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BioMed Research International
Volume 2015 (2015), Article ID 794862, 10 pages
http://dx.doi.org/10.1155/2015/794862
Research Article

Hepatocyte-Specific Ablation of PP2A Catalytic Subunit α Attenuates Liver Fibrosis Progression via TGF-β1/Smad Signaling

1Department of Anatomy, Histology and Embryology, Nanjing Medical University, Nanjing, Jiangsu 210029, China
2Model Animal Research Center of Nanjing University, Nanjing, Jiangsu 210061, China

Received 1 September 2014; Revised 18 November 2014; Accepted 18 November 2014

Academic Editor: Yury Popov

Copyright © 2015 Na Lu et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Abstract

Protein phosphatase 2A (PP2A), a family of the major serine/threonine phosphatases in cells, regulates many aspects of physiological processes. However, isoform-specific substrates and the biological role of each specific member of the PP2A family remain largely unknown. In this study, we investigated whether PP2A catalytic subunit Cα (PP2Acα) is involved in chronic hepatic injury and fibrosis. A hepatocyte-specific PP2Acα ablation mice model was established to examine the effect of PP2Acα on carbon tetrachloride- (CCl4-) induced chronic hepatic injury and fibrosis. Our results showed that PP2Acα knockout mice were less susceptible to chronic CCl4-induced liver injury as evidenced by lower levels of serum alanine aminotransferase and aspartate aminotransferase, decreased hepatocyte proliferation, and increased rate of apoptotic removal of the injured hepatocytes. PP2Acα knockout mice also displayed a lesser extent of liver fibrosis as a significant decrease in the proportion of α-smooth muscle actin-expressing cells and collagen deposition was observed in their liver tissues. Furthermore, the levels of serum TGF-β1 and hepatocytic Smad phosphorylation were reduced in the PP2Acα knockout mice. These data suggest that hepatocyte-specific ablation of PP2Acα protects against CCl4-induced chronic hepatic injury and fibrogenesis and the protective effect is mediated at least partially through the impaired TGF-β1/Smad signaling.

1. Introduction

Hepatic fibrosis is a common pathological consequence of chronic liver diseases and usually results from prolonged liver injury caused by chronic hepatitis, alcohol, or chemical insults [1]. Irrespective of the etiology, persisting liver fibrogenesis is widely recognized as the major driving force for the progression of any form of chronic liver disease (CLD) ultimately leading to liver cirrhosis and hepatic failure [25]. Among these lines, cirrhosis is currently defined as the end stage of hepatic fibrosis with high prevalence in the world and closely associated with hepatocellular carcinoma incidence. Thus, extensive efforts have been made at elucidating hepatic fibrogenesis with the aim of developing therapeutic strategies for abrogating its progression [6, 7].

Hepatic fibrosis is an abnormal response of the liver to persistent injury with an excessive and aberrant deposition of extracellular matrix (ECM) proteins in the liver, the most abundant of which is the collagen family [8]. After an injury, parenchymal cells undergo the process of regeneration and replacement of the necrotic or apoptotic cells, which requires both a well-orchestrated proliferation of cells and the reconstruction of ECM. When the injury persists, the damaged tissues would eventually suffer from extensive pathological fibrosis due to a progressive excess accumulation of ECM components in an attempt to limit the consequences of chronic parenchymal injury. In the past decade, although several novel mediators, mechanisms, and signaling pathways have been proposed to play an active role in sustaining liver fibrogenesis during CLD progression, transforming growth factor-β1 (TGF-β1) is considered as a major profibrogenic cytokine and a potent inducer of hepatic stellate cell (HSC) proliferation and collagen production [9]. Its collagen synthesis stimulatory effect is executed through intracellular signal transducers Smads whose phosphorylation and subsequent translocation into the nucleus upon TGF-β1-induced activation of the TGF-β receptor would regulate expression of profibrotic target genes [10].

Protein phosphatase 2A (PP2A) is the major eukaryotic serine/threonine phosphatase representing 0.1–1% of total cellular proteins and plays a crucial role in regulating most cellular functions [11]. The typical and primary mammalian PP2A is a heterotrimeric complex consisting of a scaffold subunit (A subunit), a catalytic subunit (PP2Ac), and a regulatory subunit (B subunit) [12]. Molecular cloning has disclosed that there are two isoforms of the mammalian PP2Ac: PP2Acα (encoded by the Ppp2ca gene) and PP2Acβ (encoded by the Ppp2cb gene). These two isoforms share 97% homology in the amino acid sequence and the difference is within the first 30 amino acids [13]. Both PP2Ac isoforms are ubiquitously expressed with PP2Acα transcripts 10-fold greater in general than PP2Acβ transcripts due to transcriptional regulation [14, 15]. However, despite the tremendous functional significance of the “PP2A” family, isoform-specific substrates and the biological role of each specific member of the “PP2A” family remain largely unknown because of the lack of valid isoform-specific PP2A antibodies or specific inhibitors/activators and activity assays, as well as the complexity of PP2A regulation. PP2A has been implicated in the TGF-β1 signaling pathway by modulating the basal level and activity of type I receptors that specifically phosphorylates Smad2 and Smad3 [1618]. We have previously shown that conditionally inactivated Ppp2ca gene in hematopoietic cells perturbed fetal liver erythropoiesis and increased apoptosis of committed erythroid cells via the STAT5 pathway [19]. In this study, we investigated whether and how PP2Acα was involved in hepatic fibrosis chronically induced by CCl4 using a genetic PP2Acα ablation mice model. We found that PP2Acα knockout mice were protected against liver injury and fibrosis development as compared with PP2Acα wild-type mice, an effect likely attributed to a defect in TGF-β1/Smad signaling.

2. Materials and Methods

2.1. Mice and Treatment

Ppp2cafl/fl mice and wild-type B6 mice were bred with AlbCre+ mice, respectively. All the mice were of a mixed 129/B6 background. After cross mating, Ppp2cafl/fl/AlbCre+ (i.e., knockout, KO), Ppp2cafl/fl and AlbCre+ were generated and used in the experiments. Since there was no significant difference in PP2Ac isoform expression, enzyme activity, and liver fibrosis phenotype between Ppp2cafl/fl mice and AlbCre+ mice, these two genotypic mice were used as control. Animal welfare and experimental procedures were approved by the Institutional Animal Care and Use Committee of Nanjing Medical University. To establish chronic liver fibrosis, male mice aged 8–10 weeks were intraperitoneally injected with 2 mg/kg body weight of 10% CCl4 dissolved in olive oil 3 times a week for 5 weeks. Mice were euthanized 48 h following the last injection. Before mice were sacrificed, serum was obtained by retroorbital bleeding from anesthetized mice following overnight fasting.

2.2. Measurement of Phosphatase Activity

Liver protein was extracted in a phosphatase extraction buffer containing 20 mmol/L imidazole-HCl, 2 mmol/L EDTA, 2 mmol/L EGTA (pH 7.0), 1 mmol/L benzamidine, 1 mmol/L phenylmethylsulfonyl fluoride, and protein inhibitor cocktails. Phosphatase activity was assayed using a malachite green-based PP2A Assay Kit (Upstate Biotechnology, Waltham, MA). Briefly, total proteins were immunoprecipitated with anti-PP2Ac, and PP2Ac-bound beads were incubated with synthetic phosphopeptide for the dephosphorylation reaction. The reaction supernatant was then mixed with malachite green reagent for color development. Changes in absorbance were measured at 650 nm.

2.3. ELISA Assay and Biochemistry Analysis

Mice serum TGF-β1 level was assayed by enzyme-linked immunosorbent assay (ELISA) with mouse TGF-β1 immunoassay kit (Sunny ELISA Kits, Mutisciences, Hangzhou, China) following manufacturer’s instructions. Serum alanine transaminase (ALT) and aspartate aminotransferase (AST) levels were measured using an autoanalyzer.

2.4. Immunohistochemistry

Immunohistochemisty was performed on paraffin embedded liver tissues using antibodies specific to PP2Ac (Abcam, Cambridge, UK), α-SMA (Abcam, Cambridge, UK), and PCNA (Abcam, Cambridge, UK). Dewaxed and rehydrated paraffin-embedded sections were incubated with methanol: hydrogen peroxide (1 : 10) to block endogenous peroxidase activity and then were washed in Tris-buffered saline (pH 7.6). The slides were then incubated with the primary antibodies overnight at room temperature. After rinsing with Tris-buffered saline for 15 min, tissues were incubated with secondary antibody (biotinylated goat anti-rabbit IgG, Sigma). Sections were then washed and incubated with the Vectastain Elite ABC reagent (Vector Laboratories, Burlingame, CA) for 45 min. Staining was developed using 3,3-diaminobenzidine (2.5 mg/mL) followed by counterstaining with Mayer’s hematoxylin. Five high-power fields (400x magnification) were randomly selected within each slide. Data are expressed as the average percentage of positive staining cells.

2.5. Histological Analysis and Collagen Content Measurement

Liver tissues were fixed in 4% formalin and embedded in paraffin according to standard procedure. 5 μm sections were cut on a rotary microtome and stained with Sirius red and trichrome for collagen content measurement. For quantification of collagen deposition, slides were prepared from the tissues of 5 individual mice of each genotype. Five fields were randomly selected per slide and calculated for collagen accumulation using Image Pro-Plus software under ×100 objective.

2.6. TUNEL Staining

For in situ detection of apoptotic cells, terminal deoxynucleotidyl transferase-mediated labeling of nick-end DNA (TUNEL) staining was performed according to the manufacturer’s instructions (Roche). Five high-power fields were randomly selected per slide at 400x magnification. Data are expressed as the average percentage of TUNEL-positive cells.

2.7. Western Blot Analysis

Lysates from liver tissues were separated on SDS-PAGE, transferred to polyvinylidene fluoride (PVDF) membranes, and blotted with primary antibodies directed against PP2Ac (Abcam, Cambridge, UK), PCNA (Abcam, Cambridge, UK), Bax (Cell Signaling Technology, Danvers, MA), cleaved caspase-3 (Abcam, Cambridge, UK), α-smooth muscle actin (α-SMA, Abcam, Cambridge, UK), Smad2, phospho-Smad2, Smad3, phospho-Smad3, Bcl-2, β-actin (all from Cell Signaling Technology, Danvers, MA), Cyclin D1 (Upstate Biotechnology, Lake Placid, NY), and Cyclin E (Merck Millipore, Billerica, MA), followed by appropriate secondary antibodies and chemiluminescent detection.

2.8. Statistical Analysis

All data are presented as means standard deviation (SD). Student’s -test was used for comparisons. was considered statistically significant.

3. Results

3.1. PP2Acα Knockout Mice Were Protected against CCl4-Induced Chronic Hepatic Injury

To examine a deletion efficiency of PP2Acα in hepatocytes of PP2Acα knockout (Ppp2cαfl/fl/AlbCre+) mice, PP2Ac protein contents and PP2A phosphatase activity were measured from the livers of Ppp2cαfl/fl/AlbCre+ mice and control Ppp2cαfl/fl and AlbCre+ mice. As shown in Figure 1(a), the expression level of PP2Ac was substantially reduced in Ppp2cαfl/fl/AlbCre+ mice livers compared to that in either Ppp2cαfl/fl or AlbCre+ control, when measured by both Western blot analysis and immunochemical staining using an antibody detecting both PP2Acα and PP2Acβ. Similarly, PP2A phosphatase activity was significantly decreased in the livers of the PP2Acα knockout mice (Figure 1(b). Since Ppp2cαfl/fl and AlbCre+ mice displayed similar level of PP2Ac protein and phosphatase activity in livers, we used Ppp2cαfl/fl mice for subsequent studies. To determine whether PP2Acα knockout mice could be protected against chronic liver injury, the mice were subjected to CCl4 treatment three times a week for 5 weeks and the two indicators of acute liver injuries, serum ALT and AST, were measured. Figure 1(c) shows that the levels of serum ALT and AST in the knockout mice were significantly lower compared with the control, suggesting that PP2Acα knockout mice were more resistant to CCl4-induced chronic hepatic damage.

Figure 1: PP2Acα knockout alleviated liver injury induced by chronic CCl4 administration. (a) PP2Ac protein levels in the livers of knockout (Ppp2cαfl/fl/AlbCre+) and control (Ppp2cαfl/fl and AlbCre+) mice were determined by Western blot analysis (left panel) and immunohistochemical staining (right panel) using an antibody detecting both PP2Acα and PP2Acβ. Magnification, ×400. Bar, 200 μm. (b) PP2A phosphatase activity of protein extracts from the mice liver tissues. Each value is mean ± SD (), . (c, d) Serum alanine aminotransferase (ALT) and aspartate aminotransferase (AST) levels in the knockout and control mice 48 h after intraperitoneal injection with 2 mg/kg CCl4 three times a week for 5 weeks. Each value is mean ± SD (), .
3.2. Knockout of PP2Acα Alleviated CCl4-Induced Chronic Hepatic Fibrosis

To assess the potential protective effect of PP2Acα deletion on liver fibrosis, collagen deposition was determined in the liver tissues of the control and PP2Acα knockout mice after the chronic CCl4 administration. Figure 2(a) shows representative micrographs of Masson’s trichrome staining of liver tissue sections 5 weeks after the CCl4 treatment. In the liver tissues of control mice, extensive fibrosis displaying a honeycomb pattern of fibrous septa (blue staining) was evident whereas much weaker collagen staining was found in the livers of PP2Acα knockout mice. The percentage of the fibrotic area per total liver area was reduced by 56% in the knockout mice when compared with the control mice. Consistently with the results obtained from Masson’s trichrome staining, Sirius red staining for collagen deposition also showed that PP2Acα knockout mice largely inhibited hepatic collagen accumulation after the chronic CCl4 challenge (Figure 2(b). These data indicated that loss of PP2Acα was capable of protecting the liver from the development of fibrotic lesions after CCl4.

Figure 2: PP2Acα ablation attenuated CCl4-induced liver fibrosis. Masson’s trichrome staining (a) and Sirius red staining (b) of liver tissue sections from the control and PP2Acα knockout mice at 5 weeks after the chronic CCl4 treatment. Magnification, ×100. Bar, 50 μm. The histograms show the mean percentage of the staining area per total liver area determined from five randomly selected fields. Values are means ± SD, . and .
3.3. PP2Acα Deletion Blocked Hepatic Stellate Cell (HSC) Activation In Vivo

Since activation of HSCs to overproduce ECM is a key event in the pathophysiology of hepatic fibrosis and α-smooth muscle actin (α-SMA) is a marker for activated HSCs, we sought to investigate whether there was different expression of α-SMA expression in livers from the control and PP2Acα knockout mice chronically treated with CCl4. As shown in Figure 3(a), stronger intensity of α-SMA immunohistochemical staining and significantly more α-SMA positive cells were observed in liver sections of the control mice than those of PP2Acα mice. Similar results were obtained from immunoblot analysis. Compared with the control, the levels of hepatic α-SMA protein were markedly reduced in the PP2Acα knockout mice (Figure 3(b). These observations imply that PP2Acα may stimulate liver fibrosis via HSC activation and therefore its deletion may reduce the liver fibrosis through abolishing the profibrogenic effect of CCl4.

Figure 3: PP2Acα deletion inhibited HSC activation. (a) Immunohistochemical analysis of α-SMA expression in liver tissues from the control and PP2Acα knockout mice at 5 weeks after the chronic CCl4 treatment. Magnification, ×100. Bar, 50 μm. The histogram shows the mean percentage of the α-SMA positive area per total liver area determined from five randomly selected fields. Values are means ± SD, . . (b) Western blot analyses of hepatic α-SMA expression in the control and PP2Acα knockout mice at 5 weeks after the chronic CCl4 treatment. Liver homogenates were probed with antibodies against α-SMA and β-actin, respectively.
3.4. Deletion of PP2Acα Reduced Hepatocyte Proliferation but Increased Hepatocyte Apoptosis

To understand the mechanism underlying the less liver fibrosis in the PP2Acα knockout mice than in the control mice, we first examined hepatocyte proliferation and apoptosis in the two strains of mice after the chronic challenge. As shown in Figure 4(a), hepatocyte proliferation was significantly reduced in the knockout mice compared to the control, as evidenced by PCNA immunohistochemical staining on liver sections. To determine whether the proliferation inhibitory effect induced by PP2Acα knockout was related to apoptosis, we assessed the frequency of apoptotic cells within the liver tissues by the in situ TUNEL staining. As shown in Figure 4(b), a marginal increase in the number of apoptotic hepatocytes was observed in the PP2Acα knockout mice compared to the control mice. However, necrosis was less pronounced in the liver of PP2Acα knockout mice (Figure 4(c). Consistently with the apoptosis data, the liver lysates from PP2Acα knockout mice showed a decrease in proliferating cell nuclear antigen PCNA, cell cycle-promoting molecule Cyclins D and E, and antiapoptotic molecule Bcl-2 expression levels but demonstrated an increased level of proapoptotic protein Bax and active caspase-3 (Figure 4(d)). These data indicated that the PP2Acα knockout mice were protected against chronic CCl4-induced liver injury, possibly due to less injurious responsiveness in the lack of PP2Acα.

Figure 4: Knockout of PP2Acα suppressed hepatocyte proliferation and enhanced hepatocyte apoptosis. (a) Immunohistochemical analysis of PCNA expression in the livers from the control and PP2Acα knockout mice at 5 weeks after the chronic CCl4 treatment. Magnification, ×400. Bar, 200 μm. The histogram shows the mean percentage of the PCNA-positive cells determined from five randomly selected fields. (b) TUNEL staining was performed on the liver sections from the control and PP2Acα knockout mice at 5 weeks after the chronic CCl4 treatment. Magnification, 400. Bar, 200 μm. The histogram shows the mean percentage of the TUNEL-positive cells determined from five randomly selected fields. (c) H&E staining of liver tissue sections from the control and PP2Acα knockout mice at 5 weeks after the chronic CCl4 treatment. Representative areas of necrosis are indicated by arrowheads. Magnification, 100. Bar, 50 μm. The histogram shows the mean percentage of the necrotic area per total liver area determined from five randomly selected fields. Values are means ± SD, . and . (d) Western blot analyses of hepatic PCNA, Cyclin D, Cyclin E, Bcl-2, Bax, and cleaved caspase-3 expression in the control and PP2Acα knockout mice at 5 weeks after the chronic CCl4 treatment. β-actin was used as a loading control.
3.5. PP2Acα Deletion Inhibited TGF-β Secretion and Impaired TGF-β Downstream Signaling

Since TGF-β and its downstream signal transducers Smads have been well established to play a vital role in the progression of fibrogenesis at both cellular and molecular levels [20], we next sought to determine whether TGFβ1/Smad signaling was altered in the PP2Acα knockout mice that may underlie the inner mechanism behind its resistance to CCl4-induced fibrosis. As shown in Figure 5(a), the serum level of TGFβ1 was significantly reduced in the PP2Acα knockout mice compared with wild-type mice. Meanwhile, the expressions of phospho-Smad2 and phospho-Smad3, mediators of the TGFβ1 signaling, were also substantially suppressed in the PP2Acα knockout mice. Thus, at least part of the observed reduction in hepatic fibrosis in the PP2Acα knockout mice can be accounted for by a decrease in TGFβ1/Smad signaling.

Figure 5: PP2Acα ablation diminished the serum level of TGF-β1 and its downstream signal transduction. (a) Quantification of serum TGF-β1 level by ELISA in the control and PP2Acα knockout mice chronically treated with CCl4 for 5 weeks. Values are means ± SD, . . (b) Western blot analysis of phospho-Smad2 (p-Smad2), total Smad2 (Smad2), phospho-Smad3 (p-Smad3), and total Smad3 (Smad3) expression levels in the livers from the control and PP2Acα knockout mice treated chronically with CCl4 for 5 weeks.

4. Discussion

This study demonstrates that PP2Acα is crucial for liver injury and fibrogenesis. Conditional genetic deletion of PP2Acα attenuated liver fibrosis in the mice following chronic CCl4 treatment, probably through impairing TGFβ1/Smad profibrotic signaling pathway. Our results indicate that PP2Acα could interfere with the TGF-β/Smad signaling pathway, which in turn modulates critical pathological events such as collagen deposition, HSC activation, and hepatocyte proliferation and apoptosis in the development of hepatic fibrosis.

PP2A regulates many key cellular processes such as the cell cycle, cell growth, apoptosis, and signal transduction. It has long been speculated that the individual, yet highly homologous, members of each subfamily of PP2A subunits would have unique and specific roles in addition to their established redundant activities. Genetic deletion of PP2A catalytic subunit Cα (PP2Acα) in mice results in embryonic lethality with no mesoderm induction [21], which implies that PP2Acα plays an important role in mesenchymal cells such as osteoblasts, adipocytes, and myoblasts. Most recently, PP2Acα has been shown to be an important regulator of adipocyte differentiation by regulating the expression of adipocyte marker genes and the Wnt/GSK-3β/β-catenin pathway [22]. However, the role of PP2Acα in liver injury and fibrosis has not been examined previously. The results of the studies reported here provide multiple lines of evidence that the expression of PP2Acα influences the consequence of hepatic damage repair and fibrogenesis under CCl4-induced liver toxicity. When treated chronically with CCl4, PP2Acα knockdown mice had less liver damage as demonstrated by lower serum ALT and AST levels consequent to a significant reduction in PP2A phosphatase activity of the mice liver tissues. Decreased mitotic activity in the liver sections was further confirmed by immunostaining for expression of PCNA, a nuclear protein highly expressed during the DNA synthesis phase of the cell cycle and closely correlated with the proliferative state of the cells [23]. The number of PCNA-positive cells was significantly reduced in the livers of CCl4-treated PP2Acα knockdown mice compared with the wild-type mice. The primary mode of cell death in response to CCl4 injury is through necrosis; however, it has been shown that apoptosis may also play a role in the elimination of damaged hepatocytes [2426]. In our mice model under chronic CCl4 administration, increased hepatocyte apoptosis and reduced antiapoptotic protein Bcl-2 expression as well as enhanced expression of proapoptotic protein Bax and activation of caspase-3 were observed in livers of PP2Acα knockdown mice. It may be noteworthy that treatment of PP2A inhibitor could augment Bcl-2 phosphorylation that also leads to a reduction in its antiapoptotic function [27]. Therefore, reduced Bcl-2 expression together with possible increased Bcl-2 phosphorylation may contribute to higher apoptotic rate in the hepatocytes of PP2Acα mice. These results suggest that the ablation of the hepatocyte-specific PP2Acα reduces the severity of CCl4-induced liver injury by masking proliferative/regenerative response and promoting apoptotic response to remove the damaged hepatocytes.

Activation of the α-SMA-positive, matrix-producing myofibroblasts has long been recognized as a major decisive event in tissue fibrogenesis after chronic injury. They are often presumed to be derived from hepatic stellate cells (HSCs) which have been considered as the main source of ECM during liver fibrosis and are the first identified fibrogenic cell population [28, 29]. In the normal liver, they display a quiescent phenotype. However, upon acute or chronic liver injury, a complex network of autocrine/paracrine fibrogenic signals promotes transdifferentiation of quiescent HSCs to a myofibroblastic phenotype characterized by the expression of α-smooth muscle actin and de novo expression of receptors for fibrogenic, chemotactic, and mitogenic factors [30]. In this study, we have shown that significantly less collagen accumulation in the livers of PP2Acα knockdown mice was accompanied by a substantial reduction in α-SMA-expressing cells. It is therefore possible that suppressed HSC activation due to PP2Acα ablation may contribute to the resistance to chronic hepatic fibrosis in the PP2Acα knockout mice compared to the similarly treated wild-type mice. HSCs are not only an important source of growth factors in the liver but also a good responder to these factors, emphasizing the importance of tightly regulated autocrine control of growth factor activity within pericellular milieu [31]. TGF-β1 is derived from both paracrine and autocrine sources and is the most potent fibrogenic cytokine in the liver [32, 33]. It is secreted in a biologically inactive form which can be converted into active form in response to injury. Once activated, TGF-β1 signals via its cognate TGF-β1 receptor that phosphorylates the transcription factor Smads (Smads 1, 2, 3, 5, and 8) forming a complex with the co-Smad (Smad4), which then translocates into the nucleus to regulate transcription of profibrotic target genes [20, 33]. TGF-β1/Smad signaling pathway can influence various aspects in the fibrogenic process including regulation of hepatocyte proliferation and apoptosis, mediation of HSC activation, and the subsequent ECM production in response to liver injury [34, 35]. In our CCl4 chronically treated mice models, the TGF-β1 serum level was significantly decreased in PP2Acα knockout mice compared with the control wild-type mice. As expected, phospho-Smad2 and phospho-Smad3 were drastically reduced in the absence of PP2Acα. In good agreement with this, we found a similar change in the expression of Cyclin D1 and Cyclin E which have been known to be TGF-β1/Smad regulated targets [36, 37]. PP2A has been reported to function as a negative regulator in TGF-β1-induced TAK1 (transforming growth factor-β-activated kinase 1) activation in mesangial cells [38]. However, it should be recognized that control of TAK1 activation may be conducted in a cell type-specific or context-dependent manner [38, 39]. Thus, it is conceivable that different protein phosphatases or even different subunits of PP2A may be compensatorily expressed due to PP2Acα ablation and play distinct and opposing roles in the regulation of TGF-β1/Smad signaling. While the exact molecular mechanisms remain to be clarified and explored, it is tempting to suggest a model in which TGF-β1/Smad signaling is impaired as a result of PP2Acα deficiency, which in turn leads to less susceptibility to hepatic damage, suppressed HSC activation, and decreased collagen production, thus protecting PP2Acα knockout mice against CCl4-induced chronic hepatic fibrosis.

In summary, our studies demonstrate that PP2Acα plays a crucial role in the progression of fibrosis using an in vivo genetic mice model. In PP2Acα knockout mice, chronic hepatic fibrosis induced by CCl4 administration is less severe compared with their wild-type littermates. The protective effect of PP2Acα ablation is mediated, at least in part, through the impaired TGF-β1/Smad signaling in PP2Acα mice. Therefore, genetic approach or pharmacological intervention targeting PP2Acα enzymatic activity or its interaction with downstream targets could potentially serve as an effective strategy to the future treatment of hepatic fibrosis.

Conflict of Interests

The authors declare that there is no conflict of interests regarding the publication of this paper.

Acknowledgment

The study is supported by the grant from Natural Science Foundation of Jiangsu Province (no. BK2011133).

References

  1. S. L. Friedman, “Evolving challenges in hepatic fibrosis,” Nature Reviews Gastroenterology & Hepatology, vol. 7, no. 8, pp. 425–436, 2010. View at Publisher · View at Google Scholar · View at Scopus
  2. S. L. Friedman, “Mechanisms of hepatic fibrogenesis,” Gastroenterology, vol. 134, no. 6, pp. 1655–1669, 2008. View at Publisher · View at Google Scholar · View at Scopus
  3. M. Parola, F. Marra, and M. Pinzani, “Myofibroblast—like cells and liver fibrogenesis: emerging concepts in a rapidly moving scenario,” Molecular Aspects of Medicine, vol. 29, no. 1-2, pp. 58–66, 2008. View at Publisher · View at Google Scholar · View at Scopus
  4. J. A. Dranoff and R. G. Wells, “Portal fibroblasts: underappreciated mediators of biliary fibrosis,” Hepatology, vol. 51, no. 4, pp. 1438–1444, 2010. View at Publisher · View at Google Scholar · View at Scopus
  5. M. Rosselli, J. MacNaughtan, R. Jalan, and M. Pinzani, “Beyond scoring: a modern interpretation of disease progression in chronic liver disease,” Gut, vol. 62, no. 9, pp. 1234–1241, 2013. View at Publisher · View at Google Scholar · View at Scopus
  6. S. L. Friedman, “Molecular regulation of hepatic fibrosis, an integrated cellular response to tissue injury,” The Journal of Biological Chemistry, vol. 275, no. 4, pp. 2247–2250, 2000. View at Publisher · View at Google Scholar · View at Scopus
  7. J. P. Iredale, “Models of liver fibrosis: exploring the dynamic nature of inflammation and repair in a solid organ,” Journal of Clinical Investigation, vol. 117, no. 3, pp. 539–548, 2007. View at Publisher · View at Google Scholar · View at Scopus
  8. K. Wallace, A. D. Burt, and M. C. Wright, “Liver fibrosis,” Biochemical Journal, vol. 411, no. 1, pp. 1–18, 2008. View at Publisher · View at Google Scholar · View at Scopus
  9. G. Eghbali-Fatourechi, G. C. Sieck, Y. S. Prakash, P. Maercklein, G. J. Gores, and L. A. Fitzpatrick, “Type I procollagen production and cell proliferation is mediated by transforming growth factor-β in a model of hepatic fibrosis,” Endocrinology, vol. 137, no. 5, pp. 1894–1903, 1996. View at Publisher · View at Google Scholar · View at Scopus
  10. A. M. Gressner and R. Weiskirchen, “Modern pathogenetic concepts of liver fibrosis suggest stellate cells and TGF-β as major players and therapeutic targets,” Journal of Cellular and Molecular Medicine, vol. 10, no. 1, pp. 76–99, 2006. View at Publisher · View at Google Scholar · View at Scopus
  11. D. M. Virshup and S. Shenolikar, “From promiscuity to precision: protein phosphatases get a makeover,” Molecular Cell, vol. 33, no. 5, pp. 537–545, 2009. View at Publisher · View at Google Scholar · View at Scopus
  12. D. M. Virshup, “Protein phosphatase 2A: a panoply of enzymes,” Current Opinion in Cell Biology, vol. 12, no. 2, pp. 180–185, 2000. View at Publisher · View at Google Scholar · View at Scopus
  13. J. Arino, C. W. Woon, D. L. Brautigan, T. B. Miller Jr., and G. L. Johnson, “Human liver phosphatase 2A: cDNA and amino acid sequence of two catalytic subunit isotypes,” Proceedings of the National Academy of Sciences of the United States of America, vol. 85, no. 12, pp. 4252–4256, 1988. View at Publisher · View at Google Scholar · View at Scopus
  14. Y. Khew-Goodall and B. A. Hemmings, “Tissue-specific expression of mRNAs encoding α- and β-catalytic subunits of protein phosphatase 2A,” FEBS Letters, vol. 238, no. 2, pp. 265–268, 1988. View at Publisher · View at Google Scholar · View at Scopus
  15. Y. Khew-Goodall, R. E. Mayer, F. Maurer, S. R. Stone, and B. A. Hemmings, “Structure and transcriptional regulation of protein phosphatase 2A catalytic subunit genes,” Biochemistry, vol. 30, no. 1, pp. 89–97, 1991. View at Google Scholar
  16. I. Griswold-Prenner, C. Kamibayashi, E. M. Maruoka, M. C. Mumby, and R. Derynck, “Physical and functional interactions between type I transforming growth factor β receptors and Bα, a WD-40 repeat subunit of phosphatase 2A,” Molecular and Cellular Biology, vol. 18, no. 11, pp. 6595–6604, 1998. View at Google Scholar · View at Scopus
  17. C. Petritsch, H. Beug, A. Baimain, and M. Oft, “TGF-β inhibits p70 S6 kinase via protein phosphatase 2A to induce G1 arrest,” Genes and Development, vol. 14, no. 24, pp. 3093–3101, 2000. View at Publisher · View at Google Scholar · View at Scopus
  18. J. Batut, B. Schmierer, J. Cao, L. A. Raftery, C. S. Hill, and M. Howell, “Two highly related regulatory subunits of PP2A exert opposite effects on TGF-β/activin/nodal signalling,” Development, vol. 135, no. 17, pp. 2927–2937, 2008. View at Publisher · View at Google Scholar · View at Scopus
  19. W. Chen, P. Gu, X. Jiang, H.-B. Ruan, C. Li, and X. Gao, “Protein phosphatase 2A catalytic subunit α (PP2Acα) maintains survival of committed erythroid cells in fetal liver erythropoiesis through the STAT5 pathway,” The American Journal of Pathology, vol. 178, no. 5, pp. 2333–2343, 2011. View at Publisher · View at Google Scholar · View at Scopus
  20. T. A. Wynn, “Cellular and molecular mechanisms of fibrosis,” Journal of Pathology, vol. 214, no. 2, pp. 199–210, 2008. View at Publisher · View at Google Scholar · View at Scopus
  21. J. Götz, A. Probst, E. Ehler, B. Hemmings, and W. Kues, “Delayed embryonic lethality in mice lacking protein phosphatase 2A catalytic subunit Cα,” Proceedings of the National Academy of Sciences of the United States of America, vol. 95, no. 21, pp. 12370–12375, 1998. View at Publisher · View at Google Scholar · View at Scopus
  22. H. Okamura, D. Yang, K. Yoshida, J. Teramachi, and T. Haneji, “Reduction of PP2A Cα stimulates adipogenesis by regulating the Wnt/GSK-3β/β-catenin pathway and PPARγ expression,” Biochimica et Biophysica Acta—Molecular Cell Research, vol. 1843, pp. 2376–2384, 2014. View at Publisher · View at Google Scholar
  23. R. Bravo, “Synthesis of the nuclear protein cyclin (PCNA) and its relationship with DNA replication,” Experimental Cell Research, vol. 163, no. 2, pp. 287–293, 1986. View at Publisher · View at Google Scholar · View at Scopus
  24. M. B. Bansal, K. Kovalovich, R. Gupta et al., “Interleukin-6 protects hepatocytes from CCl4-mediated necrosis and apoptosis in mice by reducing MMP-2 expression,” Journal of Hepatology, vol. 42, no. 4, pp. 548–556, 2005. View at Publisher · View at Google Scholar · View at Scopus
  25. W. Xu, C. Hellerbrand, U. A. Köhler et al., “The Nrf2 transcription factor protects from toxin-induced liver injury and fibrosis,” Laboratory Investigation, vol. 88, no. 10, pp. 1068–1078, 2008. View at Publisher · View at Google Scholar · View at Scopus
  26. K. Şerbetçi, O. Uysal, N. Erkasap, T. Köken, C. Baydemir, and S. Erkasap, “Anti-apoptotic and antioxidant effect of leptin on CCl4-induced acute liver injury in rats,” Molecular Biology Reports, vol. 39, no. 2, pp. 1173–1180, 2012. View at Publisher · View at Google Scholar · View at Scopus
  27. Y. Tamura, S. Simizu, and H. Osada, “The phosphorylation status and anti-apoptotic activity of Bcl-2 are regulated by ERK and protein phosphatase 2A on the mitochondria,” FEBS Letters, vol. 569, no. 1–3, pp. 249–255, 2004. View at Publisher · View at Google Scholar · View at Scopus
  28. A. Geerts, “History, heterogeneity, developmental biology, and functions of quiescent hepatic stellate cells,” Seminars in Liver Disease, vol. 21, no. 3, pp. 311–335, 2001. View at Publisher · View at Google Scholar · View at Scopus
  29. R. Safadi and S. L. Friedman, “Hepatic fibrosis—role of hepatic stellate cell activation,” MedGenMed, vol. 4, no. 3, p. 27, 2002. View at Google Scholar · View at Scopus
  30. A. Mallat and S. Lotersztajn, “Cellular mechanisms of tissue fibrosis. 5. Novel insights into liver fibrosis,” American Journal of Physiology—Cell Physiology, vol. 305, no. 8, pp. C789–C799, 2013. View at Publisher · View at Google Scholar · View at Scopus
  31. U. E. Lee and S. L. Friedman, “Mechanisms of hepatic fibrogenesis,” Best Practice & Research: Clinical Gastroenterology, vol. 25, no. 2, pp. 195–206, 2011. View at Publisher · View at Google Scholar · View at Scopus
  32. K. Breitkopf, P. Godoy, L. Ciuclan, M. V. Singer, and S. Dooley, “TGF-β/Smad signaling in the injured liver,” Zeitschrift fur Gastroenterologie, vol. 44, no. 1, pp. 57–66, 2006. View at Publisher · View at Google Scholar · View at Scopus
  33. Y. Inagaki and I. Okazaki, “Emerging insights into transforming growth factor β Smad signal in hepatic fibrogenesis,” Gut, vol. 56, no. 2, pp. 284–292, 2007. View at Publisher · View at Google Scholar · View at Scopus
  34. A. M. Gressner, R. Weiskirchen, K. Breitkopf, and S. Dooley, “Roles of TGF-beta in hepatic fibrosis,” Front Biosci, vol. 7, pp. d793–d807, 2002. View at Publisher · View at Google Scholar · View at Scopus
  35. S. Dooley and P. Ten Dijke, “TGF-β in progression of liver disease,” Cell and Tissue Research, vol. 347, no. 1, pp. 245–256, 2012. View at Publisher · View at Google Scholar · View at Scopus
  36. K. Jungert, M. Buchholz, M. Wagner, G. Adler, T. M. Gress, and V. Ellenrieder, “Smad-Sp1 complexes mediate TGFβ-induced early transcription of oncogenic Smad7 in pancreatic cancer cells,” Carcinogenesis, vol. 27, no. 12, pp. 2392–2401, 2006. View at Publisher · View at Google Scholar · View at Scopus
  37. E. Cocolakis, M. Dai, L. Drevet et al., “Smad signaling antagonizes STAT5-mediated gene transcription and mammary epithelial cell differentiation,” Journal of Biological Chemistry, vol. 283, no. 3, pp. 1293–1307, 2008. View at Publisher · View at Google Scholar · View at Scopus
  38. I. K. Sung, H. K. Joon, L. Wang, and M. E. Choi, “Protein phosphatase 2A is a negative regulator of transforming growth factor-β1-induced TAK1 activation in mesangial cells,” The Journal of Biological Chemistry, vol. 283, no. 16, pp. 10753–10763, 2008. View at Publisher · View at Google Scholar · View at Scopus
  39. T. Kajino, H. Ren, S.-I. Iemura et al., “Protein phosphatase 6 down-regulates TAK1 kinase activation in the IL-1 signaling pathway,” The Journal of Biological Chemistry, vol. 281, no. 52, pp. 39891–39896, 2006. View at Publisher · View at Google Scholar · View at Scopus