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Table of Contents

    Topic review

    Muscular Dystrophies

    Subjects: Physiology
    View times: 49
    Submitted by: László Csernoch


    Muscle dystrophy is a muscle disease that leads to a progressive loss of muscle mass and a weakened musculoskeletal system in accordance with age of onset, severity, and the group of muscles affected.

    1. Introduction

    Dystrophy is an umbrella name that encompasses more than 30 genetic disorders that progress over time, leading to degeneration and weakness of the muscles. The phenotype of muscular dystrophy is an endpoint that arises from a disparate set of genetic and biochemically heterogeneous pathways. Genes associated with muscular dystrophies encode proteins of the plasma membrane (sarcolemma), terminal cisternae, extracellular matrix, and the sarcomere, as well as nuclear membrane components (Figure 1).

    Figure 1. Mutations in skeletal muscle causing muscle disorders. . Altered lipid phosphatase activity of MTM1; . defects in microtubule dynamics or vesicular traffic (DNM2); . defective calcium release from the SR via RyRs; . mutated or missing dystrophin; . defects in alternative splicing due to MBLN1, CELF1 and DUX4 malfunction. (MTM1: myotubularin 1; DNM2: dynamin 2; SR: sarcoplasmic reticulum; RyR: ryanodine receptor; MBLN1: muscle blind-like; CELF: CUGBP/Elav-like factors; DUX4: homebox protein 4; DHPR: dihydropyridine receptor; NMJ: neuromuscular junction; SERCA: sarco(endo)plasmic reticulum calcium pump).

    Myopathies are a diversified family of disorders characterized by pathological structure and/or the functioning of skeletal muscles. Inherited myopathies include a clinically, histopathologically, and genetically heterogeneous group of rare genetic muscle diseases that are characterized by architectural anomalies in the muscle fibers.

    2. Muscular Dystrophies

    Muscular dystrophies (MDs) are a group of inherited disorders in which the voluntary muscles that control movement, in some instances the heart muscles and eventually the diaphragm, progressively weaken and lose their ability to maintain proper function. There are more than 30 types of MDs that vary in severity, symptoms, and causes. In recent years, the classification of MDs has been adjusted in order to correspond to the newly available information related to the primary protein dysfunctions and their localizations. As a consequence, by convention, the MDs had been classified according to the main clinical and biopsy findings, age of onset, and rate of progression into nine major forms: (1) Becker, (2) congenital, (3) Duchenne, (4) distal, (5) Emery–Dreifuss, (6) facioscapulohumeral, (7) limb–girdle, (8) myotonic, and (9) oculopharyngeal muscular dystrophy. In the present review, we tackle the most common forms of MDs in humans.

    2.1. Dystrophinopathies

    Dystrophinopathies cover a spectrum of X-linked muscle diseases ranging from mild to severe forms that include Duchenne muscular dystrophy (DMD), Becker muscular dystrophy (BMD), and DMD-associated dilated cardiomyopathy (DCM). DMD/BMD are neuromuscular genetic disorders characterized by progressive muscle degeneration, weakness, and wasting due to the alterations of a critical muscle protein called dystrophin, which is a relatively long (110 nm), rod-shaped intracellular protein localized at the cytoplasmic face of the sarcolemma in cardiac and skeletal muscles [1][2]. Dystrophin connects γ-actin of the subsarcolemmal cytoskeleton system to a complex of proteins in the surface membrane (dystrophin protein complex, DPC) and helps keep the muscle cell intact and orchestrates the transmission of force laterally across the muscle during contraction (see Figure 1). Growing evidence suggests that dystrophin also has a major role in regulating signaling pathways that activate nitric oxide (NO) production, Ca2+ entry, and the production of reactive oxygen species (ROS). The absence or reduced expression of dystrophin beside other members of the DPC complex causes dystrophinophathies.

    DMD is the most common muscular dystrophy in children affecting primarily boys due to classical X-linked recessive genetics according to which males who carry the mutation express the disease while females are carriers. The incidence of DMD is approximately 1 in 3500 [3][4][5][6]. DMD symptom onset is in early childhood, usually between ages 2 and 6. The symptoms of DMD include decreased muscle size accompanied by progressive weakness and atrophy of skeletal and heart muscles. Early signs of DMD are muscle weakness of weight-bearing muscles and may include delayed ability to sit, stand, or walk, difficulties learning to speak, and general cognitive impairment. Most children with DMD use a wheelchair by their early teens. Heart and breathing problems also begin in the teen years, leading to serious life-threatening complications, and patients usually die in the third or fourth decade due to respiration or cardiac failure.

    Frame-shift mutations or other genetic rearrangement in the dystrophin gene abolish protein expression that disturbs the connection between the cytoskeleton and the extracellular matrix, making muscle fibers more susceptible to contraction-induced membrane damage. As a result, the uncontrolled influx of calcium ions occurs inevitably, leading to progressive myofiber degeneration [7][8]. These pathologic processes are accompanied by chronic inflammation and fibrosis [9], as evidenced by macrophage infiltration [10]. In DMD, skeletal muscles active myofiber necrosis, and cellular infiltration can be histologically identified, furthermore regenerating myofibers containing centrally located nuclei, and a large variety of myofiber sizes are often detected. This phenotype is particularly pronounced in the diaphragm, which undergoes progressive degeneration and myofiber loss, causing an approximately 5-fold reduction in muscle isometric strength [11].

    In-frame deletions often generate truncated dystrophin and result in BMD characterized by skeletal muscle weakness with milder symptoms and later onset that appear between the ages of 2 and 16 but in some cases as late as the twenties. Its incidence has been estimated to be between 1 in 30,000 male births [12][13].

    Plentiful mouse models have been developed to better understand the basic molecular biology of DMD. Currently, there are nearly 60 different animal models for DMD, and the list keeps growing. For a comprehensive lineup, see Table 1 and the review by McGreevey and colleagues [14]. The TREAT-NMD Alliance (https://treat-nmd.org/research-overview/preclinical-research/) is an initiative to improve preclinical trial design and execution for the most common mouse models of DMD, spinal muscular atrophy (SMA), and congenital muscular dystrophy.

    Table 1. Mouse models of Duchenne muscular dystrophy.

    Model System Genetic Changes in the Mouse Model/Mutation(s) Genetic Similarity/Genetic Background Likeliness of Phenotype and Symptoms References
    Advantage Disadvantage Advantage Disadvantage
    Dystrophin-deficient mice
    Albino mdx
    Exon 23 point mutation. On the C57BL/10 background.
    mdx on the Albino background.
    mdx on the BALB/c background.
    mdx on the C57BL/6 background.
    mdx on the C3H background.
    mdx on the DBA2 background.
    mdx on the FVB background.
      The diaphragm shows progressive deterioration as in humans.
    More severe dystrophic signs.
    Minimal clinical symptoms, lifespan reduced by only 25% compared to human DMD. [15][16][17][18][19]
    Intron 42 point mutation.
    Intron 65 point mutation.
    Exon 53 point mutation.
    Exon 10 point mutation.
    On the C57BL/6 background. Chemically induced mutation.
    all dystrophin isoforms eliminated.
    Fewer revertant fibers.
    Severe disease signs.
    CRKHR1 Unsequenced, dystrophin deficiency confirmed by immunofluorescence staining. On the C3H background. ENU chemically induced mutation. Elevated CK, centrally nucleated myofibers, and dystrophin deficiency.   [21]
    mdx52 Exon 52 deletion. On the C57BL/6 background
    hot spot mutation.
    Targeted inactivation.     [22]
    mdxβgeo Insertion of the β-geo gene trap cassette in intron 63. LacZ replaced the CR and CT domain. All dystrophin isoforms are mutated.     [23]
    DMD-null Entire DMD gene deletion. Cre-loxP system. All dystrophin isoforms are eliminated.     [24]
    Dp71-null Insertion of the β-geo cassette in intron 62.   Selective elimination of Dp71. Dp71 deficiency is associated with early cataract formation in mice.   [25][26]
    Dup2 Exon 52 duplication. On the C57BL/6 background.       [27]
    Immun-deficient mdx mice
    NSG-mdx4cv Prkdc and IL2rb double deficient. On the mdx4cv background. Innate immunity deficient. B, T, and NK cell deficient.   [28]
    Rag2 IL2rb Dmd Rag2 and IL2rb double deficient. On the mdx βgeo background.   B, T, and NK cell deficient.
    No revertant fibers.
    Scid mdx Prkdc deficient. On the mdx background.   B and T cell deficient.   [31]
    W41 mdx C-kit receptor deficient On the mdx background Haematopoietic deficient. Optimal for bone marrow cell therapy studies.   [32]
    Phenotypic dko mice
    α7/dystrophin dko or mdx/α7–/– α7/dystrophin double deficient.     Severe dystrophic phenotype.   [33][34]
    Adbn–/– mdx αdystrobrevin/dystrophin double deficient.     Severe dystrophic phenotype.   [35]
    Cmah-mdx Cmah/dystrophin double deficient.     Severe dystrophic phenotype.
    d-dko δ-sarcoglycan/dystrophin double deficient.     Severe dystrophic phenotype.   [37]
    Desmin-/- mdx4cv desmin/dystrophin double deficient.     Severe dystrophic phenotype.   [38]
    Dmdmdx/Largemyd like-glycosyltransferase/dystrophin deficient.     Severe dystrophic phenotype.   [39]
    DMD null; Adam8-/- ADAM8 deficient and entire DMD gene deletion. On the DMD-null background. The injured myofibers are not efficiently removed in DMD null.     [40]
    dysferlin/dystrophin dko dysferlin/dystrophin double deficient.     Severe dystrophic phenotype.   [41][42]
    Il-10-/-/mdx interleukin-10/dystrophin double deficient. On the mdx background.   Severe dystrophic phenotype and marked cardiomyopathy.   [43]
    mdx/mTR telomerase RNA/dystrophin double deficient.   Premature depletion of myofiber repair. Severe dystrophic phenotype.   [44]
    mdx:MyoD-/- MyoD/dystrophin double deficient.   MyoD is only expressed in skeletal muscle. Severe dystrophic phenotype and prominent dilated cardiomyopathy. MyoD mutations do not occur in human DMD. [45]
    mdx:utrophin-/- utrophin/dystrophin double deficient.   Targeted mutation at the utrophin CR domain/exon 7. Severe dystrophic phenotype with cardiomyopathy, cardiac fibrosis, LV dilation.   [35][46]
    PAI-1-/--mdx plasminogen activator inhibitor-1/dystrophin double deficient.   Early onset fibrosis and higher CK.     [47]
    Transgenic mdx mice
    full-length dystrophin TG mdx transgenic over-expression of full-length dystrophin. On the mdx background.   Over-expression does not harm muscle rather it shows protection.   [48][49][50]
    Dp71 TG mdx transgenic over-expression of Dp71. On the mdx background.   Severe disease signs.   [51][52]
    Dp116 TG mdx4cv
    transgenic over-expression of Dp116. On the mdx4cv background
    on the utrophin/dystrophin dko background.
      Severe disease signs.
    Improved lifespan.
    No change in histopathology, CK, and specific force development. [53][54]
    Dp260 TG mdx
    Dp260 mdx/utrn-/-
    transgenic over-expression of Dp260. On the mdx background
    on the utrophin/dystrophin dko background.
      Slightly improved histopathology.
    Severe lethal phenotype was converted to a mild myopathy.
    No improvement of specific force. [55][56]
    micro-dystrophin TG transgenic over-expression of synthetic micro-dystrophin gene. On the mdx background.   Improved protection against disease signs. No restoration of nNOS. [57][58][59][60]
    Fiona transgenic over-expression of full-length dystrophin gene. On the mdx background.   Improved protection against disease signs. No restoration of nNOS. [61][62]
    laminin α1 TG mdx transgenic over-expression of laminin α1. On the mdx background.   Similar phenotype as mdx. No improvement but no harm. [63]

    With all its caveats, the most widely used animal model for DMD research is the C57BL/10ScSn-Dmdmdx/J (BL10-mdx; available from the Jackson laboratory, JL#001801) mouse in which the dystrophic phenotype arises because of a point mutation (C to T transition) in exon 23, which results in a stop codon and truncated dystrophin protein. This spontaneous mutation was discovered in the early 1980s in a colony of C57BL/10ScSn mice due to elevated serum creatine kinase (CK) and histological evidence of myopathy [15]. The mdx muscles seem more susceptible to contraction- and stretch-induced damage revealed as sarcolemmal tears [64]. Normal physiological control of calcium homeostasis is lost in mdx mice [65][66], and similar to the human condition, calcium levels are increased in myofibers isolated from mdx mice [67].

    DMD is a multi-systemic condition affecting many parts of the body and resulting in atrophy of the skeletal, cardiac, and respiratory muscles. DMD disease progression in mdx mice has several distinctive phases. In the first 2 weeks, the mdx muscle is indistinguishable from that of normal mice. Between 3 and 6 weeks, it undergoes astonishing necrosis. Subsequently, the majority of skeletal muscle enters a relatively robust regeneration phase. As a hallmark of the disease, mdx limb muscles often become hypertrophic during this phase. The diaphragm is an exception, as it shows progressive deterioration, as seen in affected humans [11]. Severe dystrophic phenotypes, such as muscle wasting, scoliosis, and heart failure do not occur until mdx mice are 15 months or older [68][69][70][71][72][73]. Despite being deficient for dystrophin, mdx mice display overall minimal clinical symptoms; their lifespan is only reduced by ≈25% (vs. 75% decrease in humans) without obvious signs of dilated cardiomyopathy [14][37]. The robust skeletal muscle regeneration might explain somewhat the slowly progressive phenotype observed in mdx mice.

    The mdx mouse has been crossed to several different genetic backgrounds, including the Albino, BALB/c, C3H, C57BL/6, DBA2, and FVB strains; several immune-deficient mdx strains were also engineered (see Table 1). Phenotypic variation has been observed in different backgrounds. Several other dystrophin-deficient lines (Dup2, DMD-null, Dp71-null, mdx52, and mdxβgeo) were also created using various genetic engineering techniques. The DMD-null mouse was created by deleting the entire DMD genomic region using the Cre-loxP technology [24] resulting in the ablation dystrophin isoforms expression in all tissues. Further models (mdxcv) were created by chemical mutagenesis programs by treating mice with N-ethyl-N-nitrosourea, a chemical mutagen, so that each strain carries a different point mutation [20][74]. By eliminating myogenic differentiation 1 (MyoD), a master myogenic regulator, from mdx mice, Megeney et al. obtained a MyoD/dystrophin double-mutant mouse that shows marked myopathy, dilated cardiomyopathy, and premature death [45][46][75]. Another similar approach was the generation of telomerase/mdx double-mutant mice (mTR/mdx) that show more severe muscle wasting and cardiac defects [44][76].

    Two other proteins, utrophin and α7-integrin, fulfill the same function as dystrophin, and their relative expression is upregulated in mdx mice. The genetic elimination of utrophin, which is expressed along the sarcolemma in developing muscle, exhibits 80% homology and shares structural and functional motifs with dystrophin and α7-integrin; their deletion in mdx mice lead to the creation of utrophin/dystrophin and integrin/dystrophin double-knockout (dko) mice, respectively [33][34][35][46][77]. The dko mice show much more severe muscle disease symptoms (similar to or even worse than that of humans with DMD); however, they are difficult to generate and care for. Utrophin heterozygous mdx mice might represent an intermediate model between the extreme dko mice and mildly affected mdx mice [78][79].

    Second mutations have been introduced to “humanize” mice (e.g., inactivation of cytidine monophosphate sialic acid hydrolase (Cmah)) and to mutate genes involved in cytoskeleton-ECM interactions (e.g. desmin and laminin); however, the introduction of a second mutation not present in human DMD turned out to produce a much more severe phenotype and complicated data interpretation [14][36][46][80].

    To test if the “humanization” of telomere lengths could recapitulate the DMD disease phenotype, the mdx4cv/mTRG2 dko mice were generated, which seem to recapitulate the best of both the skeletal muscle and cardiovascular features of human DMD [44]. Nevertheless, there are still a few tenable therapies for DMD, so the need for appropriate mouse models more similar to the mdx model is emphasized. Even with an improved delivery of promising strategies such as gene editing or exon skipping, testing must be done in mice with the full spectrum of DMD pathology.

    Dysferlinopathies are caused by the lack of functional dysferlin, which is a key protein involved in membrane repair processes causing Myoshi myopathy or dysferlin-related limb girdle muscular dystrophy (LGMD R2) [81]. The dysferlin-deficient mice (dysf-/-) replicate well human dysferlinopathies, showing similarities with the human condition although with milder histopathological aspects. Due to space restrictions, we did not further elaborate on these mouse models (for a comprehensive review, see [82] and more recently [83].

    2.2. Myotonic Dystrophy

    Myotonic dystrophy (DM) is an autosomal dominantly inherited disorder and the most prevalent form of muscular dystrophy in adulthood. Clinical characterization of the disease was done first by Steiner in 1909. DM is a complex genetic disease with diverse symptoms affecting multiple organs, such as skeletal muscle, cardiac muscle, the endocrine and gastrointestinal system, reproductive system, and central nervous system (CNS). Symptoms range from muscle weakness and wasting both in skeletal muscle and in heart, arrhythmias, or conduction abnormalities, disorders in the function of the neuromuscular junction, neurologic impairment such as excessive daytime sleepiness and motivation deficit, insulin resistance, cataracts, and male infertility. There are two major forms of the disease: myotonic dystrophy type I (DM1 or Steiner’s disease) and myotonic dystrophy type II (DM2 or proximal myotonic myopathy), which are associated to partially similar clinical appearances but distinct genetic defects [57].

    Several hypotheses have been suggested to explain the complex symptoms of DM. The genetic background responsible for classic myotonic dystrophy documented by Steiner was discovered in 1992. An expansion of a CTG trinucleotide repeat in the 3′ untranslated region of the dystrophia myotonica protein kinase gene (DMPK) has been identified, which is a mutation that has been transcribed into RNA but not translated into protein [57]. Based on DMPK haploinsufficiency theory, the expanded repeats inhibit DMPK mRNA or protein production, which is in agreement with observation in DM1 patient muscle and cell cultures demonstrating a decreased expression of DMPK mRNA and protein [84]. On the other hand, DMPK-knockout mice did not display myotonia but rather mild myopathy [85]. Although DMPK haploinsufficiency alone is not sufficient to explain the features of DM1, the CTG repeats might influence the expression of neighboring genes as well. The haploinsufficiency of SIX5 and of other adjacent genes such as myotonic dystrophy gene with tryptophan and aspartic acid (WD) repeats, DMWD [86], and the FCGRT gene, encoding the Immunoglobulin G Fc Fragment Receptor and Transporter, has also been suggested to contribute to DM1 pathogenesis [87]. Indeed, Six5 knockout mice develop cataracts [88][89] but without any muscular deficiency. The next concept was the RNA gain-of-function hypothesis assuming that the mutant RNA transcribed from the expanded allele is capable of inducing symptoms of the disease. The HSALR transgenic mouse model (among others) confirms this theory [90]. In HSALR mice 250 CTG repeats were expressed in the 3′ end of the human skeletal α-actin gene that implied myotonia and muscle degeneration characteristic in DM1 without a multisystem phenotype.

    DM2 was identified in 1998 with a different genetic mutation from that of DM1 [91]. In 2001, DM2 was reported as a result of CCTG repeats within intron 1 of the nucleic acid-binding protein (CNBP) gene (known also as zinc finger 9 gene, ZNF9) [92]. In both types of DM, there is a nucleotide repeat expansion; however, completely different genes are affected. Nevertheless, DM1 and DM2 have similar symptoms bringing up the idea of a common pathogenic mechanism. One candidate is a process through interaction with RNA-binding proteins. The transcripts with nucleotide repeat expansions can accumulate in the nucleus (see Figure 1) and form RNA aggregates/foci interfering with protein families such as the muscleblind-like (MBNL), CUGBP/Elav-like factors (CELF), and the RNA binding Fox (RBFOX) being the most important splicing regulators in skeletal muscle [93][94][95].

    MBNL1 is sequestered on the expanded CUG repeats producing a loss of function, while CELF1 is upregulated due to the activation of protein kinase C, leading to its stabilization. These processes result in irregular splicing profiles of MBNL1- and CELF1-regulated transcripts in adult skeletal muscle and heart, or even during embryonic to adult switch in the splicing pattern. MBNL1 (Mbnl1ΔE3/ΔE3) knockout mice with targeted deletion of MBNL1 exon 3—where an RNA-binding motif is located—underpin this model, since these animals reproduce several features of DM including muscle, eye, and RNA splicing disorders (alternative splicing regulation in the brain is slightly affected, it depends mainly on the loss of MBNL2) [96]. Moreover, the adeno-associated virus-mediated overexpression of MBNL1 in HSALR mice is able to lessen the myotonia [24]. Verification also arises from the tissue-specific induction of CELF1 overexpression in adult mouse skeletal muscle, where muscle impairment detected in DM1 has been reproduced [97], while CELF1 overexpression in the heart leads to cardiac abnormalities similar to DM1 [98] (the role of CELF1 in DM2 is not clarified). These phenotypes were related to miss-splicing. These animal models imply that the overexpression of toxic CTG or CCTG repeats, depletion of MBNL1, or overexpression of CELF1 would all eventuate in similar splicing alterations, which initiate downstream signaling pathways resulting in the phenotype and/or molecular background of myotonic dystrophies.

    The modified splicing apparatus can affect other genes in diverse signal transduction pathways leading to disrupted protein synthesis or the presence of different protein isoforms and the modified localization of proteins. Focusing on muscle, an aberrant regulation of RNA-binding proteins causes splicing alterations in the voltage-gated chloride channel 1 (CLCN1) transcript resulting in myotonia with delayed muscle relaxation in skeletal muscle cells [57][99]. Alternative splicing defects of BIN1 (bridging integrator 1), a lipid-binding protein responsible for the biogenesis of the transverse (T) tubules, has also been associated with muscle weakness. The inactive form of BIN1 causes damages of the excitation–contraction coupling (ECC) [100]. Another protein concerned is the calcium channel CaV1.1. Mis-splicing of the CACNA1S gene contributes to muscle weakness. Alternative splicing of the genes encoding ryanodine receptor 1 (RyR1) and SERCA1 expression are also altered modifying contractility of the muscles [101]. Altered splicing of several other genes encoding structural proteins has also been described in DM, as a few examples: DTNA (encoding dystrobrevin-α), MYOM1 (encoding myomesin1), NEB (encoding nebulin), TNNT3 (encoding fast troponin T3), DMD (encoding dystrophin), MTMR1 (encoding myotubularin-related protein 1), and CAPN3 (encoding intracellular protease Calpain 3). Atypical splicing of the insulin receptor (IR) may take part in the formation of insulin resistance. The genes mentioned above represent just a few examples of the more than 30 miss regulated splicing identified in DM patient’s tissue samples or of the more than 60 aberrant splicing described in mice tissues [102].

    According to the previously listed conditions, molecular, and genetic variations, an “overall DM” model system should meet several requirements. At this moment, none of the available mouse models recapitulates all aspects of DM (for a comprehensive list of these mouse models, see Table 2). At the same time, the mouse models generated so far provided us with a significant tool in understanding the disease mechanism. There are different approaches in the various models. The inactivation of DM genes, the overexpression of toxic CTG/CTGG repeats, the induced alterations in splicing through MBNL1 inactivation, or CELF1 overexpression have resulted in a transgenic mouse model that was suitable for the examination of different aspects of the disease. Despite the growing number of already identified transcripts and the increased amount of data on altered pathways, the precise mechanism of the DMs is poorly understood. The available and the new mouse models to be established in the future can help scientists to discover a disease-modifying therapy.

    Table 2. Mouse models of myotonic dystrophies.

    2.3. Facioscapulohumeral Dystrophy

    Facioscapulohumeral dystrophy (FSHD) also known as Landouzy–Dejerine syndrome is the 3rd most common autosomal dominant form of muscular dystrophy after DMD and DM. Its prevalence is 1:8500 to 15,000, and males are more often symptomatic compared to females [103]. The disease tends to progress slowly with periods of rapid deterioration, and it affects the face, shoulder blades, and upper arms muscles, leading to difficulty chewing or swallowing and slanted shoulders. Currently, there is no cure for FSHD, as no pharmaceuticals have proven effective for alleviating the disease course. Prognosis is variable, but most people with the disease have a normal lifespan.

    The FSHD is a very complex disease with primate-specific genetic and epigenetic components. It is caused by the epigenetic de-repression of the double homebox protein 4 (DUX4) retrogene on chromosome 4, in the 4q35 region that leads to a gain-of-function disease [104]. DUX4 is expressed in early human development, while in mature tissues, it is suppressed. In FSHD, DUX4 is inadequately turned off, which can be due to several different mutations. The mutation termed “D4Z4 contraction” defines the FSHD type 1 (FSHD1), making up 95% of all FSHD cases, whereas the disease caused by other mutations is classified as FSHD2 or contraction independent.

    There are a few FSHD1 mouse models available for preclinical efficiency testing prior to human clinical trials, but due to the unusual nature of the disease locus, these models will not recapitulate accurately the genetic and pathophysiological spectrum of the human condition, and overall, these models remain sub-optimal in assessing therapeutic efficacy (Table 3). The most significant hurdle that is impossible to overcome is that the D4Z4 macrosatellite encoding the toxic DUX4 retrogene is specific to primates, which impedes the possibility of working with a natural model of the disease [105]. Several xenograft models were developed in which skeletal muscle tissue from FSHD patients or muscle precursor cells were transplanted into the mouse muscle (see Table 3). There are currently no mouse models for FSHD2.

    Table 3. Mouse models of facioscapulohumeral muscular dystrophy.

    Model System Genetic Changes in the Mouse Model/Mutation(s) Genetic Similarities/Genetic Background Likeliness of Phenotype and Symptoms
    Advantage Disadvantage Advantage Disadvantage
    AAV6-DUX4 TA injection of AAV6-DUX4 in 6–8-week-old mice. On the C57BL/6 background.   Degenerating myofibers and infiltrating mononuclear cells.
    DUX4-induced cell death via p53-dependent pathway.
    Minor degeneration, increased central nuclei.
    Signs of apoptosis.
    Transgenic insertion of two and a half copies of D4Z4 from the permissive haplotype of a pathogenic allele.
    Transgenic insertion of twelve and a half copies of D4Z4 from the permissive haplotype of a pathogenic allele.
    On the C57BL/6NJ background.
    Body-wide expression of the DUX-4 transcript in all tissues.
    Keratitis leading to blindness.
    DUX4 transcript detected in myoblasts and myotubes.
    DUX4 transcript was NOT detected in tibialis anterior and pectoralis muscles.
    No muscle weakness or abnormal morphology. Satellite-cell derived myoblasts with DUX4 positive nuclei fail to fuse and form myotubes.
    Minor regeneration defect upon cardiotoxin injury.
    Doxycycline-inducible DUX4 transgene on the X-chromosome. On C57BL/6J background. Abnormal embryogenesis, mostly lethal. Surviving males lived ‹ 2 months. Weaker grip strength.
    Smaller muscles, impaired function, reduced specific force.
    Impaired myogenic regeneration. The activation of the downstream targets of DUX4 in mice differs from that in humans. Smaller and fewer myofibers, but not dystrophic.
    TA was least affected.
    Xenograft Human muscle engraftment into immunodeficient mice. “Humanized” mouse model.   FSHD biomarker profile maintained in xenograft.  
    FRG1 Transgenic insertion of FRG1 driven by a human skeletal α-actin promoter. Spinal curvature correlated with the level of FRG1 expression.
    Dystrophic features.
      Fiber size variability, necrosis, centralized nuclei. Excess collagen, selective muscle atrophy, reduced exercise tolerance. Abberant alternative splicing of specific pre-mRNAs.
    Fat1 Knockout of Fat1. Regionalized muscle and non-muscle abnormalities. Retinal vasculopathy, abnormal inner ear patterning.
    Abnormal embryogenesis.
    Muscle weakness of the face and scapulohumeral region. Altered myoblast migration polarity.
    Pitx1 Transgenic overexpression of Pitx1 induced in the absence of doxycycline. Myofiber atrophy, necrotic and centrally nucleated fibers, inflamatory infiltration. Polyadenylated DUX4 mRNA expressed at higher level in FSHD muscle. Asymmetric muscle weakness in the face and shoulders that gradually progresses into the trunk and leg muscles.
    Evidence of endomysial inflamation.
    Retinal vasculopathy hearing loss.
    Tamoxifen inducible Cre-DUX4 Reproductively viable. No functional deficit of diaphragm muscles. Progressive pathology.
    Mild alopecia. Females more affected.
    AAV-mediated follistatin gene therapy improved muscle mass and strength. No extramuscular deficits. Tamoxifen dose-dependent skeletal muscle pathology.
    Limited skeletal muscle pathology.

    This entry is adapted from 10.3390/ijms21238935


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