|
|
|
|
|
|
|
|
|||||
| Home Help Feedback Subscriptions Archive Search Table of Contents | |||||
First published online December 11, 2006
doi: 10.1242/10.1242/jcs.03300
Research Article |
1 CellStem Cell Research Institute, H. San Raffaele Scientific Institute, 20132, Milan, Italy
2 Department of Experimental, Environmental Medicine and Medical Biotechnology, University of Milano-Bicocca, 20052 Monza, Italy
3 Department of Biomedical Science, University of Modena and Reggio Emilia, 41100 Modena, Italy
4 Department of Biology, University of Milano, 20130 Milan, Italy
5 E. Medea Scientific Institute, 23842 Bosisio Parini, Italy
6 Department of Preclinical Sciences LITA-Vialba, University of Milano, 20157 Milan, Italy
Authors for correspondence (e-mail: giulio.cossu{at}unimi.it and emilio.clementi{at}unimi.it)
Accepted 12 October 2006
 |
Summary |
|---|
 Top Summary IntroductionResultsDiscussionMaterials and MethodsReferences |
|---|
-sarcoglycan-null dystrophic mice have a significantly enhanced ability to migrate to dystrophic muscles, to resist their apoptogenic environment and engraft into them, yielding a significant recovery of -sarcolgycan expression. In vitro NO-treated mesoangioblasts displayed an enhanced chemotactic response to myotubes, cytokines and growth factors generated by the dystrophic muscle. In addition, they displayed an increased ability to fuse with myotubes and differentiating myoblasts and to survive when exposed to cytotoxic stimuli similar to those present in the dystrophic muscle. All the effects of NO were cyclic GMP-dependent since they were mimicked by treatment with the membrane permeant cyclic-GMP analogue 8-bromo-cGMP and prevented by inhibiting guanylate cyclase. We conclude that NO donors exert multiple beneficial effects on mesoangioblasts that may be used to increase their efficacy in cell therapy of muscular dystrophies.
Key words: Muscular dystrophy, Stem cells, Nitric oxide, Cyclic GMP, Apoptosis, Differentiation
|
Introduction |
|---|
|
TopSummaryIntroductionResultsDiscussionMaterials and MethodsReferences |
|---|
). Inflammation is followed by sclerosis, thus starting a vicious circle that reduces oxygen supply and increases the likelihood of degeneration for surviving and regenerated fibres (Emery, 2002). In the most severe forms, such as Duchenne muscular dystrophy, regeneration is progressively exhausted, and skeletal muscle is replaced by fat and fibrous tissue. This condition leads to progressive muscle weakness and eventually paralysis, ultimately causing death by respiratory and/or cardiac failure (Emery, 2002). Although the underlying molecular defects are now known, there is still no available satisfactory therapy.
The current therapies, based on corticosteroid administration, provide only temporary improvements and are associated with severe side-effects (Manzur et al., 2004). The other pharmacological strategies attempted so far, including administration of protease inhibitors, and drugs that regulate calcium homeostasis or act on protein and lipid metabolism, have yielded no favourable outcomes in clinical trials and did not enter the clinical practice (Skuk et al., 2002).
In the past few years experimental approaches offering an alternative to classical pharmacological treatments have been developed, among which the injection of myogenic stem cells and gene therapy with adeno-associated viral vectors appear to hold particular promise (Cossu and Sampaolesi, 2004). Significant restoration of muscle structure and function in the -sarcoglycan (SG)-null mouse model of muscular dystrophy have been obtained using mesoangioblasts, a population of vessel-associated, mesoderm stem cells that express angioblast and mesoderm markers (Minasi et al., 2002; Sampaolesi et al., 2003). Although promising, this cell therapy is still far from yielding a complete reconstitution of the skeletal muscle structure. The main reasons for the only partial effect of mesoangioblasts are not yet known, but it is conceivable that it may arise from a limited homing of these cells to muscle, as well as a reduced ability of these cells to fuse and to resist the cytotoxic environment existing in the damaged muscle, where several pro-inflammatory and pro-apoptotic stimuli may be present (Tews and Goebel, 1996; Rando et al., 1998; Engvall and Wewer, 2003). To date, no studies have reported specific pharmacological approaches to enhance the therapeutic efficacy of cell therapy, even though we showed that exposure to cytokines such as high mobility group box 1 (HMGB1) and stromal cell-derived factor 1 (SDF-1) increases mesoangioblast colonisation of dystrophic muscle (Palumbo et al., 2004; Galvez et al., 2006).
A good candidate molecule to increase the efficiency of muscle repair by mesoangioblasts is nitric oxide (NO), a short-lived messenger generated by skeletal muscle to play important roles in regulating its own physiological functions (Wolosker et al., 1997; Bredt, 1998; Balon and Nadler, 1997; Stamler and Meissner, 2001; Eu et al., 2003; Shen et al., 1994; Wang et al., 1995; Clementi and Meldolesi, 1997; Nisoli et al., 2004). Several pieces of evidence support this idea. NO actively participates in processes important to muscle regeneration, such as the myogenic programme activated by insulin-like growth factor (IGF)-II (Carrasco et al., 2002; Kaliman et al., 1999) or by stimulating myoblast fusion (Pisconti et al., 2006). In addition, NO contributes to activation of satellite cells by mediating the production of hepatocyte growth factor (HGF) and follistatin (Anderson, 2000; Tatsumi et al., 2002; Pisconti et al., 2006).
Here, we report that a brief ex-vivo treatment of mesoangioblasts with NO donors enhances their ability to migrate, resist death-inducing stimuli of the type known to be present in dystrophic muscles and fuse with regenerating myofibres. The action of NO is cyclic GMP (cGMP)-dependent and appears to be mediated by classical pathways involved in myogenesis and muscle repair. Our results indicate that the treatment with NO exerts multiple actions that enable mesoangioblasts to limit muscle damage in vivo more efficiently, thus opening an opportunity for improving the efficacy of cell therapy.
|
Results |
|---|
|
TopSummaryIntroductionResultsDiscussionMaterials and MethodsReferences |
|---|
SG-null mice) and injected into the femoral artery are able to engraft into muscle and yield both morphological and functional repair in SG-null mice (Duclos et al., 1998; Sampaolesi et al., 2003).
We investigated whether NO enhanced the therapeutic function of these cells. To this end, mesoangioblasts were cultured for 12 hours in growth medium in the presence or absence of either (Z)-1-[2-(2-aminoethyl)-N-(2-ammonioethyl)amino]diazen-1-ium-1,2-diolate] (DETA-NO) (20 µM) or isosorbide mononitrate (IMN) (50 µM), two widely employed, structurally unrelated NO-releasing compounds (Yamamoto and Bing, 2000). At the concentrations used these NO-donors release concentrations of NO in the physiological range (Clementi et al., 1998). Mesoangioblasts (5x105 per animal) were then washed free of the drugs and injected into the right femoral artery of SG-null mice. Mice were sacrificed 21 days after injection, and the quadriceps, gastrocnemius, soleus and tibialis anterior muscles collected. The expression of SG, an index of wild-type mesoangioblast integration, was then evaluated, by real-time PCR, in quadriceps, gastrocnemius and soleus muscles. Expression of SG in the tibialis anterior was evaluated by western blot analyses and immunohistochemistry. Using this single-injection protocol the restoration of SG expression by untreated mesoangioblasts was clearly detectable, although lower than that obtained with repeated cell injections (Sampaolesi et al., 2003). Mesoangioblasts pretreated with DETA-NO or IMN yielded a recovery of SG mRNA levels in the various muscles that was significantly higher than that induced by untreated mesoangioblasts (Fig. 1A). Accordingly, SG expression analysed by western blotting and immunohistochemistry was also increased (Fig. 1B,C, and data not shown), and the areas in which SG expression was increased by NO-treated mesoangioblasts were larger in size than those observed with untreated mesoangioblasts and contained more SG-positive fibres. In the tibialis anterior the increase in area size was of 26.3±1.3% and 22.7±2.0% with DETA-NO- and IMN-treated mesoangioblasts, respectively (n=15, P<0.01 vs. control). In the same muscle, of a total fibre number of 418±28, the numbers of SG-positive fibres were 109±12, 184±15 and 142±9 after injection with control mesoangioblasts, DETA-NO- and IMN-treated mesoangioblasts, respectively (n=20, IMN- or DETA-NO-treated mesoangioblasts: P<0.01 vs. control). In all these experiments the effect of pretreatment with DETA-NO and IMN was dependent on NO generation because the treatments with the amine DETA or isosorbide did not yield significant effects (data not shown).
|
). Although mesoangioblasts express none of the NO-synthesizing enzymes, in preliminary experiments they were found to be endowed with the NO-dependent guanylate cyclase (data not shown). To examine the cGMP-dependency of the effect of NO, mesoangioblasts were incubated for 12 hours with the cell-permeable analogue of cGMP, 8-bromo-cGMP (8-Br-cGMP) (1 mM), or DETA-NO combined with 1H-(1,2,4) oxadiazolo [4,3-]quinoxalin-1-one (ODQ) (1 µM), a selective guanylate cyclase inhibitor that prevents NO-dependent cGMP generation (Garthwaite et al., 1995). Pretreatment of mesoangioblasts with 8-Br-cGMP enhanced SG expression in a manner similar to the pretreatment with the NO donors (Fig. 1A-C). The combined pretreatment with DETA-NO and ODQ consistently abolished this effect. Pretreatment with ODQ alone did not have significant effects (data not shown). These results indicate that the effect of NO on mesoangioblast homing is cGMP-dependent.
Mechanisms through which NO/cGMP increases homing of mesoangioblasts in vivo
Various mechanisms may conceivably explain the enhanced therapeutic efficacy of the NO-treated mesoangioblasts, including an increased ability to migrate through vessels and into the site of damage, resist the apoptogenic stimuli present in the dystrophic muscle and fuse with, and repair, existing myofibres. We decided to investigate these mechanisms in vivo separately from each other. To assess chemoattraction and cell movement, green fluorescent protein (GFP)-expressing mesoangioblasts pretreated or not with IMN, DETA-NO, 8-Br-cGMP or DETA-NO plus ODQ were injected into the right femoral artery. Mice were sacrificed 6 hours later, and the quadriceps, gastrocnemius and tibialis anterior muscles collected. Also collected were the liver, spleen and lungs, i.e. the filter organs in which mesoangioblasts tend to accumulate when injected intra-arterially (Sampaolesi et al., 2003). The percentage of cells found in the various muscles and organs was evaluated measuring GFP expression by real-time PCR. Pretreatment with DETA-NO or IMN significantly increased the ability of mesoangioblasts to reach the muscles (Fig. 2A) and reduced the percentage of mesoangioblasts retained in the filter organs (Fig. 2B).
|
To analyse the effect of NO on muscle repair, the pretreated mesoangioblasts were injected directly into the right tibialis anterior muscle as above, but muscles were removed and analysed after 21 days. The pretreatment with either NO donor resulted in a significantly increased expression of SG, measured by both quantitative real-time PCR (Fig. 2D) and western blot analyses (Fig. 2E). The fact that restoration of SG levels by untreated mesoangioblasts was reduced compared with that observed with intra-arterially delivered cells (compare NT in Fig. 1B and Fig. 2E) may reflect an increased cell death due to this specific route of administration (Beauchamp et al., 1999) (B. G. Galvez, unpublished observation).
Of importance, the pretreatment with 8-Br-cGMP mimicked the effects of NO on all the mechanisms investigated, while co-incubation with DETA-NO and ODQ abolished it (Fig. 2A-E). Pretreatment with ODQ alone did not have significant effects on either parameter investigated (data not shown). These results indicate that NO has independent effects that help to enhance homing of mesoangioblasts in a cGMP-dependent manner.
NO/cGMP enhances migration of mesoangioblasts in vitro in response to chemoattractants
We performed different sets of in vitro experiments to investigate in detail the mechanisms of the NO/cGMP effects on mesoangioblast functions observed in vivo. We evaluated the effect of NO/cGMP pretreatment on migration of mesoangioblasts using a transwell system in which the upper and lower chambers were separated by a gelatin-coated cell-permeable membrane. Mesoangioblasts pretreated or not with IMN, DETA-NO, 8-Br-cGMP or DETA-NO plus ODQ were plated into the upper chamber and serum-starved overnight. Migration was triggered by the addition of vascular endothelial growth factor (VEGF) (10 ng/ml), a known chemoattractant of these cells, in the lower chamber (Palumbo et al., 2004), transforming growth factor-ß (TGF-ß) (100 ng/ml), tumour necrosis factor- (TNF-) (10 ng/ml), hepatocyte growth factor (HGF) (10 ng/ml) or basic fibroblast growth factor (bFGF) (10 ng/ml), i.e. chemokines and growth factors known to be present in the environment of the regenerating dystrophic muscle (Charge and Rudnicki, 2004). Migration was measured after 6 hours and compared with that triggered by bovine serum albumin (BSA) (0.1%), used as a negative control. As shown in Fig. 3A, migration of mesoangioblasts was dependent on the stimulus used, with TGFß and TNF being the most powerful chemoattractants, whereas smaller but still significant migration was induced by VEGF, HGF and bFGF. As shown in the graph and representative images of Fig. 3B,C, pretreatment with either DETA-NO or IMN increased mesoangioblast migration in response to all stimuli used. The effect of NO was mimicked by 8-Br-cGMP and inhibited by ODQ, indicating the cGMP-dependence of the effect of NO. Interestingly, neither NO nor 8-Br-cGMP enhanced migration significantly in the absence of chemoattractants (Fig. 3B; data not shown).
|
We then investigated whether the stimulatory effect of NO/cGMP was still maintained in a transwell migration assay through an endothelial cell layer. To this end mouse microendothelial H5V cells were plated onto the upper membrane of the transwell insert and cultured until they reached confluence. In this assay we used LacZ-expressing mesoangioblasts so that migrated cells were distinguished from endothelial cells by ß-galactosidase staining. Under these conditions, VEGF, HGF and TNF triggered significant migration of control, untreated mesoangioblasts (Fig. 3D). Pretreatment with DETA-NO, IMN or 8-Br-cGMP increased migration further. The effect of DETA-NO was abolished when it was administered together with ODQ.
We studied whether differentiated L6E9 myotubes and non-differentiating L6E9 myoblasts attracted mesoangioblasts and whether NO affected this event. We found that a significant number of mesoangioblasts migrated through the H5V cell monolayer in the presence of myotubes. By contrast, myoblasts failed to trigger migration (Fig. 3E). Pretreatment with either DETA-NO or IMN further increased mesoangioblast migration triggered by myotubes. The effect of NO was mimicked by 8-Br-cGMP and inhibited by ODQ. Conversely, none of the pretreatments triggered migration towards undifferentiated myoblasts (Fig. 3E). Of importance, mesoangioblast pretreatment with ODQ alone had no significant effects in any of the migration experiments (data not shown).
Differentiation of mesoangioblasts into skeletal muscle cells is enhanced by NO/cGMP treatment in vitro
When co-cultured with myogenic cells, mesoangioblasts fuse with them and differentiate into skeletal muscle (Minasi et al., 2002). To investigate the effect of NO on this event we performed two different sets of experiments: in the first mesoangioblasts and L6E9 myoblasts were co-cultured and induced to differentiate together for 5 days (co-fusion experiments), whereas in the second mesoangioblasts were co-cultured with preformed L6E9 myotubes (post-fusion experiments). Cells were fixed and stained with the anti-myosin heavy-chain monoclonal antibody (mAb) MF20 to identify myotubes and differentiated myocytes and with 4',6-diamidino-2-phenylindole (DAPI). The DAPI staining allowed us to distinguish between rat nuclei (L6E9 cells) and mouse nuclei (mesoangioblasts) on the basis of the different heterochromatin distribution (Blau et al., 1983). Pretreatment of mesoangioblasts with DETA-NO, IMN or 8-Br-cGMP increased their ability to fuse to both myoblasts and myotubes. The effect of DETA-NO was no longer observed in the presence of ODQ (Fig. 3F,G). ODQ had no effects on the fusogenic ability of mesoangioblasts when administered alone (data not shown).
NO/cGMP treatment inhibits death of mesoangioblasts induced by different stimuli in vitro
NO, when generated at low concentrations often increases cell resistance to apoptosis, an effect that may persist even after its removal (Liu and Stamler, 1999; Falcone et al., 2004; Perrotta et al., 2004). We investigated whether NO/cGMP had pro-survival effects on mesoangioblasts. To this end, mesoangioblasts pretreated or not with DETA-NO, IMN, 8-Br-cGMP or DETA-NO plus ODQ were exposed for a further 24 hours to cytotoxic stimuli known to be present in the microenvironment of the dystrophic muscle, i.e. TNF (100 ng/ml) and the reactive oxygen species generating agents H2O2 (100 µM) and As2O3 (20 µM) (Tews and Goebel, 1996; Rando et al., 1998; Emery, 2002; Engvall and Wewer, 2003; Hodgetts et al., 2003). Cell death was determined 24 hours later by measuring both Annexin V staining of phosphatidylserine exposed on the outer leaflet of the plasma membrane and propidium iodide (PI) incorporation. Results obtained are summarised in Fig. 4A, and representative dot-plot analyses showing the results using As2O3 as the death-inducing stimulus are shown in Fig. 4B. Cell death-induction by all stimuli used was prevented by pretreatment with either NO donor or 8-Br-cGMP and restored by co-incubation of DETA-NO with ODQ (Fig. 4A,B). We then assessed whether NO protected against cell-mediated cytotoxicity, an event known to occur in the damaged, dystrophic muscle (Hohlfeld and Engel, 1990). To this end, mesoangioblasts, after the various pretreatments indicated above, were stained with the green fluorescent dye 5-chloromethylfluorescein (CFMDA) and then co-incubated for 16 hours with cytotoxic T lymphocytes. The results obtained show that NO conferred protection against cytotoxicity, evaluated by measuring PI incorporation (Fischer et al., 2002) (Fig. 4C). Also in this case, the effect of NO depended on cGMP generation.
|
; Horsley and Pavlath, 2004; Iezzi et al., 2004). In addition, the pretreatment with NO increased the expression of receptors for HGF, VEGF and TNF, as well as members of families of adhesion molecules known to play a role in migration, such as cadherins and integrins (Carmeli et al., 2004; Horsley and Pavlath, 2004; Krauss et al., 2005). Finally, NO increased the expression of two anti-apoptotic members of the Bcl protein family, Bcl-2 and Bcl-xL, and reduced the expression of pro-apoptotic Bax (Adams et al., 2001).
|
|
Discussion |
|---|
|
TopSummaryIntroductionResultsDiscussionMaterials and MethodsReferences |
|---|
SG-null mouse (Sampaolesi et al., 2003), a model of Duchenne muscular dystrophy (Duclos et al., 1998). Here we show that a brief ex-vivo treatment of mesoangioblasts with NO significantly increases various independent parameters important for their therapeutic activity, i.e. the ability to reach dystrophic muscles, to resist their apoptogenic environment and to engraft into them. The combination of these effects resulted in increased efficiency in homing of intra-arterially delivered mesoangioblasts that yielded an enhanced structural recovery of the damaged muscle. Of importance, the increased homing of mesoangioblasts to the muscle was accompanied by a concomitant reduction in their number in the relevant filter organs. This number is large and may cause damage to these organs (Cossu and Sampaolesi, 2004). Thus, increasing homing to the target tissue has two positive outcomes, the delivery of more cells to repair the target tissue and a reduction in the number of cells that are trapped in filter organs.
The treatment with NO shows two characteristics. First, it is persistent, since a brief exposure of mesoangioblasts yielded a long-lasting increase in their function; second, it depends on the generation of cGMP following activation of guanylate cyclase, an enzyme known to be stimulated by nanomolar concentrations of NO and to mediate physiological actions of the gas (Moncada et al., 1991). Both these characteristics are crucial from a therapeutic standpoint because the amelioration of mesoangioblast function was obtained with a short-term drug exposure, compatible with minimal manipulation of cells ex vivo, and with concentrations of NO in the physiological range.
Using in vitro experiments, we studied in further detail the mechanisms responsible for the beneficial effects of NO observed in vivo. We investigated the effect of NO on migration of mesoangioblasts towards multinucleated myotubes. These experiments were performed in the presence of an endothelial cell layer in a transwell system, an assay commonly used to examine the chemotactic properties of specific molecules, and proven as a reliable indicator of the mechanisms that govern cellular trafficking in vivo (Puri et al., 2004). Moreover, this in vitro setting mimicks the microenvironment encountered by mesoangioblasts after intra-arterial injection, since myotubes correspond to newly regenerated, immature fibres (Charge and Rudnicki, 2004). We found that pretreatment with NO significantly increased migration of mesoangioblasts towards myotubes. Interestingly, in control experiments using proliferating myoblasts, migration of mesoangioblasts was almost undetectable and not significantly modified by NO, suggesting that some factors secreted by newly-formed muscle fibres stimulate mesoangioblast migration and synergise with the action of NO.
We also investigated the ability of NO to ameliorate mesoangioblast migration triggered by cytokines and growth factors known to be produced in the pro-inflammatory environment of the regenerating dystrophic muscle, such as TNF, HGF, bFGF and TGFß (Charge and Rudnicki, 2004; Wagers and Conboy, 2005) or VEGF, a chemoattractant for mesoangioblasts (Palumbo et al., 2004). NO significantly increased mesoangioblast migration triggered by all of these chemoattractants, both in the presence and absence of an endothelial cell layer. Of importance, all the effects of NO in these in vitro assays were found to be cGMP-dependent, consistent with the in vivo migration results. The fact that NO increases migration triggered by myotubes and a variety of chemoattractants is of relevance for the therapy of muscular dystrophy, since it indicates that the beneficial actions of NO apply to the various pro-inflammatory conditions that may arise during the course of the disease.
An important aspect of damaged muscle is that it originates a pro-apoptotic microenvironment in which cytokines such as TNF, oxidative stress and immune-competent cells play a role, and that may contribute to the poor outcome of transplantation of myogenic cells (Tews and Goebel, 1996; Rando et al., 1998; Emery, 2002; Engvall and Wewer, 2003; Hohlfeld and Engel, 1990; Hodgetts et al., 2003). In vivo, we found that NO/cGMP reduced the number of apoptotic mesoangioblasts observed in muscle sections; in vitro, the exposure to NO/cGMP increases the ability of mesoangioblasts to resist the apoptogenic effects of TNF, reactive oxygen species and cytotoxic T lymphocytes. This evidence supports the fact that NO protects mesoangioblasts from apoptosis, consistent with its cGMP-dependent anti-apoptotic role described for other cell types (Liu and Stamler, 1999).
The observation that injection of NO-pretreated mesoangioblasts led to a recovery of SG expression by muscle fibres suggests an additional mechanism that may contribute to the in vivo effect of NO is an increased mesoangioblast ability to fuse to pre-existing myofibres. A role for NO in myoblast fusion has indeed been shown by some studies (Kaliman et al., 1999; Pisconti et al., 2006), although whether this also applies to mesoangioblasts is not known. To investigate this possibility we used an in vitro fusion assay in which mesoangioblasts were co-incubated with either preformed myotubes or differentiating myoblasts. Pretreatment with NO led to increased fusion of mesoangioblasts in both types of assays. Also in this case the effect was cGMP-dependent, and therefore consistent with the in vivo results.
Signalling events activated by the NO/cGMP pathway are multiple and comprise both short-term modifications of protein function and activity and long-term effects on gene transcription (Pilz and Casteel, 2003). The persistency of the effect of NO/cGMP on mesoangioblasts observed here is consistent with the latter mechanism of action. Moreover, induction and repression of specific genes is also crucial in the process of myogenesis, myoblast fusion and muscle repair (Buckingham, 2001; Charge and Rudnicki, 2004; Cossu and Biressi, 2005). We have therefore investigated whether regulation of gene transcription explained the effects of NO/cGMP on mesoangioblasts. We found that NO increased expression by mesoangioblasts of several plasma membrane receptors known to play key roles in myogenesis, such as members of metalloproteases and disintegrin families, adhesions molecules, integrins and cadherins (Carmeli et al., 2004; Horsley and Pavlath, 2004; Krauss et al., 2005). NO also increased the expression of HGF, which participates in NO-induced satellite cell activation (Anderson, 2000; Tatsumi et al., 2002), and of IGF-I and follistatin, which contribute to muscle hypertrophy (Glass, 2003; Iezzi et al., 2004), the latter recently shown to mediate NO-induced satellite cell fusion (Pisconti et al., 2006). Interestingly, NO also increased the expression of receptors for chemoattractants, and this, together with the effect on adhesion molecules, may explain why NO-treated mesoangioblasts are endowed with and increased migratory ability. NO also inhibited the mesoangioblast expression of proapoptotic Bax, while increasing the expression of anti-apoptotic Bcl-2 and Bcl-xL (Adams et al., 2001). This, together with the observation that the anti-apoptotic action of NO was not restricted to a specific stimulus, strongly suggests that NO switches off the apoptotic programme elicited by the damaged muscle environment in mesoangioblasts, rather than acting as a simple negative modulator of selected apoptotic signals. Although the changes in the levels of expression of the various genes investigated were not striking, the pattern of modifications induced in mesoangioblasts by NO/cGMP is consistent with a general switch on of signalling pathways involved in myogenesis and muscle repair. How and to what extent the changes in gene expression are integrated in shaping the enhanced function of NO-treated mesoangioblasts remains to be investigated.
Which among the various effects of NO on mesoangioblasts described here is the most relevant in in vivo conditions is difficult to predict, and enhanced migration, resistance to apoptosis and ability to fuse may conceivably all play a role. However, the anti-apoptotic effect of NO is the most dramatic in terms of fold changes and has already been shown to play a key role with other cell types in vivo (Perrotta et al., 2004). This strongly suggests that protection against apoptosis plays a crucial role in determining the NO-dependent enhanced homing of mesoangioblasts.
In conclusion, we propose that the treatment of mesoangioblasts with NO significantly enhances their homing to dystrophic muscle, yielding a recovery of its function. Since this treatment does not require extensive cell manipulation and is non-toxic it appears worth pursuing, especially in view of the new NO donors and compounds able to increase cGMP concentration that are currently undergoing validation for clinical use (Burgaud et al., 2002; Nakane, 2003). In addition, because of its simplicity, the treatment might be easily combined with other strategies to yield an enhanced therapeutic effect combining increased mesoangioblast survival and ability to reach damaged muscles and engraft into them. Finally, this therapeutic approach may be helpful not only in muscular dystrophies but also in other pathological states in which stem cell therapy has been proposed, including congenital myopathies and muscle atrophy (Wagers and Conboy, 2005).
|
Materials and Methods |
|---|
|
TopSummaryIntroductionResultsDiscussionMaterials and MethodsReferences |
|---|
SG mAbs from DSHB (University of Iowa, Iowa City, IA, USA) and NovoCastra (Newcastle, UK), respectively. In immunoblot and immunohistochemistry analyses primary Abs were detected by appropriate secondary Abs conjugated with horseradish peroxidase (BioRad, Hercules, CA, USA) or Alexa-Fluor 488 and 594, respectively (Molecular Probes, Eugene, OR, USA). Polycarbonate membrane transwell inserts used for the in vitro chemotaxis assays were purchased from Costar (Milan, Italy); mouse VEGF, TNF-, HGF, bFGF and TGF-ß from R&D Systems (Abingdon, UK); and fluorescein isothiocyanate (FITC)-Annexin V and PI from Bender MedSystem (Vienna, Austria). The reagents for RNA extraction and cDNA preparation were obtained by Invitrogen Life Technologies (Carlsbad, CA, USA). ODQ and DETA-NO were from Alexis Italia (Florence, Italy), and all the other reagents were purchased from Sigma (Milan, Italy).
Animals
SG-null C57BL/6 mice were a kind gift of K. Campbell (Iowa University, Iowa City, IA, USA). Animals were housed in the pathogen-free facility at our institution and treated in accordance with the European Community guidelines, and with the approval of the Institutional Ethical Committee. Animals were used when 4 months old, since at this stage SG-null mice are characterized by the development of histopathological features of muscle dystrophy with ongoing fibre degeneration and modest spontaneous regeneration (Duclos et al., 1998).
Cell culture
Wild-type, GFP- or LacZ-expressing D16 mesoangioblasts were generated and cultured as described (Minasi et al., 2002; Sampaolesi et al., 2003; Palumbo et al., 2004). In all experiments the pretreatment of mesoangioblasts with DETA-NO (20 µM), IMN (50 µM), 8-Br-cGMP (1 mM), ODQ (1 µM) or DETA-NO plus ODQ was for 12 hours, after which cells were washed free of the drugs and suspended in culture medium. Delivery of mesoangioblasts was either by intra-arterial injection through the right femoral artery with 5x105 mesoangioblasts per animal, performed exactly as described (Sampaolesi et al., 2003), or by injection of 5x105 cells directly into tibialis anterior muscles.
The rat skeletal muscle cell line L6E9 was cultured in Dulbecco's modified Eagle's medium (DMEM) containing 15% foetal bovine serum (FBS), 200 µM glutamine, 1000 U/ml penicillin and streptomycin growth medium (GM). Differentiation was obtained by shift to a differentiation medium (DM) containing 2% horse serum. The microendothelium cell line H5V (a kind gift of Elisabetta Dejana, University of Milano, Milan, Italy) was cultured in DMEM containing 10% FBS, 200 µM glutamine, 1000 U/ml penicillin and streptomycin.
Quantitative real-time PCR analysis
Tissue samples were homogenized and RNA extracted using TRIzol reagent (Invitrogen) and reverse transcribed into complementary DNA by using a Taqman kit (Platinum Taq DNA polymerase; Invitrogen). Real-time quantitative PCR analyses were performed using a Mx3000P real-time PCR detection system (Stratagene, La Jolla, CA, USA). Each cDNA sample was amplified in duplicate by using the SYBR Green Supermix (BioRad) for GFP (GFP primers: forward (FW), 5'-AAGTTCATCTGCACCACCG-3'; reverse (Rev), 5'-TCCTTGAAGAAGATGGT GCG-3'). Data are expressed as the percentage of migrated cells, which is calculated by comparing the level of GFP messenger in our sample with that corresponding to the total input of injected cells. Real-time PCR analyses of SG expression were performed using the Taqman Universal PCR master mixture containing AmpliTaq Gold DNA with commercial primers (Applied Biosystems, Foster City, CA, USA) for SG detection. For Taqman assays, the level of SG measured represents the specific signal detected in the sample from mesoangioblast-injected SG-null mouse muscles vs. that of a positive control for SG expression (corresponding wild-type mouse muscles).
Protein extraction and immunoblot analysis
Muscle tissues were dissected and homogenized in 100 mM NaHCO3, 1 mM EDTA, 2% sodium dodecyl sulphate and protease inhibitor cocktail (Complete, Roche Diagnostics) and centrifuged (1000 g) for 10 minutes at 4°C to discard cellular debris. Sample preparation and western blot analyses were performed as described (Bulotta et al., 2001).
Immunohistochemistry
Tibialis muscles recovered from the mesoangioblast-injected animals were dissected and frozen in liquid N2-cooled isopentane. Serial muscle sections were immunostained as previously described (Sampaolesi et al., 2003) with the anti-GFP, anti-laminin or anti-SG Abs. Primary Abs were detected using appropriate secondary Abs and nuclei were visualized with the DNA dye DAPI. Quantification of SG-positive areas and fibre number was performed in five randomly selected fields of at least three non-adjacent transverse SG-laminin double-stained sections along the longitudinal axis of the muscle.
Differentiation experiments
L6E9 myoblasts were plated in growth medium at a density of 1.5x105 and shifted in DM medium 24 hours later. D16 mesoangioblasts suspended in DM were added to L6E9 cultures either at the moment of medium shift (5x104 cells/dish, co-fusion experiments) or after 3 days (2x104 cells/dish, post-fusion experiments), i.e. when L6E9 myotubes were already formed.
After 5 days of co-culture, the medium was removed, the cells fixed and myotubes and nuclei revealed by immunofluorescence using the anti-myosin heavy-chain Ab (MF20, 1:3) and DAPI, respectively (Brunelli et al., 2004). The percentage of mesoangioblasts fused to rat myotubes was measured by counting the number of mouse nuclei in myosin heavy chain-stained rat fibres (5-8 random fields for each sample) on the basis of different staining with DAPI because of different heterochromatin distribution.
Migration assays
LacZ-expressing D16 mesoangioblasts (2x104) were plated in complete medium in the upper chamber of transwell inserts (membrane diameter: 6.5 mm; pore size: 8 µm) coated with type A gelatin from porcine skin. At the end of the pretreatments the cells were starved overnight in DMEM without serum. The following morning the lower chamber medium was substituted with DMEM containing differentiated L6E9 myotubes, undifferentiated L6E9 cells or one of the following chemotactic agents: TGFß (100 ng/ml), VEGF (10 ng/ml), TNF (10 ng/ml), HGF (10 ng/ml) or bFGF (10 ng/ml). In the transmigration experiments through endothelium, mouse microendothelial H5V cells were plated on the gelatin-coated transwell membrane (1x104 cells/dish) and grown in DMEM containing 10% FBS until they reached confluence, before the addition of mesoangioblasts. The tightness of the monolayers was checked by measuring the diffusion of BSA from the upper to the lower chamber. The number of mesoangioblasts that crossed the membrane pores was evaluated after 6 hours. To this end, non-migrated cells were mechanically removed from the upper side of the transwell system, whereas the cells in the lower side of the filter membrane were fixed in 4% paraformaldehyde for 10 minutes at 4°C and stained with crystal violet [0.1% in methanol-water (2:8) solution for 20 minutes at room temperature]. The number of migrated cells was measured using an inverted microscope and by counting 5-10 random fields of the lower face of the transwell membrane at 20x magnification or by X-Gal staining, performed according to standard protocols (Brunelli et al., 2003). Migration index was calculated by dividing the number of migrated cells in the presence of the chemotactic agents by the cells migrated in response to DMEM with 0.1% BSA (control).
Cell death experiments
After the various pretreatments, mesoangioblasts were incubated with or without TNF (100 ng/ml), H2O2 (100 µM) or As2O3 (20 µM) for 24 hours. Cells were detached and stained with FITC-Annexin V and PI according to the manufacturer's instructions and analysed by flow cytometry as described (Sciorati et al., 1997). Cells showing single staining for Annexin V or double staining for Annexin V and PI were considered dead cells. To study the effect of cytotoxic T lymphocytes, 5x104 mesoangioblasts or control cells (splenocytes and RMA cells) were stained with the vital green fluorescent dye CFMDA (Perrotta et al., 2004) and incubated with increasing numbers of cytotoxic effector T cells (1:1, 1:5, 1:10, 1:25) (Ferrarini et al., 1999). Cell death was evaluated by flow cytometry measuring PI incorporation after 16 hours (Fischer et al., 2002).
Gene expression profiling
Biotin-labelled target synthesis as well as the Affymetrix Mouse Genome MOE430 GeneChip array hybridization and scanning were performed with Affymetrix instruments and by applying standard procedures and protocols on total RNA isolated from cultured cells using the RNeasy RNA isolation kit (Qiagen, Valencia, CA, USA). The amount of a transcript mRNA (signal) was determined using the GCOS 1.2 absolute analysis algorithm as already described (Liu et al., 2002).
RT-PCR
RNA (1 µg) collected from cells using an RNeasy Mini (or Micro) kit (Qiagen) was converted into double-stranded cDNA using the Thermoscript RT-PCR System cDNA synthesis kit (Invitrogen), according to the manufacturer's instructions. cDNA was then amplified using the following primers: Adam12 FW, 5'-ATCAGTGTCTTCGGCGTTC-3'; Adam12 Rev, 5'-GGCAATTCTTCCTGTTGTTA CATACC-3'; Adam15 Fw, 5'-GACCACTCCACAAGCATCTTAGG-3'; Adam15 Rev, 5'-GGGAGAATCATGGTCCAAACC-3'; Bax Fw, 5'-GGAATTCGCCGTGATGGACGGGTCCGG-3'; Bax Rev, 5'-GGAATTCTCAGCCCATCTTCTTCCAGA-3'; Bcl-2 Fw, 5'-TTCGGTGTAACTAAAGACAC-3'; Bcl-2 Rev, 5'-CTCAAAGAAGGCCACAATCC-3'; Bcl-XL Fw, 5'-GTGAGTGGACGGTCAGTG-3'; Bcl-XL Rev, 5'-TTGGACAATGGACTGGTTGA-3'; Cdh13 Fw, 5'-GACGCCTGACAAGCCATCTCCTAA-3'; Cdh 13 Rev, 5'-GACCCCCACAGCTCCCTCCTC-3'; Cdh15 Fw, 5'-CTTGGGTGCCACGGAGA-3'; Cdh15 Rev, 5'-ATGCAGGCCCTCGGAGAC-3'; Hgf Fw, 5'-CTTGGC ATCCACGATGTTCAT-3'; Hgf Rev, 5'-TGGTGCTGACTGCATTTCTCA-3'; Igf1 Fw, 5'-GTGGATGCTCTTCAGTTCGT-3'; Igf1 Rev, 5'-ACACTCC TAAAGACGATGTT-3'; Itgb1 Fw, 5'-TGTTCAGTGCAGAGCCTTCA-3'; Itgb1 Rev, 5'-CCTCATACTTCGGATTGACC-3'; Fst Fw, 5'-CTC TTCAAGTGGATGATTTTC-3'; Fst Rev, 5'-ACAGTAGGCATTATTG GTCTG-3'; Mmp11 Fw, 5'-ATTGATGCTGCCTTCCAGGAT-3'; Mmp11 Rev, 5'-GGGCGAGGAAAGCCTTCTAG-3'; Mmp19 Fw, 5'-GCCCATTTCCGG TCAGATG-3'; Mmp19 Rev, 5'-AGGGATCCTCC AGACCACAAC-3'; Tnfr1 Fw, 5'-CCACCATCTCGGTCATCAGGATTGCCT-3'; Tnfr1 Rev, 5'-TTCTCA TGGAAGCTATGGGTATCACA-3'; Met Fw, 5'-AGAAATTCATCAGGCTGTG AA GCGCG-3'; Met Rev, 5'-TTCCTCCGATCGCACACATTTGTCG-3'; Flt1 Fw, 5'-CAATGTGGAGAGCCGAGACA-3'; Flt1 Rev, 5'-GAGGTGTTGAAAG ACTGGAACGA-3'; GAPDH Fw, 5'-TGAAGGTCGGAGTCAACGGATTTGGT-3'; GAPDH Rev, 5'-CATGTGGGCCATGAGGTCCACCAC-3'.
Statistical analysis
The results are expressed as means ± s.e.m.; n represents the number of individual experiments. Statistical analysis was performed using the Student's t-test for unpaired variables (two-tailed). Asterisks and crosses in the figure panels refer to statistical probabilities vs. untreated controls or DETA-NO-treated cells, respectively. Statistical probability values (P) of less than 0.05 were considered significant.
|
Acknowledgments |
|---|
SG-null mice. This work was supported by grants from Telethon, the Association Française contre les Myopathies, CARIPLO, the European Community, Duchenne Parent Project Italia and the Italian Association of Cancer Research (AIRC). |
Footnotes |
|---|
|
References |
|---|
|
TopSummaryIntroductionResultsDiscussionMaterials and MethodsReferences |
|---|
Adams, V., Gielen, S., Hambrecht, R. and Schuler, G. (2001). Apoptosis in skeletal muscle. Front. Biosci. 6, D1-D11.[Medline]
Anderson, J. E. (2000). A role for nitric oxide in muscle repair: nitric oxide-mediated activation of muscle satellite cells. Mol. Biol. Cell. 11, 1859-1874.
Balon, T. W. and Nadler, J. L. (1997). Evidence that nitric oxide increases glucose transport in skeletal muscle. J. Appl. Physiol. 82, 359-363.
Beauchamp, J. R., Morgan, J. E., Pagel, C. N. and Partridge, T. A. (1999). Dynamics of myoblast transplantation reveal a discrete minority of precursors with stem cell-like properties as the myogenic source. J. Cell. Biol. 144, 1113-1122.
Blau, H. M., Chiu, C. P. and Webster, C. (1983). Cytoplasmic activation of human nuclear genes in stable heterocaryons. Cell 32, 1171-1180.[CrossRef][Medline]
Bredt, D. S. (1998). NO skeletal muscle derived relaxing factor in Duchenne muscular dystrophy. Proc. Natl. Acad. Sci. USA 95, 14592-14593.
Brunelli, S., Casey, E., Bell, D., Harland, R. and Lovell-Badge, R. (2003). Expression of Sox3 throughout the developing central nervous system is dependent on the combined action of discrete, evolutionarily conserved regulatory elements. Genesis 36, 12-24.[CrossRef][Medline]
Brunelli, S., Tagliafico, E., De Angelis, F. G., Tonlorenzi, R., Baesso, S., Ferrari, S., Niinobe, M., Yoshikawa, K., Schwartz, R. J., Bozzoni, I. et al. (2004). Msx2 and necdin combined activities are required for smooth muscle differentiation in mesoangioblast stem cells. Circ. Res. 94, 1571-1578.
Buckingham, M. (2001). Skeletal muscle formation in vertebrates. Curr. Opin. Genet. Dev. 11, 440-448.[CrossRef][Medline]
Bulotta, S., Barsacchi, R., Rotiroti, D., Borgese, N. and Clementi, E. (2001). Activation of the endothelial nitric-oxide synthase by tumor necrosis factor-alpha. A novel feedback mechanism regulating cell death. J. Biol. Chem. 276, 6529-6536.
Burgaud, J. L., Riffaud, J. P. and Del Soldato, P. (2002). Nitric-oxide releasing molecules: a new class of drugs with several major indications. Curr. Pharm. Des. 8, 201-213.[CrossRef][Medline]
Carmeli, E., Moas, M., Reznick, A. Z. and Coleman, R. (2004). Matrix metalloproteinases and skeletal muscle: a brief review. Muscle Nerve 29, 191-197.[CrossRef][Medline]
Carrasco, M., Canicio, J., Palacin, M., Zorzano, A. and Kaliman, P. (2002). Identification of intracellular signaling pathways that induce myotonic dystrophy protein kinase expression during myogenesis. Endocrinology 143, 3017-3025.
Charge, S. B. and Rudnicki, M. A. (2004). Cellular and molecular regulation of muscle regeneration. Physiol. Rev. 84, 209-238.
Clementi, E. and Meldolesi, J. (1997). The cross-talk between nitric oxide and Ca2+: a story with a complex past and a promising future. Trends Pharmacol. Sci. 18, 266-269.[Medline]
Clementi, E., Brown, G. C., Feelisch, M. and Moncada, S. (1998). Persistent inhibition of cell respiration by nitric oxide: crucial role of S-nitrosylation of mitochondrial complex I and protective action of glutathione. Proc. Natl. Acad. Sci. USA 95, 7631-7636.
Cossu, G. and Sampaolesi, M. (2004). New therapies for muscular dystrophy: cautious optimism. Trends Mol. Med. 10, 516-520.[CrossRef][Medline]
Cossu, G. and Biressi, S. (2005). Satellite cells, myoblasts and other occasional myogenic progenitors: possible origin, phenotypic features and role in muscle regeneration. Semin. Cell Dev. Biol. 16, 623-631.[CrossRef][Medline]
Duclos, F., Straub, V., Moore, S. A., Venzke, D. P., Hrstka, R. F., Crosbie, R. H., Durbeej, M., Lebakken, C. S., Ettinger, A. J., van der Meulen, J. et al. (1998). Progressive muscular dystrophy in alpha-sarcoglycan-deficient mice. J. Cell Biol. 142, 1461-1471.
Emery, A. E. (2002). The muscular dystrophies. Lancet 359, 687-695.[CrossRef][Medline]
Engvall, E. and Wewer, U. M. (2003). The new frontier in muscular dystrophy research: booster genes. FASEB J. 17, 1579-1584.
Eu, J. P., Hare, J. M., Hess, D. T., Skaf, M., Sun, J., Cardenas-Navina, I., Sun, Q. A., Dewhirst, M., Meissner, G. and Stamler, J. S. (2003). Concerted regulation of skeletal muscle contractility by oxygen tension and endogenous nitric oxide. Proc. Natl. Acad. Sci. USA 100, 15229-15234.
Falcone, S., Perrotta, C., De Palma, C., Pisconti, A., Sciorati, C., Capobianco, A., Rovere-Querini, P., Manfredi, A. A. and Clementi, E. (2004). Activation of acid sphingomyelinase and its inhibition by the nitric oxide/cyclic guanosine 3',5'-monophosphate pathway: key events in Escherichia coli-elicited apoptosis of dendritic cells. J. Immunol. 173, 4452-4463.
Ferrarini, M., Imro, M. A., Sciorati, C., Heltai, S., Protti, M. P., Pellicciari, C., Rovere, P., Manfredi, A. A. and Rugarli, C. (1999). Blockade of the Fas-triggered intracellular signaling pathway in human melanomas is circumvented by cytotoxic lymphocytes. Int. J. Cancer 81, 573-579.[CrossRef][Medline]
Fischer, K., Andreesen, R. and Mackensen, A. (2002). An improved flow cytometric assay for the determination of cytotoxic T lymphocyte activity. J. Immunol. Methods 259, 159-169.[CrossRef][Medline]
Galvez, B.G., Sampaolesi, M., Brunelli, S., Covarello, D., Gavina, M., Rossi, B., Costantin, G., Torrente, Y. and Cossu, G. (2006). Complete repair of dystrophic skeletal muscle by mesoangioblasts with enhanced migration ability. J. Cell Biol. 174, 231-243.
Garthwaite, J., Southam, E., Boulton, C. L., Nielsen, E. B., Schmidt, K. and Mayer, B. (1995). Potent and selective inhibition of nitric oxide-sensitive guanylyl cyclase by 1H-[1,2,4]oxadiazolo[4,3-a]quinoxalin-1-one. Mol. Pharmacol. 48, 184-188.[Abstract]
Glass, D. J. (2003). Molecular mechanisms modulating muscle mass. Trends Mol. Med. 9, 344-350.[CrossRef][Medline]
Hodgetts, S. I., Spencer, M. J. and Grounds, M. D. (2003). A role for natural killer cells in the rapid death of cultured donor myoblasts after transplantation. Transplantation 75, 863-871.[CrossRef][Medline]
Hohlfeld, R. and Engel, A. G. (1990). Lysis of myotubes by alloreactive cytotoxic T cells and natural killer cells. Relevance to myoblast transplantation. J. Clin. Invest. 86, 370-374.[Medline]
Horsley, V. and Pavlath, G. K. (2004). Forming a multinucleated cell: molecules that regulate myoblast fusion. Cells Tissues Organs 176, 67-78.[CrossRef][Medline]
Iezzi, S., Di Padova, M., Serra, C., Caretti, G., Simone, C., Maklan, E., Minetti, G., Zhao, P., Hoffman, E. P., Puri, P. L. et al. (2004). Deacetylase inhibitors increase muscle cell size by promoting myoblast recruitment and fusion through induction of follistatin. Dev. Cell 6, 673-684.[CrossRef][Medline]
Kaliman, P., Canicio, J., Testar, X., Palacin, M. and Zorzano, A. (1999). Insulin-like growth factor-II, phosphatidylinositol 3-kinase, nuclear factor-kappaB and inducible nitric-oxide synthase define a common myogenic signaling pathway. J. Biol. Chem. 274, 17437-17444.
Krauss, R. S., Cole, F., Gaio, U., Takaesu, G., Zhang, W. and Kang, J. S. (2005). Close encounters: regulation of vertebrate skeletal myogenesis by cell-cell contact. J. Cell Sci. 118, 2355-2362.
Liu, L. and Stamler, J. S. (1999). NO: an inhibitor of cell death. Cell Death Differ. 6, 937-942.[CrossRef][Medline]
Liu, W. M., Mei, R., Di, X., Ryder, T. B., Hubbell, E., Dee, S., Webster, T. A., Harrington, C. A., Ho, M. H., Baid, J. et al. (2002). Analysis of high density expression microarrays with signed-rank call algorithms. BioInformatics 18, 1593-1599.
Manzur, A. Y., Kuntzer, T., Pike, M. and Swan, A. (2004). Glucocorticoid corticosteroids for Duchenne muscular dystrophy. Cochrane Database Syst. Rev., CD003725.
Minasi, M. G., Riminucci, M., De Angelis, L., Borello, U., Berarducci, B., Innocenzi, A., Caprioli, A., Sirabella, D., Baiocchi, M., De Maria, R. et al. (2002). The meso-angioblast: a multipotent, self-renewing cell that originates from the dorsal aorta and differentiates into most mesodermal tissues. Development 129, 2773-2783.
Moncada, S., Palmer, R. M. and Higgs, E. A. (1991). Nitric oxide: physiology, pathophysiology, and pharmacology. Pharmacol Rev. 43, 109-142.[Medline]
Nakane, M. (2003). Soluble guanylyl cyclase: physiological role as an NO receptor and the potential molecular target for therapeutic application. Clin. Chem. Lab. Med. 41, 865-870.[CrossRef][Medline]
Nisoli, E., Falcone, S., Tonello, C., Cozzi, V., Palomba, L., Fiorani, M., Pisconti, A., Brunelli, S., Cardile, A., Francolini, M. et al. (2004). Mitochondrial biogenesis by NO yields functionally active mitochondria in mammals. Proc. Natl. Acad. Sci. USA 101, 16507-16512.
Palumbo, R., Sampaolesi, M., De Marchis, F., Tonlorenzi, R., Colombetti, S., Mondino, A., Cossu, G. and Bianchi, M. E. (2004). Extracellular HMGB1, a signal of tissue damage, induces mesoangioblast migration and proliferation. J. Cell Biol. 164, 441-449.
Perrotta, C., Falcone, S., Capobianco, A., Camporeale, A., Sciorati, C., De Palma, C., Pisconti, A., Rovere-Querini, P., Bellone, M., Manfredi, A. A. et al. (2004). Nitric oxide confers therapeutic activity to dendritic cells in a mouse model of melanoma. Cancer Res. 64, 3767-3771.
Pilz, R. B. and Casteel, D. E. (2003). Regulation of gene expression by cyclic GMP. Circ. Res. 93, 1034-1046.
Pisconti, A., Brunelli, S., Di Padova, M., De Palma, C., Deponti, D., Baesso, S., Sartorelli, V., Cossu, G. and Clementi, E. (2006). Follistatin induction by nitric oxide through cyclic GMP: a tightly regulated signaling pathway that controls myoblast fusion. J. Cell Biol. 172, 233-244.
Puri, K. D., Doggett, T. A., Douangpanya, J., Hou, Y., Tino, W. T., Wilson, T., Graf, T., Clayton, E., Turner, M., Hayflick, J. S. et al. (2004). Mechanisms and implications of phosphoinositide 3-kinase delta in promoting neutrophil trafficking into inflamed tissue. Blood 103, 3448-3456.
Rando, T. A., Disatnik, M. H., Yu, Y. and Franco, A. (1998). Muscle cells from mdx mice have an increased susceptibility to oxidative stress. Neuromuscul. Disord. 8, 14-21.[CrossRef][Medline]
Sampaolesi, M., Torrente, Y., Innocenzi, A., Tonlorenzi, R., D'Antona, G., Pellegrino, M. A., Barresi, R., Bresolin, N., De Angelis, M. G., Campbell, K. P. et al. (2003). Cell therapy of alpha-sarcoglycan null dystrophic mice through intra-arterial delivery of mesoangioblasts. Science 301, 487-492.
Sciorati, C., Rovere, P., Ferrarini, M., Heltai, S., Manfredi, A. A. and Clementi, E. (1997). Autocrine nitric oxide modulates CD95-induced apoptosis in gammadelta T lymphocytes. J. Biol. Chem. 272, 23211-23215.
Shen, W., Xu, X., Ochoa, M., Zhao, G., Wolin, M. S. and Hintze, T. H. (1994). Role of nitric oxide in the regulation of oxygen consumption in conscious dogs. Circ. Res. 75, 1086-1095.
Skuk, D., Vilquin, J. T. and Tremblay, J. P. (2002). Experimental and therapeutic approaches to muscular dystrophies. Curr. Opin. Neurol. 15, 563-569.[CrossRef][Medline]
Stamler, J. S. and Meissner, G. (2001). Physiology of nitric oxide in skeletal muscle. Physiol. Rev. 81, 209-237.
Tatsumi, R., Hattori, A., Ikeuchi, Y., Anderson, J. E. and Allen, R. E. (2002). Release of hepatocyte growth factor from mechanically stretched skeletal muscle satellite cells and role of pH and nitric oxide. Mol. Biol. Cell 13, 2909-2918.
Tews, D. S. and Goebel, H. H. (1996). Cytokine expression profile in idiopathic inflammatory myopathies. J. Neuropathol. Exp. Neurol. 55, 342-347.[Medline]
Wagers, A. J. and Conboy, I. M. (2005). Cellular and molecular signatures of muscle regeneration: current concepts and controversies in adult myogenesis. Cell 122, 659-667.[CrossRef][Medline]
Wang, T., Xie, Z. and Lu, B. (1995). Nitric oxide mediates activity-dependent synaptic suppression at developing neuromuscular synapses. Nature 374, 262-266.[CrossRef][Medline]
Wolosker, H., Rocha, J. B., Engelender, S., Panizzutti, R., De Miranda, J. and de Meis, L. (1997). Sarco/endoplasmic reticulum Ca2+-ATPase isoforms: diverse responses to acidosis. Biochem. J. 321, 545-550.
Yamamoto, T. and Bing, R. J. (2000). Nitric oxide donors. Proc. Soc. Exp. Biol. Med. 225, 200-206.
CiteULike 
Complore 
Connotea 
Del.icio.us 
Digg 
Reddit 
Technorati 
Twitter What's this?
Related articles in JCS:
This article has been cited by other articles:
|
|
 |
|
  D. Deponti, R. Buono, G. Catanzaro, C. De Palma, R. Longhi, R. Meneveri, N. Bresolin, M. T. Bassi, G. Cossu, E. Clementi, et al. The Low-Affinity Receptor for Neurotrophins p75NTR Plays a Key Role for Satellite Cell Function in Muscle Repair Acting via RhoA Mol. Biol. Cell, August 15, 2009; 20(16): 3620 - 3627. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 K. Lolmede, L. Campana, M. Vezzoli, L. Bosurgi, R. Tonlorenzi, E. Clementi, M. E. Bianchi, G. Cossu, A. A. Manfredi, S. Brunelli, et al. Inflammatory and alternatively activated human macrophages attract vessel-associated stem cells, relying on separate HMGB1- and MMP-9-dependent pathways J. Leukoc. Biol., May 1, 2009; 85(5): 779 - 787. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 C. Colussi, C. Mozzetta, A. Gurtner, B. Illi, J. Rosati, S. Straino, G. Ragone, M. Pescatori, G. Zaccagnini, A. Antonini, et al. HDAC2 blockade by nitric oxide and histone deacetylase inhibitors reveals a common target in Duchenne muscular dystrophy treatment PNAS, December 9, 2008; 105(49): 19183 - 19187. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 D. Deponti, S. Francois, S. Baesso, C. Sciorati, A. Innocenzi, V. Broccoli, F. Muscatelli, R. Meneveri, E. Clementi, G. Cossu, et al. Necdin mediates skeletal muscle regeneration by promoting myoblast survival and differentiation J. Cell Biol., October 22, 2007; 179(2): 305 - 319. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 C. Perrotta, L. Bizzozero, S. Falcone, P. Rovere-Querini, A. Prinetti, E. H. Schuchman, S. Sonnino, A. A. Manfredi, and E. Clementi Nitric Oxide Boosts Chemoimmunotherapy via Inhibition of Acid Sphingomyelinase in a Mouse Model of Melanoma Cancer Res., August 15, 2007; 67(16): 7559 - 7564. [Abstract] [Full Text] [PDF]
|
|
| |||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||
