Tyrosine 705 Phosphorylation of STAT3 Is Associated with Phenotype Severity in TGF<i>β</i>1 Transgenic Mice

Guadagnin, Eleonora; Narola, Jigna; Bönnemann, Carsten G.; Chen, Yi-Wen

doi:https://doi.org/10.1155/2015/843743

BioMed Research International

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Abstract Introduction Materials and Methods Results Discussion Conclusion Acknowledgments References Copyright Related Articles

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Muscular Dystrophy: Disease Mechanisms and Therapies

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Research Article | Open Access

Volume 2015 | Article ID 843743 | https://doi.org/10.1155/2015/843743

Tyrosine 705 Phosphorylation of STAT3 Is Associated with Phenotype Severity in TGFβ1 Transgenic Mice

Eleonora Guadagnin,¹Jigna Narola,¹Carsten G. Bönnemann,²and Yi-Wen Chen^1,3

Academic Editor: Toshifumi Yokota

Received20 Jan 2015

Accepted30 Mar 2015

Published24 Aug 2015

Abstract

Transforming growth factor beta 1 (TGFβ1) is a key player in skeletal muscle degenerative and regenerative processes. We previously showed that conditionally overexpressing TGFβ1 in skeletal muscles caused myofiber atrophy and endomysial fibrosis in mice. However, the disease severity varied significantly among individual mice. While 40% of mice developed severe muscle pathology and lost body weight within 2 weeks of TGFβ1 transgene induction in muscles, the rest showed milder or no phenotype. This study aims at determining whether signal transducer and activator of transcription 3 (STAT3) plays a role in the phenotypic difference and whether it can be activated by TGFβ1 directly in muscle cells. Our results show that while total STAT3 was not differentially expressed between the two groups of mice, there was significantly higher pSTAT3 (Tyr705) in the muscles of the mice with severe phenotype. Immunohistochemistry showed that pSTAT3 (Tyr705) was localized in approximately 50% of the nuclei of the muscles. We further showed that TGFβ1 induced Tyr705 phosphorylation of STAT3 in C2C12 cells within 30 minutes of treatment while total STAT3 was not affected. Our findings suggest that TGFβ1 alone can induce Tyr705 phosphorylation of STAT3 in skeletal muscle cells and contribute to disease severity in transgenic TGFβ1 mice.

1. Introduction

TGFβ1 belongs to the TGFβ superfamily and has been shown to regulate a wide variety of biological processes, including promotion of apoptosis, inhibition of cell growth, and induction of cell differentiation, migration, and extracellular matrix (ECM) deposition [1, 2]. Several studies showed that persistent expression and activation of TGFβ1 act as negative regulator of muscle repair by inducing apoptosis in myoblasts, suppressing muscle differentiation, and causing fibrosis in the muscles [3–5]. TGFβ1 is believed to be responsible for the ECM deposition in skeletal muscle [6–9], which leads to endomysial and perimysial fibrosis in muscular dystrophies, including Duchenne muscular dystrophy and congenital muscular dystrophies [10–12]. Using animal models, we and others demonstrated that TGFβ1 alone can cause muscle atrophy and fibrosis in vivo [5, 13, 14]. However, TGFβ1 is also recognized to play critical roles in muscle regeneration process by recruiting macrophages to clean up the damaged tissues after muscle injury and in muscle diseases [15].

The signal transducer and activator of transcription (STAT) family are composed of latent cytoplasmic proteins with a dual molecular role: signal transducer and transcription activator [16, 17]. One member of the STAT family, STAT3, is expressed in most of tissue types and responds mainly to IL-6, IL-10, and EGF signals [18, 19]. Phosphorylation of specific receptor tyrosine residue (Tyr705 or Ser727) in response to ligand stimulation determines the activities of STAT3. Tyr705 phosphorylation of latent cytoplasmic STAT3 promotes STAT3 homodimerization or heterodimerization with other STATs, which leads to nucleus translocation and DNA binding. Ser727 phosphorylation takes place at the C-terminal transactivation domain of STAT3 and allows maximal activation of transcription of its target genes [20]. Within hours, STAT3 is exported back to the cytoplasm and the signaling cascade is terminated [21–23]. Previous studies showed that TGFβ1 directly activates STAT3 in other cell types, including proximal tubular cells, T-cells, and pancreas [24–26]. One study showed that STAT3 activation by TGFβ1 plays a major role in the pathological connective tissue deposition in liver via the activation of connective tissue growth factor (CTGF) in hepatic cells [27]. The same study showed that STAT3 inhibition was sufficient to prevent CTGF induction and fibrosis by TGFβ1. While it is known that STAT3 activation in response to IL-6 stimulation plays major roles in modulating muscle mass, to date there is no direct evidence that TGFβ1 activates STAT3 in skeletal muscle cells.

To study the effects of TGFβ1 on muscle fibrosis and atrophy, we generated a tet-repressible muscle-specific TGFβ1 transgenic mouse model [5]. In this model, withdrawal of oral doxycycline induces the expression of TGFβ1 transgene. The study showed that TGFβ1 overexpression in skeletal muscles causes muscle atrophy and endomysial fibrosis. Interestingly, we observed that a subgroup of the TGFβ1 transgenic mice showed more severe muscle weight loss while the rest exhibited milder pathology. The size of the myofibers was significantly smaller and the endomysial fibrosis was significantly higher in the subgroup with severe phenotypes, suggesting that activation of additional signaling pathways leads to more severe phenotypes. In this study, we investigated whether the STAT3 and phosphorylation of the protein in the mice were associated with more severe phenotype. In addition, we conducted an in vitro study using C2C12 myoblasts to determine whether TGFβ1 can activate STAT3 in muscle cells.

2. Materials and Methods

2.1. Mouse Model and Muscle Collection

All muscle samples used in this were collected as described previously [5]. Briefly, the tet-repressible muscle-specific TGF-β1 transgenic mice (TRE-TGF-β1/mCK-tTA) were generated by crossing two transgenic mouse lines (TRE-TGF-β1 and mCK-tTA). The TRE-TGF-β1 line carries a porcine TGF-β1 cDNA containing a double mutation where cysteines at positions 223 and 225 are converted to serines, which is regulated by the tetO recognition element (TRE). The mCK-tTA line carries a construct containing the tetracycline-controlled transactivator (tTA) protein driven by a muscle-specific creatine kinase promoter (mCK). The presence of doxycycline in cells inhibits binding of tTA to the TRE and blocks TGF-β1 transgene expression. After crossbreeding the TRE-TGF-β1 and mCK-tTA lines, the pregnant female mice received drinking water with doxycycline (200 μg/mL in 5.0% sucrose) in order to suppress the TGF-β1 transgene expression in the pups in utero. After weaning, all pups were maintained on water treated with doxycycline until the transgene was induced. In this study, doxycycline was removed from water to induce transgene expression in the TRE-TGFβ1/mCK-tTA mice when the mice were 6 weeks old. The muscles were collected 2 weeks after the TGFβ1 transgene was induced. Littermates with only one of the transgenes, which do not express TGFβ1 were used as controls.

2.2. Immunoblotting

Vastus lateralis muscles were sectioned with a Leica CM 1900 cryostat (Walldorf, Baden-Wurttemberg, Germany). Thirty 10 μm cryosections were lysed in 50 μL of RIPA buffer (0.1% SDS, 1% NP40, 0.5% sodium deoxycholate, 150 mM sodium chloride, and 50 mM TrisHCl pH 7.5) for 30 minutes on ice, with protease inhibitor cocktail (Complete, Roche, Mannheim, Germany) as well as phosphatase inhibitor cocktail (PhosStop, Roche, Mannheim, Germany). At the end of the incubation, the cell extracts were centrifuged for 10 minutes (12,000 g) at 4°C. The amount of protein was calculated using the Quick Start Bradford Protein Assay Kit 1 (Bio Rad Laboratories, Hercules, CA). Then 30 μg of protein in NuPAGE LDS Sample Buffer (Life Technologies, Grand Island, NY) and NuPAGE Sample Reducing Agent (Life Technologies, Grand Island, NY) was loaded to SDS-PAGE gel for immunoblotting analysis. The primary antibodies used were pSTAT3 (Y705, 1 : 1000; Cell Signaling Technology, Danvers, MA), pSTAT3 (S727, 1 : 1000; Cell Signaling Technology, Danvers, MA), and Total STAT3 (1 : 1000; Cell Signaling Technology, Danvers, MA). Bound antibodies were detected using ECL reagents. The results were normalized to GAPDH (1 : 5000; Millipore, Billerica, MA). Band intensity was evaluated by densitometry analysis, normalized to its total content, and reported as fold increase relative to respective control set as 1.

2.3. Immunofluorescence Staining

To detect pSTAT3 (Tyr705), muscle sections of 5 μm were fixed in 4% paraformaldehyde, washed 3 times in 1x PBS, permeabilized with 0.5% Triton X-100 for 10 minutes at room temperature, and blocked with 5% goat serum. The slides were incubated overnight at 4°C with the primary antibody against pSTAT3 Tyr705 (1 : 100 diluted in 5% goat serum). Secondary antibody only was used as the negative control. After 3 washes in PBS for 15 minutes each, the slides were incubated with the secondary antibody Alexa Fluor 680 Donkey Anti-Rabbit IgG (Life Technlogies, Grand Island, NY) for 1 hour at room temperature and then washed again 3 times in 1x PBS. Finally, the slides were mounted with the appropriate mounting medium (ProLong Gold Antifade Reagent with DAPI, Molecular Porbes, Life Technologies, Grand Island, NY). Images of the tissue sections (20x, 40x) were taken using Nikon Eclipse E800 microscope (Nikon, Chiyoda-ku, Tokyo, Japan), RT slider camera (Diagnostic Instrument, Sterling Height, MI), and SPOT advanced software.

2.4. Cell Culture and Treatment

Murine C2C12 myoblasts were cultured in DMEM (Life Technologies, Grand Island, NY) supplemented with 10% fetal bovine serum, 2 mM L-glutamine, and 100 U/mL penicillin/streptomycin at 37°C in 5% CO₂. Cells were seeded in 6-well plates, and when they were 70% confluent, they were induced to differentiate with DMEM supplemented with 5% horse serum, 2 mM L-glutamine, and 100 U/mL penicillin/streptomycin at 37°C in 5% CO₂. TGFβ1 (R&D SYSTEMS, Minneapolis, MN) was reconstituted at 20 μg/mL in sterile 4 mM HCl containing 1 mg/mL BSA, according to the manufacturer’s instructions. C2C12 were then treated with TGFβ1 10 ng/mL after 7 days of differentiation for 30 minutes, 2 hours, and 24 hours. The cells were harvested and lysed in 30 μL of RIPA buffer for immunoblotting.

2.5. Statistical Analysis

Data are shown as mean ± SEM. The Kruskal-Wallis test was used for determining statistical significance among different groups of mice. Values of were considered significant. Student’s -test was used for determining statistical significance in treated cells. Values of were considered significant.

3. Results

3.1. Tyr705 Phosphorylation of STAT3 Is Associated with the Severe Phenotypes Induced by TGFβ1

After the TGFβ1 transgene was induced for two weeks, approximately 40% of mice developed severe phenotypes, including early body weight loss and severe myofiber atrophy and fibrosis [5]. In the study, the mice in this group were defined as mice with early onset (EO). The rest of mice were grouped into the late onset (LO) group. To determine whether STAT3 activation, which is known to be involved in muscle atrophy induced by IL-6, is involved in the variation of phenotypic presentations, we first examined the protein expression of total STAT3 as well as two phosphorylated STAT3, pSTAT3 (Tyr705), and pSTAT3 (Ser727), in muscles collected from the two groups of mice. Littermates of these mice, which did not express TGFβ1, were used as baseline control.

Immunoblotting analysis showed that while the total STAT3 was not significantly different among the EO, LO, and control groups, pSTAT3 (Tyr705) was significantly induced in the muscles of EO mice. No pSTAT3 (Tyr705) was detected in the control or LO mice (Figure 1). The expression of pSTAT3 (Ser727) was observed in muscles of all 3 groups but no significant difference among them. Variations of expression levels of total STAT3 and pSTAT3 (Ser727) were observed among different samples in all three groups. However, no correlation between the total STAT3 and pSTAT3 (Ser727) was observed.

3.2. pSTAT3 (Tyr705) Is Localized in the Nucleus of Myofibers in the TGFβ1 Mice with Severe Phenotype

After examining the phosphorylation status of STAT3, we investigated the cellular localization of pSTAT3 (Tyr705). Immunofluorescence staining using a pSTAT3 (Tyr705)-specific antibody showed that expression of pSTAT3 (Tyr705) was visible and was localized in nuclei of the muscles of the EO mice, but was not detectable in the LO mice and controls (Figure 2). Approximately 50% of nuclei in the vastus lateralis muscles of the EO mice were positive of pSTAT3 (Tyr705). When costained with PAX7, a satellite cell marker, no pSTAT3 positive cells were costained. Our previous studies showed no overt inflammatory infiltration in the muscles of these mice [5]; therefore, most of the positive nuclei are likely myonuclei. To confirm that, we costained muscle sections with CD14 and CD11b (monocyte/macrophage markers) and CD3 (lymphocytes marker), respectively. In the few positive cells, no nuclei were costained with pSTAT3 (Tyr705).

3.3. TGFβ1 Induces Tyr705 Phosphorylation of STAT3 in C2C12 Myoblasts

In order to determine whether TGFβ1 can directly activate STAT3 in muscle cells, we treated the murine myogenic cell line, C2C12, with recombinant TGFβ1 protein. The pSTAT3 (Tyr705) level was determined by immunoblotting. The results showed that TGFβ1 significantly increased pSTAT3 (Tyr705) 30 minutes after the treatment (7.9-fold, ). The pSTAT3 (Tyr705) level descended to baseline level after 2 hours of treatment. There was no change of the total STAT3 protein during the time course examined between the treated and control groups (Figure 3).

4. Discussion

In this study, we explored the relationship between TGFβ1 and STAT3 activation using a tet-repressible muscle-specific TGFβ1 transgenic mouse and C2C12 cells. The phosphorylation of the Tyr705 residue is required for STAT3 dimerization, nuclear translocation, and DNA binding [28, 29]. Phosphorylation of the Ser727 residue is believed to promote STAT3 transcriptional activity through the enhanced recruitment of transcriptional cofactors, which is not required for functional activation of STAT3. Our data showed that overexpression of TGFβ1 increased the amount of pSTAT3 (Tyr705) significantly in the EO mice but not in the LO mice. In addition, the effect was mediated through the phosphorylation of Tyr705 but not Ser727. While TGFβ1 mediated activation of STAT3 in skeletal muscles was not reported previously, TGFβ1 activated STAT3 by phosphorylating Tyr705 has been reported in hepatic cells and a mouse model of hepatocellular carcinoma [27, 30]. Both of these studies reported a direct activation of STAT3 by TGFβ1. Interestingly, a recent study showed that hepatitis C virus (HCV) activates TGFβ1 expression via STAT3 in hepatic stellate cells [31]. These findings suggested a potential postitive feedback loop between TGFβ1 and STAT3 in the hepatic cells. In our TGFβ1 transgenic model, we previously reported that expression of endogenous TGFβ1 was induced in mice with more severe phenotypes, suggesting potential involvement of a positive feedback loop [5]. Whether the STAT3 activation directly modulates genes involved in muscle atrophy and fibrosis as reported in previous studies or it induces endogenous TGFβ1 expression which is responsible for more severe phenotypes needs to be further examined.

STAT3 was originally reported for its capacity to mediate signaling predominantly from cytokines such as IL-6, IL-11, leukemia inhibitory factor (LIF), and oncostatin M. It is expressed in a large number of tissues and its activation drives the transcription of genes encoding proteins involved in angiogenesis, inflammation, apoptosis, extracellular matrix deposition, and cellular signaling [32]. IL-6 is well known for its crucial role in maintenance of skeletal muscle metabolism [33–35]. IL-6-induced STAT3 has been shown to promote satellite cells proliferation and myoblasts differentiation. Acute and transient activation of STAT3 via Tyr705 phosphorylation by IL-6 was reported to be associated with muscle hypertrophy after 10 weeks of resistance training in rats [36]. The hypertrophic effect was associated with the early upregulation of the IL-6/STAT3 signaling pathway and the downregulation of myogenic regulatory factors, including Pax7, MyoD, Myf5, and myogenin, in the satellite cells. While well controlled IL-6 expression plays a critical role in maintaining the homeostasis of skeletal muscles, studies also showed that persistent Tyr705 phosphorylation is associated with impairment of metabolism by negatively affecting skeletal muscle insulin signaling and glucose uptake [37] and is believed to be responsible for the IL-6-induced cancer cachexia [33, 38]. Our study showed that overexpression of TGFβ1 for 2 weeks induced pSTAT3 (Tyr705) in skeletal muscles of the mice with severe phenotypes. Approximately half of the nuclei were positive for pSTAT3 (Tyr705). Since TGFβ1 was the only gene overexpressed in the mouse model and is the driving force of the disease phenotype [5], the data suggested that TGFβ1 is able to activate the STAT3 signaling directly. However, whether IL-6 signaling is involved in the process is not clear and needs further investigation. To examine the possibility and demonstrate that TGFβ1 directly activates STAT3 in skeletal muscle cells, we treated the C2C12 cells with recombinant TGFβ1 and examined the activation of STAT3 at 3 time points (30 min, 2 hrs, and 24 hrs) within 24 hours. Our findings showed that the pSTAT3 Tyr705 was transiently activated within 30 minutes. This result is in agreement with a recent study using immortalized rat hepatic stellate cells (HST) [27]. In this study, it was also shown that JAK1 is necessary for the Tyr705 phosphorylation and activation of STAT3. Knockdown of JAK1 but not JAK2 or Tyk2 is sufficient to attenuate TGFβ1 mediated STAT3 activation. STAT3 is canonically activated by JAKs (JAK1, JAK2, JAK3, and Tyk2), which in turn are activated by a large number of cytokine and growth factors, including IL-10, IL-6, and EGF, and it is well known to play a crucial role in myogenic proliferation and differentiation [39, 40]. Whether the activation of STAT3 is mediated through JAK1 in our models needs to be investigated further.

5. Conclusion

Our study demonstrated that pSTAT3 (Tyr705) activation is associated with severity of phenotypes of our mouse model overexpressing TGFβ1 in skeletal muscles. The activated STAT3 was localized in the nuclei of myofibers, suggesting transcription activation. Both in vivo and in vitro data suggested that pSTAT3 (Tyr705) can be induced by TGFβ1. These data thus point to a novel signaling pathway that may modulate and contribute to the molecular and cellular mechanism of skeletal muscle fibrosis and atrophy in various diseases.

Disclaimer

The content is solely the responsibility of the authors and does not necessarily represent the official views of the National Institutes of Health.

Conflict of Interests

The authors confirm that there is no conflict of interests.

Acknowledgments

Research reported in this paper was supported by the Department of Defense under Award no. W81XWH-10-1-0659 and the NIH/NICHD under Award no. 1R24HD050846. Yi-Wen. Chen was partially supported by NIH/NIAMS under Award no. 1R01AR052027. Carsten G. Bönnemann is supported by intramural funds of NIH/NINDS.

References

R. A. Rahimi and E. B. Leof, “TGF-β signaling: a tale of two responses,” Journal of Cellular Biochemistry, vol. 102, no. 3, pp. 593–608, 2007.
View at: Publisher Site | Google Scholar
L. M. Wakefield and C. S. Hill, “Beyond TGFβ: roles of other TGFβ superfamily members in cancer,” Nature Reviews Cancer, vol. 13, no. 5, pp. 328–341, 2013.
View at: Publisher Site | Google Scholar
F. Cencetti, C. Bernacchioni, F. Tonelli, E. Roberts, C. Donati, and P. Bruni, “TGFβ1 evokes myoblast apoptotic response via a novel signaling pathway involving S1P4 transactivation upstream of Rho-kinase-2 activation,” The FASEB Journal, vol. 27, no. 11, pp. 4532–4546, 2013.
View at: Publisher Site | Google Scholar
C. Meneses, M. G. Morales, J. Abrigo, F. Simon, E. Brandan, and C. Cabello-Verrugio, “The angiotensin-(1–7)/Mas axis reduces myonuclear apoptosis during recovery from angiotensin II-induced skeletal muscle atrophy in mice,” Pflügers Archiv—European Journal of Physiology, 2014.
View at: Publisher Site | Google Scholar
J. Narola, S. N. Pandey, A. Glick, and Y.-W. Chen, “Conditional expression of TGF-β1 in skeletal muscles causes endomysial fibrosis and myofibers atrophy,” PLoS ONE, vol. 8, no. 11, Article ID e79356, 2013.
View at: Publisher Site | Google Scholar
A. Bassols and J. Massague, “Transforming growth factor β regulates the expression and structure of extracellular matrix chondroitin/dermatan sulfate proteoglycans,” The Journal of Biological Chemistry, vol. 263, no. 6, pp. 3039–3045, 1988.
View at: Google Scholar
Y. Dong, R. Lakhia, S. S. Thomas, X. H. Wang, K. A. S. Silva, and L. Zhang, “Interactions between p-Akt and Smad3 in injured muscles initiate myogenesis or fibrogenesis,” The American Journal of Physiology—Endocrinology and Metabolism, vol. 305, no. 3, pp. E367–E375, 2013.
View at: Publisher Site | Google Scholar
W. M. Jackson, A. B. Aragon, J. Onodera et al., “Cytokine expression in muscle following traumatic injury,” Journal of Orthopaedic Research, vol. 29, no. 10, pp. 1613–1620, 2011.
View at: Publisher Site | Google Scholar
Y. Ohsawa, T. Okada, S.-I. Nishimatsu et al., “An inhibitor of transforming growth factor beta type I receptor ameliorates muscle atrophy in a mouse model of caveolin 3-deficient muscular dystrophy,” Laboratory Investigation, vol. 92, no. 8, pp. 1100–1114, 2012.
View at: Publisher Site | Google Scholar
P. Bernasconi, E. Torchiana, P. Confalonieri et al., “Expression of transforming growth factor-β1 in dystrophic patient muscles correlates with fibrosis. Pathogenetic role of a fibrogenic cytokine,” The Journal of Clinical Investigation, vol. 96, no. 2, pp. 1137–1144, 1995.
View at: Publisher Site | Google Scholar
T. N. Burks and R. D. Cohn, “Role of TGF-β signaling in inherited and acquired myopathies,” Skeletal Muscle, vol. 1, no. 1, article 19, 2011.
View at: Publisher Site | Google Scholar
M. Yamazaki, S. Minota, H. Sakurai et al., “Expression of transforming growth factor-β1 and its relation to endomysial fibrosis in progressive muscular dystrophy,” The American Journal of Pathology, vol. 144, no. 2, pp. 221–226, 1994.
View at: Google Scholar
Y. Li, W. Foster, B. M. Deasy et al., “Transforming growth factor-β1 induces the differentiation of myogenic cells into fibrotic cells in injured skeletal muscle: a key event in muscle fibrogenesis,” The American Journal of Pathology, vol. 164, no. 3, pp. 1007–1019, 2004.
View at: Publisher Site | Google Scholar
C. L. Mendias, J. P. Gumucio, M. E. Davis, C. W. Bromley, C. S. Davis, and S. V. Brooks, “Transforming growth factor-beta induces skeletal muscle atrophy and fibrosis through the induction of atrogin-1 and scleraxis,” Muscle and Nerve, vol. 45, no. 1, pp. 55–59, 2012.
View at: Publisher Site | Google Scholar
E. Ceco and E. M. McNally, “Modifying muscular dystrophy through transforming growth factor-β,” The FEBS Journal, vol. 280, no. 17, pp. 4198–4209, 2013.
View at: Publisher Site | Google Scholar
C. M. Horvath, Z. Wen, and J. E. Darnell Jr., “A STAT protein domain that determines DNA sequence recognition suggests a novel DNA-binding domain,” Genes & Development, vol. 9, no. 8, pp. 984–994, 1995.
View at: Publisher Site | Google Scholar
Z. Zhong, Z. Wen, and J. E. Darnell Jr., “Stat3: a STAT family member activated by tyrosine phosphorylation in response to epidermal growth factor and interleukin-6,” Science, vol. 264, no. 5155, pp. 95–98, 1994.
View at: Publisher Site | Google Scholar
R. Fujita, F. Kawano, T. Ohira et al., “Anti-interleukin-6 receptor antibody (MR16-1) promotes muscle regeneration via modulation of gene expressions in infiltrated macrophages,” Biochimica et Biophysica Acta—General Subjects, vol. 1840, no. 10, pp. 3170–3180, 2014.
View at: Publisher Site | Google Scholar
D. Hu, L. Wan, M. Chen et al., “Essential role of IL-10/STAT3 in chronic stress-induced immune suppression,” Brain, Behavior, and Immunity, vol. 36, pp. 118–127, 2014.
View at: Publisher Site | Google Scholar
J. Turkson, “STAT proteins as novel targets for cancer drug discovery,” Expert Opinion on Therapeutic Targets, vol. 8, no. 5, pp. 409–422, 2004.
View at: Publisher Site | Google Scholar
D. E. Levy and J. E. Darnell Jr., “STATs: transcriptional control and biological impact,” Nature Reviews Molecular Cell Biology, vol. 3, no. 9, pp. 651–662, 2002.
View at: Publisher Site | Google Scholar
K. Shuai, “Modulation of STAT signaling by STAT-interacting proteins,” Oncogene, vol. 19, no. 21, pp. 2638–2644, 2000.
View at: Publisher Site | Google Scholar
T. Tanaka, M. A. Soriano, and M. J. Grusby, “SLIM is a nuclear ubiquitin E3 ligase that negatively regulates STAT signaling,” Immunity, vol. 22, no. 6, pp. 729–736, 2005.
View at: Publisher Site | Google Scholar
S. Saito, H. Shimizu, M. Yisireyili, F. Nishijima, A. Enomoto, and T. Niwa, “Indoxyl sulfate-induced activation of (pro)renin receptor is involved in expression of TGF-β1 and α-smooth muscle actin in proximal tubular cells,” Endocrinology, vol. 155, no. 5, pp. 1899–1907, 2014.
View at: Publisher Site | Google Scholar
S. Sumitomo, K. Fujio, T. Okamura et al., “Transcription factor early growth response 3 is associated with the TGF-β1 expression and the regulatory activity of CD4-positive T cells in vivo,” Journal of Immunology, vol. 191, no. 5, pp. 2351–2359, 2013.
View at: Publisher Site | Google Scholar
J. H. Yu, K. H. Kim, and H. Kim, “SOCS 3 and PPAR-γ ligands inhibit the expression of IL-6 and TGF-β1 by regulating JAK2/STAT3 signaling in pancreas,” The International Journal of Biochemistry and Cell Biology, vol. 40, no. 4, pp. 677–688, 2008.
View at: Publisher Site | Google Scholar
Y. Liu, H. Liu, C. Meyer et al., “Transforming growth factor-β (TGF-β)-mediated connective tissue growth factor (CTGF) expression in hepatic stellate cells requires Stat3 signaling activation,” The Journal of Biological Chemistry, vol. 288, no. 42, pp. 30708–30719, 2013.
View at: Publisher Site | Google Scholar
P. A. Johnston and J. R. Grandis, “STAT3 signaling: anticancer strategies and challenges,” Molecular Interventions, vol. 11, no. 1, pp. 18–26, 2011.
View at: Publisher Site | Google Scholar
D. E. Levy and C.-K. Lee, “What does Stat3 do?” The Journal of Clinical Investigation, vol. 109, no. 9, pp. 1143–1148, 2002.
View at: Publisher Site | Google Scholar
T. V. Bagnyukova, V. P. Tryndyak, L. Muskhelishvili, S. A. Ross, F. A. Beland, and I. P. Pogribny, “Epigenetic downregulation of the suppressor of cytokine signaling 1 (Socs1) gene is associated with the STAT3 activation and development of hepatocellular carcinoma induced by methyl-deficiency in rats,” Cell Cycle, vol. 7, no. 20, pp. 3202–3210, 2008.
View at: Publisher Site | Google Scholar
L. D. Presser, S. McRae, and G. Waris, “Activation of TGF-β1 promoter by hepatitis C virus-induced AP-1 and Sp1: role of of TGF-β1 in hepatic stellate cell activation and invasion,” PLoS ONE, vol. 8, no. 2, Article ID e56367, 2013.
View at: Publisher Site | Google Scholar
M. Snyder, X.-Y. Huang, and J. Jillian Zhang, “Identification of novel direct stat3 target genes for control of growth and differentiation,” The Journal of Biological Chemistry, vol. 283, no. 7, pp. 3791–3798, 2008.
View at: Publisher Site | Google Scholar
A. Bonetto, T. Aydogdu, X. Jin et al., “JAK/STAT3 pathway inhibition blocks skeletal muscle wasting downstream of IL-6 and in experimental cancer cachexia,” The American Journal of Physiology—Endocrinology and Metabolism, vol. 303, no. 3, pp. E410–E421, 2012.
View at: Publisher Site | Google Scholar
B. R. McKay, D. I. Ogborn, J. M. Baker, K. G. Toth, M. A. Tarnopolsky, and G. Parise, “Elevated SOCS3 and altered IL-6 signaling is associated with age-related human muscle stem cell dysfunction,” The American Journal of Physiology—Cell Physiology, vol. 304, no. 8, pp. C717–C728, 2013.
View at: Publisher Site | Google Scholar
K. G. Toth, B. R. McKay, M. de Lisio, J. P. Little, M. A. Tarnopolsky, and G. Parise, “IL-6 induced STAT3 signalling is associated with the proliferation of human muscle satellite cells following acute muscle damage,” PLoS ONE, vol. 6, no. 3, Article ID e17392, 2011.
View at: Publisher Site | Google Scholar
G. Begue, A. Douillard, O. Galbes et al., “Early activation of rat skeletal muscle IL-6/STAT1/STAT3 dependent gene expression in resistance exercise linked to hypertrophy,” PLoS ONE, vol. 8, no. 2, Article ID e57141, 2013.
View at: Publisher Site | Google Scholar
F. Mashili, A. V. Chibalin, A. Krook, and J. R. Zierath, “Constitutive STAT3 phosphorylation contributes to skeletal muscle insulin resistance in type 2 diabetes,” Diabetes, vol. 62, no. 2, pp. 457–465, 2013.
View at: Publisher Site | Google Scholar
M. Gilabert, E. Calvo, A. Airoldi et al., “Pancreatic cancer-induced cachexia is Jak2-dependent in mice,” Journal of Cellular Physiology, vol. 229, no. 10, pp. 1437–1443, 2014.
View at: Publisher Site | Google Scholar
Y. N. Jang and E. J. Baik, “JAK-STAT pathway and myogenic differentiation,” JAK-STAT, vol. 2, no. 2, Article ID e23282, 2014.
View at: Publisher Site | Google Scholar
A. Mohr, N. Chatain, T. Domoszlai et al., “Dynamics and non-canonical aspects of JAK/STAT signalling,” European Journal of Cell Biology, vol. 91, no. 6-7, pp. 524–532, 2012.
View at: Publisher Site | Google Scholar

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Copyright © 2015 Eleonora Guadagnin 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.

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