Connexin-43 reduction prevents muscle defects in a mouse model of manifesting Duchenne muscular dystrophy female carriers

Nouet, Julie; Himelman, Eric; Lahey, Kevin C.; Zhao, Qingshi; Fraidenraich, Diego

doi:10.1038/s41598-020-62844-9

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Published: 30 March 2020

Connexin-43 reduction prevents muscle defects in a mouse model of manifesting Duchenne muscular dystrophy female carriers

Julie Nouet ORCID: orcid.org/0000-0002-6140-1604¹,
Eric Himelman¹,
Kevin C. Lahey¹,
Qingshi Zhao¹ &
…
Diego Fraidenraich¹

Scientific Reports volume 10, Article number: 5683 (2020) Cite this article

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Abstract

Duchenne muscular dystrophy (DMD) is a severe X-linked neuromuscular disorder that affects males. However, 8% of female carriers are symptomatic and underrepresented in research due to the lack of animal models. We generated a symptomatic mouse model of DMD carriers via injection of mdx (murine DMD) embryonic stem cells (ESCs) into wild-type (WT) blastocysts (mdx/WT chimera). mdx/WT chimeras developed cardiomyopathic features and dystrophic skeletal muscle phenotypes including elevated mononuclear invasion, central nucleation, fibrosis and declined forelimb grip strength. The disease was accompanied by connexin-43 (Cx43) aberrantly enhanced in both cardiac and skeletal muscles and remodeled in the heart. Genetic reduction of Cx43-copy number in mdx/WT-Cx43(+/−) chimeras protected them from both cardiac and skeletal muscle fiber damage. In dystrophic skeletal muscle, Cx43 expression was not seen in the fibers but in adjacent F4/80+ mononuclear cells. Ethidium Bromide uptake in purified F4/80+/CD11b+ mdx macrophages revealed functional activity of Cx43, which was inhibited by administration of Gap19 peptide mimetic, a Cx43 hemichannel-specific inhibitor. Thus, we suggest that Cx43 reduction in symptomatic DMD carrier mice leads to prevention of Cx43 remodeling in the heart and prevention of aberrant Cx43 hemichannel activity in the skeletal muscle macrophages neighboring Cx43 non-expressing fibers.

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Introduction

Duchenne muscular dystrophy (DMD) is an incurable X-linked recessive disorder characterized by mutations in the dystrophin gene. The dystrophin protein is an essential part of the dystrophin-glycoprotein complex (DGC), which provides structure and mechanically-induced signal propagation between intracellular and extracellular environments¹. X-linked disorders only affect male patients; however, a percentage of female DMD heterozygotes are symptomatic. Symptomatic female carriers consist of about 8–40% of definite DMD carriers and begin to present symptoms between the ages of 2–47 years old^2,3. Patients display a range of severe to less severe phenotypes. It is generally accepted to affect 8% of female carriers, yet this statistic aligns with those affected by dilated cardiomyopathy. A higher percentage (17%) suffer from muscle weakness^{3,4,5,6,7,8,9,10}. Heart complications can be further expanded to include left-ventricle dilation (40%)¹⁰.

Research on symptomatic carriers has been confined to clinical observations largely due to the absence of a representative animal model^2,3,9,11,12. These epidemiological studies are subject to a larger margin of error from confounding variables, necessitating a DMD animal model that successfully recapitulates the symptomatic carrier phenotypes and mosaicism. X-linked muscular dystrophy mice (mdx)¹³ heterozygotes, mdx(+/−), show normal muscle histology and do not develop cardiomyopathy^11,12. Recently, we described the generation of a model to study symptomatic DMD carriers that faithfully recapitulates the pathology and symptoms (mdx/WT mouse chimeras)¹⁴. Symptomatic mdx mouse chimeras were generated via injection of mdx embryonic stem cells (ESCs) into wild-type (WT) blastocysts. Mdx/WT chimeras feature patches of dystrophin negative(−) and dystrophin positive(+) cells¹⁴. This mosaic model resembles well-documented dystrophin mosaicism in human female DMD carriers due to randomized X-inactivation^14,15.

Cardiomyopathy and arrhythmias are tightly correlated with dysregulation of gap junction (GJ) transmembrane protein connexin-43 (Cx43) based on its critical role in synchronous electrical impulse propagation between ventricular contractile cardiomyocytes^16,17,18,19. Cx43 is increasingly recognized as being pathologically disrupted in ischemia leading to cell death and tissue damage, and in Duchenne muscular dystrophy associated cardiomyopathy^20,21,22,23. Mdx hearts display increased protein levels and pathological remodeling of Cx43 away from the cell-to-cell junction intercalated disc (ID) compared to wild-type (WT) mice^16,24,25. Cx43 hemichannel remodeling to the lateral side of the cardiomyocyte and internalization leads to electrical uncoupling and arrhythmogenesis²⁶. Normalization of Cx43 levels through genetic reduction in mdx:Cx43(+/−) mice prevented Cx43 mislocalization to the lateral borders as well as cardiac dysfunction in aged mdx mice^16,24. Reduction of Cx43 hemichannel activity through treatment with Gap19 selective peptide mimetic inhibitor, improved myocardial ischemia, reperfusion, and cardiac damage by lowering the occurrence of arrhythmias, metabolic injury, and mortality^16,23,27. Pathology of mdx cardiomyopathy can be attenuated by preventing lateralized Cx43 hemichannels or blocking hemichannel activity^28,29.

The role of Cx43 in skeletal muscle pathology is less known. In contrast to cardiac muscle that requires constant GJ intracellular communication between cardiomyocytes to synchronize heart contraction, mature skeletal muscle cells fuse to form a syncytium, therefore the formation of GJs is unnecessary in mature muscle fibers. Expression of Cx43 is absent in control, uninjured tissues, and increases after denervation or injury and can be seen as punctate staining; however, it does not overlap with muscle stem cell marker (Pax7+)^30,31. Cx43 becomes dysregulated in many injured or infectious environments including ischemia/reperfusion injury, denervation, and infection/sepsis^31,32,33. In mdx mice, Cx43 has been associated with apoptosis and necrosis in myofibers³⁴. As the role of Cx43 in cardiac myocytes became clear in DMD patients, we sought to investigate the understudied pathological role of Cx43 in the skeletal muscle. In the present study, we explore a rescue role of Cx43 reduction in both the cardiac and skeletal muscle of mdx/WT chimeras.

Results

Genetic reduction of Cx43 rescues the mdx/WT-Cx43(+/−) chimeric heart

We generated mdx/WT and mdx/WT-Cx43(+/−) chimeras by injecting mdx (dystrophin−) murine embryonic stem cells (ESCs) into WT:Cx43(+/+) and WT:Cx43(+/−) (dystrophin+) blastocysts¹⁴. Seven day-old pups were genotyped for the presence of a heterozygous mutation in the Cx43 gene using DNA from tail tips. Half of the littermates contained the mutation and half did not (data not shown). Mdx ESCs contain a reporter DsRed transgene inserted into their genome whose ratio of band intensities compared to internal control, supplied by Jax labs, was used to determine the degree of ESC-derived cells (degree of chimerism)¹⁴. The presence of the DsRed transgene was assessed in pups tail tips (data not shown)¹⁴ and then confirmed at time of sacrifice using heart (Fig. 1A), diaphragm (Fig. 2A), and pectoralis (Supplementary Fig. S3). Tissue from mice transgenic for DsRed and mdx mice were used as a positive (100%) control and a negative (0%) control, respectively. Mouse chimeras in the range of 10–30% (DsRed) contained 10–30% of ESC-derived cells and 90–70% of blastocyst-derived cells respectively. Results obtained from DsRed inversely correlated with those obtained by western blot analysis of the dystrophin protein in heart, diaphragm, and pectoralis extracts (Figs. 1B and 2B, Supplementary Fig. S3). Quantification of dystrophin in mdx/WT and mdx/WT-Cx43(+/−) chimeras compared to WT (positive control) and mdx (negative control) showed a range of dystrophin expression (Supplementary Fig. S1). The presence of dystrophin+ and dystrophin− patches in the heart were observed in both mdx/WT and mdx/WT-Cx43(+/−) chimeras by immunofluorescence detection in cardiac cryosections (Fig. 1C). Variations in dystrophin levels became evident when comparative analysis was conducted across individual chimeras (Supplementary Fig. S1). For example, chimera 1 showed similar levels of dystrophin expression in heart, diaphragm, and pectoralis, but chimera 4 showed higher levels of dystrophin expression in heart than those in diaphragm or pectoralis.

Cx43 protein reduction in the heart and skeletal muscle of mdx:Cx43(+/−) mice and mdx/WT-Cx43(+/−) chimeras was confirmed through Cx43 immunoblotting (Figs. 1D and 2C). Quantification of Cx43 showed significantly higher Cx43 levels in mdx and mdx/WT with respect to WT, mdx:Cx43(+/−), mdx/WT-Cx43(+/−) despite variations in the degree of chimerism (Supplementary Fig. S1).

To study the pattern of Cx43 expression we performed immunofluorescence analysis. Cx43 was confined to the intercalated disc (ID) of the cardiomyocytes in WT, mdx:Cx43(+/−) mice and mdx/WT-Cx43(+/−) chimeric heart sections (Fig. 1E). Cx43 was additionally detected on the lateral cell borders (see white arrows) of cardiomyocytes in mdx hearts and mdx/WT chimera hearts (Fig. 1E). Cx43 retention to the ID, marked by N-Cadherin (N-Cad), was quantified (Fig. 1E-right). This suggests that Cx43 remodeling (lateral distribution) is prevented in the heart of both mdx:Cx43(+/−) mice and mdx/WT-Cx43(+/−) chimeras. Furthermore, evidence of fibrosis (Masson trichrome, MT) and mononuclear invasion (H&E) was observed in aged (10–14 months) mdx mice and mdx/WT chimeric hearts but not in WT, WT:Cx43(+/−), mdx:Cx43(+/−) mice and mdx/WT-Cx43(+/−) chimeric hearts (Fig. 1F,G). Lower magnifcation photos have been provided in Supplementary Fig. S2. This suggests that lack of Cx43 remodeling as the result of Cx43 reduction in mdx and chimeric mice may prevent cardiac histopathology. In line with this, restored cardiac function left ventricle (LV) ejection fraction (%EF) and fractional shortening (%FS) was observed in mdx:Cx43(+/−)²⁴ mice and mdx/WT-Cx43(+/−) chimeras (Fig. 1H,I). Altogether, the results suggest that genetic reduction of Cx43, Cx43(+/−), prevents muscular dystrophy associated cardiomyopathy in the heart of manifesting DMD carrier mice.

Genetic reduction of Cx43 rescues the mdx/WT-Cx43(+/−) chimeric skeletal muscle

We also studied the dystrophic skeletal muscle in chimeric mice to test a potential rescue role of genetic Cx43 reduction. We focused primarily on the diaphragm as it is the most affected skeletal muscle tissue in DMD patients and mdx mice^35,36 and confirmed our observations, with similar results, in the pectoralis muscle (Supplementary Figs. S2 and S3). Histopathological analysis revealed augmented fibrosis (MT), central nucleation and mononuclear invasion (H&E) in the diaphragm muscle of mdx and mdx:Cx43(+/−) mice, relative to that of WT mice (Fig. 2D–F). This suggests that genetic reduction of Cx43 does not benefit the mdx skeletal muscle. However, fibrosis, mononuclear infiltration, and central nucleation were reduced in the diaphragm muscle of mdx/WT-Cx43(+/−) chimeras relative to that of mdx/WT chimeras (Fig. 2D–F). This suggests that genetic reduction of Cx43 prevents pathology in the skeletal muscle of the mdx/WT-Cx43(+/−) chimeras. Accordingly, the skeletal muscle fiber cross-sectional area (CSA) distribution profile was assessed. While most of the fibers in WT diaphragm were in the range of 1,200–1,600 µm², fibers in mdx diaphragm were in a broader range, spanning from 400 µm² to 2,000 µm² at the expense of a reduced number of fibers in the 1,200–1,600 µm² range. mdx/WT-Cx43(+/−) chimeric diaphragm muscle was alike to that of WT, in which most fibers were in the range of 1200–1600 µm² (Fig. 2G). mdx/WT had less medium caliber (1,200–1,600 µm²), and more high caliber (2000+ µm²) fibers, shifting towards the mdx phenotype (Fig. 2G). Lastly, grip strength was improved in mdx/WT-Cx43(+/−) chimeras but not in mdx/WT chimeras or mdx:Cx43(+/−) mice relative to WT mice (Fig. 2H). Taken all together, the results suggest that genetic reduction of Cx43 corrects muscular dystrophy in DMD carrier mice, but not in DMD mice.

Cx43 is enhanced and functional in mdx but not in WT skeletal muscle macrophages

Our results suggest that Cx43 is enhanced in the skeletal muscle of mdx mice and mdx/WT chimeras relative to WT mice (Fig. 2C and Supplementary Fig. S1). Our results also suggest that Cx43 reduction prevents the development of skeletal muscle dystrophy in mdx/WT-Cx43(+/−) chimeras, but not in mdx:Cx43(+/−) mice (Fig. 2D–H). This finding in the skeletal muscle contrasts with that in the heart, where Cx43 reduction leads to corrections in both mdx/WT-Cx43(+/−) chimeras and mdx:Cx43(+/−) mice hearts (Fig. 1F–I). To begin to reconcile this dissimilar role of Cx43, we examined the Cx43 pattern of expression in skeletal muscle by immunofluorescence. We did not detect Cx43 on any part of the mdx or WT mature skeletal muscle fibers (Fig. 3A,B). This suggests that there may be other cell types distinct from the fibers that express Cx43 in the skeletal muscle, particularly in dystrophic mice, because Cx43 was seemingly in areas occupied by mononuclear cells (Fig. 3A,B). Due to previous reports of Cx43 in macrophages^37,38 we performed immunofluorescent analysis for Cx43 and F4/80 macrophage marker. This revealed that Cx43 was detected only in mdx F4/80+ mononuclear cells in the interstitial space between skeletal muscle fibers, areas where mononuclear invasion occurs (Fig. 3B).

To further investigate the role of Cx43 in DMD skeletal muscle macrophages, macrophage-enriched FACS-sorted F4/80+/Cd11b+ cells were purified from mdx and WT diaphragms (Fig. 3C,D). We obtained a higher percentage of the macrophage-enriched F4/80+/Cd11b+ population in mdx diaphragms relative to WT diaphragms (Fig. 3C,D). Furthermore, Cx43 protein expression in the F4/80+/Cd11b+ macrophages was enhanced in mdx versus WT (Fig. 3E,F).

To test the activity of Cx43 hemichannels in diaphragm F4/80+/Cd11b+ cells, we performed Ethidium Bromide (EthBr) uptake assays (Fig. 3G). Gap19 was used as a Cx43 hemichannel-specific peptide mimetic inhibitor. Mdx F4/80+/Cd11b+ cells exhibited a faster rate of EthBr uptake relative to WT F4/80+/Cd11b+ cells (Fig. 3G). However, Gap19 administration resulted in a dose-dependent slowing of EthBr uptake activity in mdx F4/80+/Cd11b+ cells, with negligible impact on WT F4/80+/Cd11b+ cells (Fig. 3G).

Because cardiac macrophages were also observed in the dystrophic heart, we performed F4/80 and Cx43 immunofluorescence in WT and mdx hearts to study a potential overlap. However, unlike the presence of overlap in the dystrophic diaphragm (Fig. 3B), there was no co-staining in the heart (Supplementary Fig. S4). Furthermore, macrophage-enriched FACS-sorted F4/80+/Cd11b+ cells purified from mdx hearts revealed negligible detection of Cx43 protein expression. Gravity-settled mdx heart myocytes were used as a Cx43 positive control (Supplementary Fig. S4). Altogether, the results open the possibility that detrimental activity of enhanced Cx43 hemichannels from resident skeletal muscle macrophages may be mitigated by Cx43 reduction in a dystrophic, chimeric environment.

Discussion

In this study, we show that Cx43-copy number reduction in mdx/WT-Cx43(+/−) chimeras result in a rescue of DMD pathology in both the heart and the skeletal muscle. These results are aligned with previous studies in the heart, in which normalized Cx43 levels benefit mdx cardiac pathology^16,24; but are unlike the observations in mdx skeletal muscle, in which normalized Cx43 levels do not benefit skeletal muscle pathology. We suggest aberrant Cx43 hemichannel activity in mdx macrophages promotes the dystrophic phenotype in the skeletal muscle. We also suggest the lack of rescue in mdx:Cx43(+/−) skeletal muscle compared to mdx/WT-Cx43(+/−) chimeras can be explained by the presence of some dystrophin in the symptomatic DMD carrier and the lack of dystrophin in mdx:Cx43(+/−) mice. Complete absence of dystrophin in mdx:Cx43(+/−) skeletal muscle may lead to exacerbation of a more oxidative environment that may ultimately impinge on the state of the macrophages. Overall, we propose symptomatic mdx carrier skeletal muscle, in addition to the heart, benefit from Cx43 normalization in the presence of some dystrophin+ fibers.

DMD patients exhibit chronic inflammation of the heart and skeletal muscle in the form of fibrosis, necrosis, and functional deficiencies. In mdx mice there is an upregulation of Cx43 in the affected muscles, possibly to compensate for increased injury, satellite cell exhaustion and increased myotube regeneration of the muscle^{39,40,41,42,43}. Similar to the heart, Cx43 is required for myoblast differentiation in vitro^44,45,46. In contrast with the heart where gap junction intracellular communication (GJIC) is essential, mature skeletal muscle cells fuse to form a syncytium, therefore they do not rely on GJ formation^44,45. Although absent from control, basal tissues Cx43 is expressed post-muscle injury and can be seen as punctate staining^30,31. Under similar circumstances including ischemia/reperfusion injury, denervation, and infection/sepsis, this study supports that macrophages upregulate Cx43^31,32,33. Despite the different roles of Cx43 in response to cardiac and skeletal muscle damage, higher expression is correlated to enhanced cell death^34,47,48.

Current treatments only provide short-term relief for DMD patients and carriers, although promising findings have been shown to attenuate the inflammatory phenotype. One of the most commonly prescribed treatments, Dexamethasone (DEX), is a glucocorticoid used to build strength and muscle. However, DEX has led to an increase in Cx43 hemichannels that can exacerbate skeletal muscle atrophy⁴⁹. In sepsis, Cx43 normalization via deletion or pharmacological inhibition is associated with a reduction of secreted necrotic factors, including cytokines and ATP, thereby increasing survival³⁸. Peptide mimetics, like Gap19, have been successful because they are capable of inhibiting Cx43 hemichannel dysregulation, but maintain gap junction function in other cell types³⁷.

In mdx mice, Cx43 is expressed in between mature skeletal muscle fibers, where lymphocytes, neutrophils, and macrophages reside. However, lymphocytes and neutrophils do not express Cx43³⁸. Macrophages also have the capability to fuse with adjacent fibers, which may contribute to DMD pathology^37,46,50,51. Aberrant hemichannel activity has also been observed in mdx mouse myofibers to cause apoptosis^22,33,48,52. Based on localization of Cx43 to the mononuclear cells, we postulate that reduction of hemichannel activity in skeletal muscle macrophages is linked to decreased cell death, suppressed activation of pro-inflammatory factors, and therefore, slowed muscle deterioration^17,34,53.

In our mouse model of symptomatic DMD carriers, we have shown that Cx43 has divergent roles in skeletal and cardiac tissue. Cardiomyocytes are post-mitotic, therefore post-translational effects of Cx43 better address the tissue environment^28,29. One major contributor to stress signals in the DMD heart is oxidative stress^24,54,55. In contrast, skeletal muscle is a syncytium in which fibers fuse and macrophages remain outside of the fibers. Insight for understanding the role of Cx43 may be further addressed by testing the response and modulation of reactive oxygen species in mdx versus WT macrophages. Data presented here suggest treatments limiting Cx43 and Cx43 hemichannel activity may also target Cx43+ skeletal muscle macrophages, which have roles in tissue repair and injury resolution. Macrophages have recently been shown to be essential for uptake and slow release of antisense oligonucleotides via Cx43^54,56,57. The role as a reservoir is necessary for therapeutic administration of partially-functional dystrophin to skeletal fibers and muscle stem cell regeneration for DMD patients^39,43. Cx43 is not enriched in mdx cardiac macrophages compared to the adjacent cardiomyocytes, reserving a larger role for Cx43 in the cardiomyocytes and skeletal-specific macrophages. We cannot rule out, however, a potential role for Cx43 in the cardiac macrophages, for example, at later stages of the disease.

Further investigation is necessary to determine if dystrophin from healthy fibers of a chimeric environment modulates Cx43 expression and function in neighboring macrophages, which in turn, modulate death of the neighboring fibers. In addition, we would like to investigate how this study translates to younger symptomatic carrier mice as we conducted studies in 6-month-old mdx/WT and mdx/WT-Cx43(+/−) chimeras with fibrosis in the former and no fibrosis in the latter (Supplementary Fig. S4).

As a limitation of the study, we cannot rule out an early developmental and postnatal contribution of Cx43 expression, which may still be highly expressed in the skeletal muscle, as the mixing of the WT blastocysts and the mdx ESCs takes place at pre-implantation stages of development. Thus, an early, developmental/postnatal effect of Cx43 may be a contributor to the long-term phenotype.

These results importantly contribute to research towards improved cardiomyopathic understanding and development towards target-specific (Cx43) skeletal muscle anti-inflammatory treatments for symptomatic DMD carriers.

Methods

Animals

WT (C57BL/6J), mdx (C57BL/10ScSn-Dmdmdx/J), and DsRed (B6.Cg-Tg(CAG- DsRed*MST)1Nagy/J), mice were purchased from Jackson Laboratories (Bar Harbor, ME, https://www.jax.org). Chimeras: Mouse and embryonic stem cell derivation and maintenance, and mouse chimera generation have been previously described in Gonzalez et al.¹⁴. We generated mdx/WT and mdx/WT-CX43(+/−) chimeras by injecting mdx ESCs into WT:Cx43(+/−) blastocysts. Quantification of ESC incorporation by genotyping of inserted genomic DsRed gene in mdx ESCs using primers fwd: 5′-GGTGATGTCCAGCTTGGAGT-3′ and rev: 5′-CCCCGTAATGCAGAAGAAGA-3′ (DsRed Jax) or previously published sequences⁵⁸ and protocols¹⁴. Internal positive control primers provided by Jax Labs were used: fwd: 5′-CTAGGCCACAGAATTGAAAGATCT and rev: 5′-GTAGGTGGAAATTCTAGCATCATCC-3′. Chimeric and non-chimeric control animals were sacrificed and analyzed between 10–14 months (sample size has been incorporated into figures). A few chimeras were also sacrificed at 6 months of age. Chimeras were characterized and matched in pairs according to similar chimeric signatures determined by DsRed fluorescence from tail tip sections collected postnatally¹⁴ and DsRed genomic PCR of tissues collected at sacrifice (Figs. 1A and 2A, Supplementrary Fig. 3A), and dystrophin expression (Fig. S1A). Both males and females were combined due to the long history of the lab to obtain a lack of deviations at these time-points. Individual data points have been color-coded for transparency; red dots represent females and black dots represent males. All animal experiments were approved by the IACUC of Rutgers New Jersey Medical School and performed following relevant guidelines and regulations.

Western blot

Western Blot analyses were previously described^14,24. Following euthanasia in 10–14-month-old mice, tissues were rinsed in sterile PBS, flash-frozen in liquid nitrogen, and homogenized in RIPA buffer supplemented with protease and phosphatase inhibitors (Roche). Protein concentrations of tissue lysates were estimated using a BCA kit (Pierce). 15 μg protein (heart), or 30 μg protein (skeletal), per sample, was separated on 8% gels (Bio-Rad) 100–130 V for 90 minutes (heart), or 4–12% gradient gels (Bio-Rad) 100 V for 120 minutes (pectoralis, diaphragm). Gels were transferred to 0.45 µm nitrocellulose membrane 30 V for 16 hours at 4 °C. Ponceau S stain determined initial transfer success Blots were blocked in 5% non-fat laboratory-grade milk power (BioRad) in TBS-T. FACS cells were pelleted and lysed in RIPA buffer for 30 min with gentle agitation at 4 °C. Protein (normalized by cell number) approximated a volume relative to 60,000 macrophages was ran on a 10% gel for 100V-120V for 60–90 minutes. Gels were transferred to a 0.20 µm nitrocellulose membrane at 75 V for 2 hours. Probing steps were completed in 2% BSA. All gels were probed for Cx43 (Sigma, C6219, 1:10000), Dystrophin (Mandys8, 1:100, DSHB), GAPDH (Sigma, G9295, 1:10000), and Vinculin (1:2000, Sigma V9131). Blots were imaged and quantified using ECL reagent (Bio-Rad), Bio-Rad imaging box and image lab software.

Immunofluorescence

Following euthanasia mouse hearts and skeletal muscle were harvested and rinsed in sterile PBS and frozen in Tissue-Tek^® OCT filled cryomolds using isopentane cooled on dry ice. Cryosections, 6 μm (heart) and 10 μm (skeletal muscle), were cut onto Precleaned Superfrost^® Plus slides (VWR Micro Slides) using Leica Cryostat with a −20 °C chamber. Sections were used immediately or stored at short-term(−20 °C) or long-term(−80 °C). Heart sections, stained for Cx43, were placed in chilled acetone for 10 minutes, washed, blocked in 10% Goat Serum in PBS-T (0.1% tween20 in 1X PBS) at room temperature (RT) and probed with the primary antibody Cx43 (1:1000, C6219, Sigma) and/or N-Cadherin (1:300, 33-3900, Invitrogen) overnight at 4 °C. Heart sections stained for dystrophin were thawed at RT for 30 minutes, washed with 1X PBS for 5 min, blocked for 1 hour in M.O.M.™ mouse IgG blocking reagent (BMK-2202, Vector M.O.M.™ immunodetection Kit, Vector Laboratories) and probed for using primary antibodies reactive to dystrophin (1:10, Mandys8, DSHB) in M.O.M.™ diluent overnight at 4 °C. All sections were washed 3 × 3 minutes in PBS-T (0.1% tween20 in 1X PBS) and probed with Alexa Fluor secondary antibodies (1:250, Invitrogen).

Skeletal muscle sections were thawed at RT and washed with 1X PBS. Sections, probed for Cx43 or F4/80, were fixed using 4% paraformaldehyde (PFA) for 10 minutes and then blocked for 1 hour in 10% Goat Serum in PBS-T at RT. Tissue sections were then probed with primary Cx43 (1:10,000, custom, generously supplied by Dr. Lampe) or F4/80 (1:100, MCA497RT, Bio-Rad). All sections were washed 3 × 3 minutes in PBS-T (0.1% tween20 in 1X PBS) and probed with Alexa Fluor secondary antibodies (1:250, Invitrogen). Cell borders were outlined with secondary conjugated WGA (1:500, W32464 Invitrogen, Thermo Fisher Scientific).

Afterward, muscle sections were washed in PBS-T and mounted using ProLong^TM Diamond antifade mountant with DAPI (P36962, Thermo Fisher Scientific). At least 3–5 sections (40x or 100x)were examined. Images were taken using a Nikon Eclipse T1 (Melville, NY, http://www.nikonusa.com) for immunoflourescence images, and an Olympus BX51 microscope for histological samples and processed using NIS-Elements BR software in a blinded fashion. Cross- sectional area (CSA) was measured using at least 200 fibers across 4–5 sections (100x and 200x). Colocalization was analysed using an Olympus Fluoview 1000 Confocal Laser Scanning Microscope and Z-stacks 0.5 µm thick at 600x magnification using Fluorview software and then processed in Fiji for maximum intensity. Cell counting and CSA were determined in Fiji in a blinded fashion.

H&E and Masson trichrome

Skeletal and heart muscles were fixed in 4% paraformaldehyde overnight and embedded in paraffin, following euthanasia in 10–14-month-old mice. Sections were cut at 6 μm from each tissue and stained for histopathology utilizing an H&E kit (Vector, Torrance, CA) or Masson Trichrome kit (Richard-Allen Scientific, Thermo Fisher Scientific, Waltham, MA). Images were taken using a Nikon Eclipse T1 microscope and processed using NIS-Elements BR software. Fibrosis was quantified, blinded, by subtracting blue fibrotic regions from the total muscle area in Fiji and repeated in 5 images.

Echocardiography

Animals were anesthetized with Avertin (290 mg/kg, IP) and maintained on a heated platform at 37 °C. Transthoracic echocardiography was performed using a 30-MHz ultrasound transducer (RMV707B) using VisualSonics Vevo 770 High-Resolution In-Vivo Micro-Imaging System. Mice, oriented in a shallow left lateral position, had warm coupling gel applied to the chest. Two-dimensional B-mode images and left ventricular M-mode tracings were acquired from the parasternal short-axis view at a sweeping speed of 100–200 mm/s at the level of the mid-papillary muscle. In a blinded fashion, M-mode measurements of left ventricular internal diameter (LVID) and wall thickness were acquired over eight consecutive beats and averaged using the leading-edge convention of the American Society of Echocardiography. Left ventricular ejection fraction (EF) was calculated following the cubed method using the following formula: EF(%) = 100 × [(LVIDd)³ − (LVIDs)³]/(LVIDd)³. Fractional Shortening (FS) was calculated following %FS = [LVIDd − LVIDs/LVIDd] × 100%. LVIDd: left ventricular end-diastolic dimension. LVID: left ventricular end-systolic dimension⁵⁹. 2 echocardiographic determinations per mouse.

Grip strength

An assessment of muscular function was recorded using a grip strength meter in a blinded fashion (Columbus Instruments). The grip strength meter was positioned horizontally, and mice, held by their tails, were lowered toward the pull bar. Mice (10–12 months) were allowed to get a good grip on the triangular bar with only their forelimbs. Once they had a good grasp, the mouse was pulled backward parallel to the device, until the mouse let go. This was completed in 2 runs: 5 pulls each. Run #1 trained and conditioned the mice to the apparatus. The top 3 scores from run #2 were averaged for the final value. This process was repeated 3-times over the 10–12 month period for each mouse, and the average used in statistical analysis. The force that was applied to the bar at the time of release was recorded as Gram-force.

Fluorescent activated cell sorting (FACS)

Following euthanasia, diaphragms were dissected from 8–10-month-old WT and mdx mice, washed in 1% Pen/Strep in PBS, and minced. Digestion was completed using Liberase TL (Sigma) for 2 hours at 37 °C on an orbital shaker (20 rpm). Heart: the heart was dissected from 13–16-month-old mdx mice using a Lagendorff-free method⁶⁰ describe below. Cells were filtered through a 40 μm cell strainer and incubated with antibodies F4/80, Cd11b and DAPI (Thermo Fisher Scientific) for 20 minutes on the benchtop covered from light. Samples were washed and sorted by the Flow Cytometry/Cell Sorting Rutgers Core Facility.

Ethidium bromide uptake in vitro

Cells post-FACS-sort, from 8–10-month-old WT and mdx mice, were concentrated, mounted, and allowed to attach for 20-minutes on a chamber for confocal imaging. Ethidium Bromide (EthBr) was added during the first few frames of imaging (20 μM). A scanning confocal microscope (Olympus, FluoView1000) with a 600x objective lens captured an image every 10 seconds for 20 minutes (120 total images).

Gap19 Cx43 hemichannel-specific blocker (Sigma peptide mimetic) was added to chamber cells at the time of mounting for 20-minute incubation. While blinded to the treatment group, Fiji software was used to measure the fluorescence of a circle drawn around each cell in each frame (F). Values were normalized to the 3^rd frame (F₀) after the addition of EthBr to account for variability induced by different rates of diffusion. Results are displayed as F/F₀.

Laggendorff-free isolation method for cardiac myocytes and nonmyocytes

The heart was dissected from 13–16-month-old mdx mice (N = 3). Single ventricular cardiomyocytes and mononuclear cells were isolated with Collagenase Type II (Worthington LS004176) and Protease XIV (Sigma P5147) by Laggendorf-free digestion of heart ventricle⁶⁰. Myocyte and non-myocyte populations were separated by 20 minute of gravity filtration. Langendorff-free supernatant cell suspension was filtered through a 40 μm cell strainer and underwent the FACS preparation and sorting. The settled pellet of cardiomyocytes underwent two additional 15 minute gravity settlings in 4 mL of Perfusion buffer in a 15 mL tube⁶⁰. The final pellet of myocytes was gently homogenized to obtain a protein sample used in western blot (Supplementary Fig. S4B,C).

Statistics

Data was analyzed for statistical significance using parametric analysis in GraphPad Prism 8. Statistical significance was determined using one-way Brown-Forsythe and Welch analysis of variance statistical models (ANOVA) tests and Dunnett’s T3 multiple comparison test. Cross-sectional area (Fig. 2G) was assessed using Two-way ANOVA and Tukey’s multiple comparisons test. Alpha= 0.05. Two-tailed. Data are expressed as mean ± SEM. ^####P < 0.0001, ^###P < 0.0005, ^##P < 0.005, ^#P < 0.05 versus WT. ****P < 0.0001, ***P < 0.0005, **P < 0.005 *P < 0.05 versus mdx. ^$$$$P < 0.0001, ^$$P < 0.005, ^$P < 0.05 for mdx/WT versus mdx/WT-Cx43(+/−) chimeras.

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Acknowledgements

We thank Drs. J.E. Contreras and N.Shirokova for advisement on Cx43 and in-vitro experiments, Dr. J.P. Gonzalez for initial experiments and Dr. P.D. Lampe for providing the Cx43 antibody. We also thank Dr. Ghassan Yehia and Peter Romanieko at Rutgers Transgenic Core Services for their help making the chimeras, The Flow Cytometry/Cell Sorting Core, and the Rutgers Department of Cell Biology and Molecular Medicine at RBHS for histology and support. We also thank Mr. I. Campell and NERA students S. Acevedo, J. Caballero, L Perez and B. Ojeda for help with grip strength and histological experiments. This work was supported by NIH 1R01HL141170 to D.F., MDA Research Grant 416281 to D.F., MDA Research Grant 602349 to D.F., AHA predoctoral fellowship 17PRE33660354 to E.H.

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Department of Cell Biology and Molecular Medicine, Rutgers Biomedical and Health Sciences, New Jersey Medical School, Newark, NJ, USA
Julie Nouet, Eric Himelman, Kevin C. Lahey, Qingshi Zhao & Diego Fraidenraich

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Julie Nouet
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Eric Himelman
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Kevin C. Lahey
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Qingshi Zhao
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Diego Fraidenraich
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Contributions

Conception and Design: J.N. and D.F. Experiments: J.N., E.H., Q.Z. and K.C.L. Analysis and interpretation of data: J.N., E.H., K.C.L. and D.F. Manuscript writing: J.N., Manuscript editions: J.N. and D.F. All authors reviewed and approved the manuscript.

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Correspondence to Diego Fraidenraich.

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J.N., E.H. and K.C.L. have no competing interests D.F. is a member of the Editorial Board of Scientific Reports. Q.Z. and D.F. have the following patent: “Corrective roles of insulin-like growth factor-binding protein-3 in cardiomyopathy”. United States Patent No. 8,802,629, issued on Aug. 12, 2014, assigned to Rutgers, The State University of New Jersey (New Brunswick, New Jersey).

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Nouet, J., Himelman, E., Lahey, K.C. et al. Connexin-43 reduction prevents muscle defects in a mouse model of manifesting Duchenne muscular dystrophy female carriers. Sci Rep 10, 5683 (2020). https://doi.org/10.1038/s41598-020-62844-9

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Received: 04 September 2019
Accepted: 18 March 2020
Published: 30 March 2020
DOI: https://doi.org/10.1038/s41598-020-62844-9

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Abstract

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Human skeletal muscle aging atlas

Duchenne muscular dystrophy

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Introduction

Results

Genetic reduction of Cx43 rescues the mdx/WT-Cx43(+/−) chimeric heart

Genetic reduction of Cx43 rescues the mdx/WT-Cx43(+/−) chimeric skeletal muscle

Cx43 is enhanced and functional in mdx but not in WT skeletal muscle macrophages

Discussion

Methods

Animals

Western blot

Immunofluorescence

H&E and Masson trichrome

Echocardiography

Grip strength

Fluorescent activated cell sorting (FACS)

Ethidium bromide uptake in vitro

Laggendorff-free isolation method for cardiac myocytes and nonmyocytes

Statistics

References

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