The dystrophin glycoprotein complex links laminin in the extracellular matrix to the cell cytoskeleton. Loss of dystrophin causes Duchenne muscular dystrophy, the most common human X-chromosome-linked genetic disease. The α7β1 integrin is a second transmembrane laminin receptor expressed in skeletal muscle. Mutations in the α7 integrin gene cause congenital myopathy in humans and mice. The α7β1 integrin is increased in the skeletal muscle of Duchenne muscular dystrophy patients and mdx mice. This observation has led to the suggestion that dystrophin and α7β1 integrin have complementary functional and structural roles. To test this hypothesis, we generated mice lacking both dystrophin and α7 integrin (mdx/α7-/-). The mdx/α7-/- mice developed early-onset muscular dystrophy and died at 2-4 weeks of age. Muscle fibers from mdx/α7-/- mice exhibited extensive loss of membrane integrity, increased centrally located nuclei and inflammatory cell infiltrate, greater necrosis and increased muscle degeneration compared to mdx or α7-integrin null animals. In addition, loss of dystrophin and/or α7 integrin resulted in altered expression of laminin-α2 chain. These results point to complementary roles for dystrophin and α7β1 integrin in maintaining the functional integrity of skeletal muscle.
Duchenne muscular dystrophy (DMD) is the most common X-chromosome-linked human disease that affects approximately 1 in 3,500 males. DMD patients suffer from severe, progressive muscle wasting with clinical symptoms first detected between 2 and 5 years of age. As the disease progresses, patients are confined to a wheelchair in their early teens and die in their early twenties from cardiopulmonary failure (Emery, 1993; Moser, 1984). DMD patients and mdx mice have dystrophin gene mutations that result in an absence of the dystrophin protein (Bulfield et al., 1984; Campbell, 1995; Matsumura et al., 1992; Monaco et al., 1986; Sicinski et al., 1989). Dystrophin is localized to the cytoplasmic face of the plasma membrane and mediates the interaction between the cell cytoskeleton and the extracellular matrix (ECM) through a complex of associated glycoproteins called the dystrophin-glycoprotein complex (DGC). In skeletal muscle, the DGC is localized along muscle fibers and at myotendinous and neuromuscular junctions (MTJs and NMJs, respectively). This complex includes dystroglycans, sarcoglycans and syntrophins (Suzuki et al., 1994). Dystrophin interacts with F-actin through its N-terminus (Way et al., 1992). The C-terminus interacts with syntrophins and with the cytoplasmic tail of β-dystroglycan (Henry and Campbell, 1996). α-dystroglycan binds to laminin in the extracellular matrix. Overall, the DGC links the muscle cell cytoskeleton to the extracellular matrix and maintains sarcolemmal integrity.
In DMD patients, loss of dystrophin results in a disruption of the DGC-extracellular matrix linkage. This leads to the loss of sarcolemmal integrity, unregulated influx of Ca2+ into muscle cells, activation of Ca2+-dependent proteases and muscle degeneration (Gillis, 1996). Muscle degeneration is accompanied by regeneration through the activation of muscle satellite cells; however, regenerative capacity in DMD patients is exceeded by progressive muscle degeneration. This results in the replacement of muscle fibers with adipose and connective tissue (O'Brien and Kunkel, 2001).
The mdx mouse is a valuable model for DMD and has been used extensively to analyze the progression of muscle disease. Although DMD patients (Monaco et al., 1986) and mdx mice (Bulfield et al., 1984; Sicinski et al., 1989) both lack dystrophin, the mdx mouse develops less severe muscle pathology compared with DMD patients, and has a normal life span. Several factors may explain the reduced pathology in mdx mice including differences in muscle use between humans and captive mice. In addition, mdx mice might compensate for the loss of dystrophin, possibly by overexpressing one or more proteins with functional similarity to dystrophin. One candidate protein is utrophin, an autosomal homolog of dystrophin that is expressed at the post-synaptic membrane of the NMJ in adult skeletal muscle. Utrophin is upregulated in the muscle of both DMD patients and mdx mice and is localized at extrajunctional sites (Ohlendieck et al., 1991; Pons et al., 1991). Overexpression of utrophin can rescue the dystrophic phenotype in mdx mice (Deconinck et al., 1997b; Rafael et al., 1998; Squire et al., 2002; Tinsley et al., 1998; Tinsley et al., 1996). Mice that lack utrophin show mild neuromuscular defects (Deconinck et al., 1997a; Grady et al., 1997a). By contrast, mice lacking both utrophin and dystrophin (mdx/utr-/- mice) develop severe muscular dystrophy and cardiomyopathy similar to that of DMD patients, and die between 4-14 weeks of age (Deconinck et al., 1997b; Grady et al., 1997b).
The α7β1 integrin is a second laminin receptor in skeletal muscle (Burkin and Kaufman, 1999). Like the DGC, α7β1 integrin serves as a structural link between the cell cytoskeleton and laminin in the basal lamina and, therefore, contributes to the overall integrity of the sarcolemma. Mutations in the α7-integrin gene are responsible for human congenital myopathy, in which patients exhibit delayed motor milestones (Hayashi et al., 1998). Mice that lack α7 integrin develop myopathy and demonstrate altered force transmission, compliance and viscoelasticity in diaphragm muscle (Lopez et al., 2005; Mayer et al., 1997). In addition, α7β1 integrin plays an important role in the development of NMJs (Burkin et al., 1998; Burkin et al., 2000) and MTJs (Mayer et al., 1997; Nawrotzki et al., 2003). These junctional sites are often damaged in diseased muscle (Lyons and Slater, 1991; Nagel et al., 1990; Nawrotzki et al., 2003; Rafael et al., 2000).
Increased amounts of α7 integrin are found in DMD patients and mdx mice (Hodges et al., 1997). These observations suggest that enhanced α7 integrin expression is a mechanism by which muscle can compensate for the loss of dystrophin. This hypothesis was supported by transgenic overexpression of the α7-integrin chain which alleviated the severe muscular dystrophy and extended the life-span of mice that lacked dystrophin and utrophin (Burkin et al., 2001; Burkin et al., 2005). These observations suggest potential structural and functional overlap between the α7β1 integrin and DGC.
To explore the structural and functional overlap between dystrophin and α7β1 integrin, we generated mice that lack both laminin-binding complexes (mdx/α7-/- mice). These mice exhibited more severe muscular dystrophy than either mdx- or α7-integrin-deficient animals and died at 2-4 weeks of age. In addition, the muscle of 3-week-old mdx/α7-/- mice showed inflammation and centrally located nuclei, indicative of severe muscle damage and increased requirement for muscle repair. Finally, loss of dystrophin and/or α7 integrin resulted in reduced laminin-α2-chain expression in skeletal muscle, demonstrating regulation of laminin expression by α7β1 integrin. Collectively, these studies support functional and structural overlap between DGC and α7β1 integrin in maintaining the integrity of skeletal muscle.
mdx/α7-/- mice exhibit muscle wasting and reduced viability
To determine whether functional overlap exists between dystrophin and α7β1 integrin, mdx mice were bred with mice that lack the α7-integrin gene (Flintoff-Dye et al., 2005) to produce mice that lack both dystrophin and α7 integrin (mdx/α7-/-). Mutations in the dystrophin and α7 integrin genes were confirmed by genotyping (Fig. 1A). Multiplex PCR detected a 482 bp product representing the targeted α7-integrin allele in both the α7-/- and mdx/α7-/- mice, whereas the wild-type allele was 727 bp. Amplification-resistant mutation system (ARMS) PCR yielded a 275 bp product and confirmed the presence of the mdx mutation in mdx and mdx/α7-/- mice (Fig. 1A). Loss of α7 protein was confirmed by immunoblotting. Western analysis demonstrated that both α7A-integrin and α7B-integrin isoforms were missing in mdx/α7-/- mice (Fig. 1B). The absence of both dystrophin and α7 integrin in the skeletal muscle of mdx/α7-/- mice was confirmed by immunofluorescence (Fig. 1C).
At 10 days of age, the average weight of male wild-type, mdx, α7-/- or mdx/α7-/- pups was 7.9±0.2 g, 6.3±0.9 g, 7.8±0.17 g or 5.6±0.45 g, respectively (Fig. 2B). The weight of mdx and mdx/α7-/- littermates was statistically different from wild-type and α7-/- mice (P<0.05), but was not different from each other. By day 18, mdx/α7-/- mice exhibited a failure to thrive and appeared smaller compared with mdx littermates (Fig. 2A). By day 21, male mdx/α7-/- mice weighed only 5.05±0.51 g (n=8), less than half the weight of wild-type (11.89±0.83 g, n=5), mdx (9.86±0.15 g, n=7) or α7-/- (13.04±0.54 g, n=9) animals, indicating that double-knockout mice failed to gain weight (Fig. 2C). mdx/α7-/- animals displayed kyphosis, joint contractures of the limbs, an abnormal waddling gate, tremors and reduced mobility (a movie that contrasts mobility, joint contractures, tremor and gait in mdx and mdx/α7-/- mice can be viewed as supplementary material, Movie 1). This debilitating phenotype progressed rapidly, resulting in the death of these mice at day 16-26 (Fig. 2D).
Muscle membrane integrity is compromised in mdx/α7-/- mice
To evaluate skeletal muscle integrity, mice were injected with Evan's Blue dye (EBD). EBD binds albumin, fluoresces red and can enter cells with compromised plasma membranes. At 3 weeks, wild-type and α7-/- mice showed no evidence of EBD uptake, signifying that the sarcolemma was undamaged in these animals (Fig. 3A). By contrast, myofibers from both mdx and dystrophin/α7 double-knockout mice showed considerable EBD uptake (Fig. 3A). Muscle from mdx and mdx/α7-/- mice had 14.6% and 18.9% EBD-positive fibers, respectively; however, these were not significantly different from each other (Fig. 3B). These data indicate that the loss of dystrophin but not α7 integrin, in the skeletal muscle of 3-week-old mice decreases sarcolemmal integrity.
mdx/α7-/- mice exhibit severe muscle pathology
To investigate whether the skeletal muscle from mdx/α7-/- mice exhibited greater pathology compared with controls, muscle sections were stained with hematoxylin and eosin. Skeletal muscle from 3-week-old wild-type and α7-/- mice showed no pathology (Fig. 4A). By comparison, skeletal muscle from 3-week-old mdx mice exhibited small necrotic lesions (Fig. 4A). By contrast, skeletal muscle from mdx/α7-/- mice exhibited severe pathology including variation in myofiber size, large necrotic regions and areas of mononuclear cell infiltration (Fig. 4A). These data demonstrate that the skeletal muscle of 3-week-old mdx/α7-/- mice has undergone increased muscle degeneration compared with wild-type, mdx or α7-integrin null animals.
Earlier studies have implicated inflammation in the pathogenesis of muscular dystrophy (McDouall et al., 1990; Tews and Goebel, 1996). To assess the inflammatory response in mice lacking dystrophin and α7 integrin, tissue cryosections from the triceps muscle of 3-week-old wild-type, mdx, α7-/- and mdx/α7-/- mice were incubated with anti-CD4 antibody. CD4 is a type-I membrane glycoprotein expressed on thymocytes, and to some extent, monocytes and macrophage-related cells. There was on average less than 1 CD4-positive cell per field of view from each of the control genotypes (Fig. 4B). By contrast, an average of 44 CD4-positive cells per field was observed in the muscle of mdx/α7-/- mice. These results demonstrate that mdx/α7-/- mice experienced an increased inflammatory response in skeletal muscle compared with wild-type, mdx or α7-integrin null animals at 3 weeks of age.
Increased muscle regeneration in mdx/α7-/- mice
To examine the extent of skeletal muscle regeneration in mdx/α7-/- mice, fibers containing centrally located nuclei in triceps and tibialis anterior muscles were counted and compared with control genotypes. As expected, skeletal muscle from wild-type mice had few centrally located nuclei (Fig. 5A-B). By comparison, the tibialis anterior muscle from 3-week-old mdx and α7-/- mice showed 4.1% and 3.2% fibers with centrally located nuclei, respectively (Fig. 5B). Their triceps muscle showed 2.8% and 0.3% of muscle fibers with centrally located nuclei, respectively, which was not statistically significant from the wild-type controls (Fig. 5B). By contrast, 17.8% of muscle fibers in the tibialis anterior muscle and 40.1% of muscle fibers from the triceps muscle from mdx/α7-/- contained centrally located nuclei (Fig. 5B). These results suggest an earlier onset of regeneration in response to muscle fiber damage in mdx/α7-/- mice.
Embryonic myosin heavy chain (eMyHC) expression was examined as a second measure of muscle regeneration. Consistent with data obtained from the analysis of centrally located nuclei in muscle fibers, a significant increase in the number of eMyHC-positive fibers was observed in 3-week-old mdx/α7-/- muscle. As expected, wild-type muscle showed only 0.3 eMyHC-positive fibers per field. Muscle from 3-week-old mdx and α7-/- mice showed 0.2 and 0.1 eMyHC-positive fibers per field, respectively. By contrast, 7.5 eMyHC-positive fibers per field of view were counted in muscle from mdx/α7-/- mice (Fig. 6B). Collectively, these data indicate that loss of dystrophin and α7 integrin results in more muscle regeneration in mdx/α7-/- mice at the age of 3 weeks compared with wild-type, mdx or α7 integrin deficient animals.
Altered expression of laminin-α2-chain expression in α7-/- and mdx/α7-/- mice
In mature skeletal muscle, the α7-integrin chain preferentially associates with the β1D subunit and binds to laminin-211 and laminin-221 in the extracellular matrix. The α7β1 integrin has also been shown to regulate laminin deposition (Li et al., 2003). Immunoblotting and immunofluorescence were undertaken to determine whether the absence of α7, coupled with the loss of dystrophin, affected the expression and localization of β1D integrin, utrophin and/or laminin. Wild-type, mdx, α7-/- and mdx/α7-/- mice exhibited similar amounts of β1D integrin in skeletal muscle (Fig. 7A), which was confirmed by western analysis (data not shown).
Immunofluorescence revealed an increase in laminin-α2-chain expression in mdx mice and downregulation in the muscle of α7-/- and mdx/α7-/- mice (Fig. 7A). This was confirmed by quantitative western analysis with laminin-α2 bands normalized for protein loading to the constitutively and ubiquitously expressed protein cyclooxygenase-1 (Cox-1). Expression of Cox-1 did not appear to change in wild-type or diseased states. In mdx mice an increase in laminin-α2 chain was detected compared with wild-type muscle. By contrast, a 7.4-fold decrease in laminin-α2 protein was observed in the muscle of α7-integrin-deficient mice and a 3.3-fold decrease was observed in mdx/α7-/- mice compared with wild-type animals (Fig. 7B). These results indicate that loss of α7 integrin led to reduced deposition of laminin-211 or laminin-221 in the basal lamina of muscle.
Utrophin expression was assayed with two independent anti-utrophin antibodies (MANCHO3 and MANCHO7). Utrophin is normally localized at MTJs and NMJs in adult mice (Law et al., 1994). Utrophin was localized at the NMJs of 3-week-old wild-type mice. As previously reported, utrophin expression was increased and localized at neuromuscular and extrajunctional sites in 3-week-old mdx mice (Law et al., 1994). In α7-/- and mdx/α7-/- mice, utrophin appeared localized at junctional and extrajunctional sites (Fig. 8A). Western blot analysis revealed a significant increase in utrophin expression in mdx mice (P<0.05, n=3 mice per genotype) compared with wild-type animals (Fig. 8B), which confirms previous reports. Utrophin levels in the gastrocnemius muscle from α7 and mdx/α7-/- mice were similar to those observed in wild-type animals (Fig. 8). These results indicate that the loss of dystrophin alone resulted in increased utrophin. However, the additional loss of the α7 integrin did not result in an increase in utrophin expression in the skeletal muscle of mdx/α7-/- mice.
Structural changes in the MTJs of α7 and mdx/α7-/- mice
Since the α7β1 integrin and dystrophin are localized at MTJs and loss of α7 integrin has been shown to result in defective matrix deposition at this site (Mayer et al., 1997; Nawrotzki et al., 2003), we compared the ultrastructure of the MTJs from 3-week-old wild-type, mdx, α7-/- and mdx/α7-/- mice (Fig. 9). Longitudinal sections were prepared from the gastrocemius muscle and examined by electron microscopy. The MTJs of wild-type and mdx mice showed extensive sarcolemmal folding (Fig. 9, arrows) increasing the contact area between muscle and tendon; also, a highly organized, continuous and dense extracellular matrix was observed. By contrast, the MTJs of α7-/- mice showed few sarcolemmal folds (Fig. 9, arrows) indicating loss of structural integrity at this site. The extracellular matrix appeared less organized and was not as electron-dense as wild-type or mdx tissue confirming previous observations (Fig. 9, arrowheads) (Mayer et al., 1997; Nawrotzki et al., 2003). Like those of α7-integrin-deficient mice, the MTJs of mdx/α7-/- mice showed few sarcolemmal folds (arrow) and altered deposition of extracellular matrix (Fig. 9, arrowheads). In addition to these structural changes, mdx/α7-/- mice also showed mononuclear cell infiltrate at this junctional site.
The dystrophin glycoprotein complex and α7β1 integrin are transmembrane receptors in skeletal muscle that provide molecular continuity between laminin in the extracellular matrix and the cell cytoskeleton. Disruption of either receptor leads to neuromuscular disease in both humans and mice reflecting the importance of both complexes in maintaining muscle integrity (Emery, 1993; Hayashi et al., 1998; Mayer et al., 1997; Monaco et al., 1986; Moser, 1984; Sicinski et al., 1989). Levels of the α7-integrin chain are increased twofold in the muscle of DMD patients and mdx mice (Hodges et al., 1997). Transgenic overexpression of α7 integrin in the skeletal muscle of severely dystrophic mdx/utr-/- mice can partially rescue the diseased phenotype and extend the lifespan of these animals without restoring the expression of DGC components (Burkin et al., 2001; Burkin et al., 2005). Together, these results suggest the DGC and α7β1 integrin have overlapping and compensatory functions. The severe muscle phenotype and premature death of the mdx/α7-/- mice reported in this study further extends these studies, and supports the hypothesis that dystrophin and the α7β1 integrin have overlapping roles in maintaining the structural and functional integrity of skeletal muscle. We observed only mild muscle pathology in 3-week-old α7-/- and mdx mice, which is consistent with previously reported studies (Grady et al., 1997b; Mayer et al., 1997). By contrast, the absence of both proteins in mdx/α7-/- mice results in severe muscle degeneration, variation in myofiber size and inflammatory cell infiltration.
The muscle pathology of mice that lack dystrophin and utrophin is similar to that seen in DMD patients (Deconinck et al., 1997b; Grady et al., 1997b). Utrophin is an autosomal homolog of dystrophin localized to junctional sites in adult skeletal muscle (Blake et al., 1996). In mdx mice, utrophin is increased and is localized at extrajunctional sites were it replaces dystrophin and associates with an otherwise normal dystrophin-associated protein complex (Matsumura et al., 1992). Mice that lack dystrophin and utrophin have a mean life span of 14 weeks (Burkin et al., 2001; Deconinck et al., 1997b; Grady et al., 1997b), whereas mice that lack dystrophin and α7 integrin all die before the age of 4 weeks. These results indicate that compensation by α7 integrin allows mdx/utr-/- mice to live longer. This hypothesis is supported by the partial rescue of the dystrophic phenotype in mdx/utr-/- mice by transgenic expression of α7 integrin, which extends the life span of these animals approximately threefold (Burkin et al., 2001; Burkin et al., 2005). By contrast, endogenous expression of utrophin in mdx/α7-/- mice appears to be unable to compensate to the same extent for the loss of α7 integrin and dystrophin. Interestingly, the loss of dystrophin and α7 integrin does not result in increased utrophin expression as seen in the skeletal muscle of mdx mice.
The mdx/α7-/- mice analyzed in this study exhibit a phenotype similar to mice deficient in α7-integrin and γ-sarcoglycan (Allikian et al., 2004). The phenotypic similarity between these mice suggests that functional overlap exists between γ-sarcoglycan in the dystrophin complex and α7β1 integrin. Alternatively, loss of γ-sarcoglycan might affect the stability of the dystrophin-glycoprotein complex, resulting in the observed phenotypic similarity (Hack et al., 2000b; Hack et al., 2000a; Zhu et al., 2001). The production and analysis of double-knockout mice lacking α7 integrin and other sarcoglycan subunits may elucidate further the functional overlap between members of the sarcoglycan complex and α7 integrin.
EBD uptake in the muscle of mdx/α7-/- mice was similar to that observed in mdx animals, implying that loss of dystrophin is responsible for the observed membrane damage in both groups of animals. Prior investigations have shown that the height of muscle degeneration and its ensuing regeneration in mdx mice occurs at 4-6 weeks of age (Grady et al., 1997b; McGeachie et al., 1993). By conducting the present studies in 3-week-old mice, only the onset of changes in membrane permeability in mdx muscle fibers was observed. This concept of age-dependency was further supported by the extensive muscle damage and centrally located nuclei observed in mdx/α7-/- mice compared with the single-knockout phenotypes. The absence of both dystrophin and α7 integrin resulted in significantly more centrally located nuclei and eMyHC expression in skeletal muscle fibers compared with control genotypes. Therefore, our data indicate that mdx/α7-/- mice have a requirement for increased muscle regeneration compared with mdx or α7-integrin null animals. Compromised contractile function or too little muscle regeneration might be mechanisms underlying the severe muscle damage observed in the mdx/α7-/- mice.
The severe muscle pathology observed in mdx/α7-/- mice is similar to that reported in laminin-α2-deficient mice (Miyagoe-Suzuki et al., 2000). The skeletal muscle of laminin-α2 null mice show reduced expression of α7 integrin (Hodges et al., 1997). Our data showed increased endogenous expression of both α7-integrin and laminin-α2 proteins in the muscle of mdx mice. Although α7 deficient mice exhibit decreased levels of laminin-α2 in skeletal muscle, these mice live beyond 20 weeks of age. These observations suggest that levels of laminin, dystrophin and utrophin in α7-integrin-deficient mice are sufficient to maintain muscle integrity. A further reduction in laminin-α2-chain expression was not observed in mdx/α7-/- mice compared with α7-/- animals, indicating that the loss of the laminin-α2 chain is primarily due to the loss of α7 integrin. Together, these data support the idea that, in skeletal muscle, a regulatory mechanism exists between the expression of α7 integrin and the laminin-α2 chain. This mechanism might also be involved in the rescue of severely dystrophic mice by the transgenic overexpression of α7 integrin (Burkin et al., 2001). Interestingly, utrophin and laminin expression are upregulated in mdx mice, but not mdx/α7-/- mice, suggesting the possibility that utrophin expression is regulated by laminin.
The inflammatory response to chronic muscle-fiber damage is believed to be a major factor contributing to the progression of pathology observed in DMD patients (Gorospe et al., 1994; Gosselin and McCormick, 2004). Muscle of mdx mice shows changes in the expression of genes involved in the inflammatory response (Porter et al., 2002). A significant inflammatory response was observed in the skeletal muscle and MTJs of mdx/α7-/- mice compared with mdx or α7-integrin-deficient animals at 3 weeks of age. These observations suggest that loss of dystrophin and integrin protein complexes lead to decreased extracellular matrix-to-muscle-cell contacts within muscle and at critical junctional sites, resulting in increased muscle-fiber damage and inflammation.
Although our data support the model of overlapping structural roles for dystrophin and α7 integrin in maintaining the integrity of the sarcolemma, it is also possible that these proteins have functionally intersecting cell-signaling pathways that regulate muscle survival because both mdx and laminin-deficient mice show increased apoptosis (Ruegg et al., 2002; Tidball et al., 1995; Tombes et al., 1995). Integrins exhibit mechanotransduction ability, and the binding of extracellular ligands or integrin-clustering can initiate cell signaling through proteins such as focal adhesion kinase or phosphoinisitol-3-kinase (Schlaepfer et al., 1999; Schwartz, 2001). Interestingly, signaling through FAK and the adaptor molecule growth-factor-receptor-binding protein 2 (Grb2) can lead to activation of the mitogen-activated protein kinase (MAPK) pathway (Schlaepfer et al., 1994), which promotes cell survival (Bonni et al., 1999).
Evidence that dystrophin and other members of the DCG have cell-signaling capacities that regulate cell survival and growth is beginning to emerge. Dystrophin itself can become phosphorylated, which can alter its affinity for actin (Senter et al., 1993). Calmodulin binding sites are present on both dystrophin and syntrophin (Madhavan et al., 1992), which link the DGC to Ca2+/calmodulin-dependent protein kinase II (CaMKII)-mediated signaling (Rando, 2001). Neuronal nitric oxide synthase (nNOS), which regulates many signaling pathways, is also associated with DGC (Abdelmoity et al., 2000). Finally, Grb2 can bind to β-dystroglycan (Yang et al., 1995) and may therefore be a point of convergence between dystrophin and integrins.
Recently, several genes have been identified that appear to compensate for the loss of dystrophin. Using a complementary gene therapy approach, these `booster' genes have been overexpressed in skeletal muscle of dystrophic mouse models and were shown to rescue the diseased phenotype (Engvall and Wewer, 2003). These complementary proteins include utrophin, α7 integrin, GalNac, nNOS and Adam12 (Burkin et al., 2001; Moghadaszadeh et al., 2003; Nguyen et al., 2002; Tidball and Wehling-Henricks, 2004; Tinsley et al., 1998). By taking advantage of single- and double-knockout mice, this study has identified areas of structural and functional convergence and independence between the α7β1 integrin and dystrophin protein complexes. Understanding the functional overlap between each of the complementary proteins and dystrophin might identify new pathways that can be targeted to treat muscular dystrophy.
Materials and Methods
Generation of mdx/α7-/- mice
α7-/- mice (C57BL6-α7βgal strain) produced in the Nevada Transgenic Center (Flintoff-Dye et al., 2005) were bred with mdx (C57BL10ScSn-Dmd strain) female animals. The resulting F1 males, which were heterozygous at the α7 locus, were backcrossed with mdx (C57BL10ScSn-Dmd strain) females. Males and females produced in the F2 generation that were heterozygous at the α7 locus were bred to generate mdx/α double-knockout mice. The wild-type control strain used in this study was C57BL10ScSn. Male littermates or age-matched mice were used for analysis.
To genotype mice, genomic DNA was isolated from tail clips using a Wizard SV DNA purification system (Promega, Madison, WI) following the manufacturer's instructions. Mice were genotyped by multiplex PCR to detect the wild-type and targeted α7-integrin alleles with the following primers: α7PF10 (5′-TGAAGGAATGAGTGCACAGTGC-3′), α7exon1R1 (5′-AGATGCCTGTGGGCAGAGTAC-3′) and βgalR2 (5′-GACCTGCAGGCATGCAAGC-3′). PCR conditions were as follows: 95°C for 4 minutes then 34 cycles at 95°C for 1 minute, 62°C for 1 minute and 72°C for 1 minute. A wild-type band was 727 bp, whereas the α7-integrin-targeted allele produced a 482 bp band.
The mutation in the dystrophin gene was detected by a modified ARMS assay (Amalfitano and Chamberlain, 1996; Burkin et al., 2001). The following primers were used: p259E (5′-GTCACTCAGATAGTTGAAGCCATTTAA-3′), p260E (5′-GTCACTCAGATAGTTGAAGCCATTTAG-3′) and p306F (5′-CATAGTTATTAATGCATAGATATTCAG-3′). PCR conditions were as follows: 95°C for 4 minutes then 34 cycles at 95°C for 1 minute, 55°C for 1 minute and 72°C for 1 minute. Primer set p259 and p306 produced a 275 bp wild-type dystrophin allele. Primer set p260 and p306 detects the mdx point mutation and produced a 275 bp product. To genotype the dystrophin gene, separate PCR reactions were performed because the product sizes are identical in wild-type and mdx mice.
Isolation of skeletal muscle
Three-week-old wild-type, mdx, α7-/- and mdx/α7-/- male mice were euthanized by CO2 inhalation in accordance with a protocol approved by the University of Nevada, Reno Animal Care and Use Committee. The gluteus, gastrocnemius, triceps and tibialis anterior muscles from these mice were dissected, flash-frozen in liquid nitrogen and stored at -80°C.
The gastrocnemius muscle from 3-week-old male mice was ground in liquid nitrogen. Protein was extracted in 200 mM octyl-β-D-glucopyranoside (Sigma Aldrich, St Louis, MO), 50 mM Tris-HCl pH 7.4, 150 mM NaCl, 1 mM CaCl2, 1 mM MgCl2, 2 mM PMSF and a 1:200 dilution of Protease Inhibitor Cocktail Set III (Calbiochem, EMD Biosciences, San Diego, CA) for the detection of the α7 and β1 integrins. Protein was quantified by Bradford assay and 80 μg of total protein were separated on 8% SDS-PAGE gels under non-reduced conditions, and transferred to nitrocellulose membranes. Membranes were blocked in Odyssey Blocking Buffer (LiCor Biosciences, Lincoln, NE) that was diluted 1:1 in phosphate-buffered saline (PBS). The α7 integrin was detected with a 1:500 dilution of rabbit anti-α7A (A2 345) and rabbit anti-α7B (B2 347) polyclonal antibodies. β1D integrin was detected with a 1:500 dilution of rabbit anti-β1D polyclonal antibody (a kind gift of Woo Keun Song, Gwanju Institute for Science and Technology, South Korea). Blots were incubated with a 1:5000 dilution of Alexa Fluor 680-coupled goat anti-rabbit IgG (Molecular Probes, Eugene, OR) to detect primary antibodies.
To analyze laminin-α2, protein was extracted from gastrocnemius muscle with a buffer containing 2% NP40 and 2% Triton X-100. Protein was quantified by a Bradford assay. 60 μg of protein were loaded per well, separated on a 7.5% polyacrylamide gel and transferred for 1 hour to nitrocellulose. Laminin-α2 was detected with an anti-laminin-α2 antibody (sc-20142, Santa Cruz Biotechnology, Santa Cruz, CA) at 1:200 followed by a 1:5000 dilution of Alexa Fluor 680-labeled goat anti-rabbit IgG. The 300 kDa laminin-α2 band was normalized for protein loading by re-probing the blot with goat anti-Cox-1 polyclonal antibody (Santa Cruz Biotechnology, Santa Cruz, CA). Blots were visualized with the Odyssey Imaging System and band intensities determined by using Odyssey Imaging software.
To examine utrophin expression, protein was extracted from the gastrocnemius muscle with RIPA buffer (50 mM Hepes pH 7.4, 150 mM NaCl, 1 mM Na3VO4, 10 mM NaF, 0.5% Triton X-100, 0.5% NP40, 10% glycerol, 2 mM PMSF and a 1:200 dilution of Protease Inhibitor Cocktail Set III) and quantified by a Bradford Assay (BioRad Laboratories Inc., Hercules, CA). 80 μg of total protein were separated on a 7.5% SDS-PAGE gel and transferred to nitrocellulose. The blot was incubated with a 1:200 dilution of anti-utrophin mouse monoclonal antibody (MANCHO3 8A4, a kind gift of Glenn Morris, Center for Inherited Neuromuscular Disease, Shropshire, UK) followed by a 1:50,000 dilution of horseradish peroxidase (HRP)-labeled goat anti-mouse secondary antibody. The 395 kDa utrophin band was detected by chemiluminescence and normalized for protein loading by probing the same blot with anti-Cox-1 antibody (Santa Cruz Biotechnology, Santa Cruz, CA). Band intensities were quantified by using ImageQuant TL software (Amersham Biosciences, Piscataway, NJ).
Triceps muscles were embedded in Tissue-TEK Optimal Cutting Temperature compound (Sakura Finetek USA Inc., Torrance, CA). Ten-μm sections were cut using a Leica CM1850 cryostat and placed onto Surgipath microscope slides (Surgipath Medical Industries, Richmond, IL). The α7 integrin was detected with a 1:1000 dilution of anti-CA5.5 rat monoclonal antibody (Sierra Biosource, Morgan Hill, CA) followed by a 1:1000 dilution of FITC-conjugated anti-rat secondary antibody. The β1D integrin was detected with a 1:500 dilution of rabbit polyclonal antibody followed by a 1:500 dilution of FITC-conjugated anti-rabbit antibody. Laminin-α2 chain was detected with a 1:500 dilution of rabbit anti-α2G polyclonal antibody (a kind gift from Peter Yurchenco, Robert Wood Johnson Medical School, Department of Pathology, Piscataway, NJ). Dystrophin was detected with the mouse monoclonal anti-Dys2 antibody (Novacastra Laboratories, Ltd, Newcastle upon Tyne, UK) and utrophin was detected with MANCHO7 7F3 monoclonal antibody against utrophin (a kind gift from Glenn Morris, Center for Inherited Neuromuscular Disease, Shropshire, UK) at a dilution of 1:200. Anti-CD4 monoclonal antibody (a kind gift from Dorothy Hudig, University of Nevada, Reno) was used to assay muscle inflammation at a dilution of 1:200. The mouse monoclonal antibodies were used in conjunction with a mouse-on-mouse (MOM) immunodetection kit (Vector Laboratories, Burlingame, CA) to block mouse immunoglobulin and a 1:500 dilution of FITC-conjugated anti-mouse secondary antibody. Acetylcholine receptors at NMJs were detected with Rhodamine-labeled α-bungarotoxin at 1:1000 (Molecular Probes). Fluorescence was observed with a Zeiss Axioskop 2 Plus fluorescent microscope and images were captured with a Zeiss AxioCam HRc digital camera and Axiovision 4.1 software.
Embryonic myosin heavy chain
Embryonic myosin heavy chain (eMyHC) was used in immunofluorescence experiments to measure muscle regeneration. Immunofluorescence was performed on 10-μm sections from tibialis anterior muscle from 3-week-old wild-type, mdx, α7-/- and mdx/α7-/- mice with a 1:500 dilution of anti-eMyHC antibody (F1.652, Developmental Studies Hybridoma Bank, University of Iowa, IA). The primary antibody was detected with a 1:500 dilution of FITC-conjugated anti-mouse secondary antibody. A 1 μg/ml concentration of tetramethylrhodamine-conjugated wheat-germ agglutinin (WGA) (Molecular Probes, Eugene, OR) was used to define muscle fibers. Multiple adjacent sections were analyzed with ten random, non-overlapping microscopic fields that were counted per animal at 630× magnification. Data was reported as the number of eMyHC-positive fibers per field.
Hematoxylin and eosin staining
Tibialis anterior and triceps muscles were cryosectioned and 10-μm sections were placed on Surgipath microscope slides. Tissue sections were fixed in ice-cold 95% ethanol for 2 minutes followed by 70% ethanol for 2 minutes and then re-hydrated in running water for 5 minutes. The tissue sections were then stained with Gill's hematoxylin (Fisher Scientific, Fair Lawn, NJ) and rinsed in water for 5 minutes. Tissue sections were placed in Scott's solution (0.024 M NaHCO3, 0.17 M MgSO4) for 3 minutes and rinsed in water for 5 minutes. Tissue sections were stained in eosin solution (Sigma-Aldrich, St Louis, MO) for 2 minutes. Tissue sections were then dehydrated in ice-cold 70% and 95% ethanol for 30 seconds each, followed by 100% ethanol for 2 minutes. Tissue sections were then cleared in xylene for 5 minutes prior to mounting with DePeX mounting medium (Electron Microscopy Sciences, Washington, PA). Centrally located nuclei were counted at 630× magnification by bright-field microscopy. The number of central nuclei per muscle fiber was determined by counting 1000 muscle fibers for triceps muscle and 700 muscle fibers for tibialis anterior muscle per animal. At least five animals from each genotype (wild-type, mdx, α7-/- and mdx/α7-/-) were analyzed.
Evan's Blue dye uptake
Mice were injected intraperitoneally with 50 μl per 10 g of body weight sterile Evans Blue dye solution (10 mg/ml). After 3 hours, the gastrocnemius muscle was harvested and flash-frozen in liquid nitrogen. 10-μm cryosections were placed on microscope slides and fixed in 4% paraformaldehyde. To outline muscle fibers, tissue sections were incubated with 2 μg/ml Oregon Green-488-conjugated WGA (Molecular Probes, Eugene, OR). Muscle fibers positive for Evans Blue dye were counted in a minimum of 1000 fibers per animal, and at least three animals from each phenotype were analyzed. Counting was conducted and images captured at 630× magnification.
The gastrocnemius muscle and tendon were dissected from 3-week-old animals and fixed in 2% glutaraldehyde and 2.5% paraformaldehyde in 0.2% Sorenson's phosphate buffer. Tissue was embedded in LX-112 epoxy (Ladd Research Industries), sectioned at 0.1 μm wirth a Reichert Ultracut E Ultramicrotome, stained with uranyl actetate and lead citrate and viewed with a Hitachi H-600 transmission electron microscope at 5000× magnification.
All averaged data are reported as the mean ± s.d. Comparisons between multiple groups were performed by one-way-analysis of variance (ANOVA) for parametric data or by Kruskal-Wallis one-way-analysis of variance on ranks for non-parametric data using SigmaStat 1.0 software (Jandel Corporation, San Rafael, CA). P<0.05 was considered statistically significant.
The authors thank Glenn Morris (Center for Inherited Neuromuscular Disease, Shropshire, UK) for the MANCHO3 and MANCHO7 anti-utrophin antibodies, Peter Yurchenco (Robert Wood Johnson Medical School, Piscataway, NJ) for the anti-laminin-α2G antibody, Woo Keun Song (Gwanju Institute for Science and Technology, South Korea) for the anti-β1D antibody and Dorothy Hudig (University of Nevada, Reno) for the anti-CD4 antibody. The authors also thank Eric Chaney and Paul Scowen for technical assistance and Dr Heather Burkin for critically reading the manuscript. This work was supported by grants from the NIH/NCRR P20 RR018751-01 and P20 RR15581-04 to D.J.B.