An improved method for culturing myotubes on laminins for the robust clustering of postsynaptic machinery


Motor neurons form specialized synapses with skeletal muscle fibers, called neuromuscular junctions (NMJs). Cultured myotubes are used as a simplified in vitro system to study the postsynaptic specialization of muscles. The stimulation of myotubes with the glycoprotein agrin or laminin-111 induces the clustering of postsynaptic machinery that contains acetylcholine receptors (AChRs). When myotubes are grown on laminin-coated surfaces, AChR clusters undergo developmental remodeling to form topologically complex structures that resemble mature NMJs. Needing further exploration are the molecular processes that govern AChR cluster assembly and its developmental maturation. Here, we describe an improved protocol for culturing muscle cells to promote the formation of complex AChR clusters. We screened various laminin isoforms and showed that laminin-221 was the most potent for inducing AChR clusters, whereas laminin-121, laminin-211, and laminin-221 afforded the highest percentages of topologically complex assemblies. Human primary myotubes that were formed by myoblasts obtained from patient biopsies also assembled AChR clusters that underwent remodeling in vitro. Collectively, these results demonstrate an advancement of culturing myotubes that can facilitate high-throughput screening for potential therapeutic targets for neuromuscular disorders.


Vertebrate neuromuscular junctions (NMJs) are synapses between motor neurons and skeletal muscle fibers. The function of this type of synapse is to transmit signals from the central nervous system to muscles and thus stimulate their contraction. The nerve terminal releases the neurotransmitter acetylcholine (ACh), which binds to postsynaptic ACh receptors (AChRs) that are located on the surface of muscle fibers. For efficient synaptic transmission, muscle fibers need to accumulate a high density of AChRs in their postsynaptic membrane1,2,3,4. Rodent muscles cluster components of postsynaptic machinery around day 12 of embryonic development (i.e., before motor neuron axons approach muscle fibers)5,6. Innervation leads to the dispersion of preexisting AChR clusters2,7. A single postsynaptic machinery is formed per muscle fiber directly below the nerve terminal. The nerve plays a crucial role in organizing NMJ postsynaptic machinery by secreting signaling molecules, such as agrin and ACh, which regulate the clustering and dispersion of AChRs, respectively2,8,9,10,11,12. Nerve-derived agrin binds to the surface of low-density lipoprotein receptor-related protein (Lrp4), which activates muscle-specific kinase (MuSK)13. This triggers an intracellular signaling cascade that activates AChR clustering by the scaffold protein rapsyn2. In mice during the first postnatal weeks, NMJs grow in size and undergo developmental remodeling from simple plaque-shaped structures to topologically complex assemblies2,14. During this process, postsynaptic machinery becomes perforated with scattered openings that, with time, become more numerous and fuse with each other to form indentations between AChR-rich branches that transform synapses into pretzel-like shapes15,16. The molecular mechanisms that underlie developmental remodeling are poorly understood.

The clustering process and synapse remodeling are facilitated by macromolecular complexes that are involved in cellular adhesion that interact with extracellular matrix (ECM) components and the cytoskeleton. The major ECM receptors contain integrin complexes and the dystrophin-associated glycoprotein complex17,18,19. These protein assemblies stabilize postsynaptic components and provide a platform for the recruitment of signaling molecules that regulate postsynaptic specialization18,20. Muscle cells form a thick ECM around the fiber that contains various laminins, collagens, fibronectin, and other glycoproteins21. Laminins are heterotrimeric glycoproteins that are composed of α, β, and γ chains that are encoded by different genes22,23. The different laminin trimers have various specificities for cellular receptors and can regulate different signaling pathways24,25,26,27. The basal lamina (BL) at the synaptic cleft has a specific molecular composition that contains laminin α4, α5, and β2 isoforms that are mostly absent in extrasynaptic regions of muscle fibers22,28. These ECM components are crucial for the proper development of NMJs. Laminin β2 knock-out mice have severe phenotypes of reduced synaptic folding and drastically decreased synaptic transmission29,30. In laminin α4/α5 double-mutant mice, NMJs form normally but fail to undergo developmental remodeling31,32,33. A similar phenotype was observed with the muscle-specific deletion of dystroglycan, the laminin receptor in muscle cells31. This indicates that the laminin-dystroglycan interaction is crucial for regulating NMJ developmental remodeling. Studies of postnatal NMJ reorganization in vivo are complicated by the fact that different cells (e.g., motor neurons and Schwann cells) may contribute to this process. Aneurally cultured differentiated myotubes are often used as a simplified model to study postsynaptic machinery34,35,36. The stimulation of cultured myotubes with agrin is the most commonly used method to induce the formation of AChR clusters in vitro35,36. The major limitation of this approach, however, is that AChR clusters do not undergo the remodeling process. The formation of AChR clusters in cultured myotubes can also be stimulated by laminins34,37. Recent studies demonstrated that the culturing of muscle cells on mouse laminin-111-coated surfaces leads to the formation of topologically complex clusters of postsynaptic machinery that resemble clusters at the NMJ in vivo34. Moreover, the complex shape of the cluster is achieved through morphological transformation that is similar to such transformation at the NMJ and involves the formation of perforations in the initially plaque-shaped clusters. Cultured myotubes that were derived from primary myoblasts or C2C12 myoblasts were shown to utilize podosomes to remodel postsynaptic machinery38,39. These actin-rich organelles are involved in cellular adhesion and the degradation of ECM components, including laminins40,41. Little is known about the mechanisms of postsynaptic machinery remodeling in vivo. Myotubes cultured on laminin are the only in vitro system where the AChR clusters undergo developmental remodeling, providing the model to study the underlying mechanisms.

Myotubes that form AChR clusters can be used to study the mechanisms that underlie pathological processes in both congenital and autoimmune muscle disorders42,43. Defects in NMJ remodeling from “plaque” to “pretzel” shapes are frequently observed in many rodent models of neuromuscular disorders16,44. Some of these disorders still have an unknown etiology, thus highlighting the importance of studying the mechanisms of NMJ development.

The present study demonstrated an improved protocol for culturing myoblasts that allowed the reproducible formation of AChR clusters. We tested several commercially available recombinant human laminin isoforms for their ability to induce AChR cluster formation and their ability to promote AChR cluster remodeling. Our observations provide an important basis for high-throughput genetic screening and potential drug development. We also found that human primary myotubes that were derived from myoblasts obtained from patient biopsies were also able to form AChR clusters with complex topology that contained synaptic podosomes.


Optimal culturing of myoblasts for efficient AChR clustering

The postsynaptic machinery at NMJs is a topologically complex structure (Fig. 1a) that contacts hundreds of different proteins. Studying postsynaptic machinery organization in vivo in tissues can be experimentally challenging. Differentiated myotubes that are cultured in vitro provide a simplified model to study basic processes that underlie postsynaptic specialization34,36. Three methods are the most commonly used to stimulate myotubes for AChR cluster formation. The recombinant, neuron-derived glycoprotein agrin can be added to the media or deposited at the culturing surface35,36. Soluble agrin triggered the formation of small AChR aggregates at apical and lateral surfaces of myotubes (Fig. 1b), whereas precoated agrin induced the formation of much larger oval assemblies (Fig. 1c)36. Alternatively, myotubes can be stimulated for AChR clustering by precoating the culture surface with laminins34. Myotubes derived from C2C12 cells or primary myoblasts that were cultured on murine laminin formed numerous large AChR clusters at the bottom of myotubes that often acquired a complex topology that was reminiscent of postsynaptic machinery at the NMJ (Fig. 1d)34,45,46.

Figure 1

Models for studying muscle postsynaptic machinery. (a) Complex structure of postsynaptic machinery at the murine NMJ (b) Differentiated C2C12 myotubes that were stimulated with a neuron-specific splice variant of the glycoprotein agrin that was supplemented to the media formed small, elongated AChR clusters on the lateral and apical sides of the myotubes. (c) C2C12 myotubes that were grown on a laminin substratum with deposited agrin patches formed large uniform AChR assemblies at the basal surface of the myotubes. (d) C2C12 myotubes that were grown on mouse laminin-111-coated surfaces formed clusters of postsynaptic machinery that underwent developmental remodeling to topologically complex assemblies that resembled the shape of postsynaptic machinery at the NMJ. Scale bar = 6 μm. AChRs were visualized with α-bungarotoxin.

Laminin-cultured myotubes are particularly useful because they can provide insights into the mechanism of postsynaptic machinery remodeling. This system has been used by many laboratories because it is relatively easy. Nonetheless, some groups have experienced problems with obtaining a reproducibly high number of AChR clusters that is sufficient for downstream experiments. Our laboratory found that most problems with laminin-cultured myotubes result from the inappropriate culturing of cells before dedifferentiation. The most common source of such problems is the culturing of myoblasts at an inappropriate density. The present study reports a relatively simple method of myoblast culturing that yields the most reliable results. Figure 2a shows images of the optimal density for cell splitting (green frame, approximately 1.0 × 106 cells/cm2) and cells that were grown too densely or too sparsely (red frames). Myoblasts that are too sparse in cultures grow slowly and tend to form clusters. Conversely, excessive cell-cell contacts lead to dedifferentiation and the loss of myogenic potential. In such case, the cells can still form elaborate myotubes but fail to cluster AChRs or the clusters are too small, underdeveloped, or scarce. Consequently, every subsequent generation of myoblasts has a lower capacity to form numerous and mature AChR clusters. Thus if cells are seeded at the 1.0 × 106 cells/cm2 density, they should be passaged maximum 48 hours after initial seeding as the number of C2C12 usually doubles after 18 hours. For optimal experimental reproducibility, myoblasts should be of a low passage number and should be analyzed after the same number of amplifications. Figure 2b shows an optimal scheme of passaging that we implement in our laboratory to obtain a large number of cells (up to 1000 vials) at passage 5 (P5).

Figure 2

Method for culturing of C2C12 cells to obtain high yields of AChR clusters. (a) Examples of suboptimal (red boxes) and optimal (green box) cell densities for passaging. Yellow arrows show the area of excessive cell contacts that should be avoided. Cells were plated at the same time at varying densities. Cells highlighted by the green box were seeded at approximately 1.0× 106 cells/cm2 cultured on a 10 cm dish. (b) Schematic diagram of C2C12 cell passages to obtain a high number of cell stocks at an equally low number of passages. (c) Schematic diagram of the key steps during C2C12 cells culturing that are important for obtaining high yields of AChR clusters. The images show optimal (green box) and suboptimal (red boxes) cell densities for fusion initiation. Red arrowheads show areas that are not covered by cells. Yellow arrows show regions where single-cell morphology can be observed. For the highest amount of fully differentiated myotubes with AChR clusters, myoblasts should form a dense cell layer in which cell morphology is difficult to distinguish. (d) Schematic diagram of the key steps during human primary myoblast culturing that are important for obtaining high yields of AChR clusters. The differences in the protocol for handling of C2C12 cells and human primary myoblasts are highlighted in blue. Scale bar = 600 μm in a and 450 μm in c.

The next critical step for obtaining a large number of AChR clusters in cultures involves performing appropriate steps for cell preparation for differentiation on laminin-coated surfaces. After thawing, frozen cells (2.0 × 105 cells per vial) are plated on gelatin-coated dish and should be passaged twice (up to P7) and seeded on laminin in sufficient density (0.8 × 105 cells/cm2) for fusion between 24 and 48 h. The prolongation of cell growth on laminin could result in substrate degradation and a poor yield of AChR clusters. Obtaining a high density of cells upon differentiation induction is critical (Fig. 2c) because a culture that is too sparse results in poorly differentiated myotubes and myoblasts that are too dense and lose their myogenic potential47,48. Finally, differentiating myotubes should not be agitated during the fusion process. Larger myotubes tend to detach easily during medium washes, which should be avoided. Rapid shifts in temperature also result in myotube detachment. Therefore, we do not recommend removing differentiating cells from the incubator during the fusion process.

We use the same protocol for culturing human primary myoblasts, with the notable exceptions of higher seeding density (1.0 × 105 cells) on laminins and longer fusion time (8 days) (Fig. 2d). All other steps, including thawing, passaging and general handling remain the same as described above for C2C12 cell line.

AChR clustering in C2C12 myotubes that are cultured on different laminins

Myotubes grown on plain plastic, glass or gelatin-covered surface spontaneously form a small number of topologically simple AChR clusters (Fig. S1a). Mouse laminin-111 has been routinely used to induce AChR clustering34. Various laminin isoforms have different properties. We examined the ability of different laminin isoforms to induce the clustering of muscle postsynaptic machinery in cultured C2C12 myotubes. We cultured cells on recombinant human laminin-111, laminin-121, laminin-211, laminin-221, laminin-411, laminin-421, laminin-511, and laminin-521. Coating the culture surfaces with laminin-111, laminin-121, laminin-211, laminin-221, laminin-511, and laminin-521 led to the formation of numerous AChR clusters (Fig. 3a). Because myotubes grown in absence of laminin do not form complex AChR clusters (Fig. S1a), we used the most commonly implemented laminin-111 as a reference while assessing the properties of other laminin isoforms (Fig. 3a,b). Surprisingly, laminin-111 reproducibly yielded a lower number of clusters compared with the several other laminins (Fig. 3a,b). In contrast, laminin trimers that contained the α4 chain (i.e., laminin-411 and laminin-421) were very inefficient in inducing AChR aggregates (Fig. 3a,b), and AChR aggregates that formed had a fragmented appearance (Fig. 3a, insets). This could be because of the lack of N-terminal domain in the α4 chain, which is present in other α isoforms and which serves as a binding site for integrin and other cell surface receptors (Fig. 3d). We have also evaluated the effects of combining two different human recombinant laminin isoforms on AChR clustering. Our results suggest that certain laminins have a synergistic effect on the efficiency of AChR clustering. As such, combining laminin-121 with laminin-221 for coating of culturing surface doubled the number of clusters produced by myotubes when compared to results of these isoforms on their own (Figs. 3e,f; S1b).

Figure 3

Clustering of AChRs in C2C12 myotubes cultured on different human laminins. (a) Representative images of AChR clusters in myotubes that were cultured on Permanox slides coated with the indicated laminins. Scale bar = 150 μm. (b) Quantification of AChR clusters formed by myotubes that were grown on Permanox slides coated with the indicated laminins. Quantifications represent the average number of clusters. For all laminins except laminin-111, laminin-411, and laminin-421, the total number of clusters that were used for the analysis was> 300. For laminin-111, 216 clusters were used. For laminin-411, 25 clusters were used. For laminin-421, 30 clusters were used. The clusters were collected from five independent experiments performed on different days. (c) Different laminins induced similar levels of AChR-α1 subunit expression in myotubes. HEK293 cell lysates were used as a negative control. Tubulin was used as a loading control. (d) Schematic representation of laminin-111, 211, 411, 511. LN domains are shown in green, L4 domains in red, LF domain in yellow and LG domains in orange. (e) Representative images of AChR clusters in myotubes that were cultured on the indicated laminin combinations. (f) Quantification of AChR clusters formed by myotubes grown on indicated combinations of laminin isoforms. The total number of clusters used in the analysis was>160 for 121 + 221 and 211 + 221; for 121 + 211 it was 71 and for 111 + 221 it was 99. Quantifications represent the average number of clusters. Scale bar = 150 μm. *p < 0.05, **p < 0.005, ***p < 0.0005. For statistical analysis we used one way ANOVA with Dunnett test; laminin-111 used as a reference. Error bars represent SEM values. AChRs were visualized with α-bungarotoxin.

The culturing of myotubes on various laminins led to the similar induction of AChR production, analyzed by Western blot (Figs. 3c; S1c). To exclude the possibility that the observed differences were attributable to varying levels of laminins that adhered to the surfaces during coating, we analyzed material that adhered to the culture wells after coating using silver staining. As shown in Supplementary Fig. S2a and b, similar amounts of each laminin were recovered in three independent experiments. Thus, the differences that we observed likely reflected the ability of individual laminins to induce AChR clustering. We have also calculated the myotube diameter in order to exclude the possibility that the observed differences are attributable to better myotube quality. Additionally we measured the average size of cluster stimulated by each laminin and found that while the myotube diameter remained similar for each laminin, laminin-511 led to production of slightly larger clusters than any other isoform (Fig. S2c and d).

Myoblast fusion in vitro is dependent on the cell attachment, which can be different for various laminins49,50. More efficient fusion and better attachment are both factors that affect the quality and the number of AChR clusters produced by myotubes31. We thus measured the fusion index of cells grown on each tested laminin isoform. For C2C12 the fusion index directly correlated to the number of AChR clusters. As such, laminin-221 and laminin-121 produced the highest number of clusters and had the highest fusion index (Fig. S3a and c).

Effect of different laminins on AChR cluster formation in C2C12 myotubes

The assemblies of postsynaptic machinery in laminin-cultured C2C12 myotubes underwent developmental remodeling that resembled maturation of rodent NMJ in vivo (Fig. 4a)34,51. During this process, oval, plaque-shaped AChR clusters (Fig. 4a,c) became perforated and acquired a much more complex topology. Some of the remodeled clusters acquired C-shaped topology, in which a large portion of AChRs was removed from the center of the assembly (Fig. 4a,e)34. Other clusters had a perforated pretzel-like shape with actin-rich structures, known as synaptic podosomes, that interdigitated AChR-rich domains (Fig. 4a,g)38,51.

Figure 4

Different AChR cluster morphologies in C2C12 myotubes grown on various human laminins. (a) Schematic diagram showing developmental remodeling of postsynaptic machinery. Actin-rich podosomes are represented as red spheres. (b) Quantification of plaque-shaped clusters, presented as the average percentage of clusters. (c) Example of plaque-shaped cluster. (d) Quantification of C-shaped clusters, presented as the average percentage of clusters. (e) Example of C-shaped cluster. (f) Quantification of perforated clusters that contained synaptic podosomes, presented as the average percentage of clusters. (g) Example of cluster that contained actin-rich podosomes. Scale bar = 6 μm. Quantifications represent the average number of clusters. For all laminins except laminin-111, laminin-411, and laminin-421, the total number of clusters that were used for the analysis was> 300. For laminin-111, 216 clusters were used. For laminin-411, 25 clusters were used. For laminin-421, 30 clusters were used. Clusters were collected from five independent experiments performed on five different days. *p < 0.05, **p < 0.005, ***p < 0.0005. For statistical analysis we used one way ANOVA with Dunnett test; laminin-111 used as a reference. Error bars represent SEM values. AChR (green) was visualized with α-bungarotoxin. F-actin (red) was visualized with phalloidin.

Interestingly, C2C12 myotubes that were cultured on different human laminins exhibited alterations of the maturation of AChR clusters. Of the tested laminin isoforms, none increased plaque-shaped clusters compared with isoform-111 (Fig. 4b,c). Cultures on laminin-121 and laminin-211, which led to the formation of numerous clusters (Fig. 3a,b), produced significantly fewer immature plaque-like AChR aggregates (Fig. 4b,c). Laminin-121 and laminin-211 appeared to induce fewer C-shaped clusters than laminin-111, although the effect of laminin-211 did not reach statistical significance (Fig. 4d). The highest percentage of C-shaped structures was observed in myotubes that were cultured on laminin-221 (Fig. 4d,e). Laminin-221, similar to laminin-511, induced significantly fewer perforated clusters with actin-rich podosomes compared with laminin-111 (Fig. 4f,g). The highest percentage of perforated clusters (>70%) was formed by cells that were grown on laminin-121 and laminin-211 (Fig. 4f,g). Interpreting the types of clusters formed by cells that were cultured on laminins that contained the α4 isoform (i.e., laminin-411 and laminin-421) was more difficult because these cells made hardly any aggregates (Fig. 3a,b). These findings indicate that different types of laminins that are used for coating exert differential effects on the developmental remodeling of AChR clusters in cultured C2C12 myotubes.

We also evaluated presence of rapsyn, a scaffold protein present at the postsynaptic machinery that is crucial for AChR assembly2. As expected, rapsyn was similarly localized to the AChR clusters irrespectively of the used laminin isoform, and its expression levels were comparable for each culture (Fig. S4a and b).

AChR cluster formation and remodeling in primary human myotubes

Myotubes that are derived from human patients myoblasts can be used to study the molecular processes that underlie pathological alterations associated with neuromuscular disease and screening novel therapeutics52. We analyzed the ability of human primary myotubes to form clusters of postsynaptic machinery on different laminins. In contrast to C2C12 myotubes, most of the laminins that were used for coating did not significantly influence the efficiency of AChR clustering (Fig. 5a) or cell fusion (Fig. S3b). Most of the AChR clusters that formed in human myotubes had a simple, plaque-like shape (Fig. 5b,c). However, some AChR clusters underwent topological reorganization, with visible perforations within the clusters (Fig. 5d,e). These perforations appeared to be similar to those in C2C12-derived myotubes (Figs. 1, 4g). Perforations in C2C12 clusters are formed by synaptic podosomes38. Therefore, we examined whether human myotubes also form these organelles during cluster remodeling. Immunocytochemical analysis revealed that perforated areas in AChR assemblies in human myotubes contained actin-rich cores38,40. In typical podosomes, these actin-rich structures are surrounded by the cortex domain that is enriched in proteins that are associated with cellular adhesion38,40,45,53. As expected, AChR clusters in human myotubes also had strong vinculin and LL5β immunoreactivity in the cortex-like domain that abutted actin-rich cores (Fig. 5e,f). Interestingly, most of the tested laminins produced more clusters with complex topology than laminin-111 (Fig. 5d). Thus, AChR clusters in human primary myotubes were able to undergo developmental remodeling, and this process involved podosome formation.

Figure 5

Effect of various laminins on AChR cluster formation and remodeling in human primary myotubes. (a) Quantification of AChR clusters formed by human primary myotubes that were cultured on the indicated laminins. (b) Quantification of plaque-shaped AChR clusters formed by human primary myotubes that were cultured on the indicated laminins, presented as the average percentage of clusters. (c) Example of plaque-shaped cluster. (d) Quantification of perforated clusters that contained synaptic podosomes, presented as the average percentage of clusters. (e, f) Examples of clusters that contained actin-rich podosomes that were immunostained for podosome cortex protein markers vinculin (e) and LL5β (f). Scale bar = 6 μm. Quantifications represent the average number of clusters. For all laminins except laminin-221, the total number of clusters that were used for the analysis was> 140. For laminin-221, 83 clusters were used. Clusters were collected from three independent experiments performed on three different days. *p < 0.05, **p < 0.005, ***p < 0.0005. For statistical analysis we used one way ANOVA with Dunnett test; laminin-111 used as a reference. Error bars represent SEM values. AChR (red) was visualized with α-bungarotoxin. F-actin (blue) was visualized with phalloidin.


Myotubes that are cultured on laminin-coated surfaces provide a unique in vitro system whereby clusters of muscle postsynaptic machinery undergo robust developmental remodeling31,34,38. Several laboratories, however, have experienced difficulties in culturing myotubes that reproducibly form AChR clusters with complex topology. Herein, we describe an improved protocol for culturing C2C12 muscle cells as well as a description for culturing human primary myotubes to study the mechanisms that govern postsynaptic machinery development and remodeling. Our protocol is useful for obtaining and freezing a large number of cell stocks and utilizing cells for experimentation with a constant and low passage number, which significantly increases experimental reproducibility. However, we observe the decline of cells ability to form complex AChR clusters after 8–10 passages in the laboratory. It is worth mentioning, that commercially acquired C2C12 cells are an immortalized cell line generated decades ago, thus their actual passage number may vary depending on the supplier and particular lots that have been ordered. We tested several laminin isoforms that are commercially available and found that laminin-121, laminin-211, laminin-221, laminin-511, and laminin-521 induced significantly more AChR clusters in C2C12 myotubes than the commonly used laminin-111. Moreover, we found that clusters of postsynaptic machinery that were formed in C2C12 myotubes cultured on laminin-121 and laminin-221 were the most developed. It is interesting that laminin-121 induced efficiently AChR clustering although this isoform is absent in the synaptic basal lamina. It is possible, however, that this trimer facilitates adhesion and stimulates AChR clustering despite being absent at the NMJ. Myotubes that were derived from human primary myoblasts obtained from human biopsies also formed AChR clusters that underwent developmental remodeling. Although human NMJs acquire the “en grape” shape rather than a more complex”pretzel”-like topology observed in rodents, we observed that synaptic podosomes also form in cultured human myotubes. This may suggest that initial steps of postsynaptic machinery remodeling are similar in both species. Unfortunately, there is no data about developmental remodeling of human NMJ and how the “en grape” shape of the junction is achieved thus our method may be useful in future studies regarding this process. We also show that laminin-421 and laminin-511 were the isoforms that promoted formation of the most podosome-containing AChR clusters in human primary myotubes.

The AChR clustering depends on the attachment to the substratum31. C2C12 cells fusion index was significantly different on various laminins. Human primary myoblasts also exhibit some variations in fusion, however the differences did not reach statistical significance.

The molecular mechanisms that underlie the developmental remodeling of NMJs and muscle postsynaptic machinery are poorly understood, likely because of the various cell types (e.g., muscle cells, Schwann cells, and motor neurons) that could contribute to this process. In vitro-cultured myotubes provide a minimalistic system whereby at least some aspects of AChR regulation can be studied14. C2C12 and mouse primary myotubes utilize podosomes to remodel postsynaptic machinery when cultured on laminin38. There is no evidence, however, of the presence of podosomes at NMJs in vivo. Several podosome-associated proteins have been shown to be present at the muscle postsynaptic specialization, and they may be involved in the remodeling process45,51.

NMJ postnatal transformation from”plaques” to “pretzels” has been shown to depend on the laminin-dystroglycan signaling pathway31. Integrins are also involved in the organization and stabilization of postsynaptic machinery, but their direct roles in developmental synapse remodeling is unclear54. Laminin trimers contain several binding sites for their surface receptors. The N’-terminal portion of most of α isoforms (missing in laminin α4) interacts with integrins and globular domains located at the C-terminus of laminin α chains bind α-dystroglycan24 (Fig. 3d). Each α chain contains five laminin globular subunits (LG1–5)27. Depending on the isoform of the α chain, different modules are utilized for the interaction with α-dystroglycan25. Despite differences in the localization of interaction sites, they all share the common feature of being calcium-dependent. Interestingly, agrin also interacts with α-dystroglycan in a calcium-dependent manner through its own laminin globular module26. Our observation that laminins containing the α4 chain induce clustering of AChRs in human primary muscles but not in C2C12, hints toward possibility that the formation of AChR clusters in C2C12 cells have different molecular requirements. It is also a possibility that efficiency of laminin polymerization through their LN domains is different for each tested isoform. This could result in differences in the accessibility to surface receptors, altered stiffness of the culturing surface, or ability of cells to produce and deposit endogenous laminins. All these are factors that may influence the efficiency of AChR clustering and remodeling. Another interesting line of investigation would be to test the affinities of laminin globular domains to α-dystroglycan in our experimental system, which may provide insights into the mechanisms of AChR cluster assembly.

In addition to being an intriguing biological process, the postnatal reorganization of synapses in topologically complex structures appears to be affected in many models of neuromuscular disorders2,44,55. Aberrant synaptic maturation may be linked to various pathological processes2,16. Several neuromuscular myopathies have an unknown etiology. This highlights the importance of studying the molecular aspects of NMJ development. The present method for culturing and stimulating myotubes to form and remodel AChR clusters may facilitate the identification of novel synaptic regulators. The high reproducibility of culturing and robust formation of AChR clusters are important prerequisites for establishing high-throughput screening. While our studies were performed using permanox slides, the method that we describe can also be implemented in other formats, such as glass surfaces38 as well as multi-well culturing dishes. The present study found that human cells that were derived from patient muscle biopsies formed AChR clusters in vitro that underwent the remodeling process, thus demonstrating the potential utility of this methodology for further studies that seek to improve diagnoses of neuromuscular disorders and elucidate their underlying mechanisms.

Materials and Methods

Passaging C2C12 cells

C2C12 myoblasts (catalog no. 13K011, Sigma) were cultured on 10 cm gelatin-coated plates. The surface of the plate was coated with 0.2% gelatin in double-distilled H2O that was then discarded after a few minutes. The plate was allowed to dry for 1–2 h in the laminar tissue culture. Cells (1 × 106/10 cm dish) were cultured in Dulbecco’s Modified Eagle Medium (DMEM; catalog no. 12–604 F, Lonza) with 20% fetal bovine serum (FBS; catalog no. E5050–02, lot no. 70932, EURx), 0.1% fungizone, and 1% penicillin/streptomycin. Different lots of FBS from the same suppliers may vary and can affect AChR clustering. Therefore, testing different lots of FBS and selecting the one that efficiently facilitates the clustering of postsynaptic machinery are important. At all stages of culturing, the cells were evenly spread on the dish to prevent dedifferentiation. Cells were passaged every 3 days and before they reached 30% confluence (see Fig. 2 for recommended densities). After trypsinization, the cells were collected by centrifugation at 419 g for 3 min, resuspended in fresh culture medium, and split according to a 1:6 ratio onto fresh gelatin-coated dishes that contained warm culture medium. Cells that are passaged this way take ~2 days to reach 30% confluence.

Freezing C2C12 cells

Each 10-cm dish that contained 4.0 × 105 cells C2C12 myoblasts was split between two freezing vials. After trypsinization, the cells were resuspended in 0.5 ml/vial of freezing medium I (DMEM with glutamine and 20% FBS at room temperature) and aliquoted into two separate vials. Pre-chilled freezing medium II (0.5 ml; DMEM with glutamine, 20% FBS, and 14% dimethylsulfoxide [DMSO; catalog no. A994.1, Roth]) was added. The vials were placed in a pre-chilled freezing container and moved immediately to −80 °C. After 1–2 days, frozen cell stocks were placed in a liquid nitrogen container that was suitable for long-term storage. The protocol for freezing human primary muscle cells was the same as for C2C12 cells.

Thawing frozen cells

To prevent cell damage that could be caused by DMSO, the cells were thawed quickly in a 37°C water bath and immediately placed on a gelatin-coated dish that contained 10 ml of pre-warmed culture medium. The medium that contained remnants of the freezing medium was replaced the next day.

Differentiation into myotubes

For myoblast fusion, we routinely use Permanox slides (catalog no. 160005, Thermo Fisher Scientific) and reusable Flexiperm eight-well grids (0.9 cm2 surface area/well), which is a suitable format for immunocytochemical microscopy and small-scale biochemical analysis. Flexiperm grids (catalog no. 6032039, Sarstedt) were sterilized by dipping in 100% ethanol, dried, and attached to Permanox slides. To induce AChR cluster formation, the Permanox surface was covered with mouse laminin 111 (catalog no. L2020-1MG, Sigma) or with recombinant human laminins (111; 121; 211; 221; 411; 421; 511; 521) provided with “Lamscreen” kit available through Biolamina (catalog no. LNKT-0201, Biolamina). For coating, 2 µg of each laminin (or mixture of laminins when indicated) was diluted in DMEM (200 µl/well). Frozen laminins were slowly thawed on ice to avoid aggregation that can result in uneven distribution on the slide. Importantly, the laminin solution needs to cover the well area evenly because uneven coating can affect the formation of AChR clusters and lead to the detachment of myotubes during differentiation. The Permanox slides were incubated with laminin overnight at 37 °C in the tissue culture incubator. The next day, 1 × 105 myoblasts were seeded per Flexiperm well (cell density of 1.4–1.6 × 105/ml). Myoblast differentiation into myotubes was induced 24 h after cell seeding on laminin-coated Permanox slides because a longer incubation time can result in the degradation of laminin, which would affect AChR cluster formation. Myotube differentiation was induced by gentle replacement of the culture medium with fusion medium (DMEM with glutamine, 2% horse serum [HS], 0.1% fungizone, and 1% penicillin/streptomycin). Importantly, a substantial volume of the medium (~700 µl/Flexiperm well) had to be added because replacing media during differentiation is not recommended. The cells were allowed to fuse for 4 days, with no cell agitation during that time because moving the slide or removing it from the incubator for microscopic inspection or medium replacement can significantly affect the attachment of large myotubes and interfere with their ability to form complex AChR clusters. For culturing cells on agrin-coated surface we used a previously described protocol36. Briefly, HEK293 cells were transfected with a plasmid coding for neuron-specific z-splice variant of agrin and seeded on Permanox slides. After 28 hours cells were treated with 2% Triton X-100 in PBS for 1 hour and washed 6 times in PBS. Myoblasts were then seeded on the same surface and fusion was carried out as described before.

Fixation and fluorescent staining

For fixation, the Permanox slides that contained differentiated myotubes were removed from the incubator and placed on a heat block at 37°C. The fusion medium was gently replaced with 4% paraformaldehyde (PFA) in phosphate-buffered saline (PBS). After the addition of PFA, the slides were removed from the heat block, followed by fixation for 7 min at room temperature. Paraformaldehyde was then removed, and each well was washed three times with PBS. For immunocytochemistry, the cells were blocked with blocking buffer (2% bovine serum albumin [BSA; catalog no. SC-2323, ChemCruz], 0.2% normal goat serum [NGS], and 0.05% Triton-X 100 [catalog no. T8787-100ML, Sigma]) for 30 min at room temperature. To visualize AChR clusters, F-actin cells were incubated for 30 min with AlexaFluor 488-α-bungarotoxin (1 ng/µl; catalog no. B13422, Invitrogen) and 100 nM Actistain conjugated to AlexaFluor 555 (catalog no. PHDH1, Cytoskeleton) in blocking buffer, followed by three washes with PBS. The Flexiperm grid was then gently removed, and 120 µl of Fluoromount was added to the Permanox slide, which was then sealed with a coverslip. For vinculin staining, primary antibody against vinculin (catalog no. V4506, Sigma) was used. For Ll5β staining, a previously described antibody was used45. For myosin II heavy chain staining a primary antibody against myosin II heavy chain (catalog no. 21-55-4, DSHB) was used.

Microscopic analysis

Microscopic analysis was performed at the Confocal Microscopy Facility, Nencki Institute, using a Zeiss Spinning Disc confocal microscope or Leica TCS SP8 scanning confocal microscope that was equipped with a diode or white light laser, respectively. Images were collected using ZEN software (ZEISS International) and analyzed using ImageJ/Fiji software. All measurements were taken using the ZEN software from photos acquired by the Zeiss Spinning Disc confocal microscope. Entire cluster area (including the perforations) was measured for all clusters used in the analysis of cluster size.

Fusion assay

For the fusion index analysis, C2C12 and primary human cells were stained with DAPI to visualize nuclei and anti-myosin heavy chain antibody to label differentiating cells. For fusion analysis, the ratio of nuclei present in myosin-positive cells to the total nuclei in the sample was calculated.

Silver staining

For silver staining analysis, Flexiperm wells were incubated with laminins overnight. The medium was then aspirated and 30 µl of 2× sample buffer (62.5 mM Tris-HCl [pH 6.8], 2.5% sodium dodecyl sulfate [SDS], 0.002% bromophenol blue, 0.7135 M [5%] β-mercaptoethanol, and 10% glycerol) that was added to each well. The solution was pipetted up and down 2–4 times, and the samples were then boiled at 95 °C for 5 min. Proteins were resolved by SDS-polyacrylamide electrophoresis (PAGE). The gels were silver-stained according to the standard protocol.

Western blot

The cells were lysed in lysis buffer (50 mM Tris-HCl, 150 mM NaCl, 1% Nonidet-P40, 0.5% SDS, 10% glycerol, 1 mM dithiothreitol [DTT], 1 mM NaF, and ethylenediaminetetraacetic acid-free mini protease inhibitor cocktail [catalog no. 11873580001, Roche], pH 8.0) and scraped off the dish. The lysates were briefly incubated on ice, passed three times through a 25-gauge needle, incubated on ice for 15 min, and centrifuged at 20,000 × g for 30 min at 4 °C. For Western blot, the supernatant samples were mixed with sample buffer and boiled for 5 min. The proteins were then resolved by SDS-PAGE and transferred to nitrocellulose membranes (catalog no. 66485, Pall Corporation) using Trans Blot Turbo (catalog no. 1704270, Bio-Rad). Membranes were blocked with 5% milk in TBST (20 mM Tris-HCl, 150 mM NaCl [pH 7.6], and 0.1% Tween20) and probed with anti-AChR-α1 antibody (catalog no. 10613-1-AP, Proteintech), anti-rapsyn antibody (catalog no. ab156002, Abcam) or anti-tubulin antibody (catalog no. ab18251, Abcam) in 5% milk in TBST. After washing with TBST buffer, the membranes were incubated with appropriate secondary antibodies conjugated to horseradish peroxidase. For protein detection, we used Clarity chemiluminescent substrate (catalog no. 1705060, Bio-Rad).

Culturing human primary myoblasts

Human primary myoblasts were obtained from EuroBioBank. The donor was a healthy female aged 29 during tissue sampling. The myoblasts were at passage 4 upon reception. Cells were plated in F-10 Ham nutrient mixture (catalog no. N6908-500ML, Sigma) that contained L-glutamine, sodium bicarbonate, 20% FBS, 0.1% fungizone, and 1% penicillin/streptomycin. The medium was supplemented with 0.5 mg/ml fetuin (catalog no. F3385-100MG, Sigma), 0.39 μg/ml dexametazon (catalog no. D4902-25MG, Sigma), and 20 ng/ml basic fibroblast growth factor (catalog no. G507A, Promega). Human primary myoblasts were passaged the same way as C2C12 cells, with the exception of using 0.7% gelatin for coating the culture plates. Fusion was initiated 2 days after seeding 1 × 105 cells/Flexiperm well by replacing the culture medium with 2% HS in DMEM (the same as for C2C12). The cells were allowed uninterrupted fusion for 8 days, after which they were fixed for microscopy.

Data availability

The datasets generated during and/or analysed during the current study are available from the corresponding author on a reasonable request.


  1. 1.

    Tintignac, L. A., Brenner, H. R. & Ruegg, M. A. Mechanisms Regulating Neuromuscular Junction Development and Function and Causes of Muscle Wasting. Physiol. Rev. 95, 809–852 (2015).

    CAS  PubMed  Article  Google Scholar 

  2. 2.

    Li, L., Xiong, W. C. & Mei, L. Neuromuscular Junction Formation, Aging, and Disorders. Annu. Rev. Physiol. 80, 159–188 (2018).

    CAS  PubMed  Article  Google Scholar 

  3. 3.

    Strack, S., Khan, M. M., Wild, F., Rall, A. & Rudolf, R. Turnover of acetylcholine receptors at the endplate revisited: novel insights into nerve-dependent behavior. J. Muscle Res. Cell Motil. 36, 517–524 (2015).

    CAS  PubMed  Article  Google Scholar 

  4. 4.

    Martinez-Pena y Valenzuela, I. et al. Nicotinic acetylcholine receptor stability at the NMJ deficient in alpha-syntrophin in vivo. J. Neurosci. 31, 15586–15596 (2011).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  5. 5.

    Frank, E. & Fischbach, G. D. Early events in neuromuscular junction formation in vitro: induction of acetylcholine receptor clusters in the postsynaptic membrane and morphology of newly formed synapses. J. Cell Biol. 83, 143–158 (1979).

    CAS  PubMed  Article  Google Scholar 

  6. 6.

    Wu, H., Xiong, W. C. & Mei, L. To build a synapse: signaling pathways in neuromuscular junction assembly. Dev. 137, 1017–1033 (2010).

    CAS  Article  Google Scholar 

  7. 7.

    Lin, W. et al. Distinct roles of nerve and muscle in postsynaptic differentiation of the neuromuscular synapse. Nat. 410, 1057–1064 (2001).

    ADS  CAS  Article  Google Scholar 

  8. 8.

    McMahan, U. J. The agrin hypothesis. Cold Spring Harb. Symp. Quant. Biol. 55, 407–418 (1990).

    CAS  PubMed  Article  Google Scholar 

  9. 9.

    Ruegg, M. A. & Bixby, J. L. Agrin orchestrates synaptic differentiation at the vertebrate neuromuscular junction. Trends Neurosci. 21, 22–27 (1998).

    CAS  PubMed  Article  Google Scholar 

  10. 10.

    Zong, Y. & Jin, R. Structural mechanisms of the agrin-LRP4-MuSK signaling pathway in neuromuscular junction differentiation. Cell Mol. Life Sci. 70, 3077–3088 (2013).

    CAS  PubMed  Article  Google Scholar 

  11. 11.

    Lin, W. et al. Neurotransmitter acetylcholine negatively regulates neuromuscular synapse formation by a Cdk5-dependent mechanism. Neuron 46, 569–579 (2005).

    CAS  PubMed  Article  Google Scholar 

  12. 12.

    Burden, S.J., Huijbers, M.G. & Remedio, L. Fundamental Molecules and Mechanisms for Forming and Maintaining Neuromuscular Synapses. Int J Mol Sci 19 (2018).

  13. 13.

    Kim, N. et al. Lrp4 is a receptor for Agrin and forms a complex with MuSK. Cell 135, 334–342 (2008).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  14. 14.

    Kummer, T. T., Misgeld, T. & Sanes, J. R. Assembly of the postsynaptic membrane at the neuromuscular junction: paradigm lost. Curr. Opin. Neurobiol. 16, 74–82 (2006).

    CAS  PubMed  Article  Google Scholar 

  15. 15.

    Marques, M. J., Conchello, J. A. & Lichtman, J. W. From plaque to pretzel: fold formation and acetylcholine receptor loss at the developing neuromuscular junction. J. Neurosci. 20, 3663–3675 (2000).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  16. 16.

    Shi, L., Fu, A. K. & Ip, N. Y. Molecular mechanisms underlying maturation and maintenance of the vertebrate neuromuscular junction. Trends Neurosci. 35, 441–453 (2012).

    CAS  PubMed  Article  Google Scholar 

  17. 17.

    Ervasti, J. M. & Campbell, K. P. A role for the dystrophin-glycoprotein complex as a transmembrane linker between laminin and actin. J. Cell Biol. 122, 809–823 (1993).

    CAS  PubMed  Article  Google Scholar 

  18. 18.

    Singhal, N. & Martin, P. T. Role of extracellular matrix proteins and their receptors in the development of the vertebrate neuromuscular junction. Dev. Neurobiol. 71, 982–1005 (2011).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  19. 19.

    Heino, J. & Kapyla, J. Cellular receptors of extracellular matrix molecules. Curr. Pharm. Des. 15, 1309–1317 (2009).

    CAS  PubMed  Article  Google Scholar 

  20. 20.

    Gawor, M. & Proszynski, T. J. The molecular cross talk of the dystrophin-glycoprotein complex. Ann. N. Y. Acad. Sci. 1412, 62–72 (2018).

    ADS  CAS  PubMed  Article  Google Scholar 

  21. 21.

    Gillies, A. R. & Lieber, R. L. Structure and function of the skeletal muscle extracellular matrix. Muscle Nerve 44, 318–331 (2011).

    CAS  PubMed  PubMed Central  Google Scholar 

  22. 22.

    Patton, B. L., Miner, J. H., Chiu, A. Y. & Sanes, J. R. Distribution and function of laminins in the neuromuscular system of developing, adult, and mutant mice. J. Cell Biol. 139, 1507–1521 (1997).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  23. 23.

    Aumailley, M. et al. A simplified laminin nomenclature. Matrix Biol. 24, 326–332 (2005).

    CAS  PubMed  Article  Google Scholar 

  24. 24.

    Hohenester, E., Tisi, D., Talts, J. F. & Timpl, R. The crystal structure of a laminin G-like module reveals the molecular basis of alpha-dystroglycan binding to laminins, perlecan, and agrin. Mol. Cell 4, 783–792 (1999).

    CAS  PubMed  Article  Google Scholar 

  25. 25.

    Dempsey, C. E., Bigotti, M. G., Adams, J. C. & Brancaccio, A. Analysis of alpha-Dystroglycan/LG Domain Binding Modes: Investigating Protein Motifs That Regulate the Affinity of Isolated LG Domains. Front. Mol. Biosci. 6, 18 (2019).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  26. 26.

    Hohenester, E. Laminin G-like domains: dystroglycan-specific lectins. Curr. Opin. Struct. Biol. 56, 56–63 (2018).

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  27. 27.

    Colognato, H. & Yurchenco, P. D. Form and function: the laminin family of heterotrimers. Dev. Dyn. 218, 213–234 (2000).

    CAS  PubMed  Article  Google Scholar 

  28. 28.

    Patton, B. L. Laminins of the neuromuscular system. Microsc. Res. Tech. 51, 247–261 (2000).

    CAS  PubMed  Article  Google Scholar 

  29. 29.

    Noakes, P. G., Gautam, M., Mudd, J., Sanes, J. R. & Merlie, J. P. Aberrant differentiation of neuromuscular junctions in mice lacking s-laminin/laminin beta 2. Nat. 374, 258–262 (1995).

    ADS  CAS  Article  Google Scholar 

  30. 30.

    Knight, D., Tolley, L. K., Kim, D. K., Lavidis, N. A. & Noakes, P. G. Functional analysis of neurotransmission at beta2-laminin deficient terminals. J. Physiol. 546, 789–800 (2003).

    CAS  PubMed  Article  Google Scholar 

  31. 31.

    Nishimune, H. et al. Laminins promote postsynaptic maturation by an autocrine mechanism at the neuromuscular junction. J. Cell Biol. 182, 1201–1215 (2008).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  32. 32.

    Lee, K. M., Chand, K. K., Hammond, L. A., Lavidis, N. A. & Noakes, P. G. Functional decline at the aging neuromuscular junction is associated with altered laminin-alpha4 expression. Aging 9, 880–899 (2017).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  33. 33.

    Chand, K. K., Lee, K. M., Lavidis, N. A. & Noakes, P. G. Loss of laminin-alpha4 results in pre- and postsynaptic modifications at the neuromuscular junction. FASEB J. 31, 1323–1336 (2017).

    CAS  PubMed  Article  Google Scholar 

  34. 34.

    Kummer, T. T., Misgeld, T., Lichtman, J. W. & Sanes, J. R. Nerve-independent formation of a topologically complex postsynaptic apparatus. J. Cell Biol. 164, 1077–1087 (2004).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  35. 35.

    Godfrey, E. W., Nitkin, R. M., Wallace, B. G., Rubin, L. L. & McMahan, U. J. Components of Torpedo electric organ and muscle that cause aggregation of acetylcholine receptors on cultured muscle cells. J. Cell Biol. 99, 615–627 (1984).

    CAS  PubMed  Article  Google Scholar 

  36. 36.

    Schmidt, N., Basu, S., Kroger, S. & Brenner, H. R. A Cell Culture System to Investigate the Presynaptic Control of Subsynaptic Membrane Differentiation at the Neuromuscular Junction. Methods Mol. Biol. 1538, 3–11 (2017).

    CAS  PubMed  Article  Google Scholar 

  37. 37.

    Sugiyama, J. E., Glass, D. J., Yancopoulos, G. D. & Hall, Z. W. Laminin-induced acetylcholine receptor clustering: an alternative pathway. J. Cell Biol. 139, 181–191 (1997).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  38. 38.

    Proszynski, T. J., Gingras, J., Valdez, G., Krzewski, K. & Sanes, J. R. Podosomes are present in a postsynaptic apparatus and participate in its maturation. Proc. Natl Acad. Sci. USA 106, 18373–18378 (2009).

    ADS  CAS  PubMed  Article  Google Scholar 

  39. 39.

    Bernadzki, K. M., Rojek, K. O. & Proszynski, T. J. Podosomes in muscle cells and their role in the remodeling of neuromuscular postsynaptic machinery. Eur. J. Cell Biol. 93, 478–485 (2014).

    CAS  PubMed  Article  Google Scholar 

  40. 40.

    Paterson, E. K. & Courtneidge, S. A. Invadosomes are coming: new insights into function and disease relevance. FEBS J. 285, 8–27 (2018).

    CAS  PubMed  Article  Google Scholar 

  41. 41.

    Gimona, M., Buccione, R., Courtneidge, S. A. & Linder, S. Assembly and biological role of podosomes and invadopodia. Curr. Opin. Cell Biol. 20, 235–241 (2008).

    CAS  PubMed  Article  Google Scholar 

  42. 42.

    Maselli, R. A. et al. Mutations in MUSK causing congenital myasthenic syndrome impair MuSK-Dok-7 interaction. Hum. Mol. Genet. 19, 2370–2379 (2010).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  43. 43.

    Phillips, W. D. et al. Guidelines for pre-clinical animal and cellular models of MuSK-myasthenia gravis. Exp. Neurol. 270, 29–40 (2015).

    CAS  PubMed  Article  Google Scholar 

  44. 44.

    Lee, Y. I., Mikesh, M., Smith, I., Rimer, M. & Thompson, W. Muscles in a mouse model of spinal muscular atrophy show profound defects in neuromuscular development even in the absence of failure in neuromuscular transmission or loss of motor neurons. Dev. Biol. 356, 432–444 (2011).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  45. 45.

    Proszynski, T. J. & Sanes, J. R. Amotl2 interacts with LL5beta, localizes to podosomes and regulates postsynaptic differentiation in muscle. J. Cell Sci. 126, 2225–2235 (2013).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  46. 46.

    Lee, C. W. et al. Regulation of acetylcholine receptor clustering by ADF/cofilin-directed vesicular trafficking. Nat. Neurosci. 12, 848–856 (2009).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  47. 47.

    Chowdhury, S. R. et al. Growth and differentiation potentials in confluent state of culture of human skeletal muscle myoblasts. J. Biosci. Bioeng. 109, 310–313 (2010).

    CAS  PubMed  Article  Google Scholar 

  48. 48.

    Tanaka, K. et al. Evidence for cell density affecting C2C12 myogenesis: possible regulation of myogenesis by cell-cell communication. Muscle Nerve 44, 968–977 (2011).

    CAS  PubMed  Article  Google Scholar 

  49. 49.

    Melo, F., Carey, D. J. & Brandan, E. Extracellular matrix is required for skeletal muscle differentiation but not myogenin expression. J. Cell Biochem. 62, 227–239 (1996).

    CAS  PubMed  Article  Google Scholar 

  50. 50.

    Hinterberger, T. J. & Barald, K. F. Fusion between myoblasts and adult muscle fibers promotes remodeling of fibers into myotubes in vitro. Dev. 109, 139–147 (1990).

    CAS  Google Scholar 

  51. 51.

    Pęziński, M. & Prószyński, T. Domain organization of synaptic components. Curr. Opin. Physiol. 4, 7–14 (2018).

    Article  Google Scholar 

  52. 52.

    Clausen, L., Cossins, J. & Beeson, D. Beta-2 Adrenergic Receptor Agonists Enhance AChR Clustering in C2C12 Myotubes: Implications for Therapy of Myasthenic Disorders. J. Neuromuscul. Dis. 5, 231–240 (2018).

    PubMed  PubMed Central  Article  Google Scholar 

  53. 53.

    Linder, S. & Aepfelbacher, M. Podosomes: adhesion hot-spots of invasive cells. Trends Cell Biol. 13, 376–385 (2003).

    CAS  PubMed  Article  Google Scholar 

  54. 54.

    Ross, J. A. et al. Multiple roles of integrin-alpha3 at the neuromuscular junction. J. Cell Sci. 130, 1772–1784 (2017).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  55. 55.

    Slater, C. R. Structural factors influencing the efficacy of neuromuscular transmission. Ann. N. Y. Acad. Sci. 1132, 1–12 (2008).

    ADS  PubMed  Article  Google Scholar 

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We thank Dr. Marta Gawor for providing an image of AChR clusters in myotubes that were grown on agrin-coated substratum. This work was supported by Polish National Science Center Opus grant no. UMO-2018/29/B/NZ3/02675 (awarded to T.J.P.) and Preludium grant no. UMO-2018/29/N/NZ4/02724 (awarded to M.P). M.P was also supported by the European Union Horizon 2020 research and innovation program under Marie Sklodowska-Curie grant no. 665735 (Bio4Med) and the Polish Ministry of Science and Higher Education within 2016–2020 funds for the implementation of international projects (agreement no. 3548/H2020/COFUND/2016/2). The project was performed using the CePT infrastructure, financed by the European Union, European Regional Development Fund, within the Operational Program “Innovative Economy” for 2007–2013.

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M.P. designed and carried out the experiments and analyzed the data included in this publication. P.D. carried out the preliminary experiments. H.L. provided the primary human muscle cell line, analyzed the data and reviewed the manuscript. B.S.P. analyzed results and edited the manuscript and figures. T.J.P. designed the experiments, analyzed the data, and provided scientific supervision. M.P. and T.J.P. wrote and reviewed the manuscript.

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Correspondence to Tomasz J. Prószyński.

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Pęziński, M., Daszczuk, P., Pradhan, B.S. et al. An improved method for culturing myotubes on laminins for the robust clustering of postsynaptic machinery. Sci Rep 10, 4524 (2020).

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