µM.

We also examined whether MTA could affect myofibroblast proliferation. Figure 12A shows that MTA reduced FCS-triggered DNA synthesis, without causing any toxicity (determined by lactate dehydrogenase release, not shown). Additionally we observed that MTA did not induce apoptosis in cultured myofibroblasts (data not shown). Our [3H]thymidine incorporation experiments suggested that MTA inhibited cell cycle progression through the S phase (DNA synthesis), therefore we examined the expression of cyclin D1, a key cyclin in the transition from G0/G1 to S phase. We found that cyclin D1 expression was reduced by MTA treatment both at the mRNA and protein levels (Figure 12B). The expression of cyclin D1 can be regulated by AP-1 transcription factors, and among the components of the AP-1 complex JunD has been identified as a critical transcription factor in liver fibrogenesis [27], [42]. Therefore we examined the binding of JunD to a region of the cyclin D1 promoter that contains a key AP-1 binding site [25] by ChIP analysis. As depicted in Figure 12C, MTA treatment almost completely blunted JunD association with cyclin D1 promoter in this regulatory region. In view of this response we examined the expression of JunD in cultured myofibroblasts treated with MTA, and observed that MTA significantly reduced JunD protein levels (Fig. 12D). These data suggested that the reduction of cyclin D1 expression by MTA could be mediated in part through the downregulation of JunD levels. Nevertheless, in spite of this effect of MTA on JunD cellular contents this compound almost totally inhibited cyclin D1 expression, and our ChIP experiment showed a near complete inhibition of JunD binding to the cyclin D1 promoter. This suggested that MTA could also affect the interaction of the remaining JunD protein with this cyclin D1 regulatory region. MTA is a well known inhibitor of methylation reactions [15], and it has been shown to inhibit H3K4 trimethylation, a hallmark of open chromatin conformation and transcriptional activation [43], in different cell types [18], [44]. In view of this we examined the levels of tri-methylated-H3K4 in chromatin associated with this region of the cyclin D1 promoter. We detected increased levels of tri-methylated-H3K4 upon FCS stimulation, and observed that this modification was lowered by MTA treatment (Fig. 12E).

Figure 12. MTA inhibits DNA synthesis in myofibroblasts.

MTA Effects on cyclin D1 and JunD expression. Effect of MTA on FCS-induced [3H]thymidine incorporation in myofibroblasts treated as indicated (24 h) (A). Cyclin D1 mRNA expression in myofibroblasts treated (12 h) with 10% FCS and MTA as indicated. Inset shows a Western blot analysis of cyclin D1 protein (B). ChIP assay measuring the binding of JunD to the −905 to −725 cyclin D1 promoter region encompassing a key AP-1 binding site in myofibroblasts treated as indicated (12 h). Immunoprecipitated genomic DNA corresponding to the −905 to −725 cyclin D1 promoter region was quantified by real time PCR as indicated in Methods section. A representative gel picture of amplified DNA fragments is shown (C). Western blot analysis of JunD protein levels in myofibroblasts treated as indicated for 6 h (D). ChIP assay measuring the binding of tri-methylated-H3K4 (H3K4me3) to the same cyclin-D1 promoter region in myofibroblasts treated as indicated (12 h). A representative gel picture of amplified DNA fragments is shown (E). *P<0.05 vs FCS, #P<0.05 vs FCS+MTA 200 µM.

The relevance of these in vitro effects of MTA on the expression of fibrogenic and cell proliferation-related genes was supported by the observation of reduced α1(I)procollagen, αSMA, tenascin-C, TGFβ1, TGFβ2, JunD and cyclin D1 expression in myofibroblasts isolated from Mdr2−/− mice treated for 3 weeks with MTA when compared to cells isolated from untreated mice (Fig.13).

Figure 13. Expression of fibrogenic activation and cellular proliferation-related genes in myofibroblasts isolated from the liver of control and MTA-treated Mdr2−/− mice.

Mdr2−/− mice were treated for three weeks with MTA or vehicle as described in the Methods section. At the end of the treatments hepatic myofibroblasts were isolated and the mRNA levels of the indicated genes were measured. Data are means ±SEM of three independent cell preparations per condition. *P<0.05 vs vehicle-treated Mdr2−/− mice.

Finally, to gain additional insight into the mechanisms of the antifibrogenic effects of MTA we explored the direct effects of this molecule on the activity of intracellular signalling pathways related to the proliferation and fibrogenic activation of myofibroblasts [27][30]. As depicted in Fig. 14A, while MTA treatment was not able to directly modify the phosphorylation of Erk1/2 elicited by FCS, it reduced the levels of phospho-c-Jun, a target of the pro-fibrogenic JNK signalling pathway in liver extracellular matrix producing cells [29]. Interestingly, MTA significantly attenuated the phosphorylation of the mTOR and p70S6 kinase downstream target S6 ribosomal protein triggered by the pro-fibrogenic growth factor PDGF (Fig. 14B). p70S6 kinase activity is required for G1 cell cycle progression, and it has been also identified as a signal transducer for liver fibrogenic cell growth [45].

Figure 14. Effect of MTA on liver myofibroblast intracellular signalling pathways.

Liver myofibroblasts were pre-treated with MTA for 30 min in the absence of serum and then stimulated with 10% FCS for 30 min or PDGF (20 ng/ml) for 60 min. Phosphorylation levels of Erk1/2 and c-Jun upon FCS stimulation (A), and S6 ribosomal protein after PDGF treatment (B) were analyzed by western blotting. Representative blots are shown.


We have shown that oral administration of the nucleoside MTA significantly ameliorates liver injury in Mdr2−/− mice. These mice represent a clinically relevant model of spontaneous chronic liver disease, spanning from peribiliary inflammation and fibrosis to HCC development [9][14]. MTA was well tolerated and a significant improvement in serum markers of hepatic injury and function was observed. This was accompanied by reduced hepatic fibrosis and fibrogenic cell abundance. Accordingly, α1(I)procollagen mRNA levels were lowered, and TIMP1 expression tended to decrease. The fact that MTA also reduced the expression of MMP13, the interstitial collagenase in rodents, suggests that MTA down-regulates overall tissue remodelling activity, inhibiting fibrosis progression rather than stimulating fibrosis resolution [3].

Previous studies have shown that MTA exerts remarkable biological effects, its pharmacologic administration modulates different pathways and cellular responses, including gene expression, cell cycle progression and inflammation [15][20]. Therefore, the mechanisms behind MTA therapeutic action on a complex model such as Mdr2−/− mice are likely multifaceted. Our current findings agree with those reported by Simile et al., who showed that parenteral MTA administration to rats undergoing chronic CCl4-induced liver injury reduced fibrosis [19]. This effect was mechanistically related to MTA antioxidant properties, that counteracted the oxidative stress and subsequent injury generated by CCl4 metabolism [19]. However, oxidative stress is not a prominent feature in Mdr2−/− mice [14]. Accordingly, we found that GSH levels were unaltered in Mdr2−/− mouse liver, and were not affected by MTA, suggesting that MTA effects were not attributable to its antioxidant potential. In vivo MTA is metabolized to methionine in the so called methionine salvage pathway, and in the liver methionine is efficiently metabolized into SAMe [15]. SAMe is a key methyl donor with significant hepatoprotective properties, including antifibrotic activity in experimental cholestasis [31], [46]. In view of the metabolic links between MTA and SAMe, we measured SAMe levels in control and MTA-treated Mdr2−/− mouse liver but did not observe major differences, indicating that MTA effects were not likely mediated through its potential contribution to the SAMe pool. Moreover, this may suggest that the antifibrotic effects of SAMe in experimental cholestasis [46] could be mediated in part by the metabolic or non-enzymatic conversion of SAMe into MTA [15].

Interestingly, MTA reduced the expression of the extracellular matrix protein tenascin-C in the liver of Mdr2−/− animals. This may be directly related to MTA antifibrotic effects, since tenascin-C is required for the development of experimental liver fibrosis [24]. Furthermore, tenascin-C is up-regulated in chronic hepatitis C, and its expression in peritumoral activated stellate cells in HCC associates with poor clinical prognosis [26], [38], [47]. In view of this, tenascin-C may be a previously unrecognized player in fibrosis and HCC development in Mdr2−/− mice, and its attenuation by MTA a key event in the anti-fibrotic and anti-neoplastic properties of this molecule [20]. Moreover, tenascin-C binds and activates αvβ6 integrin, a recently identified pharmacological target in biliary fibrosis [13].

As occurs in human chronic liver disease, progression of liver injury in Mdr2−/− mice is associated with persistent inflammation. The observation that anti-inflammatory compounds like ibuprofen or curcumin ameliorate injury and fibrosis in Mdr2−/− mice [6], [30], and that TNFα blockade prevents hepatocarcinogenesis in these animals [6], underscore the role played by inflammation in this model. We and others have previously shown that MTA has a significant immunomodulatory potential. MTA inhibits NF-κB mediated signalling, reduces inflammatory cytokine production by macrophages and lymphocytes, and attenuates the cellular effects of these cytokines [16][18]. We now observed that in Mdr2−/− mice MTA reduced the expression of IL6, Mcp-1, the NO-generating enzyme iNOS, and the profibrogenic factor TGFβ2. Accordingly MTA attenuated the activation of Erk1/2, JNK and Smad2, intracellular pathways triggered by these cytokines and which are directly implicated in fibrogenesis [3], [5], [27][30]. Therefore, interference with inflammatory cytokine and NO generation likely contributes to MTA hepatoprotective and anti-fibrogenic effects in this model [10], [48].

From a mechanistic perspective, and in view of the remarkable anti-inflammatory effects of MTA, we cannot overlook the fact that this molecule is structurally very close to adenosine, a purine nucleoside released form cells with notorious anti-inflammatory properties [15], [33]. Adenosine interacts with different G-protein-coupled cell surface receptors including the A1, A2A, A2B and A3 receptors. Until recently adenosine anti-inflammatory effects were mainly attributed to its interaction with the high affinity A2A receptor subtype [49], however an important role for the low affinity A2B receptor in the anti-inflammatory response to adenosine is currently emerging [34], [38], [40]. Using specific pharmacological antagonists of the A2A and A2B receptors we evaluated their potential implication in the immunomodulatory effects of MTA on mouse RAW 264.7 monocytes/macrophages challenged with bacterial LPS, a prototypic model of the inflammatory response. We found that the inhibition of LPS-elicited TNFα production by MTA was not impaired in the presence of these drugs, suggesting that MTA effects were not mediated through these receptors. Nevertheless, the involvement of the adenosine signalling system in the biological effects of MTA cannot be completely disregarded. Interestingly we observed that MTA treatment resulted in a remarkable potentiation of the expression of A2B receptors triggered by LPS, and this effect was not shared by the adenosine receptor agonist NECA. As previously mentioned A2B receptors display low affinity for adenosine, but their expression is up-regulated during tissue injury and inflammation, conditions in which interstitial adenosine concentrations raise. The expression of A2B receptors seems to be very important for the attenuation of the systemic inflammatory response, as illustrated by the fact that A2B knockout mice show enhanced cytokine production and overall mortality during sepsis [39], [50]. Therefore the stimulatory effect of MTA on A2B receptor expression could also contribute to dampen inflammation in the chronically injured Mdr2−/− mouse liver.

In addition to these responses, a direct cytoprotective effect of MTA on hepatocytes may also be involved, as we previously observed that MTA can prevent hepatocyte death in vitro [51], [52]. Mechanistically, the attenuation of JNK activity found in MTA-treated Mdr2−/− mice could be related to the hepatoprotective effects of this molecule, given that inhibition of JNK has been demonstrated to prevent liver damage in different in vitro and in vivo experimental models of hepatocellular injury [53][55]. In this context the reduced hepatocyte proliferation found in MTA-treated mice may be related in part to the attenuation of liver damage, since liver regeneration occurs in response to injury.

We also observed that MTA has direct effects on liver fibrogenic cells. A previous study had reported that MTA could reduce collagen gene expression in primary hepatic stellate cells [56]. Here we confirmed this observation in liver myofibroblasts, and we also found that MTA down-regulated also the expression of αSMA, TGFβ1 and TGFβ2, and Mcp-1, all markers of activated fibrogenic cells [3], [6], [57]. However, MTA did not modify IL6 mRNA levels in myofibroblasts. This supports the specificity of MTA effects on gene expression, and indicates that the downregulation of IL6 observed in vivo could be attributed to the interaction of MTA with other cell types, likely inflammatory cells. The reduction of TGFβ isoforms and Mcp-1 expression by MTA found in vivo as well as in cultured myofibroblasts may be important effects regarding the mechanisms of action of this molecule. TGFβ1 and TGFβ2 are key cytokines in the development of liver fibrosis that can be expressed in a variety of cells including activated stellate cells, myofibroblats, macrophages and activated cholangiocytes [58], [59]. The inhibition of TGFβ1 and TGFβ2 expression and activation has been demonstrated to attenuate liver fibrosis, including biliary fibrosis [59]. On the other hand, Mcp-1 participates in the recruitment of inflammatory cells during liver injury, and has been cogently demonstrated to contribute to hepatic parenchymal damage [60]. Moreover, besides expressing Mcp-1 liver fibrogenic cells can be activated and induced to proliferate by this chemokine [61], [62]. Together these findings suggest that attenuation of TGFβ1/2 and Mcp-1 expression could have important mechanistic roles in the therapeutic action of MTA.

Increased proliferation and survival of ECM-producing cells are central events in the development of liver fibrosis [5], [58]. MTA has been shown to induce apoptosis of different cell types, including HCC cells [51]. However, we did not observe any pro-apoptotic or cytotoxic effect of MTA in liver myofibroblasts. What we found was a significant inhibition by MTA of FCS-stimulated DNA synthesis. In line with this response we observed that MTA reduced the expression of cyclin D1, a key G1 cyclin associated with liver fibrogenic cell proliferation [63]. AP-1 transcription factors can stimulate the expression of genes involved in the activation and proliferation of liver fibrogenic cells, and among them JunD is known to play an important role in liver fibrogenesis [27], [42]. To gain further insight into the mechanism of action of MTA, we examined the binding of JunD to cyclin D1 promoter and found that it was markedly reduced in myofibroblasts treated with this compound. This can be due in part to the observed downregulation of JunD levels in MTA-treated cells, and therefore reduction of JunD expression may be a relevant mechanism in the antifibrogenic action of MTA.

In order to better understand the mechanisms behind the antiproliferative effects of MTA, we examined the activity of three signalling pathways that are involved in fibrogenic cell proliferation. We found that while MTA did not affect FCS-triggered Erk1/2 phosphorylation, it reduced phopho-c-Jun levels and significantly attenuated PDGF elicited ribosomal S6 protein phosphorylation. Both, the JNK and the mTOR and p70S6 kinase pathways have been demonstrated as key regulators of hepatic fibrogenic cell proliferation [29], [45], and therefore their inhibition by MTA could be relevant in the mechanism of action of this compound. The selective interaction of MTA with protein kinase-mediated intracellular signalling pathways as described here is likely to have profound effects on cellular behaviour and thus deserves further examination.

We also noticed that MTA could attenuate the increase in H3K4 trimethylation elicited by FCS stimulation in the cyclin D1 promoter. H3K4 trimethylation is a marker of transcriptional active chromatin, and this modification contributes to gene activation [64]. MTA is an inhibitor of methylation reactions [15], including histone methylation [18], our observations suggest that interference with this epigenetic mechanism could account in part for the effects of MTA on cyclin D1 gene expression. Moreover, this finding makes it tempting to speculate that MTA could exert its antifibrogenic effects also through an overall action on the epigenetic programming. In this regard 3 deazaneplanocin, another methyltransferase inhibitor, has been recently reported to prevent the activation of liver fibrogenic cells, however its efficacy and tolerability in chronic in vivo models of liver fibrosis have not been tested yet [65]. Together these findings suggest that the antifibrogenic effects of MTA observed in vivo may be mediated in part through the direct inhibition of myofibroblast activation and proliferation. Nevertheless, a direct effect of MTA on bile duct epithelial cell damage and cholangiocyte activation, important events in the pathogenesis of liver injury in Mdr2−/− mice [30], cannot be discarded and merit future evaluation. Figure 15 summarizes the proposed mechanisms of action of MTA in Mdr2−/− mice mainly based on the observations reported in this study.

Figure 15. Potential mechanisms of action of MTA in Mdr2−/− mice.

Our in vivo and in vitro observations indicate that MTA displays different actions that may underlie its beneficial effects on the course of liver injury and fibrosis in Mdr2−/− mice. MTA may exert a direct cytoprotective effect on hepatocytes by reducing JNK activity, preventing hepatocellular death and further inflammation. MTA also inhibits the production of cytokines by inflammatory cells, likely through interference with NFκB activity as described before [16][18]. In addition, enhanced expression of adenosine A2B receptors may contribute to the anti-inflammatory pharmacological profile of MTA. This compound can also exert direct effects on extracellular matrix (ECM) producing cells (myofibroblasts), reducing their activation, proliferation and the production of pro-fibrogenic factors. Inhibition of JunD expression may be an important event in the antifibrogenic action of MTA.

In summary, here we have demonstrated that oral MTA administration is an effective therapeutic strategy to attenuate disease progression in a relevant model of liver injury and fibrosis. In addition to our current study, MTA has been previously tested in in vivo experimental models never showing untoward effects [16], [17], [66], [67], and an ID50 of 2.9±0.4 g/kg was estimated when administered intramuscularly to rats [19]. In humans MTA administration is also well tolerated [68], [69]. These considerations, together with the efficacy described herein, suggest that MTA could be a good candidate to be clinically tested in the context of liver injury and fibrosis.

Author Contributions

Conceived and designed the experiments: MAA. Performed the experiments: MUL CG-P MGF-B CMR-O MM JMB SG SA NJ RU JL FJC. Analyzed the data: FJC MUL RU JP JL CB MAA. Contributed reagents/materials/analysis tools: JMB SL JAR. Wrote the paper: JL MAA.


  1. 1. Williams R (2006) Global challenges in liver disease. Hepatology 44: 521–6.
  2. 2. Siegel AB, Zhu AX (2009) Metabolic syndrome and hepatocellular carcinoma. Cancer 115: 5651–5661.
  3. 3. Bataller R, Brenner DA (2005) Liver fibrosis. J Clin Invest 115: 209–218.
  4. 4. Elsharkawy AM, Mann DA (2007) Nuclear factor-κB and the hepatic inflammation-fibrosis-cancer axis. Hepatology 46: 590–597.
  5. 5. Lotersztajn S, Julien B, Teixeira-Clerc F, Grenard P, Mallat A (2005) Hepatic fibrosis: molecular mechanisms and drug targets. Annu Rev Pharmacol Toxicol 45: 605–628.
  6. 6. Pikarski E, Porat RM, Stein I, Abramovitch R, Amit S, et al. (2004) NF-κB functions as a tumour promoter in inflammation-associated cancer. Nature 431: 461–466.
  7. 7. Berasain C, Castillo J, Perugorria MJ, Latasa MU, Prieto J, et al. (2009) Inflammation and liver cancer: new molecular links. Ann NY Acad Sci; 1155: 206–221.
  8. 8. Pinzani M, Rombouts K, Colagrande S (2005) Fibrosis in chronic liver diseases: diagnosis and management. J Hepatol. 42. (Suppl): pp. S22–S36.
  9. 9. Popov Y, Schuppan D (2009) Targeting liver fibrosis: strategies for development and validation of antifibrotic therapies. Hepatology 50: 1294–1306.
  10. 10. Fickert P, Fuchsbichler A, Wagner M, Zollner G, Kaser A, et al. (2004) Regurgitation of bile acids from leaky bile ducts causes sclerosing cholangitis in Mdr2 (Abcb4) knockout mice. Gastroenterology 127: 261–274.
  11. 11. Popov Y, Patsenker E, Fickert P, Trauner M, Schuppan D (2005) Mdr2 (Abcb4)-/- mice spontaneously develop severe biliary fibrosis via massive dysregulation of pro- and antifibrogenic genes. J Hepatol 43: 1045–1054.
  12. 12. Nakken KE, Nygård S, Haaland T, Berge KE, Arnkværn K, et al. (2007) Multiple inflammatory-, tissue remodelling- and fibrosis genes are differentially transcribed in the livers of Abcb4 (-/-) mice harbouring chronic cholangitis. Scand J Gastroenterol 42: 1245–1255.
  13. 13. Patsenker E, Popov Y, Stickel F, Jonczyk A, Goodman SL, et al. (2008) Inhibition of integrin αvβ6 on cholangiocytes blocks transforming growth factor-β activation and retards biliary fibrosis progression. Gastroenterology 135: 660–670.
  14. 14. Katzenellenbogen M, Pappo O, Barash H, Klopstock N, Mizrahi L, et al. (2006) Multiple adaptive mechanisms to chronic liver disease revealed at early stages of liver carcinogenesis in the Mdr2-knockout mice. Cancer Res 66: 4001–4010.
  15. 15. Avila MA, Garcia-Trevijano ER, Lu SC, Corrales FJ, Mato JM (2004) Methylthioadenosine. Int J Biochem Cell Biol 36: 2125–2130.
  16. 16. Hevia H, Varela-Rey M, Corrales FJ, Berasain C, Martínez-Chantar ML, et al. (2004) 5′-Methythioadenosine modulates the inflammatory response to endotoxin in mice and in rat hepatocytes. Hepatology 39: 1088–1098.
  17. 17. Moreno B, Hevia H, Santamaria M, Sepulcre J, Muñoz J, et al. (2006) Methylthioadenosine reverses brain autoimmune disease. Ann Neurol 60: 323–334.
  18. 18. Iglesias-Ara A, Xia M, Ramani K, Mato JM, Lu SC (2008) S-Adenosylmethionine inhibits lipopolysaccharide-induced gene expression via modulation of histone methylation. Hepatology 47: 1655–1666.
  19. 19. Simile MM, Banni S, Angioni E, Carta G, De Miglio MR, et al. (2001) 5′-Methylthioadenosine administration prevents lipid peroxidation and fibrogenesis induced in rat liver by carbon-tetrachloride intoxication. J Hepatol 34: 386–394.
  20. 20. Pascale RM, Simile MM, De Miglio MR, Feo F (2002) Chemoprevention of hepatocarcinogenesis: S-adenosyl-L-methionine. Alcohol 27: 193–198.
  21. 21. Berasain C, Hevia H, Fernández-Irigoyen J, Larrea E, Caballería J, et al. (2004) Methylthioadenosine phosphorylase gene expression is impaired in human liver cirrhosis and hepatocarcinoma. Biochim Biophys Acta 1690: 276–284.
  22. 22. Perugorria MJ, Latasa MU, Nicou A, Cartagena-Lirola H, Castillo J, et al. (2008) The epidermal growth factor receptor ligand amphiregulin participates in the development of mouse liver fibrosis. Hepatology 48: 1251–1261.
  23. 23. Li LY, Grenard P, Van Nhieu JT, Julien B, Mallat A, et al. (2003) Heme oxygenase-1 is an antifibrogenic protein in human hepatic myofibroblasts. Gastroenterology 125: 460–469.
  24. 24. El-Karef A, Yoshida T, Gabazza EC, Nishioka T, Inada H, et al. (2007) Deficiency of tenascin-C attenuates liver fibrosis in immune-mediated chronic hepatitis in mice. J Pathol 211: 86–94.
  25. 25. Eto IMolecular cloning and sequence analysis of the promoter region of mouse cyclin D1 gene. Cell Prolif 2000; 33: 167–187.
  26. 26. El-Karef A, Kaito M, Tanaka H, Ikeda K, Nishioka T, et al. (2007) Expression of large tenascin-C splice variants by hepatic stellate cells/myofibroblasts in chronic hepatitis C. J Hepatol 46: 664–673.
  27. 27. Mann J, Mann DA (2009) Transcriptional regulation of hepatic stellate cells. Adv Drug Delivery Rev 61: 497–512.
  28. 28. Tao J, Mallat A, Gallois C, Belmadani S, Méry PF, et al. (1999) Biological effects of C-type natriuretic peptide in human myofibroblastic hepatic stellate cells. J Biol Chem 274: 23761–23769.
  29. 29. Kluwe J, Pradere JP, Gwak GY, Mencin A, De Minicis S, et al. (2010) Modulation of hepatic fibrosis by c-Jun-N-terminal kinase inhibition. Gastroenterology 138: 347–359.
  30. 30. Baghdasaryan A, Claudel T, Kosters A, Gumhold J, Silbert D, et al. (2010) Curcumin improves sclerosing cholangitis in Mdr2-/- mice by inhibition of cholangiocyte inflammatory response and portal myofibroblast proliferation. Gut 59: 521–530.
  31. 31. Mato JM, Martínez-Chantar ML, Lu SC (2008) Methionine metabolism and liver disease. Annu Rev Nutr 28: 273–293.
  32. 32. Katzenellenbogen M, Mizrahi L, Pappo O, Klopstock N, Olam D, et al. (2007) Molecular mechanisms of liver carcinogenesis in the Mdr2-knockout mice. Mol Cancer Res 5: 1159–1170.
  33. 33. Jacobson KA, Gao Z (2006) Adenosine receptors as therapeutic targets. Nat Rev Drug Discovery 5: 247–264.
  34. 34. Haskó G, Csóka B, Németh ZH, Vizi ES, pacher P (2009) A2B adenosine receptors in immunity and inflammation. Trends Immunol. 30: 263–270.
  35. 35. Munshi R, Clanachan AS, Baer HP (1988) 5′-deoxy-5′-methylthioadenosine: a nucleoside which differentiates between adenosine receptor types. Biochem Pharmacol 37: 2085–2089.
  36. 36. Németh ZH, Leibovich SJ, Deitch EA, Vizi S, Szabó C, et al. (2003) cDNA Microarray analysis reveals a nuclear factor-κB-independent regulation of macrophage function by adenosine. J Pharmacol Exp Ther 306: 1042–1049.
  37. 37. Németh ZH, Lutz CS, Csóka B, Deitch EA, Leibovich SJ, et al. (2005) Adenosine augments IL-10 production by macrophages through an A2B recptor-mediated posttranscriptional mechanism. J Immunol 175: 8260–8270.
  38. 38. Kreckler LM, Wan TC, Ge Z, Auchampach JA (2006) Adenosine inhibits tumor necrosis factor-α release from mouse peritoneal macrophages via A2A and A2B but not the A3 adenosine receptor. J Pharmacol Exp Ther 317: 172–180.
  39. 39. Ryzhov S, Zaynagetdinov R, Goldstein AE, Novitskiy SV, Blackburn MR, et al. (2008) Effetc of A2B adenosine receptor gene ablation on adenosine-dependent regulation of proinflammatory cytokines. J Pharm Exp Ther 324: 694–700.
  40. 40. Aherne CM, Kewley EM, Eltzschig HK (2010) The resurgence of A2B adenosine receptor signalling. Biochim Biophys Acta May 27. [Epub ahead of print].
  41. 41. Dranoff JA, Wells RG (2010) Portal fibroblasts: underappreciated mediators of biliary fibrosis. Hepatology 51: 1438–1444.
  42. 42. Smart DE, Green K, Oakley F, Weitzman JB, Yaniv M, et al. (2006) JunD is a profibrogenic transcription factor regulated by Jun N-terminal kinase-independent phosphorylation. Hepatology 44: 1432–1440.
  43. 43. Guenther MG, Levine SS, Boyer LA, Jaenisch R, Young RA (2007) A chromatin landmark and transcription initiation at most promoters in human cells. Cell 130: 77–88.
  44. 44. Song M-R, Ghosh A (2004) FGF2-induced chromatin remodelling regulates CNTF-mediated gene expression and astrocyte differentiation. Nat Neurosci 7: 229–235.
  45. 45. Gäbele E, Reif S, Tsukada S, Bataller R, Yata Y, et al. (2005) The role of p70S6K in hepatic stellate cell collagen gene expression and cell proliferation. J Biol Chem 280: 13374–13382.
  46. 46. Yang H, Ramani K, Xia M, Ko KS, Li TWH, et al. (2009) Dysregulation of glutathione synthesis during cholestasis in mice: molecular mechanisms and therapeutic implications. Hepatology 49: 1982–1991.
  47. 47. Ju M, Qiu S, Fan J, Xiao Y, Gao Q, et al. (2009) Peritumoral activated hepatic stellate cells predict poor clinical outcome in hepatocellular carcinoma. Am J Clin Pathol 131: 498–510.
  48. 48. Spirli C, Fabris L, Duner E, Fiorotto R, Roskams T, et al. (2003) Cytokine-stimulated nitric oxide production inhibits adenylyl cyclase and cAMP-dependent secretion in cholangiocytes. Gastroenterology 124: 737–753.
  49. 49. Sitkovsky MV (2003) Use of the A2A adenosine receptor as a physiological immunosuppressor and to engineer inflammation in vivo. Biochem Pharmacol 65: 493–501.
  50. 50. Csóka B, Németh ZH, Rosenberger P, Eltzschig HK, Spolarics Z, et al. (2010) A2B adenosine receptors protect against sepsis-induced mortality by dampening excessive inflammation. J Immunol 185: 542–550.
  51. 51. Ansorena E, Garcia-Trevijano ER, Martinez-Chantar ML, Huang Z, Chen L, et al. (2002) S-Adenosylmethionine and methylthioadenosine are antiapoptotic in cultured rat hepatocytes but proapoptotic in human hepatoma cells. Hepatology 35: 274–280.
  52. 52. Ansorena E, Berasain C, López Zabalza MJ, Avila MA, García-Trevijano ER, et al. (2006) Differential regulation of the JNK/AP-1 pathway by S-adenosylmethionine and methylthioadenosine in primary rat hepatocytes versus HuH7 hepatoma cells. Am J Physiol Gastrointest Liver Physiol 290: G1186–G1193.
  53. 53. Marderstein EL, Bucher B, Guo Z, Feng X, Reid K, et al. (2003) Protection of rat hepatocytes from apoptosis by inhibition of c-Jun N-terminal kinase. Surgery 134: 280–284.
  54. 54. Uehara T, Bennett B, Sakata ST, Satoh Y, Bilter G, et al. (2005) JNK mediates hepatic ischemia reperfusion injury. J Hepatol 42: 850–859.
  55. 55. Gunawan BK, Liu ZX, Hanawa N, Gaarde WA, Kaplowitz N (2006) c-Jun N-terminal kinase plays a major role in murine acetaminophen hepatotocicity. Gastroenterology 131: 165–178.
  56. 56. Nieto N, Cederbaum AI, S-Adenosylmethionine blocks collagen I production by preventing transforming growth factor-β induction of the COL1A2 promoter (2005) J Biol Chem 280: 30963–30974.
  57. 57. Marra F, DeFranco R, Grappone C, Milani S, Pastacaldi S, et al. (1998) Increased expression of monocyte chemotactic protein-1 during active hepatic fibrogenesis: correlation with monocyte infiltration. Am J Pathol 152: 423–430.
  58. 58. Friedman SL (2008) Mechanisms of hepatic fibrogenesis. Gastroenterology 134: 1655–1669.
  59. 59. Schuppan D, Popov Y (2009) Rationale and targets for antifibrotic therapies. Gastroenterol Clin Biol 33: 949–957.
  60. 60. Zamara E, Galastri S, Aleffi S, Petrai I, Aragno M, et al. (2007) Prevention of severe toxic liver injury and oxidative stress in MCP-1-deficient mice. J Hepatol 46: 230–238.
  61. 61. Marra F, Valente AJ, Pinzani M, Abboud HE (1993) Cultured human liver fat-storing cells produce monocyte chemotactic protein-1. Regulation by proinflammatory cytokines. J Clin Invest 92: 1674–1680.
  62. 62. Kruglov EA, Nathanson RA, Nguyen T, Dranoff JA (2006) Secretion of MCP-1/CCL2 by bile duct epithelia induces myofibroblastic trasndifferentiation of portal fibroblasts. Am J Physiol Gastrointest Liver Physiol 290: G765–G771.
  63. 63. Kawada N, Ikeda K, Seki S, Kuroki T (1999) Expression of cyclins D1, D2 and E correlates with proliferation of rat stellate cells in culture. J Hepatol 30: 1057–1064.
  64. 64. Wysoka J, Swigut T, Xiao H, Milne TA, Kwon SY, et al. (2006) A PHD finger of NURF couples histone H3 lysine 4 trimethylation with chromatin remodelling. Nature 442: 86–90.
  65. 65. Mann J, Chu DCK, Maxwell A, Oakley F, Zhu N, Tsukamoto H, Mann DAMeCP2 controls an epigenetic pathway that promotes myofibroblast transdifferentiation and fibrosis. Gastroenterology 2010; 138: 705–714.
  66. 66. Chen H, Xia M, Lin M, Yang H, Kuhlenkamp J, et al. (2007) Role of methionine adenosyltransferase 2A and S-adenosylmethionine in mitogen-induced growth of human colon cancer cells. Gastroenterology 133: 207–219.
  67. 67. Andreu-Perez P, Hernandez-Losa J, Moline T, Gil R, Grueso J, et al. (2010) Methylthioadenosine (MTA) inhibits melanoma cell proliferation and in vivo tumor growth. BMC Cancer 10: 265.
  68. 68. Stramentinoli G, Gennari FAdenosine derivatives of anti- inflammatory and analgesic activity, and therapeutic compositions which contain them as their active principle. Stramentinoli patent 4,454,122. Filed: Aug 6, 1982; Issued: Jun 12, 1984.
  69. 69. Moratti EPharmaceutical compositions containing 5-deoxy-5-methylthioadenosine s-adenosylmethionine and their salts for reducing seborrhoea. Moratti patent 5,753,213. Filed: Mar 13, 1990; Issued: May 19, 1998.