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BioMed Research International
Volume 2014 (2014), Article ID 235426, 14 pages
Local Overexpression of V1a-Vasopressin Receptor Enhances Regeneration in Tumor Necrosis Factor-Induced Muscle Atrophy
1DAHFMO Unit of Histology and Medical Embryology, Interuniversity Institute of Myology, Sapienza University of Rome, Via A. Scarpa 16, 00161 Rome, Italy
2Institute of Histology and Embryology, Catholic University School of Medicine, L.go F. Vito, 1, 00168 Rome, Italy
Received 27 January 2014; Revised 22 April 2014; Accepted 23 April 2014; Published 20 May 2014
Academic Editor: Marina Bouché
Copyright © 2014 Alessandra Costa 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.
Skeletal muscle atrophy occurs during disuse and aging, or as a consequence of chronic diseases such as cancer and diabetes. It is characterized by progressive loss of muscle tissue due to hypotrophic changes, degeneration, and an inability of the regeneration machinery to replace damaged myofibers. Tumor necrosis factor (TNF) is a proinflammatory cytokine known to mediate muscle atrophy in many chronic diseases and to inhibit skeletal muscle regeneration. In this study, we investigated the role of Arg-vasopressin-(AVP-)dependent pathways in muscles in which atrophy was induced by local overexpression of TNF. AVP is a potent myogenesis-promoting factor and is able to enhance skeletal muscle regeneration by stimulating Ca2+/calmodulin-dependent kinase and calcineurin signaling. We performed morphological and molecular analyses and demonstrated that local over-expression of the AVP receptor V1a enhances regeneration of atrophic muscle. By upregulating the regeneration/differentiation markers, modulating the inflammatory response, and attenuating fibrogenesis, the stimulation of AVP-dependent pathways creates a favourable environment for efficient and sustained muscle regeneration and repair even in the presence of elevated levels of TNF. This study highlights a novel in vivo role for AVP-dependent pathways, which may represent an interesting strategy to counteract muscle decline in aging or in muscular pathologies.
Skeletal muscle is a dynamic tissue capable of extensive regeneration in response to injury. Nevertheless, regeneration may be hindered in the case of aging, extended injury, or pathological conditions, leading to functional impairment. Although the general mechanisms underlying muscle regeneration have been identified, little is known about the factors limiting efficient repair in pathological muscle. Reduction in the number of satellite cells, poor recruitment of circulating stem cells within the damaged area, chronic inflammation, and formation of fibrotic tissue represent important factors contributing to limited or impaired regeneration. Inflammation is an important phase in the muscle regeneration process [1, 2]. Cytokines expressed during the early phase of inflammatory responses, such as interferon-γ (IFN-γ), interleukin-1 (IL-1), and TNF, drive the differentiation and activation of macrophages towards the M1 phenotype. These classically activated M1 macrophages represent a proinflammatory population of cells capable of amplifying and perpetuating the inflammatory response . After M1 macrophages reach their peak concentration, they are replaced by a population of alternatively activated M2 macrophages, which are activated by anti-inflammatory cytokines such as interleukin-4 (IL-4), interleukin-10 (IL-10), express CD-163 [1, 3, 4], and attenuate the inflammatory response and promote tissue repair. Perturbations in the spatial distribution of inflammatory cells, changes in the type and magnitude of the inflammatory cell infiltrate, and disrupted temporal sequence, result in a persistent rather than resolved inflammatory phase  and functional impairment of skeletal muscle .
The nuclear-factor-kappa B (NF-κB) transcription factor is one of the most important molecules, which has been linked to the loss of skeletal muscle mass in various physiopathological conditions. Activation of NF-κB in skeletal muscle leads to degradation of muscle specific proteins, inflammation, and fibrosis and blocks myofiber regeneration after injury/atrophy [7, 8]. Interestingly, NF-κB regulates the expression of a number of inflammatory molecules including proinflammatory cytokines such as TNF, which is also a potent activator of NF-κB, thus establishing a positive feedback loop leading to muscular abnormalities . Although the autoactivation of NF-κB requires proteolytic processing of NF-κB and IκB family of proteins by the ubiquitin-proteasome system [9, 10], NF-κB can induce the expression of FoxO transcription factors by modulating the Akt signaling pathways . Nuclear translocation and activation of FoxO transcription factors results in the upregulation of atrogin-1/MAFbx and MuRF1, thus promoting atrophy and muscle loss [12–14].
In this study, we examined the effects of local V1a-vasopressin receptor overexpression on TNF-induced muscle atrophy. The neurohypophyseal nonapeptide Arg8-vasopressin (AVP), oxytocin (OT), and related peptides constitute a family of positive regulators of terminal differentiation in myogenic cell lines (L5 and L6) and primary satellite cells [15–17]. V1aR is the only vasopressin receptor expressed in skeletal muscle [18–20]. Previously, we demonstrated that V1aR expression is modulated during skeletal muscle regeneration, and that AVP-V1aR signaling is a powerful enhancer of muscle regeneration through mechanisms involving calcineurin A (CnA), GATA2, MEF2, and IL-4 . There is now extensive evidence showing that the AVP system is impaired in several neuromuscular diseases, such as amyotrophic lateral sclerosis and multiple sclerosis [22, 23], suggesting that AVP may act as a physiologic factor in skeletal muscle homeostasis.
Here we demonstrate that local V1aR overexpression enhances regeneration in TNF-induced muscle atrophy. By modulating the inflammatory response, attenuating fibrogenesis, and upregulating the regeneration/differentiation markers, the stimulation of AVP-dependent pathways creates a favourable environment for sustained and efficient muscle regeneration and repair even in the presence of elevated levels of TNF. In addition, we demonstrate that the positive effect of V1aR overexpression in muscle homeostasis involves Akt-mediated inhibition of FoxO transcription factors.
The findings of this research are expected to lead to the identification of new pharmacological or gene therapy targets that may delay the progression of muscular wasting associated with numerous myopathies.
2. Materials and Methods
C57 transgenic desmin/nls-lacZ mice used in this study bear a transgene in which the 1-κB DNA 5′ regulatory sequence of the desmin gene is linked to a reporter gene coding for Escherichia coli--galactosidase . The desmin/nls-lacZ transgene labels muscle cells in which the desmin synthesis program has commenced . Mice were treated according to the guidelines of the Institutional Animal Care and Use Committee. They were housed in a temperature-controlled (°C) and humidity-controlled (%) room regulated to provide a 12 h light, 12 h dark cycle. Mice were allowed to feed and drink ad libitum. Animals were anesthetized with an intraperitoneal injection of Avertin A (a mix of tribromoethanol and 2-methyl-2-butanol diluted in physiological solution) before gene delivery by electroporation or muscle damage. Injury of mock-, V1aR-, TNF-, and V1aR+TNF-transfected Tibialis anterior (TA) muscles of 2-month-old mice was induced along the entire length of the muscle with a total of four cardiotoxin (CTX) injections (5 μL of 10 μM CTX per injection). In our previous study, regeneration was fully active at 7 days after injury .
Therefore, mice were sacrificed 7 days after injury and the regeneration process in the injured muscle was examined by assessing the number and size of regenerating fibers as previously described .
2.2. Plasmid Construction
The MLC-Myc-V1aR plasmid was derived from MLC-Myc and PCD3-V1aR (kindly provided by Prof. S.J. Lolait, University of Bristol, UK) expression vectors, as previously described by Toschi et al. . To induce expression of the secreted form of murine TNF-α, we used the construct pBabe-mTNF-α (kindly provided by Dr. Gokhan Hotamisligil, Harvard University, Boston, MA) under control of the SV40 promoter. The SV40 promoter has been shown to be efficient for driving exogenous cDNA expression in skeletal muscle .
2.3. Gene Delivery by Electroporation
The TA in each mouse hind limb was injected with the indicated amount of cDNA: 20 μg of MLC-Myc-V1aR (V1aR), or pcDNA3 (mock) , or pBabe-mTNF-α (TNF)m or 10 μg of MLC-Myc-V1aR plus 10 μg of pBabe-mTNF-α (V1aR+TNF), in combination with 5 μg of pCMV-SNAP-GFP (kindly provided by Dr. Pozzan, University of Padua, Italy), as a marker of transfection efficiency. The electric pulses were delivered using 3 × 5 mm gene paddles electrodes (BTX, San Diego, CA) placed on either side of the muscle, as described by Donà et al. . This protocol of gene delivery by electroporation guarantees stable DNA expression for more than four months. After electroporation, mice rapidly recovered and did not show any locomotor impairment or particular sign of pain or stress.
2.4. Histological and Histochemical Analysis
TA muscles from mock-, V1aR-, TNF or TNF+V1aR-transfected 7-8-week-old desmin/nls-lacZ mice were embedded in Jung tissue freezing medium (Leica, Wetzlar, Germany) and frozen in liquid nitrogen-cooled isopentane. Frozen sections (7 μm) were obtained using a Leica cryostat. Sections were observed under the green activation filter of the Axioskop 2 plus system (Zeiss). For histological analysis, sections were stained with hematoxylin and eosin (H&E) using standard methods .
Esterase staining was adapted from Davis  as previously reported . Cryosections of each muscle were incubated for 5 min in a staining solution containing 3 mg alpha-naphthyl acetate, 0.375 mL acetone, 6.25 mL 0.2 M sodium phosphate, and 0.4 mL of a solution containing equal volumes of 2% pararosaniline (Sigma-Aldrich) and 2% sodium nitrite. Photomicrographs were obtained using an Axioscop2 plus system equipped with an AxiocamHRc (Zeiss, Oberkochen, Germany) at 1300 × 1030 pixel resolution and analyzed using 10x NA 0.30 air objective lens or 20x NA 0.50 air objective lens.
The trichrome stain (Masson) kit (Sigma-Aldrich Procedure number HT15) was used for distinguishing collagen from muscle tissue. Tissue sections were treated with Bouin’s solution to intensify the final coloration. Nuclei were stained with Weigert’s iron hematoxylin, and the cytoplasm and muscle were stained with Biebrich scarlet-acid fuchsin. After treatment with phosphotungstic and phosphomolybdic acid, collagen was demonstrated by staining with aniline blue.
2.5. Immunofluorescence Analysis
Frozen sections were fixed in 4% paraformaldehyde for 10 min on ice, washed with PBS, incubated in PBS containing 1% BSA (Sigma-Aldrich) and 1 : 100 goat serum for 30 min at room temperature, and then incubated overnight at 4°C with the selected primary antibody at the appropriate dilution. The following antibody was used: mouse monoclonal antiembryonic MHC (Developmental Hybridoma-Bank number BF-G6, University of Iowa, Iowa City, IA). Samples were then washed with PBS containing 1% BSA and incubated for 1 h at room temperature with the appropriate secondary antibody, Alexafluor 568-conjugated anti-mouse (Molecular Probes, Eugene, OR, USA) 1 : 500 in 1% BSA. Nuclei were visualized with Hoechst 33342 (Sigma-Aldrich). The sections were mounted with Vectashield mounting medium (Vector Laboratories, Burlingame, CA) and examined in a Zeiss Axioplan (Zeiss, Thornwood, NY) fluorescence microscopy using a 10x and 20x objective lens.
2.6. Morphometric Analysis
Photomicrographs of regenerating muscle fibers (identified by morphological criteria, i.e., centrally located nuclei in H&E stained sections) were taken at standard resolution (1.300 × 1030 pixel) and analyzed using ImageJ, Scion Image software. For morphometric evaluation of fiber size, 200–1000 cross-sectioned fibers per sample were analyzed. Quantitative data were obtained from three independent experiments in triplicate. The values are expressed as mean ± SD.
2.7. Gene Expression Analysis
TA muscles were dissected, and total RNA extraction was performed with tissue lyser (QIAGEN) in TriRagent (Invitrogen, Carlsbad, CA), according to the manufacturer’s protocol, and was reverse-transcribed using Moloney Murine Leukemia Virus Reverse Transcriptase (M-MLV RT; Invitrogen, Carlsbad, CA). cDNA preamplification was performed with TaqMan PreAmp Master Mix Kit (Applied Biosystems) according to the manufacturer’s instructions [31–33] to accurately detect the expression pattern of the following cytokines: IL4, IL10, IL6, IL1, and the chemokine ligand CCL2 and scavenger receptor CD163. Quantitative PCR was performed on an ABI PRISM 7500 SDS (Applied Biosystems, USA), using premade 6-carboxyfluorescein (FAM)-labeled TaqMan assay for: TNF (Mm00443258_m1), V1aR (Mm00444092_m1), CCL2 (Mm00441242-m1), IL1- (Mm01336189_m1), IL6 (Mm0120733_m1), CD163 (Mm004744096_m1), IL10 (Mm00439616_m1), IL-4 (Mm00445260_m1) Pax7 (Mm00834082_m1), desmin (Mm00802455_m1), myogenin (Mm00446194_m1), atrogin-1 (Mm01207878_m1), and HPRT (Mm00446968_m1) as internal controls. Real-time PCR was performed using RNA preparations from three different animals for each group.
2.8. Immunoblotting Analysis
TA muscles were dissected, minced, and homogenized with RIPA buffer (20 mMTris/HCl pH 7.5, 2 mM EDTA, 2 mM EGTA, 0.25 M Sucrose, 5 mM DTT, 0,1% Triton X-100, 10 mM NaF, 200 μM sodium orthovanadate) containing a protease inhibitor cocktail (Roche, Indianapolis, IN). Equal amounts of protein (20–30 μg), determined by Pierce BCA Protein Assay Reagents, were separated by SDS PAGE and transferred electrophoretically to a hybond-C extra nitrocellulose membrane (Amersham Biosciences, Piscataway, NJ). Nonspecific binding was blocked in Tris-buffered saline with Tween 20 (TBST) containing 5% nonfat milk for 1 h at room temperature, and the membrane was then incubated overnight at 4°C in TBST containing primary antibodies. The following antibodies were used: mouse monoclonal anti-MHC (Developmental Hybridoma-Bank), monoclonal anti-NFκB-p65 (C22B4), and monoclonal anti-phosphoNFκB-p65 (Ser563) (93H1) (Cell Signaling), rabbit polyclonal anti-IκBα (Santa Cruz Biotechnologies), polyclonal anti-phospho-Akt (Ser473), monoclonal anti-FoxO3a (75D8), and polyclonal anti-phospho-FoxO3a (Ser253) (Cell signaling). Monoclonal anti-tubulin-α (Sigma-Aldrich) or mouse monoclonal anti-GAPDH (Santa Cruz Biotechnologies) was used for normalization, as indicated. Blots were washed in TBST and then incubated with the appropriate secondary antibodies, goat anti-mouse, or anti-rabbit HRP-conjugated (Bio-Rad Laboratories, Hercules, CA) in TBST containing 1% nonfat milk. Blots were extensively washed and the antibody binding was detected by means of Super Signal West Pico Chemiluminescent Substrate (Pierce, Rockford, IL).
2.9. Statistical Analysis
The Student’s -test was used throughout this paper for statistical analyses.
3.1. Local V1aR Overexpression Counteracts the Negative Effects of TNF on Muscle Regeneration
Our previous data demonstrated that muscle specific overexpression of the AVP receptor V1a enhances skeletal muscle regeneration after CTX induced damage, by stimulating satellite cell activation and increasing the expression of differentiation markers . We also demonstrated that TNF administration is sufficient to induce inhibition of muscle regeneration by activating a nonapoptotic, caspase-dependent process, ultimately leading to muscle wasting . Therefore, in this study we investigated whether local overexpression of V1aR protects the muscle from the effects of high TNF levels. To this end, we overexpressed the myosin-light-chain (MLC)-myc-V1a AVP receptor construct  alone or in combination with the TNF construct [21, 35] in TA muscles, by means of gene delivery by electroporation. Controls consisted of mock-transfected samples (i.e., muscles transfected with pcDNA3) and, when indicated, in nonelectroporated muscles (WT). In order to assess the efficacy of the transfections, we used real-time PCR analysis, to verify the V1aR and TNF expression levels in muscle extracts one week after electroporation (Figures 1(a) and 1(b)). V1aR expression was strongly upregulated in TA muscles electroporated with the V1aR construct, both in the presence and in the absence of TNF, demonstrating that TNF did not interfere with the electroporation efficiency or with the forced expression of V1aR (Figure 1(a)). As expected, TNF expression was high in samples electroporated with the TNF construct alone or in combination with V1aR (Figure 1(b)). The expression of V1aR and TNF did not differ significantly between the V1aR and V1aR+TNF samples (Figures 1(a) and 1(b)).
Morphological analysis showed that 1 week after electroporation, local overexpression of TNF (Figure 2(a), panel (B)) caused an accumulation of mononucleated infiltrating cells, compared with mock-transfected and V1aR overexpressing muscle alone (Figure 2(a), panels (A) and (C) resp.). In addition, a regeneration response occurred in the muscle rendered atrophic by TNF overexpression, as demonstrated by the presence of central nucleated fibers in TNF overexpressing muscle (Figure 2(b)). By contrast, cotransfection of V1aR and TNF did not significantly modify the number of regenerating fibers compared with TNF transfection alone. It did, however, affect the fiber size distribution by favoring the accumulation of larger fibers, as shown in Figure 2(c). It is noteworthy that the overexpression of V1aR induced a slight, yet significant increase in the fiber cross-sectional area compared with mock-transfected muscle (15% increase, ) (data not shown). In conclusion, V1aR overexpression leads to more efficient regeneration than that observed in muscles overexpressing TNF alone.
3.2. Muscle V1aR Overexpression Modulates the Inflammatory Response and Attenuates the Fibrosis Induced by High Levels of TNF
TNF is a proinflammatory cytokine capable of activating macrophages, thereby inducing the production of other proinflammatory cytokines and perpetuating the inflammatory response. To verify whether the enhanced regenerative response in V1aR overexpressing muscle is associated with a modulation of inflammation, we examined the presence of macrophages by esterase staining. Figure 3(a) shows a high number of esterase-positive, macrophages in TNF over-xpressing muscles, whereas the concomitant overexpression of V1aR significantly attenuated their number.
Efficient muscle repair is accompanied by and/or requires the migration and proliferation of fibroblasts needed to produce additional extracellular matrix (ECM) components acting as a scaffold for regenerating myofibers [3, 36, 37] and substituting the basement membrane and ECM components degraded during the inflammatory phases [38–40]. However, if inflammatory cell infiltration and fibroblast activation persist, an aberrant tissue repair response will produce a nonfunctional mass of fibrotic tissue . In order to visualize the extent of fibrosis, we performed Masson’s trichrome staining under the indicated experimental conditions. Figure 3(b) shows the normal presence of connective tissue in mock muscle and in muscle overexpressing V1aR, while muscles expressing TNF display increased amounts of ECM in skeletal muscle tissue. In the presence of high TNF and V1aR levels, the extent of fibrosis was significantly attenuated in comparison with muscle overexpressing TNF alone. Taken together, these data demonstrate that V1aR overexpression leads to a more efficient regeneration process, characterized by attenuated inflammatory response and reduced fibrosis.
3.3. V1aR Overexpression Modulates the Molecular Mechanisms Involved in the Inflammatory Response
It has been demonstrated that NF-κB is one of the central players of the inflammatory system [2, 42] and that TNF, along with other proinflammatory cytokines, stimulates the NF-κB signaling pathway, promoting muscle catabolism [5, 7]. Western blot and densitometric analysis (Figures 4(a), 4(b), and 4(c)) revealed that TNF overexpression promotes a strong upregulation of phospho-NF-κB expression and a concomitant downregulation of the NF-κB inhibitory factor, namely, IκBα. By contrast, phospho-NF-κB expression was significantly reduced in muscle overexpressing both TNF and V1aR, demonstrating that V1aR overexpression attenuates the effects of TNF on inflammation.
3.4. Inflammatory Cytokine Production Is Modulated in V1aR Overexpressing Muscle
To gain further insight into the mechanism by which V1aR modulates the resolution of inflammation and contributes to muscle repair, we performed real-time PCR, to analyse the expression patterns of specific cytokines and chemokines secreted by M1 macrophages, a proinflammatory cell population capable of perpetuating the inflammatory response . Figure 5(a) demonstrates that the expression of CCL2, IL1 and IL6 was strongly upregulated in the presence of high levels of TNF compared with mock- and V1aR-transfected muscles. TNF overexpression was also accompanied by a slight increase in CD163 expression. By contrast, the overexpression of V1aR, in TNF expressed muscle, significantly reduced the expression of the proinflammatory cytokines. Interestingly, the reduction in M1 macrophages, promoted by V1aR overexpression, was associated with an upregulation of M2 macrophage markers such as CD163, IL-10, and IL-4 (Figure 5(b)). Notably, CD163 is a macrophage-specific receptor for complexes of hemoglobin and haptoglobin, and ligation of CD163 can contribute to the regulation of macrophage phenotype by increasing the expression of anti-inflammatory cytokines, especially IL-10 . IL-4 is involved in muscle regeneration by promoting satellite cell fusion and differentiation [44–46], and we have previously demonstrated that stimulation of AVP signaling induces calcineurin-dependent expression of IL-4 in muscle cells. These results demonstrate that a high level of V1aR accelerates the resolution of TNF-dependent inflammation, modulating the muscle milieu by favoring the shift from M1 to M2 macrophage phenotype, thereby stimulating the secretion of anti-inflammatory cytokines and thus promoting regeneration.
3.5. Stimulation of AVP Signaling Modifies the Effects of TNF on Myogenesis and Promotes Muscle Maturation
Regeneration consists of a sequence of phenomena including the activation of satellite cells, and their differentiation and fusion into fibers expressing muscle specific products. Therefore, we first analyzed the expression of Pax7 and desmin, which are relevant markers of activated and proliferating satellite cells, 1 week after TNF and/or V1aR electroporation in muscles. Real-time PCR analysis demonstrated that TNF overexpression greatly increased the levels of Pax7 and desmin expression, when compared with WT and mock-transfected muscle, whereas the transfection of V1aR alone induced lower but significant changes in the expression of these proteins (Figures 6(a) and 6(b)). By contrast, the combination of V1aR and TNF overexpression promoted a significant increase in Pax7 and desmin expression. We then analyzed the expression of molecular markers characteristic of the terminal phases of muscle differentiation, such as myogenin and MHC. It is noteworthy that TNF overexpression downregulated the expression levels of MHC (but not of myogenin) compared with mock-transfected samples (Figure 6(c) and densitometry Figure 6(e)). By contrast, V1aR overexpression counteracted the negative effect of TNF on muscle differentiation, stimulating myogenin and MHC expression (Figures 6(c) and 6(d) and densitometry Figure 6(e)). Moreover, immunofluorescence analysis for embryonic-myosin heavy chain (embryonic-MHC), a marker of regenerating myofibers, revealed a significant increase in the number of embryonic-MHC positive fibers in muscles overexpressing both TNF and V1aR, compared with control and V1aR-alone transfected samples (Figure 6(f)).
Taken together, these results suggest that TNF stimulates satellite cell activation and muscle regeneration but, as expected, impinges on the maturation process. By contrast, overexpression of V1aR counteracts the negative effects of TNF, stimulating muscle growth and maturation.
3.6. V1aR Counteracts the Effect of TNF on Protein Degradation by Stimulating PI3K/Akt/FoxO Signaling
TNF is known to induce protein degradation as a result of activation of the ubiquitin-dependent proteasome pathway . On the other hand, the PI3K/Akt signaling is one of the most critical pathways involved in the regulation of skeletal muscle mass [8, 12]. Akt phosphorylates FoxO transcription factors in multiple sites, leading to the exclusion of phosphorylated FoxO proteins from the nucleus and inhibition of atrogin-1 expression . We therefore analyzed the effect of TNF on Akt and FoxO3a expression in the presence and absence of V1aR overexpression. Here we demonstrate that, in muscle overexpressing TNF, the phosphorylated form of Akt is downregulated compared with mock-transfected muscle, while the expression of native FoxO (FoxO3a) is high. The double band of native FoxO3a is ascribable to the presence of posttranslational modifications of FoxO3a, such as acetylation or ubiquitination. By contrast, phospho-Akt is upregulated in V1aR overexpressing muscles, either alone or in combination with a high TNF level (Figure 7(a)). Indeed, phospho-FoxO3a is downregulated only in samples overexpressing TNF alone, and the expression of atrogin-1 in this condition is strongly upregulated (Figures 7(a) and 7(e)). These results demonstrate that V1aR overexpression stimulates the PI3K/Akt pathways leading to phosphorylation of FoxO transcription factors, which in turn results in downregulation of atrogin-1 expression.
In this study, we show that the negative effects of TNF on muscle regeneration and inflammation are strongly counteracted by stimulation of AVP signaling. AVP, a neurohypophyseal nonapeptide, is a potent myogenesis-promoting factor both in vitro and in vivo. By interacting with V1aR, AVP increases cytosolic Ca2+ concentrations, upregulates Myf-5 and myogenin expression, and activates Ca2+/calmodulin-dependent protein kinase (CaMK) and CnA signaling pathways [16, 17, 48–51]. Moreover, local V1aR overexpression results in acceleration of the regeneration process, as demonstrated by rapid resolution of inflammation, earlier activation and fusion of satellite cells, and formation of regenerating fibers compared with the mock-transfected muscles .
To better clarify the molecular pathways involved in the positive effects of V1aR overexpression in muscle homeostasis, we induced morphological alterations in TA muscles by local overexpression of TNF and analyzed the effects of high levels of V1aR on TNF-induced muscle atrophy.
TNF is a proinflammatory cytokine known to induce murine myoblast apoptosis  and block human muscle satellite cell differentiation . Chronic exposure to low levels of circulating TNF inhibits muscle regeneration and induces cachexia [35, 54].
Morphological analysis clearly demonstrated that the accumulation of infiltrating cells in muscle overexpressing TNF alone dramatically decreases when TNF and V1aR are overexpressed together. Moreover, while V1aR does not significantly modify the number of regenerating fibers compared with samples overexpressing TNF alone, it does affect the fiber size distribution suggesting that it may play a role in acceleration of the regeneration process. Furthermore, a comparison between mock and V1aR-transfected muscles indicated that V1aR overexpression exerts a hypertrophic effect on the fibers, regardless of the regeneration process, which may be attributable to either increased fusion of satellite cells or increased synthesis and accumulation of contractile proteins. Inflammation is a critical component of muscle physiology that represents an important phase in regeneration and is often associated with severe and progressive fibrosis [3, 36, 37, 55]. Invasion by neutrophils and macrophages characterizes the initial phases of inflammation. This is followed by downregulation of the inflammatory response, thus preventing further damage and favouring regeneration . The shift from the M1-macrophage-dependent necrotic environment to the M2-macrophage phase characterized by stem cell recruitment and differentiation is important insofar as it promotes regeneration [57, 58]. This could also explain the slight increase in CD163 (involved in anti-inflammatory responses) expression occurring in TNF overexpressing muscles [2, 3]. Our data are in line with recent findings demonstrating that the V1aR agonist dramatically reduces the mRNA level of proinflammatory cytokines in astrocytes .
The enhanced regenerative capacity of V1aR overexpressing muscles correlated with dampening of inflammation and connective tissue accumulation; consequently, fibrosis and prolonged infiltration by monocytes/macrophages typical of TNF overexpressing muscle were more rapidly resolved in the presence of high levels of V1aR. This finding is supported by the V1aR-dependent modulation of NF-κB expression, one of the most important molecular players in the activation and maintenance of inflammation in response to TNF stimuli [9, 60].
Local overexpression of V1aR selectively downregulated the proinflammatory cytokines, CCL2, IL1, IL-6, whose expression is associated with sustained mononuclear cell influx and the switch from acute to chronic inflammatory process [3, 5]. Interestingly, V1aR upregulated the expression of anti-inflammatory cytokines, including CD163, IL-10, and IL-4, which play a major role in promoting growth and regeneration . In particular, several works have identified IL-4 as a key cytokine in myogenic fusion processes. Being directly correlated with CnA activity, IL-4 is synthesized and secreted after the translocation of nuclear factor of activated T-cells into the nucleus and stimulates fusion of myoblasts to preformed myotubes [44–46]. Moreover, we previously demonstrated that IL-4 represents a key cytokine in the mediation of the effects of AVP on skeletal muscle homeostasis . In the present study we found that TNF stimulates satellite cell activation and muscle regeneration, as demonstrated by the upregulation of Pax7 and desmin expression, but, as expected, impinges on the maturation process as shown by the low levels of the late differentiation marker MHC. By contrast, the overexpression of V1aR counteracted the negative effects of TNF, stimulating muscle growth and maturation as demonstrated by the increased expression levels of myogenin and MHC in TNF+V1aR overexpressing muscles.
One of the most important mechanisms controlling cellular and protein turnover is mediated by Akt-FoxO. A reduction in the activity of the Akt pathway, as observed in different models of muscular atrophy, results in decreased levels of phosphorylated FoxO and consequent upregulation of atrophy related genes [14, 62], which are responsible for increased protein degradation through the ubiquitin-proteasome system [7, 63, 64]. Here we demonstrate that TNF overexpression upregulates dephosphorylated FoxO expression, thus promoting the transcriptional activation of atrogin-1. By contrast, V1aR overexpression stimulated the PI3K/Akt pathways, leading to phosphorylation of FoxO transcription factors and resulting in the inhibition of atrogin-1 expression.
Since neurohypophyseal hormones are not canonical regulators of skeletal muscle structure and function, the physiological relevance of our findings merits discussion. A large body of evidence indicates that AVP and/or OT play a significant role in promoting differentiation and hypertrophy of myogenic cells in culture. Recently, Breton et al. provided evidence that functional oxytocin receptors are present in human primary myoblasts . The finding that levels of immunoreactive AVP, which are high in embryonic skeletal muscle, decline during gestation and reach very low levels at birth points to a role of AVP in muscle development . These data, combined with our results demonstrating a modulation of V1aR endogenous expression during the regeneration process, suggest that AVP signaling plays a significant role in skeletal muscle homeostasis . Interestingly, several authors have shown that exercise, a physiological hypertrophic cue, significantly increases circulating AVP, both in humans and in other mammals, thus posing the theoretical basis for the physiological regulation of muscle hypertrophy by neurohypophyseal hormones [49, 66–69]. De Jager et al. recently reported that treatment of cattle with anabolic steroids unexpectedly led to a high expression of mRNA encoding oxytocin in muscle, accompanied by a high level of circulating oxytocin in the plasma , suggesting that OT is involved in mediating the anabolic effects of the treatment.
Our findings show that the stimulation of AVP signaling in muscle enhances the regeneration process by attenuating inflammation and fibrosis and by modulating protein degradation. Stimulation of AVP signaling might represent an interesting novel strategy to counteract muscle decline in aging or in muscular pathologies.
Conflict of Interests
The authors declare that there is no conflict of interests regarding the publication of this paper.
The authors are indebted to Dr. Biliana Lozanoska-Ochser for critically revising the paper. This paper is supported in part by PRIN 2009 WBFZYM and by 2012 N8YJC3 and by Sapienza University Project C26A12ENW, to S.A.
- S. Gordon and P. R. Taylor, “Monocyte and macrophage heterogeneity,” Nature Reviews Immunology, vol. 5, no. 12, pp. 953–964, 2005.
- J. G. Tidball, “Inflammatory processes in muscle injury and repair,” American Journal of Physiology: Regulatory Integrative and Comparative Physiology, vol. 288, no. 2, pp. R345–R353, 2005.
- Y. Kharraz, J. Guerra, C. J. Mann, A. L. Serrano, and P. Muñoz-Cánoves, “Macrophage plasticity and the role of inflammation in skeletal muscle repair,” Mediators of Inflammation, vol. 2013, Article ID 491497, 9 pages, 2013.
- M. Saclier, S. Cuvellier, M. Magnan, R. Mounier, and B. Chazaud, “Monocyte/macrophage interactions with myogenic precursor cells during skeletal muscle regeneration,” The FEBS Journal, vol. 280, no. 17, pp. 4118–4130, 2013.
- M. R. Douglas, K. E. Morrison, M. Salmon, and C. D. Buckley, “Why does inflammation persist: a dominant role for the stromal microenvironment?” Expert Reviews in Molecular Medicine, vol. 4, no. 25, pp. 1–18, 2002.
- S. Carosio, M. G. Berardinelli, M. Aucello, and A. Musarò, “Impact of ageing on muscle cell regeneration,” Ageing Research Reviews, vol. 10, no. 1, pp. 35–42, 2011.
- Y.-P. Li and M. B. Reid, “NF-κB mediates the protein loss induced by TNF-α in differentiated skeletal muscle myotubes,” American Journal of Physiology: Regulatory Integrative and Comparative Physiology, vol. 279, no. 4, pp. R1165–R1170, 2000.
- S. Schiaffino, K. A. Dyar, S. Ciciliot, B. Blaauw, and M. Sandri, “Mechanisms regulating skeletal muscle growth and atrophy,” The FEBS Journal, vol. 280, no. 17, pp. 4294–4314, 2013.
- A. Kumar, Y. Takada, A. M. Boriek, and B. B. Aggarwal, “Nuclear factor-κB: its role in health and disease,” Journal of Molecular Medicine, vol. 82, no. 7, pp. 434–448, 2004.
- M. S. Hayden and S. Ghosh, “Shared principles in NF-κB signaling,” Cell, vol. 132, no. 3, pp. 344–362, 2008.
- F. Mourkioti, P. Kratsios, T. Luedde et al., “Targeted ablation of IKK2 improves skeletal muscle strength, maintains mass, and promotes regeneration,” The Journal of Clinical Investigation, vol. 116, no. 11, pp. 2945–2954, 2006.
- P. Bonaldo and M. Sandri, “Cellular and molecular mechanisms of muscle atrophy,” Disease Models & Mechanisms, vol. 6, no. 1, pp. 25–39, 2013.
- C.-M. Liu, Z. Yang, C.-W. Liu et al., “Effect of RNA oligonucleotide targeting Foxo-1 on muscle growth in normal and cancer cachexia mice,” Cancer Gene Therapy, vol. 14, no. 12, pp. 945–952, 2007.
- M. Sandri, C. Sandri, A. Gilbert et al., “Foxo transcription factors induce the atrophy-related ubiquitin ligase atrogin-1 and cause skeletal muscle atrophy,” Cell, vol. 117, no. 3, pp. 399–412, 2004.
- S. Minotti, B. M. Scicchitano, C. Nervi et al., “Vasopressin and insulin-like growth factors synergistically induce myogenesis in serum-free medium,” Cell Growth & Differentiation, vol. 9, no. 2, pp. 155–163, 1998.
- C. Nervi, L. Benedetti, A. Minasi, M. Molinaro, and S. Adamo, “Arginine-vasopressin induces differentiation of skeletal myogenic cells and up-regulation of myogenin and Myf-5,” Cell Growth & Differentiation, vol. 6, no. 1, pp. 81–89, 1995.
- A. Teti, F. Naro, M. Molinaro, and S. Adamo, “Transduction of arginine vasopressin signal in skeletal myogenic cells,” American Journal of Physiology: Cell Physiology, vol. 265, no. 1, part 1, pp. C113–C121, 1993.
- M. Alvisi, V. de Arcangelis, L. Ciccone et al., “V1a vasopressin receptor expression is modulated during myogenic differentiation,” Differentiation, vol. 76, no. 4, pp. 371–380, 2008.
- C. Breton, C. Haenggeli, C. Barberis et al., “Presence of functional oxytocin receptors in cultured human myoblasts,” The Journal of Clinical Endocrinology & Metabolism, vol. 87, no. 3, pp. 1415–1418, 2002.
- M. Thibonnier, M. K. Graves, M. S. Wagner, C. Auzan, E. Clauser, and H. F. Willard, “Structure, sequence, expression, and chromosomal localization of the human vasopressin receptor gene,” Genomics, vol. 31, no. 3, pp. 327–334, 1996.
- A. Toschi, A. Severi, D. Coletti, et al., “Skeletal muscle regeneration in mice is stimulated by local overexpression of V1a-vasopressin receptor,” Molecular Endocrinology, vol. 25, no. 9, pp. 1661–1673, 2011.
- J.-L. G. de Aguilar, J. W. Gordon, F. René, B. Lutz-Bucher, P. Kienlen-Campard, and J.-P. Loeffler, “A mouse model of familial amyotrophic lateral sclerosis expressing a mutant superoxide dismutase 1 shows evidence of disordered transport in the vasopressin hypothalamo-neurohypophysial axis,” European Journal of Neuroscience, vol. 11, no. 12, pp. 4179–4187, 1999.
- D. Michelson, L. Stone, E. Galliven et al., “Multiple sclerosis is associated with alterations in hypothalamic-pituitary-adrenal axis function,” The Journal of Clinical Endocrinology & Metabolism, vol. 79, no. 3, pp. 848–853, 1994.
- L. Lescaudron, Z. Li, D. Paulin, and J. Fontaine-Perus, “Desmin-lacZ transgene, a marker of regenerating skeletal muscle,” Neuromuscular Disorders, vol. 3, no. 5-6, pp. 419–422, 1993.
- L. Lescaudron, S. E. Creuzet, Z. Li, D. Paulin, and J. Fontaine-Pérus, “Desmin-lacZ transgene expression and regeneration within skeletal muscle transplants,” Journal of Muscle Research and Cell Motility, vol. 18, no. 6, pp. 631–641, 1997.
- V. A. Lupa-Kimball and K. A. Esser, “Use of DNA injection for identification of slow nerve-dependent regions of the MLC2s gene,” American Journal of Physiology: Cell Physiology, vol. 274, no. 1, part 1, pp. C229–C235, 1998.
- M. Donà, M. Sandri, K. Rossini, I. Dell'Aica, M. Podhorska-Okolow, and U. Carraro, “Functional in vivo gene transfer into the myofibers of adult skeletal muscle,” Biochemical and Biophysical Research Communications, vol. 312, no. 4, pp. 1132–1138, 2003.
- A. H. Fischer, K. A. Jacobson, J. Rose, and R. Zeller, “Hematoxylin and eosin staining of tissueand cell sections,” Cold Spring Harbor Protocols, vol. 3, no. 5, 2008.
- B. J. Davis, “Histochemical demonstration of erythrocyte esterases,” Experimental Biology and Medicine, vol. 101, no. 1, pp. 90–93, 1959.
- E. Berardi, P. Aulino, I. Murfuni et al., “Skeletal muscle is enriched in hematopoietic stem cells and not inflammatory cells in cachectic mice,” Neurological Research, vol. 30, no. 2, pp. 160–169, 2008.
- I. Desitter, B. S. Guerrouahen, N. Benali-Furet, et al., “A new device for rapid isolation by size and characterization of rare circulating tumor cells,” Anticancer Research, vol. 31, no. 2, pp. 427–441, 2011.
- A. London, E. Itskovich, I. Benhar et al., “Neuroprotection and progenitor cell renewal in the injured adult murine retina requires healing monocyte-derived macrophages,” The Journal of Experimental Medicine, vol. 208, no. 1, pp. 23–39, 2011.
- A. Turchinovich, L. Weiz, A. Langheinz, and B. Burwinkel, “Characterization of extracellular circulating microRNA,” Nucleic Acids Research, vol. 39, no. 16, pp. 7223–7233, 2011.
- V. Moresi, A. Pristerà, B. M. Scicchitano et al., “Tumor necrosis factor-α inhibition of skeletal muscle regeneration is mediated by a caspase-dependent stem cell response,” Stem Cells, vol. 26, no. 4, pp. 997–1008, 2008.
- D. Coletti, V. Moresi, S. Adamo, M. Molinaro, and D. Sassoon, “Tumor necrosis factor-α gene transfer induces cachexia and inhibits muscle regeneration,” Genesis, vol. 43, no. 3, pp. 120–128, 2005.
- C. M. Murphy, A. Matsiko, M. G. Haugh, J. P. Gleeson, and F. J. O'Brien, “Mesenchymal stem cell fate is regulated by the composition and mechanical properties of collagen-glycosaminoglycan scaffolds,” Journal of the Mechanical Behavior of Biomedical Materials, vol. 11, pp. 53–62, 2012.
- A. L. Serrano, C. J. Mann, B. Vidal, E. Ardite, E. Perdiguero, and P. Muñoz-Cánoves, “Cellular and molecular mechanisms regulating fibrosis in skeletal muscle repair and disease,” Current Topics in Developmental Biology, vol. 96, pp. 167–201, 2011.
- A. K. Gulati, A. H. Reddi, and A. A. Zalewski, “Changes in the basement membrane zone components during skeletal muscle fiber degeneration and regeneration,” The Journal of Cell Biology, vol. 97, no. 4, pp. 957–962, 1983.
- V. Moresi, G. Garcia-Alvarez, A. Pristerà et al., “Modulation of caspase activity regulates skeletal muscle regeneration and function in response to vasopressin and tumor necrosis factor,” PLoS ONE, vol. 4, no. 5, Article ID e5570, 2009.
- C. M. Overall and C. P. Blobel, “In search of partners: linking extracellular proteases to substrates,” Nature Reviews Molecular Cell Biology, vol. 8, no. 3, pp. 245–257, 2007.
- C. J. Mann, E. Perdiguero, Y. Kharraz et al., “Aberrant repair and fibrosis development in skeletal muscle,” Skeletal Muscle, vol. 1, article 21, 2011.
- C. Smith, M. J. Kruger, R. M. Smith, and K. H. Myburgh, “The inflammatory response to skeletal muscle injury: illuminating complexities,” Sports Medicine, vol. 38, no. 11, pp. 947–969, 2008.
- K. Yunoki, T. Inoue, K. Sugioka et al., “Association between hemoglobin scavenger receptor and heme oxygenase-1-related anti-inflammatory mediators in human coronary stable and unstable plaques,” Human Pathology, vol. 44, no. 10, pp. 2256–2265, 2013.
- S. Chargé and M. A. Rudnicki, “Fusion with the fused: a new role for interleukin-4 in the building of muscle,” Cell, vol. 113, no. 4, pp. 422–423, 2003.
- V. Horsley, K. M. Jansen, S. T. Mills, and G. K. Pavlath, “IL-4 acts as a myoblast recruitment factor during mammalian muscle growth,” Cell, vol. 113, no. 4, pp. 483–494, 2003.
- G. K. Pavlath and V. Horsley, “Cell fusion in skeletal muscle: central role of NFATC2 in regulating muscle cell size,” Cell Cycle, vol. 2, no. 5, pp. 419–422, 2003.
- E. Andres-Mateos, H. Brinkmeier, T. N. Burks, et al., “Activation of serum/glucocorticoid-induced kinase 1 (SGK1) is important to maintain skeletal muscle homeostasis and prevent atrophy,” EMBO Molecular Medicine, vol. 5, no. 1, pp. 80–91, 2013.
- B. M. Scicchitano, L. Spath, A. Musarò, M. Molinaro, S. Adamo, and C. Nervi, “AVP induces myogenesis through the transcriptional activation of the myocyte enhancer factor 2,” Molecular Endocrinology, vol. 16, no. 6, pp. 1407–1416, 2002.
- B. M. Scicchitano, L. Spath, A. Musarò et al., “Vasopressin-dependent myogenic cell differentiation is mediated by both Ca2+/calmodulin-dependent kinase and calcineurin pathways,” Molecular Biology of the Cell, vol. 16, no. 8, pp. 3632–3641, 2005.
- V. de Arcangelis, D. Coletti, M. Canato et al., “Hypertrophy and transcriptional regulation induced in myogenic cell line L6-C5 by an increase of extracellular calcium,” Journal of Cellular Physiology, vol. 202, no. 3, pp. 787–795, 2005.
- F. Naro, V. de Arcangelis, D. Coletti et al., “Increase in cytosolic Ca2+ induced by elevation of extracellular Ca2+ in skeletal myogenic cells,” American Journal of Physiology: Cell Physiology, vol. 284, no. 4, pp. C969–C976, 2003.
- C. E. H. Stewart, P. V. Newcomb, and J. M. P. Holly, “Multifaceted roles of TNF-α in myoblast destruction: a multitude of signal transduction pathways,” Journal of Cellular Physiology, vol. 198, no. 2, pp. 237–247, 2004.
- E. J. Foulstone, C. Huser, A. L. Crown, J. M. P. Holly, and C. E. H. Stewart, “Differential signalling mechanisms predisposing primary human skeletal muscle cells to altered proliferation and differentiation: roles of IGF-I and TNFα,” Experimental Cell Research, vol. 294, no. 1, pp. 223–235, 2004.
- D. Coletti, L. Belli, and S. Adamo, “Cachexia: novel perspectives for an old syndrome,” Basic Applied Myology, vol. 16, no. 5-6, pp. 131–139, 2006.
- C. M. Hogaboam, M. L. Steinhauser, S. W. Chensue, and S. L. Kunkel, “Novel roles for chemokines and fibroblasts in interstitial fibrosis,” Kidney International, vol. 54, no. 6, pp. 2152–2159, 1998.
- L. Pelosi, C. Giacinti, C. Nardis, et al., “Local expression of IGF-1 accelerates muscle regeneration by rapidly modulating inflammatory cytokines and chemokines,” The FASEB Journal, vol. 21, no. 7, pp. 1393–1402, 2007.
- F. O. Martinez, A. Sica, A. Mantovani, and M. Locati, “Macrophage activation and polarization,” Frontiers in Bioscience, vol. 13, no. 2, pp. 453–461, 2008.
- D. Ruffell, F. Mourkioti, A. Gambardella et al., “A CREB-C/EBPβ cascade induces M2 macrophage-specific gene expression and promotes muscle injury repair,” Proceedings of the National Academy of Sciences of the United States of America, vol. 106, no. 41, pp. 17475–17480, 2009.
- L. Zhao and R. D. Brinton, “Suppression of proinflammatory cytokines interleukin-1β and tumor necrosis factor-α in astrocytes by a V1 vasopressin receptor agonist: a cAMP response element-binding protein-dependent mechanism,” The Journal of Neuroscience, vol. 24, no. 9, pp. 2226–2235, 2004.
- M. Sandri, “Signaling in muscle atrophy and hypertrophy,” Physiology, vol. 23, no. 3, pp. 160–170, 2008.
- J. G. Tidball and S. A. Villalta, “Regulatory interactions between muscle and the immune system during muscle regeneration,” American Journal of Physiology: Regulatory Integrative and Comparative Physiology, vol. 298, no. 5, pp. R1173–R1187, 2010.
- J. M. Sacheck, J.-P. Hyatt, A. Raffaello et al., “Rapid disuse and denervation atrophy involve transcriptional changes similar to those of muscle wasting during systemic diseases,” The FASEB Journal, vol. 21, no. 1, pp. 140–155, 2007.
- S. C. Bodine, E. Latres, S. Baumhueter et al., “Identification of ubiquitin ligases required for skeletal Muscle Atrophy,” Science, vol. 294, no. 5547, pp. 1704–1708, 2001.
- M. D. Gomes, S. H. Lecker, R. T. Jagoe, A. Navon, and A. L. Goldberg, “Atrogin-1, a muscle-specific F-box protein highly expressed during muscle atrophy,” Proceedings of the National Academy of Sciences of the United States of America, vol. 98, no. 25, pp. 14440–14445, 2001.
- A. Smith, R. I. Stephen, M. M. Arkley, and N. McIntosh, “Immunoreactive arginine vasopressin in human fetal and neonatal skeletal muscle,” Early Human Development, vol. 28, no. 3, pp. 215–222, 1992.
- S. L. Alexander, C. H. G. Irvine, M. J. Ellis, and R. A. Donald, “The effect of acute exercise on the secretion of corticotropin-releasing factor, arginine vasopressin, and adrenocorticotropin as measured in pituitary venous blood from the horse,” Endocrinology, vol. 128, no. 1, pp. 65–72, 1991.
- V. A. Convertino, L. C. Keil, E. M. Bernauer, and J. E. Greenleaf, “Plasma volume, osmolality, vasopressin, and renin activity during graded exercise in man,” Journal of Applied Physiology: Respiratory Environmental and Exercise Physiology, vol. 50, no. 1, pp. 123–128, 1981.
- B. Melin, J. P. Eclache, G. Geelen et al., “Plasma AVP, neurophysin, renin activity, and aldosterone during submaximal exercise performed until exhaustion in trained and untrained men,” European Journal of Applied Physiology and Occupational Physiology, vol. 44, no. 2, pp. 141–151, 1980.
- B. Melin, C. Jimenez, G. Savourey et al., “Effects of hydration state on hormonal and renal responses during moderate exercise in the heat,” European Journal of Applied Physiology and Occupational Physiology, vol. 76, no. 4, pp. 320–327, 1997.
- N. de Jager, N. J. Hudson, A. Reverter et al., “Chronic exposure to anabolic steroids induces the muscle expression of oxytocin and a more than fifty fold increase in circulating oxytocin in cattle,” Physiological Genomics, vol. 43, no. 9, pp. 467–478, 2011.