Abstract
In addition to the highly specialized contractile apparatus, it is becoming increasingly clear that there is an extensive actin cytoskeleton which underpins a wide range of functions in striated muscle. Isoforms of cytoskeletal actin and actin-associated proteins (non-muscle myosins, cytoskeletal tropomyosins, and cytoskeletal α-actinins) have been detected in a number of regions of striated muscle: the sub-sarcolemmal costamere, the Z-disc and the T-tubule/sarcoplasmic reticulum membranes. As the only known function of these proteins is through association with actin filaments, their presence in striated muscles indicates that there are spatially and functionally distinct cytoskeletal actin filament systems in these tissues. These filaments are likely to have important roles in mechanical support, ion channel function, myofibrillogenenous and vesicle trafficking.
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The contractile apparatus of skeletal muscle is composed of repeating units of interdigitating actin thin and myosin thick filaments (the sarcomeres). The sarcomeric actin thin filaments are anchored at the lateral boundary of the sarcomere, the Z-disc or Z-line. The Z-disc forms a structural scaffold for the sarcomere and provides a site for attachment for a network of filaments that links individual contractile bundles (myofibrils) to each other and to the plasma membrane (sarcolemma) (Clark et al. 2002). This complex network of cytoskeletal arrays allows the coordinated and rapid translation of the molecular force production by the sarcomeres into macroscopic contraction of myofibers. The attachment of the sarcomeres to the sarcolemma occurs at the costameres, sub-sarcolemmal cytoskeletal complexes aligned with the Z-disc and M-line (Clark et al. 2002; Pardo et al. 1983b). Two major cytoskeletal systems in striated muscle make up the costameric cytoskeleton: desmin intermediate filaments and actin microfilaments. Desmin filaments link Z-discs of adjacent myofibrils with the plasma membrane (through the costameres) and other organelles within the cell (mitochondria and nuclei) (Clark et al. 2002). The intermediate filaments are thought be one of the major elements responsible for maintaining the highly ordered myofibrillar alignment of striated muscle and for the precise positioning of intracellular organelles within the myofiber.
Three main actin-associated costameric complexes have been identified: (1) the focal adhesion complex, (2) the dystrophin-glycoprotein complex and (3) the spectrin-based filament network (Clark et al. 2002). Mutations in many costameric proteins (e.g., dystrophin, integrins) result in muscular dystrophy (Blake et al. 2002). This highlights the importance of the costamere in maintaining the structural integrity of the muscle. The cytoskeletal actin isoform, γ-cytoskeletal actin, is thought to be the major actin found at the costamere and has been proposed to be a critical element linking the membrane bound dystroglycan complex to the sarcomeres (Ervasti 2003). In addition to the costameric actin cytoskeleton there is now good evidence for the existence of a number of spatially and functionally distinct cytoskeletal actin-based filaments in the interior of the myofiber associated particularly with the sarcoplasmic reticulum/T-tubule membranes. It is becoming clear that these cytoskeletal actin filaments perform similar functions to those identified in non-muscle cells, e.g., vesicle trafficking, ion channel tethering (Bennett and Baines 2001; Clark et al. 2002; Rudich and Klip 2003). In this review we will examine the evidence for these internal actin cytoskeletons and their potential roles in striated muscle. We will restrict discussion to studies that show direct evidence for the presence of “non-muscle” cytoskeletal forms of actin and actin-associated proteins in cardiac and skeletal muscle with particular emphasis on actin filaments that are located not at the sarcolemma but in the internal areas of the myofiber (summarized in Table 1; Fig. 1).
Cytoskeletal (non-muscle) actins
Six actin isoforms have been identified in mammalian cells: cytoskeletal/cytoplasmic β- and γ-actins (main isoforms in non-muscle cells), cardiac muscle α-actin, skeletal muscle α-actin, and smooth muscle α- and γ-actins (Tondeleir et al. 2009; Vandekerckhove and Weber 1978). In undifferentiated muscle cells (myoblasts), β- and γ-cytoskeletal isoforms are the predominate actins (Schwartz and Rothblum 1981). γ-Cytoskeletal actin is believed to an have important role in the organization of the early developing sarcomeres (Lloyd et al. 2004). Critical to the process of sarcomere formation and complete muscle differentiation is a replacement of the cytoskeletal isoforms with the muscle isoforms (Lloyd et al. 2004; Schwartz and Rothblum 1981; Shani et al. 1981; von Arx et al. 1995). However, low levels of β- and γ-cytoplasmic actin remain in adult muscle (Hanft et al. 2006, 2007; Kee et al. 2004; Nakata et al. 2001; Otey et al. 1987; Sonnemann et al. 2006) associated with specialized membrane domains (costamere, T-tubule, sarcoplasmic reticulum and the neuromuscular junction).
Using an antibody that specifically recognizes β-cytoskeletal actin (Lubit and Schwartz 1980), Lubit and colleagues showed that this actin isoform was concentrated at the neuromuscular junctions (NMJ) of adult rat skeletal muscle fibers in areas closely associated with acetylcholine receptors (AChR) (Hall et al. 1981; Lubit 1984). β-cytoskeletal actin is present in the neuromuscular junction before the development of the postsynaptic folds (embryonic day 18) suggesting that it has a role in the development of the postsynaptic folds and/or the clustering of the AChR at the NMJ in association with the spectrin/ankyrin filaments (see Section “Spectrin-actin cytoskeleton”).
Using an antibody that recognizes both γ-actin isoforms (cytoskeletal and smooth muscle), Pardo and Craig found that γ-actin localized to the submembraneous costameric lattice and to mitochondria in skeletal muscle (Craig and Pardo 1983; Pardo and Craig 1983a). More recent studies have provided evidence for a costameric γ-cytoskeletal actin filament network linking the peripheral sarcomeres with the dystroglycan complex at the sarcolemma (Ervasti 2003; Hanft et al. 2006; Rybakova et al. 2000, 2002; Rybakova and Ervasti 2005). They proposed that this γ-cytoskeletal actin filament system is a critical component of the costameric cytoskeleton contributing to the mechanical stability of the sarcolemma (Ervasti 2003; Rybakova et al. 2000). However, recent studies of a skeletal muscle-specific γ-actin knock-out (KO) mouse question this hypothesis (Sonnemann et al. 2006; Prins et al. 2008). In this mouse, the dystroglycan costameric complex is not disrupted and the mouse does not have dystrophic features that are normally associated with disruptions to the costameric network (Sonnemann et al. 2006). This is consistent with the work of Corrado et al. (1996) who showed in transgenic mouse models that mutations to the actin-binding domain of dystrophin was less severe than mutations in the dystroglycan-binding domain. Thus, it would appear that γ-cytoskeletal actin’s role in skeletal muscle is not simply one of mechanical support for the sarcolemma. However, this mouse does have histological features of progressive centronuclear fiber myopathy (CNM) (Sonnemann et al. 2006), a condition characterized by the presence of a high proportion of fibers with centrally located nuclei. In humans, the genes that are mutated in CNM have roles in vesicle trafficking, and membrane structure and function (myotubulin, dynamin-2, amphiphysin-2, ryanodine receptor) indicating disruption to membrane function is the cause of CNM (Bitoun et al. 2009; Cao et al. 2008; Jungbluth et al. 2008; Laporte et al. 1996). This raises the possibility that disruption to these processes may also be the cause of the CNM-like features in the γ-cytoskeletal actin KO mouse as these same processes are known to be dependent on the actin cytoskeleton (see Sections “Spectrin-actin cytoskeleton”, “Actin and ion channels: role in the internal membrane systems”, “Cytoskeletal α-actinins (α-actinin-1 and -4)”, and “Actin and GLUT4 trafficking: at the sarcolemma and the T-tubule”).
Apart from costameric actin there is now good evidence for additional cytoskeletal actin filament networks in the interior of skeletal muscle fibers (Kee et al. 2004; Nakata et al. 2001; Papponen et al. 2009; Vlahovich et al. 2008, 2009). Nakata et al. (2001) using a γ-cytoskeletal-actin-specific polyclonal antibody (raised against a N-terminal peptide) showed in mouse skeletal muscle sections that γ-cytoskeletal actin is located throughout the myofiber co-localizing with the Z-disc. Surprisingly, unlike that reported by Hanft et al. (2006) they failed to detect γ-cytoskeletal actin at the sarcolemma presumably due to differences in the epitopes recognized by the two antibodies. The antibody used by Hanft et al. (2006) is a monoclonal raised against a combination of purified bovine brain γ-cytoskeletal actin and the keyhole limpet hemocyanin-conjugated 14 amino acid N-terminal peptide, while the antibody used in Nakata et al. (2001) is a polyclonal against a shorter 7 amino acid N-terminal peptide. We also examined the location of γ-cytoskeletal actin in adult mouse skeletal muscle (Kee et al. 2004; Vlahovich et al. 2008), again with a different antibody (Schevzov et al. 2005b) [polyclonal against the same 14 amino acid N-terminal peptide as in Hanft et al. (2006)]. In this case, γ-cytoskeletal actin was detected both at the sarcolemma and also in a novel region adjacent to the Z-disc (Kee et al. 2004; Vlahovich et al. 2008, 2009) which we have called the Z-LAC (Z-Line Adjacent Cytoskeleton) (Kee et al. 2004).
Because of the variable staining with the γ-cytoskeletal actin antibodies, Papponen et al. (2009) used GFP- and myc-tagged γ-cytoskeletal actin constructs to examine its localization in skeletal muscle. Consistent with the findings of Nakata et al. (2001), the tagged γ-cytoskeletal actin constructs localized specifically to the Z-disc and not the sarcolemma in cultured rat skeletal myofibers and electroporated skeletal muscles of mice (Papponen et al. 2009). In conclusion, although there are some differences in immuno-staining patterns with the various γ-cytoskeletal antibodies, there are now a number of studies using different approaches that show γ-cytoskeletal actin not just at the sarcolemma, but also at or in close proximity to the Z-disc throughout the muscle fiber. This speaks to the existence of multiple spatially and functionally distinct actin filament systems in skeletal muscle fibers as have been observed in other cell types (Gunning et al. 2005, 2008). One would predict that cytoskeletal actin filaments would be present in cardiac muscle but surprisingly the presence of γ-cytoskeletal actin in mature cardiac muscle has not been reported.
Cytoskeletal (non-muscle) tropomyosins
Tropomyosins (Tms) are filamentous proteins associated with the actin cytoskeleton. Three isoforms are striated-muscle-specific, or sarcomeric, and they bind to the sarcomeric actin thin filament where they regulate actin–myosin interactions and give strength and stability to the contractile apparatus (Gunning et al. 2008). All other Tm isoforms are considered to be non-sarcomeric or cytoskeletal. Previous studies from our laboratory (Bryce et al. 2003; Dalby-Payne et al. 2003; Gunning et al. 1998; Hook et al. 2003; Hughes et al. 2003; Kee et al. 2004; Percival et al. 2000, 2004; Schevzov et al. 2005a, 2008; Vrhovski et al. 2003) and others (Lin et al. 1997) have demonstrated that both Tm and actin isoforms segregate into functionally distinct compartments in different cell types. This provides a means to independently regulate the cytoskeleton at different sites and to tailor the function of actin filaments at these different sites (Gunning et al. 2008). For example, we have shown that Tm isoforms can regulate actin filament turnover (Creed et al. 2008) and interact with specific myosin motors in neuroblastoma-derived cells (Bryce et al. 2003).
Using antibodies that recognize specific cytoskeletal Tm isoforms, cytoskeletal Tms have been detected in a number of different regions of skeletal and cardiac muscle (Kee et al. 2004; Schevzov et al. 2008; Vlahovich et al. 2008, 2009). Two different Tm isoforms, Tm5NM1 and Tm4, have been found adjacent to the Z-disc (at the Z-LAC) throughout the myofiber in association with γ-cytoskeletal actin (Kee et al. 2004; Schevzov et al. 2008; Vlahovich et al. 2008). More recent studies in skeletal muscle have shown that the two Tm isoforms define two independent filament systems. Tm5NM1 is closely associated with the transverse-tubules (T-tubules) as it co-localizes with the T-tubule specific dihydropyridine receptor, while Tm4, using immuno-electron microscopy, has been precisely localized to the terminal region of the sarcoplasmic reticulum (SR) (Vlahovich et al. 2009). As Tms are typically associated with actin filaments (Gunning et al. 2008) these studies suggest that there are two novel cytoskeletal actin/Tm filament populations associated with the two specialized membrane systems in skeletal muscle, the T-tubules and the SR. In keeping with Tm5NM1 associating with T-tubules, lack of Tm5NM1 in a knockout mouse leads to T-tubule dysmorphology and altered skeletal muscle contractile function (Vlahovich et al. 2009). As yet the function of Tm4-defined actin filaments at this site is not known, but one would predict that because they are associated with the terminal SR that these filaments would have some role in SR Ca2+ storage and/or release during skeletal muscle excitation and contraction.
A further set of Tm4-defined actin filaments, independent of the Z-LAC, have been detected in skeletal muscle fibers, oriented parallel to the sarcomeres (Vlahovich et al. 2008). These “longitudinal” Tm4 filaments co-localize with γ-cytoskeletal actin and are prevalent during myofiber formation, growth and repair/regeneration. The increase in the amounts of both Tm4 (Vlahovich et al. 2008) and γ-cytoskeletal actin (Hanft et al. 2006, 2007) in dystrophic muscle and the co-localization of Tm4 and γ-cytoskeletal actin in skeletal muscles undergoing chronic repair, suggests that γ-cytoskeletal actin filaments decorated by this Tm isoform may play a role in myofibrillar formation (Lloyd et al. 2004; Sanger et al. 2006).
Recent studies on a transgenic mouse that expresses a Tm not normally detected in muscle (Tm3) suggest the cytoskeletal Tm-containing actin filaments adjacent to the Z-disc (Z-LAC) have a role in protecting the muscle from contractile stress (Kee et al. 2009). Ectopic Tm3 localizes to the Z-LAC and results in a dystrophic phenotype (Kee et al. 2004, 2009) and increased susceptibility to contractile stress (Kee et al. 2009), presumably through disruption of an endogenous cytoskeletal actin filament system in muscle. The phenotype of the Tm3 mouse is very distinct from the Tm5NM1 KO mouse (dystrophy in the former; no dystrophy in the latter, but an alteration to excitation–contraction coupling) indicating that Tm3 is not disrupting the Tm5NM1-defined actin filaments, but yet another distinct population of microfilaments (Kee et al. 2004, 2009). Taken together the data on the cytoskeletal Tm isoforms in skeletal muscle is consistent with the concept of Tm isoforms defining functionally distinct actin filament populations in skeletal muscle.
Non-muscle myosins
In striated muscle, non-muscle (NM) myosin II isoforms are thought to play a role in the formation of myofibrils. Studies in cardiomyocytes and explants of precardiac mesoderm from quail embryos indicate that one of the first stages in the development of the myofibril is the formation of premyofibrils containing α-actinin-rich Z-bodies, with NM myosin IIB and myosin light chain kinase (MLCK; the principle Ca2+-activated regulator of myosin II) at the edges of the developing cardiomyocyte (Dabiri et al. 1997; Du et al. 2003; Dudnakova et al. 2006; LoRusso et al. 1997). During the transition from premyofibrils to mature myofibrils there is a replacement of NM myosin IIB filaments with muscle-specific myosin II filaments and the fusion of Z-bodies into mature Z-discs (Dabiri et al. 1997; Du et al. 2003; LoRusso et al. 1997). However, Takeda et al. (2000) and Dudnakova et al. (2006) using polyclonal antibodies to NM myosin heavy chains (MyHC) II isoforms and MLCK, respectively, found that these NM myosin proteins were still expressed in adult cardiac and skeletal muscle. NM MyHC IIB was found at the Z-disc and intercalated disc in adult human cardiac and skeletal muscle while NM MyHC IIA was found at or near the Z-discs in skeletal muscle only (non-stretched muscle). Confocal Z-scans showed that the NM MyHC II isoforms (A and B) were located near the Z-discs throughout the myofiber (Takeda et al. 2000). MLCK was also found near the Z-disc co-localized with NM MyHC IIB in cultured chicken embryonic cardiomyocytes and adult chicken and human heart (Dudnakova et al. 2006). The presence of all the major components of the actin cytoskeleton (NM MyHC, MLCK, γ-cytoskeletal actin and cytoskeletal Tms) in close proximity to the Z-disc provides additional evidence that there is a functional actin cytoskeleton at this site. One possible role of these actin filaments is to maintain the structural integrity of the Z-disc and perhaps perform a dynamic function in muscle relaxation. Alternatively, these filaments may be involved in the function of the muscle T-tubule/SR membranes which are located in proximity to the Z-disc as has been shown for the Z-LAC tropomyosin, Tm5NM1, in skeletal muscle and the spectrin/ankyrin network in cardiac muscle (see Sections “Cytoskeletal (non-muscle) tropomyosins”, “Spectrin-actin cytoskeleton” respectively).
Spectrin-actin cytoskeleton
Spectrin is an actin-binding protein that forms the major membrane cytoskeleton in erythrocytes and many other cells including striated muscle. In cardiac and skeletal muscle, spectrin is enriched in specialized membrane domains (costameres, T-tubules/SR, neuromuscular junction) and in association with ankyrin plays a prominent role in anchoring a diverse range of integral membrane proteins (ion channels and cell adhesion molecules) with the actin cytoskeleton (Baines and Pinder 2005; Bennett and Baines 2001; Kordelli 2000). There is now a large body of evidence for spectrin and ankyrin in the internal membranes (the T-tubules and the SR) of cardiac and skeletal muscle where they play a similar role as at the sarcolemma (Bennett and Baines 2001; Bennett et al. 2004; Chen et al. 1997; Flucher et al. 1990; Hayes et al. 2000; Kordeli et al. 1998; Kostin et al. 1998; Li et al. 1993; Messina and Lemanski 1989; Mohler et al. 2004, 2005; Mohler and Wehrens 2007).
In cardiac muscle, spectrin II isoforms (α and β) are found at the plasma membrane, the Z-disc and regions of the myofibril consistent with the SR (Bennett et al. 2004; Hayes et al. 2000). Multiple isoforms of ankyrins are also present at these sites in association with specific ion channels. Early studies using an antibody to erythrocyte ankyrin (ankyrin-R) detected ankyrin at the triads (surrounding the T-tubules and the terminal SR cisternae) in skeletal muscle (Flucher et al. 1990) and at the sarcolemma and the T-tubules in cardiac muscle (Chen et al. 1997; Li et al. 1993). More recent studies in cardiac muscle have localized ankyrin-G to the intercalated disc and the transverse tubules where it has a role in tethering the voltage-gated Nav to these membranes (Lowe et al. 2008). Ankyrin-B plays a similar role of organizing and stabilizing ion channels in the T-tubule/SR membranes; its absence, in ankyrin-B knockout mice, leads to the loss of the Na/K ATPase, the Na/Ca exchanger and inositol 1,4,5-trisphosphate receptors from the Z-disc/T-tubule location (Mohler et al. 2005). Thus, it is clear that the spectrin/ankyrin networks have important roles in maintaining localized concentrations of ion-channels in specialized membrane domains in striated muscle. However, the specific role of actin in these spectrin/ankyrin networks has yet to be determined. Indeed, which actin associates with the spectrin/ankyrin filaments has not been defined, although β-cytoplasmic actin is concentrated at the postsynaptic membrane of the neuromuscular junction (Hall et al. 1981; Lubit 1984). It has been known for some time that disruption to the actin cytoskeleton alters ion channel function (see Section “Actin and ion channels: role in the internal membrane systems”). Part of this effect may be due to impact on the actin-spectrin cytoskeleton.
Actin and ion channels: role in the internal membrane systems
There is a large body of research demonstrating a direct role of the actin cytoskeleton in ion channel function; sodium, calcium, potassium and stretch-activated channels have all been shown to be altered when the actin cytoskeleton is disrupted in cardiomyocytes (Calaghan et al. 2004). Much of this data has come from studies where the actin cytoskeleton is altered using cytochalasin D (inhibits actin polymerization) or phalloidin (stabilizes actin filaments). The actin cytoskeleton effects ion channels in the sarcolemma as well as channels located specifically in the T-tubules (the L-Type Ca2+ channel, the dihydropyridine receptor) (Lader et al. 1999; Rueckschloss and Isenberg 2001). The mechanisms for these effects are unknown, although alteration to the ankyrin/spectrin network is one potential mechanism (reviewed above). However, there is also evidence for a direct linkage between the actin cytoskeleton and the L-type Ca2+ channel via the actin-binding protein Ahnak (Hohaus et al. 2002). Ahnak is a ubiquitously expressed giant protein (700 kDa) that has been implicated in cell differentiation and signal transduction (Haase 2007). It associates with the regulatory subunit of the cardiac L-type Ca2+ channel (Haase et al. 2004) and binds to F-actin (Hohaus et al. 2002). In human heart, Ahnak was shown to be present at the sarcolemma and intercalated disc and areas that on immunofluorescent staining were consistent with T-tubules (Hohaus et al. 2002).
There is less direct evidence for an effect of the actin cytoskeleton on ion channels in skeletal muscle. Much of the data comes from investigations using dystrophin null myofibers from the mdx mouse model where the costameric γ-actin network is thought to be disrupted (Rybakova et al. 2000). In this case the major impact of loss of dystrophin appears to be a dysregulation of the spontaneous (resting) Ca2+ channel activity (so called Ca2+ sparks) (Allard 2006). Johnson et al. (2005) recently provided more direct evidence for a role of the actin cytoskeleton in Ca2+ channel activity in skeletal muscle. They showed that the voltage dependence of L-type Ca2+ channel activation was shifted positively in skeletal myotubes derived from neonatal mdx mice and potentiation of the channel was significantly reduced in the presence of the actin filament stabilizer phalloidin. These results suggest that loss of dystrophin impacts on the T-tubule membrane system as well as the sarcolemma. However, the internal membrane systems (T-tubule and SR) are not as well developed in neonatal myotubes compared to adult myofibers (Flucher et al. 1993). Thus, the role of actin in ion channel function in adult skeletal muscle has still to be defined.
Actin has also been implicated in the ordered arrangement of ion channels in the T-tubule membranes. In the process of establishing cardiomyocytes in culture there is an initial dedifferentiation process that involves loss of T-tubule structure and relocation of the L-type Ca2+ channels to the perinuclear space (Leach et al. 2005). Treatment with cytochalasin D (inhibits actin polymerization) lessened the changes to T-tubule morphology and density of the L-type Ca2+ channels with dedifferentiation (Leach et al. 2005). Disrupting the microtubules with nocadazole or colchicine had little effect on T-tubule morphology or channel density, suggesting that microtubules are not involved in this process. Thus, actin may be involved in trafficking or localization of ion channels to the T-tubules and other membranes perhaps mediated via disruptions to the the linkage between the actin cytoskeleton and the spectrin/ankyrin complexes (see Section “Spectrin-actin cytoskeleton”) or alterations to membrane trafficking pathways (see Section “Actin and GLUT4 trafficking: at the sarcolemma and the T-tubule”).
Cytoskeletal α-actinins (α-actinin-1 and -4)
The α-actinin proteins (4 isoforms) are multifunctional scaffolding proteins that cross-link actin filaments and bind many other structural and regulatory proteins (Sjoblom et al. 2008). α-Actinin-2 and -3 are muscle specific and are the integral components of the Z-disc, where they help anchor the myofibrillar actin filaments (Sjoblom et al. 2008). In contrast, α-actinin-1 and -4 are expressed predominately in nonmuscle cells in association with microfilament bundles and adherens-type junctions, where they crosslink actin filaments (Sjoblom et al. 2008). However, two recent studies indicate that these cytoskeletal α-actinins have important roles in skeletal muscle (Amsili et al. 2008; Talior-Volodarsky et al. 2008). In the first study, α-actinin-1 was shown (with BIAcore analysis and co-immunoprecipitation studies) to interact with UDP-N-Acetylglucosamine 2-Epimerase/NAcetylmannosamine Kinase (GNE) an enzyme involved in sialic acid metabolism (Amsili et al. 2008). The GNE gene is mutated in patients with hereditary inclusion body myopathy (HIDM), a neuromuscular disorder characterized by adult-onset muscle weakness and pathological features including cytoplasmic rimmed vacuoles and cytoplasmic or nuclear inclusions composed of tubular filaments (Argov and Mitrani-Rosenbaum 2008). Interestingly, in stretched adult mouse skeletal muscle, α-actinin-1 was found to be located adjacent to the Z-disc (the Z-LAC) (Amsili et al. 2008) an area occupied by cytoskeletal Tms (Kee et al. 2004; Vlahovich et al. 2008, 2009), NM myosins (Takeda et al. 2000) and γ-cytoskeletal actin (Kee et al. 2004; Nakata et al. 2001; Vlahovich et al. 2008, 2009). This provides added support for a Z-line adjacent actin cytoskeleton (Z-LAC) in skeletal muscle. In mouse skeletal muscle, GNE was found in a distinct but overlapping region of the sarcomere (mainly at the Z-line) to α-actinin-1 indicating that the interaction detected between these two proteins in vitro may also occur in vivo. It is unclear why an enzyme involved in sialic acid metabolism should be localized to such a specific site within skeletal myofibers and equally why a mutation in this enzyme leads to HIDM. Regardless, that GNE is located at such a specific area in muscle suggests that this localization is important for its function. The Z-LAC may be important to tether GNE to this specific region of the sarcomere.
An indication of the multifunctionality of the α-actinin proteins is the recent report linking α-actinin-4 to insulin-stimulated glucose transporter 4 (GLUT4) translocation (Talior-Volodarsky et al. 2008). Insulin-stimulated movement of GLUT4 from intracellular storage sites to the surface membranes is the rate-limiting step in insulin-stimulated glucose uptake (see Section “Actin and GLUT4 trafficking: at the sarcolemma and the T-tubule”). The initial indication that α-actinin-4 may be involved in glucose transport came from a study that showed an insulin-dependent interaction between GLUT4 and α-actinin-4 in L6 muscle cells (Foster et al. 2006). In a follow-up study, the same group showed in L6 muscle cells that siRNA-mediated α-actinin-4 knockdown (KD) inhibited insulin-stimulated GLUT4 trafficking and insertion into the plasma membrane (Talior-Volodarsky et al. 2008). They also showed that α-actinin-4 co-localized with GLUT4 in the insulin-stimulated cortical actin network and that α-actinin-4 KD had little impact on actin remodeling. KD of α-actinin-1 had no impact on insulin-stimulated GLUT4 translocation indicating the specificity of the effect of α-actinin-4 on GLUT4 trafficking. The mechanism for α-actinin-4’s effect on GLUT4 was not examined but it is likely to involve cross-linking cytoskeletal actin filaments.
Actin and GLUT4 trafficking: at the sarcolemma and the T-tubule
That the actin cytoskeleton has a role in GLUT4 trafficking is well-established (Kanzaki 2006). In insulin responsive tissues (adipose tissue and striated muscle) an obligatory step in GLUT4 translocation is a process of insulin-induced actin remodeling that leads to the formation of a dense actin network at the inner-surface of the plasma membrane (Brozinick et al. 2004; Kanzaki 2006; Tong et al. 2001; Tsakiridis et al. 1994). Inhibition of this remodeling leads to abrogation of GLUT4 translocation and inhibition of glucose uptake (Brozinick et al. 2004; Kanzaki 2006; Tong et al. 2001; Tsakiridis et al. 1994). The actin cytoskeleton has been implicated in many steps in the GLUT4 trafficking pathway: insulin signaling, intracellular GLUT4-vesicle movement, and GLUT4-vesicle tethering/docking/fusion with the plasma membrane (Kanzaki 2006). Thus, it is possible that distinct actin filaments are involved in different aspects of the GLUT4 trafficking pathway. Indeed there is now evidence for different NM myosin isoforms being involved in different parts of the GLUT4 trafficking pathway: Myo1c appears to be associated with GLUT4-vesicle docking (Chen et al. 2007) while Myo5a has been linked with GLUT4 vesicle transport (Yoshizaki et al. 2007).
In striated muscle, insulin-stimulated GLUT4 translocation occurs both at the plasma membrane (sarcolemma) and the T-tubule membrane (Khan et al. 2001; Lauritzen et al. 2006; Ploug et al. 1998). In fact, because of its very large surface area, the T-tubules are a very significant site of glucose uptake in striated muscle (Eisenberg 1983). As the T-tubules are continuations of the sarcolemma and extend throughout the myofiber to surround each myofibril they are perfectly situated to deliver glucose to the major site of utilization, the contracting myofibrils. Therefore, one would expect similar actin filament networks involved in GLUT4 trafficking associated with both the T-tubules and the sarcolemma.
Multiple functionally distinct actin cytoskeletons in striated muscle
Previous studies in non-muscle cells have demonstrated that isoforms of actin and actin-binding proteins (Tms and myosins) segregate into functionally distinct compartments (Gunning et al. 2008). This provides a means to independently regulate the cytoskeleton at different sites and to tailor the function of actin filaments at these different sites. From the proceeding discussion it is apparent that a similar situation exists in striated muscle where major components of the actin cytoskeleton (cytoskeletal actin and Tms, NM myosins, MLCK, cytoskeletal α-actinins) are found at diverse sites in striated muscle cells: the costamere, the Z-disc region and the T-tubules/SR membranes (see Table 1; Fig. 1 for a summary).
Many of the same cytoskeletal proteins are located in a number of different regions of muscle cells (see Table 1; Fig. 1). For example, cytoskeletal Tm isoforms, spectrins and ankyrin are at the sarcolemma and also at the triad membranes. This raises the possibility that actin filaments with the same composition will be present in a number of different cellular locations. Indeed this appears to be the case for GLUT4 trafficking where this actin-dependent process occurs both at the sarcolemma and the T-tubule membrane (reviewed above). The sarcolemma and the T-tubule membranes perform many similar functions in striated muscle; this includes propagation of signals from the extracellular to intracellular environment (e.g., insulin) and the transport of ions and metabolites into and out of the cell. Therefore, it is not particularly surprising that various membrane associated cytoskeletal proteins are found at both sites. The challenge will be to define the function of each of these proteins in processes that are common and specific to each of these membrane systems.
There is a need to more completely and systematically define the composition and nature of the actin filaments in striated muscle. In particular there is a need to more clearly define which of these filament systems are present in skeletal versus cardiac muscle. The majority of studies to date have used conventional confocal microscopy (axial resolution >200 nm) on muscle at non-physiological lengths to examine localization of cytoskeletal proteins in differentiated muscle cells. More detailed immuno-electron microscopy studies will be required to precisely define the location of different cytoskeletal proteins in striated muscle. With the recent development of super high-resolution fluorescent microscopy techniques (e.g., PALM, STED microscopy, etc.) (Huang et al. 2009) it should be possible to visualize individual filament populations in striated muscle cells. Specific questions that need to be addressed include: (1) how are these actin filaments organized in muscle, (2) do they resemble actin filament structures observed in other cell types, (3) are the proteins that have been detected at the Z-line (γ-cytoskeletal actin, NM myosins) truly Z-line or do they associate with structures close to the Z-line, i.e., T-tubule/SR membranes or other intermyofibrillar structures, (4) are the isoforms of Tms and other cytoskeletal proteins that are located in similar locations part of separate filament populations, and (5) are all the actin filament populations identified in striated muscle based on a γ-cytoskeletal actin backbone or do other nonsarcomeric actins exist in striated muscle (β-cytoskeletal actin, smooth muscle isoforms)?
Whatever the answers prove to be, the discovery of multiple populations of cytoskeletal actin filaments in striated muscle will contribute to our understanding of the organization of striated muscle. Our ability to visualize different populations with different antibodies will allow us to follow the establishment and regulation of these structures. The use of gene targeting techniques and overexpression approaches will allow us to establish the role of these cytoskeletal compartments. This is almost certain to reveal new levels of architectural structure and function in striated muscle.
References
Allard B (2006) Sarcolemmal ion channels in dystrophin-deficient skeletal muscle fibres. J Muscle Res Cell Motil 27:367–373
Amsili S, Zer H, Hinderlich S, Krause S, Becker-Cohen M, MacArthur DG, North KN, Mitrani-Rosenbaum S (2008) UDP-N-acetylglucosamine 2-epimerase/N-acetylmannosamine kinase (GNE) binds to alpha-actinin 1: novel pathways in skeletal muscle? PLoS ONE 3:e2477
Argov Z, Mitrani-Rosenbaum S (2008) The hereditary inclusion body myopathy enigma and its future therapy. Neurotherapeutics 5:633–637
Baines AJ, Pinder JC (2005) The spectrin-associated cytoskeleton in mammalian heart. Front Biosci 10:3020–3033
Bennett V, Baines AJ (2001) Spectrin and ankyrin-based pathways: metazoan inventions for integrating cells into tissues. Physiol Rev 81:1353–1392
Bennett PM, Baines AJ, Lecomte MC, Maggs AM, Pinder JC (2004) Not just a plasma membrane protein: in cardiac muscle cells α-II spectrin also shows a close association with myofibrils. J Muscle Res Cell Motil 25:119–126
Bitoun M, Durieux A-C, Prudhon B, Bevilacqua JA, Herledan A, Sakanyan V, Urtizberea A, Cartier L, Romero NB, Guicheney P (2009) Dynamin 2 mutations associated with human diseases impair clathrin-mediated receptor endocytosis. Hum Mutat 30:1–9
Blake DJ, Weir A, Newey SE, Davies KE (2002) Function and genetics of dystrophin and dystrophin-related proteins in muscle. Physiol Rev 82:291–329
Brozinick JT, Hawkins ED, Strawbridge AB, Elmendorf JS (2004) Disruption of cortical actin in skeletal muscle demonstrates an essential role of the cytoskeleton in GLUT4 translocation in insulin sensitive tissues. J Biol Chem 279:40699–40706
Bryce NS, Schevzov G, Ferguson V, Percival JM, Lin JJ, Matsumura F, Bamburg JR, Jeffrey PL, Hardeman EC, Gunning P, Weinberger RP (2003) Specification of actin filament function and molecular composition by tropomyosin isoforms. Mol Biol Cell 14:1002–1016
Calaghan SC, Le Guennec JY, White E (2004) Cytoskeletal modulation of electrical and mechanical activity in cardiac myocytes. Prog Biophys Mol Biol 84:29–59
Cao C, Backer JM, Laporte J, Bedrick EJ, Wandinger-Ness A (2008) Sequential actions of myotubularin lipid phosphatases regulate endosomal PI(3)P and growth factor receptor trafficking. Mol Biol Cell 19:3334–3346
Chen F, Mottino G, Shin VY, Frank JS (1997) Subcellular distribution of ankyrin in developing rabbit heart-relationship to the Na+–Ca2+ exchanger. J Mol Cell Cardiol 29:2621–2629
Chen XW, Leto D, Chiang SH, Wang Q, Saltiel AR (2007) Activation of RalA is required for insulin-stimulated GLUT4 trafficking to the plasma membrane via the exocyst and the motor protein Myo1c. Dev Cell 13:391–404
Clark KA, McElhinny AS, Beckerle MC, Gregorio CC (2002) Striated muscle cytoarchitecture: an intricate web of form and function. Annu Rev Cell Dev Biol 18:637–706
Corrado K, Rafael JA, Mills PL, Cole NM, Faulkner JA, Wang K, Chamberlain JS (1996) Transgenic mdx mice expressing dystrophin with a deletion in the actin-binding domain display a “mild Becker” phenotype. J Cell Biol 134:873–884
Craig SW, Pardo JV (1983) Gamma actin, spectrin, and intermediate filament proteins colocalize with vinculin at costameres, myofibril-to-sarcolemma attachment sites. Cell Motil 3:449–462
Creed SJ, Bryce N, Naumanen P, Weinberger R, Lappalainen P, Stehn J, Gunning P (2008) Tropomyosin isoforms define distinct microfilament populations with different drug susceptibility. Eur J Cell Biol 87:709–720
Dabiri GA, Turnacioglu KK, Sanger JM, Sanger JW (1997) Myofibrillogenesis visualized in living embryonic cardiomyocytes. Proc Nat Acad Sci USA 94:9493–9498
Dalby-Payne JR, O’Loughlin EV, Gunning P (2003) Polarization of specific tropomyosin isoforms in gastrointestinal epithelial cells and their impact on CFTR at the apical surface. Mol Biol Cell 14:4365–4375
Du A, Sanger JM, Linask KK, Sanger JW (2003) Myofibrillogenesis in the first cardiomyocytes formed from isolated quail precardiac mesoderm. Dev Biol 257:382–394
Dudnakova TV, Stepanova OV, Dergilev KV, Chadin AV, Shekhonin BV, Watterson DM, Shirinsky VP (2006) Myosin light chain kinase colocalizes with nonmuscle myosin IIB in myofibril precursors and sarcomeric Z-lines of cardiomyocytes. Cell Motil Cytoskelet 63:375–383
Eisenberg BR (1983) Quantitative ultrastructure of mammalian skeletal muscle. In: Peachey LD, Adrian RH, Geiger SR (eds) Handbook of physiology. Section 10: skeletal muscle. Amercian Physiology Society, Bethesda
Ervasti JM (2003) Costameres: the Achilles’ heel of Herculean muscle. J Biol Chem 278:13591–13594
Flucher BE, Morton ME, Froehner SC, Daniels MP (1990) Localization of the alpha 1 and alpha 2 subunits of the dihydropyridine receptor and ankyrin in skeletal muscle triads. Neuron 5:339–351
Flucher BE, Takekura H, Franzini-Armstrong C (1993) Development of the excitation–contraction coupling apparatus in skeletal muscle: association of sarcoplasmic reticulum and transverse tubules with myofibrils. Dev Biol 160:135–147
Foster LJ, Rudich A, Talior I, Patel N, Huang X, Furtado LM, Bilan PJ, Mann M, Klip A (2006) Insulin-dependent interactions of proteins with GLUT4 revealed through stable isotope labeling by amino acids in cell culture (SILAC). J Proteome Res 5:64–75
Gunning P, Weinberger R, Jeffrey P, Hardeman E (1998) Isoform sorting and the creation of intracellular compartments. Annu Rev Cell Dev Biol 14:339–372
Gunning PW, Schevzov G, Kee AJ, Hardeman EC (2005) Tropomyosin isoforms: divining rods for actin cytoskeleton function. Trends Cell Biol 15:334–341
Gunning P, O’Neill G, Hardeman E (2008) Tropomyosin-based regulation of the actin cytoskeleton in time and space. Physiol Rev 88:1–35
Haase H (2007) Ahnak, a new player in beta-adrenergic regulation of the cardiac L-type Ca2+ channel. Cardiovasc Res 73:19–25
Haase H, Pagel I, Khalina Y, Zacharzowsky U, Person V, Lutsch G, Petzhold D, Kott M, Schaper J, Morano I (2004) The carboxyl-terminal ahnak domain induces actin bundling and stabilizes muscle contraction. FASEB J 18:839–841
Hall ZW, Lubit BW, Schwartz JH (1981) Cytoplasmic actin in postsynaptic structures at the neuromuscular junction. J Cell Biol 90:789–792
Hanft LM, Rybakova IN, Patel JR, Rafael-Fortney JA, Ervasti JM (2006) Cytoplasmic γ-actin contributes to a compensatory remodeling response in dystrophin-deficient muscle. Proc Natl Acad Sci USA 103:5385–5390
Hanft LM, Bogan DJ, Mayer U, Kaufman SJ, Kornegay JN, Ervasti JM (2007) Cytoplasmic γ-actin expression in diverse animal models of muscular dystrophy. Neuromuscul Disord 17:569–574
Hayes NV, Scott C, Heerkens E, Ohanian V, Maggs AM, Pinder JC, Kordeli E, Baines AJ (2000) Identification of a novel C-terminal variant of βII spectrin: two isoforms of βII spectrin have distinct intracellular locations and activities. J Cell Sci 113:2023–2034
Hohaus A, Person V, Behlke J, Schaper J, Morano I, Haase H (2002) The carboxyl-terminal region of ahnak provides a link between cardiac L-type Ca2+ channels and the actin-based cytoskeleton. FASEB J 16:1205–1216
Hook J, Lemckert F, Qin H, Schevzov G, Gunning P (2003) Gamma tropomyosin gene products are required for embryonic development. Mol Cell Biol 24:2318–2323
Huang B, Bates M, Zhuang X (2009) Super-resolution fluorescence microscopy. Annu Rev Biochem 78:993–1016
Hughes JA, Cooke-Yarborough CM, Chadwick NC, Schevzov G, Arbuckle SM, Gunning P, Weinberger RP (2003) High-molecular-weight tropomyosins localize to the contractile rings of dividing CNS cells but are absent from malignant pediatric and adult CNS tumors. Glia 42:25–35
Johnson BD, Scheuer T, Catterall WA (2005) Convergent regulation of skeletal muscle Ca2+ channels by dystrophin, the actin cytoskeleton, and cAMP-dependent protein kinase. Proc Natl Acad Sci USA 102:4191–4196
Jungbluth H, Wallgren-Pettersson C, Laporte J (2008) Centronuclear (myotubular) myopathy. Orphanet J Rare Dis 3:26
Kanzaki M (2006) Insulin receptor signals regulating GLUT4 translocation and actin dynamics. Endocr J 53:267–293
Kee AJ, Schevzov G, Nair-Shalliker V, Robinson CS, Vrhovski B, Ghoddusi M, Qiu MR, Lin JJC, Weinberger R, Gunning PW, Hardeman EC (2004) Sorting of a nonmuscle tropomyosin to a novel cytoskeletal compartment in skeletal muscle results in muscular dystrophy. J Cell Biol 166:685–696
Kee AJ, Gunning PW, Hardeman EC (2009) A cytoskeletal tropomyosin can compromise the structural integrity of skeletal muscle. Cell Motil Cytoskelet 66:710–720
Khan AH, Thurmond DC, Yang C, Ceresa BP, Sigmund CD, Pessin JE (2001) Munc18c regulates insulin-stimulated glut4 translocation to the transverse tubules in skeletal muscle. J Biol Chem 276:4063–4069
Kordeli E (2000) The spectrin-based skeleton at the postsynaptic membrane of the neuromuscular junction. Microsc Res Tech 49:101–107
Kordeli E, Ludosky MA, Deprette C, Frappier T, Cartaud J (1998) AnkyrinG is associated with the postsynaptic membrane and the sarcoplasmic reticulum in the skeletal muscle fiber. J Cell Sci 111:2197–2207
Kostin S, Scholz D, Shimada T, Maeno Y, Mollnau H, Hein S, Schaper J (1998) The internal and external protein scaffold of the T-tubular system in cardiomyocytes. Cell Tissue Res 294:449–460
Lader AS, Kwiatkowski DJ, Cantiello HF (1999) Role of gelsolin in the actin filament regulation of cardiac L-type calcium channels. Am J Physiol 277:C1277–C1283
Laporte J, Hu LJ, Kretz C, Mandel JL, Kioschis P, Coy JF, Klauck SM, Poustka A, Dahl N (1996) A gene mutated in X-linked myotubular myopathy defines a new putative tyrosine phosphatase family conserved in yeast. Nat Genet 13:175–182
Lauritzen HP, Ploug T, Prats C, Tavare JM, Galbo H (2006) Imaging of insulin signaling in skeletal muscle of living mice shows major role of T-tubules. Diabetes 55:1300–1306
Leach RN, Desai JC, Orchard CH (2005) Effect of cytoskeleton disruptors on L-type Ca channel distribution in rat ventricular myocytes. Cell Calcium 38:515–526
Li ZP, Burke EP, Frank JS, Bennett V, Philipson KD (1993) The cardiac Na+–Ca2+ exchanger binds to the cytoskeletal protein ankyrin. J Biol Chem 268:11489–11491
Lin JJ, Warren KS, Wamboldt DD, Wang T, Lin JL (1997) Tropomyosin isoforms in nonmuscle cells. Int Rev Cytol 170:1–38
Lloyd CM, Berendse M, Lloyd DG, Schevzov G, Grounds MD (2004) A novel role for non-muscle gamma-actin in skeletal muscle sarcomere assembly. Exp Cell Res 297:82–96
LoRusso SM, Rhee D, Sanger JM, Sanger JW (1997) Premyofibrils in spreading adult cardiomyocytes in tissue culture: evidence for reexpression of the embryonic program for myofibrillogenesis in adult cells. Cell Motil Cytoskelet 37:183–198
Lowe JS, Palygin O, Bhasin N, Hund TJ, Boyden PA, Shibata E, Anderson ME, Mohler PJ (2008) Voltage-gated Nav channel targeting in the heart requires an ankyrin-G dependent cellular pathway. J Cell Biol 180:173–186
Lubit BW (1984) Association of beta-cytoplasmic actin with high concentrations of acetylcholine receptor (AChR) in normal and anti-AChR-treated primary rat muscle cultures. J Histochem Cytochem 32:973–981
Lubit BW, Schwartz JH (1980) An antiactin antibody that distinguishes between cytoplasmic and skeletal muscle actins. J Cell Biol 86:891–897
Messina DA, Lemanski LF (1989) Immunocytochemical studies of spectrin in hamster cardiac tissue. Cell Motil Cytoskelet 12:139–149
Mohler PJ, Wehrens XHT (2007) Mechanisms of human arrhythmia syndromes: abnormal cardiac macromolecular interactions. Physiology 22:342–350
Mohler PJ, Rivolta I, Napolitano C, LeMaillet G, Lambert S, Priori SG, Bennett V (2004) Nav1.5 E1053K mutation causing Brugada syndrome blocks binding to ankyrin-G and expression of Nav1.5 on the surface of cardiomyocytes. Proc Nat Acad Sci USA 101:17533–17538
Mohler PJ, Davis JQ, Bennett V (2005) Ankyrin-B coordinates the Na/K ATPase, Na/Ca exchanger, and InsP3 receptor in a cardiac T-tubule/SR microdomain. PLoS Biol 3:e423
Nakata T, Nishina Y, Yorifuji H (2001) Cytoplasmic γ-actin as a Z-disc protein. Biochem Biophys Res Commun 286:156–163
Otey CA, Kalnoski MH, Bulinski JC (1987) Identification and quantification of actin isoforms in vertebrate cells and tissues. J Cell Biochem 34:113–124
Papponen H, Kaisto T, Leinonen S, Kaakinen M, Metsikko K (2009) Evidence for γ-actin as a Z disc component in skeletal myofibers. Exp Cell Res 315:218–225
Pardo JV, Pittenger MF, Craig SW (1983a) Subcellular sorting of isoactins: selective association of gamma actin with skeletal muscle mitochondria. Cell 32:1093–1103
Pardo JV, Siliciano JD, Craig SW (1983b) A vinculin-containing cortical lattice in skeletal muscle: transverse lattice elements (“costameres”) mark sites of attachment between myofibrils and sarcolemma. Proc Natl Acad Sci USA 80:1008–1012
Percival JM, Thomas G, Cock TA, Gardiner EM, Jeffrey PL, Lin JJ, Weinberger RP, Gunning P (2000) Sorting of tropomyosin isoforms in synchronised NIH 3T3 fibroblasts: evidence for distinct microfilament populations. Cell Motil Cytoskelet 47:189–208
Percival JM, Hughes JAI, Brown DL, Schevzov G, Heimann K, Vrhovski B, Bryce N, Stow JL, Gunning PW (2004) Targeting of a tropomyosin isoform to short microfilaments associated with the golgi complex. Mol Biol Cell 15:268–280
Ploug T, van Deurs B, Ai H, Cushman SW, Ralston E (1998) Analysis of GLUT4 distribution in whole skeletal muscle fibers: identification of distinct storage compartments that are recruited by insulin and muscle contractions. J Cell Biol 142:1429–1446
Porter GA, Dmytrenko GM, Winkelmann JC, Bloch RJ (1992) Dystrophin colocalizes with beta-spectrin in distinct subsarcolemmal domains in mammalian skeletal muscle. J Cell Biol 117:997–1005
Prins KW, Lowe DA, Ervasti JM (2008) Skeletal muscle-specific ablation of γ-cyto-actin does not exacerbate the mdx phenotype. PLoS ONE 3:e2419
Rudich A, Klip A (2003) Push/pull mechanisms of GLUT4 traffic in muscle cells. Acta Physiol Scand 178:297–308
Rueckschloss U, Isenberg G (2001) Cytochalasin D reduces Ca2+ currents via cofilin-activated depolymerization of F-actin in guinea-pig cardiomyocytes. J Physiol 537:363–370
Rybakova IN, Ervasti JM (2005) Identification of spectrin-like repeats required for high affinity utrophin–actin interaction. J Biol Chem 280:23018–23023
Rybakova IN, Patel JR, Ervasti JM (2000) The dystrophin complex forms a mechanically strong link between the sarcolemma and costameric actin. J Cell Biol 150:1209–1214
Rybakova IN, Patel JR, Davies KE, Yurchenco PD, Ervasti JM (2002) Utrophin binds laterally along actin filaments and can couple costameric actin with sarcolemma when overexpressed in dystrophin-deficient muscle. Mol Biol Cell 13:1512–1521
Sanger JW, Kang S, Siebrands CC, Freeman N, Du A, Wang J, Stout AL, Sanger JM (2006) How to build a myofibril. J Muscle Res Cell Motil 26:1343–1354
Schevzov G, Bryce NS, Monte-Baldonado R, Joya J, Lin JJ, Hardeman E, Weinberger R, Gunning P (2005a) Specific features of neuronal size and shape are regulated by tropomyosin isoforms. Mol Biol Cell 16:3425–3437
Schevzov G, Vrhovski B, Bryce NS, Elmir S, Qiu MR, O’Neill GM, Yang N, Verrills NM, Kavallaris M, Gunning PW (2005b) Tissue-specific tropomyosin isoform composition. J Histochem Cytochem 53:557–570
Schevzov G, Fath T, Vrhovski B, Vlahovich N, Rajan S, Hook J, Joya JE, Lemckert F, Puttur F, Lin JJC et al (2008) Divergent regulation of the sarcomere and the cytoskeleton. J Biol Chem 283:275–283
Schwartz RJ, Rothblum KN (1981) Gene switching in myogenesis: differential expression of the chicken actin multigene family. Biochemistry 20:4122–4129
Shani M, Zevin-Sonkin D, Saxel O, Carmon Y, Katcoff D, Nudel U, Yaffe D (1981) The correlation between the synthesis of skeletal muscle actin, myosin heavy chain, and myosin light chain and the accumulation of corresponding mRNA sequences during myogenesis. Dev Biol 86:483–492
Sjoblom B, Salmazo A, Djinovic-Carugo K (2008) Alpha-actinin structure and regulation. Cell Mol Life Sci 65:2688–2701
Sonnemann KJ, Fitzsimons DP, Patel JR, Liu Y, Schneider M, Moss RL, Ervasti J (2006) Cytoplasmic γ-actin is not required for skeletal muscle development but its absence leads to a progressive myopathy. Dev Cell 11:387–397
Takeda K, Yu ZX, Qian S, Chin TK, Adelstein RS, Ferrans VJ (2000) Nonmuscle myosin II localizes to the Z-lines and intercalated discs of cardiac muscle and to the Z-lines of skeletal muscle. Cell Motil Cytoskelet 46:59–68
Talior-Volodarsky I, Randhawa VK, Zaid H, Klip A (2008) Alpha-actinin-4 is selectively required for insulin-induced GLUT4 translocation. J Biol Chem 283:25115–25123
Tondeleir D, Vandamme D, Vandekerckhove J, Ampe C, Lambrechts A (2009) Actin isoform expression patterns during mammalian development and in pathology: insights from mouse models. Cell Motil Cytoskelet 66:798–815
Tong P, Khayat ZA, Huang C, Patel N, Ueyama A, Klip A (2001) Insulin-induced cortical actin remodeling promotes GLUT4 insertion at muscle cell membrane ruffles. J Clin Invest 108:371–381
Tsakiridis T, Vranic M, Klip A (1994) Disassembly of the actin network inhibits insulin-dependent stimulation of glucose transport and prevents recruitment of glucose transporters to the plasma membrane. J Biol Chem 269:29934–29942
Vandekerckhove J, Weber K (1978) At least six different actins are expressed in a higher mammal: an analysis based on the amino acid sequence of the amino-terminal tryptic peptide. J Mol Biol 126:783–802
Vlahovich N, Schevzov G, Nair-Shaliker V, Ilkovski B, Artap ST, Joya JE, Kee AJ, North KN, Gunning PW, Hardeman EC (2008) Tropomyosin 4 defines novel filaments in skeletal muscle associated with muscle remodelling/regeneration in normal and diseased muscle. Cell Motil Cytoskelet 65:73–85
Vlahovich N, Kee AJ, van der Poel C, Kettle E, Hernandez-Deviez D, Lucas C, Lynch GS, Parton RG, Gunning PW, Hardeman EC (2009) Cytoskeletal tropomyosin Tm5NM1 is required for normal excitation–contraction coupling in skeletal muscle. Mol Biol Cell 20:400–409
von Arx P, Bantle S, Soldati T, Perriard JC (1995) Dominant negative effect of cytoplasmic actin isoproteins on cardiomyocyte cytoarchitecture and function. J Cell Biol 131:1759–1773
Vrhovski B, Schevzov G, Dingle S, Lessard JL, Gunning P, Weinberger RP (2003) Tropomyosin isoforms from the gamma gene differing at the C-terminus are spatially and developmentally regulated in the brain. J Neurosci Res 72:373–383
Yoshizaki T, Imamura T, Babendure JL, Lu JC, Sonoda N, Olefsky JM (2007) Myosin 5a is an insulin-stimulated Akt2 (Protein Kinase B{β}) substrate modulating GLUT4 vesicle translocation. Mol Cell Biol 27:5172–5183
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Kee, A.J., Gunning, P.W. & Hardeman, E.C. Diverse roles of the actin cytoskeleton in striated muscle. J Muscle Res Cell Motil 30, 187–197 (2009). https://doi.org/10.1007/s10974-009-9193-x
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DOI: https://doi.org/10.1007/s10974-009-9193-x