Low intensity training improves redox status and reduces collagen fibers on dystrophic muscle
Article information
Abstract
Exercise therapy on skeletal muscle of muscular dystrophies has no defined parameters. The effect of low-intensity treadmill training on the oxidative stress markers and fibrosis on hindlimb muscles was investigated. Sixteen dystrophic male mdx animals were separated in trained (mdxT/n=8) and untrained (mdxNT/n=8) groups. Wild type animals (WT/n=8) were used as healthy control. The mdxT group runned at a horizontal treadmill (9 m/min, 30 min/day, 3 times/wk, 8 weeks). Gastrocnemius and tibial anterior muscles were collected for analysis of enzymatic/non-enzymatic oxidant activity, oxidative damage concentration, collagen fibers area morphometry. The mdxT group presented a lower collagen fiber area compared to mdxNT for gastrocnemius (P=0.025) and tibial anterior (P=0.000). Oxidative damage activity was higher in the mdxT group for both muscles compared to mdxNT. Catalase presented similar activity for tibial anterior (P=0.527) or gastrocnemius (P=0.323). Superoxide dismutase (P=0.003) and total antioxidant capacity (P=0.024) showed increased activity in the mdxT group at tibial anterior with no difference for gastrocnemius. Low-intensity training is considered therapeutic as it reduces collagen deposition while improving tissue redox status.
INTRODUCTION
Duchenne muscular dystrophy (DMD) is a genetic disease caused by the absence of dystrophin protein which promotes sarcoplasmatic membrane stability (Comim et al., 2016; Kostek and Gordon, 2018). Its absence makes skeletal muscle susceptible to contraction-induced injuries (Schill et al., 2016; Van Putten et al., 2012), as well as weakness and muscle loss (Gianola et al., 2013), with muscle tissue showing a chronic inflammatory feature (Mann et al., 2011).
Inflammation is an early event in DMD which leads to an excessive influx of electrolytes in the form of calcium and sodium. The accumulation of acidic metabolites and the increased inflammatory substances lead to muscle fibers apoptosis, necrosis and to degeneration/regeneration cycles. Over time, there is a reduction in the regenerative capacity of muscle fibers and an accumulation of collagen fibers in the extracellular matrix resulting in fibrosis and generating weakness in the diaphragm and limb muscles (Kim et al., 2013; Klingler et al., 2012; Kostek and Gordon, 2018; Smith et al., 2016).
In DMD, this microenvironment of regeneration without synchrony is exacerbated by inflammatory cytokines and by oxidative stress, frequently associated with the fibrogenesis process (Barbieri and Sestili, 2012; Chazaud, 2016; Mann et al., 2011; Zanotti et al., 2016). Redox equilibrium is essential for cellular homeostasis (Pérez-Torres et al., 2017), being a key modulator of skeletal muscle plasticity/dysfunction (Espinosa et al., 2016). Oxidant enzymes can interfere with skeletal muscle fibrosis deposition progression (Kozakowska et al., 2015) showing efficacy on dystrophic phenotype improvement, reducing muscle damage, loss of muscle strength, inflammatory process and fibrosis (Comim et al., 2016).
In a systematic review, elaborated by Hyzewicz et al. (2015a) whose sample includes 16 studies in horizontal treadmill, only 25% used low-intensity training (9 m/min), demonstrating the positive effects in the physiological parameters of the mdx model. Rota-rod (Frinchi et al., 2014), swimming (Hyzewicz et al., 2015b) and horizontal treadmill (Gaiad et al., 2017) are modalities of low-intensity training and authors observed improvement on mitochondrial gene expression, muscle differentiation on degeneration/regeneration process and turnover of extracellular matrix of the skeletal dystrophic muscle.
Low-intensity training has been seen as a promising form of treatment. Oxidative stress, in addition to damaging cell structures, can interfere with the inflammation/regeneration process of muscle fibers, resulting in fibrosis that impairs muscle function. These two parameters can help us clarify the role of low-intensity training on the dystrophic muscle. We tested the hypothesis that low-intensity training leads to adaptation of antioxidant enzymes reducing deleterious effects of reactive oxygen species (ROS) produced during exercise training leading to a reduced fibrosis deposition on skeletal muscle of the mdx model.
MATERIALS AND METHODS
Experimental design
Sixteen male mdx mice (C57BL/10ScSn-Dmdmdx/J) and eight wild-type mice (C57BL/10) acquired from the FioCruz Institute (Rio de Janeiro, Brazil) were used in this study. This research was approved by the Ethics Committee on Animal Use of the Universidade Federal University of Vales do Jequitinhonha e Mucuri under protocol n° 017/2011. Animals were maintained in cages under 12 hr day/night cycle, 22°C, supplied with food and water ad libitum Animals were aleatory randomized in two groups: trained group (mdxT, n=8) and untrained group (mdxNT, n=8). Wild-type (WT) mice composed the control group (n=8). Exercise protocol started when animals were 11 weeks old. At this age fibrosis and muscle lesion are similar between mdx mice and age-matched humans. (Grounds et al., 2008).
Low-intensity training protocol
A low-intensity training protocol on a horizontal treadmill (EP 131; Insight, Ribeirão Preto, Brazil) 30 min/day, 3 times a week for 60 days at a velocity of 9 m/min were performed by the animals of the mdxT group. The speed of the protocol was of 9 m/min so that the therapeutic training was considered low intensity (De Luca, 2014). The animals of the mdxNT group were placed on the off treadmill (0 m/min) with the same duration and frequency as the animals of the mdxT group to cause the same environmental stimuli to all mice.
Biological sample collection
After 8 weeks of low-intensity training protocol, samples of the tibial anterior and gastrocnemius muscle of all 3 groups (mdxT, mdxNT, and WT) were gathered for morphological, histochemical and redox status analysis. Muscle samples of the right hindlimb of approximately 2 cm2 were fixed in a paraformaldehyde solution at 4% to further histological and histochemical analysis. Muscle samples of the left hindlimb were immersed in a phosphate buffer pH 7.2 to wash and stored at −80°C for redox status markers assays.
Histological and histochemical analysis
The muscle samples of tibial anterior and gastrocnemius were fixed in paraformaldehyde solution and were processed to be embedded in paraffin. Sections of 5 μm in thickness were obtained and were oven-dried (60°C) in a horizontal position. Slides were reacted with Picrossirius red, a combination of Sirius red F3BA (Colour Index 35780, Sigma-Aldrich, St. Louis, MO, USA) dissolved in a saturated picric acid solution. Photomicrographs were made using an optical microscope (LABOMED LxPol, Labo America, Fremont, Canada) coupled to with an Axio CAM HRc camera and Software Capture Pro 2.9.0.1.
Intramuscular collagen deposition
Slides reacted with picrossirius red to exhibit collagen-positive areas from fifteen randomly selected fields ×100 per animal (~2.000 fibers/group) were quantified (Smith and Barton, 2014). The images were analyzed using ImageJ software (ver. 1.50i, National Institute Health, Bethesda, MD, USA), with a threshold was applied to each image, first converting it to 8-bit (blue), then subtracting the background and images automatically scaled from 0 to 255. Intramuscular collagen analysis are shown in percentage of the total area (964,819.05 μm2).
Redox status markers
Samples were macerated for 3 min (Corning, Potter-Elvehjem Tissue macerator) maintained on ice in PBS (0.05 M, pH 7.34, 4°C). The homogenate was divided into two parts and one part was centrifuged (Thermo Electron Led GmbH D37520 Osterode, Kalkberg, Germany) at 5.000 g for 5 min at 4°C and was analyzed on the basis of thiobarbituric reactive substances and the total antioxidant capacity (ferric reducing ability of plasma, FRAP) method. The sediment was used to measure the carbon content in proteins. The second part was centrifuged at 10.000 g for 10 min at 4°C and was used to analyze the activity of superoxide dismutase and catalase enzymes. All analyzes were performed in duplicates.
Lipid peroxidation
Thiobarbituric reactive substances concentration was measured in the muscle according to the method described Ohkawa et al. (1979). Aliquots of the tibial anterior and gastrocnemius samples (0.15 mL) were added to 8% sodium dodecyl sulfate, 2.5 M acetic acid (pH, 3.4) and 0.8% thiobarbituric acid. The samples were incubated for 90 min at 95°C and read on a spectrophotometer at 532 nm (SpectraMax 190, Molecular Devices, San Jose, CA, USA). The concentrations of thiobarbituric reactive substances in the samples were determined from the standard curve of known concentrations of malondialdehyde (MDA) and expressed in nmol MDA/mg protein.
Carbonyl derivatives in proteins
The tibial anterior and gastrocnemius homogenate pellet was suspended in 1 mL of 50 mM potassium phosphate buffer pH 6.7 containing 1 mM ethylenediamine-tetra-acetic acid. Each sample was homogenized and divided in to blank and test. Ten percent of trichloroacetic acid was added to all samples which were then centrifuged at 5.000 g for 10 min at 4°C and the supernatant discarded. 2,4-dinitrophenylhydrazine (10 mM DNPH) (Sigma-Aldrich) diluted in 2 mM hydrochloric acid was added to the test pellet. When white is added only HCl 2 mM. The samples were kept in the dark at room temperature for 30 min and homogenized in Vortex every 15 min. After, 10% trichloroacetic acid was added to the samples, which were homogenized and centrifuged at 5.000 g for 10 min at 4°C. The supernatant was discarded, and the pellet washed in 1 mL of ethanol and ethyl acetate (1:1) and centrifuged at 5.000 g for 10 min and at 4°C twice. Finally, the pellet was dissolved in 6% sodium dodecyl sulfate and centrifuged at 10.000 g for 10 min at 4°C. The supernatant was evaluated in a spectrophotometer at 370 nm (SpectraMax 190, Molecular Devices). A molar absorption coefficient of 22.000 M/cm was considered (Dalle-Donne et al., 2003; Levine et al., 1994).
Superoxide dismutase activity
The test of superoxide dismutase activity (EC 1.15.1.1) was performed according to Del Maestro and McDonald (1987) and as described by Barreto et al. (2012). Samples from each gastrocnemius (0.03 mL) and tibial anterior (0.1 mL) tissue were added to 0.6 mL potassium phosphate buffer (50 mM, pH 8.2, 37°C) containing 1 mM DTPA (diethylenetriamine penta-acetic acid) (Sigma-Aldrich). The reaction started by adding 0.003 mL of pyrogallol (1,2,3-benzenetriol, Sigma-Aldrich) to 0.2 mM. The reaction was determined by spectrophotometer on a microplate reader at 420 nm, 37°C, for 4 min (SpectraMax 190, Molecular Devices). The activity of superoxide dismutase was expressed as U/mg protein, where one unit of enzyme is the amount that causes inhibition of autoxidation of pyrogallol by 50%.
Catalase activity
The catalase activity test (EC 1.11.1.6) was performed as described by Barreto et al. (2012). The following were added: 0.7 mL of phosphate buffer (50 mM, pH 7.0) and an aliquot of 0.015 mL gastrocnemius and 0.025 mL tibial anterior of the homogenate, and then added gastrocnemius (0.02 mL) and tibial anterior (0.01 mL) of substrate (H2O2, 0.03 M) (Sigma-Aldrich). The hydrogen peroxide decline was performed for 1 min at 25°C in a spectrophotometer at 240 nm (Libra S22 spectrophotometer, Biochrom, UK) in quartz cuvettes. The catalase was expressed as ΔE/min/mg protein, where ΔE corresponds to the variation of enzyme activity for 1 min.
Non-enzymatic antioxidant capacity
The non-enzymatic antioxidant capacity of the samples was determined by the total antioxidant capacity method Benzie and Strain (1996). To a 0.528 mL aliquot of the total antioxidant capacity reagent, 0.072 mL of the sample homogenate was added. This mixture was homogenized and incubated in the dark at 37°C for 30 min. The samples were then centrifuged at 300 g for 5 min and the supernatant was spectrophotometrically analyzed in a microplate reader at 593 nm (SpectraMax 190, Molecular Devices). The total antioxidant capacity of the samples was expressed as Fe2+ equivalents, determined from the standard curve of known concentrations of FeSO4 and normalized by the amount of protein in the sample. The results were expressed as μM FeSO4/mg protein.
Dosage of proteins
The protein concentration of the samples was determined by the method of Bradford quantification (Comassie blue assay) (Bradford, 1976). The duplicate reading was performed on the spectrophotometer in a microplate reader (SpectraMax 190, Molecular Devices) at 590 nm and the protein values determined by Softmaxpro Software (ver. 5.4, Molecular Devices) in mg/mL.
Statistical analysis
The descriptive statistical analysis was performed via mean and standard deviation calculations to intramuscular collagen fiber quantification, markers of oxidative damage (thiobarbituric reactive substances and Carbonyl derivatives in proteins) and antioxidant defense (superoxide dismutase, catalase and total antioxidant capacity). For the analysis of oxidative damage and antioxidant defenses, mean values of the WT group were used to normalize the values of mdxT and mdxNT groups. Analysis of the normality of the data was performed by the Shapiro–Wilk test. To detect difference between groups, the analysis of variance was performed and the Bonferroni test was used as post hoc. The variables which were normally distributed were analyzed by independent t-test and the variables not normally distributed were analyzed by the Mann–Whitney U-test. Correlation analysis was performed using Pearson correlation coefficient and Spearman correlation coefficient tests according to the distribution of normality of the samples. Correlations were considered weak to values less than 0.50, moderate 0.50 to 0.75, strong 0.75 to 0.90, very strong when greater than 0.90 (Koo and Li, 2016). The IBM SPSS Statistics ver. 19.0 (IBM Co., Armonk, NY, USA) was used for data analysis, considering P≤0.05.
RESULTS
Qualitative analysis of tibial anterior and gastrocnemius muscles showed that collagen fibers are organized in thick tracts mainly of perimysium and thin bundles in the endomysium. The mdxT group presented thinner bundles of perimysium covering larger muscular areas when compared to mdxNT. Collagen fibers of WT animals are organized in thin tracts of perimysium and endomysium as shown in Figs. 1 and 2.
Morphological analysis of the deposition of collagen fibers on gastrocnemius muscle. Picrossirius red reaction (A–C) and picrossirius red under polarized light (D–F). Scale bar=200 μm. WT, wild-type; mdxT, trained mdx animals; mdxNT, untrained mdx animals. >>Deposition of collagen fibers in the perimysium. >Deposition of collagen fibers in endomysium. *Deposition of collagen fibers in polarized light.
Morphological analysis of the deposition of collagen fibers on tibial anterior muscle. Picrossirius red reaction (A–C) and picrossirius red under polarized light (D–F). Scale bar=200 μm. WT, wild-type; mdxT, trained mdx animals; mdxNT, untrained mdx animals. Anterior >>Deposition of collagen fibers in the perimysium. >Deposition of collagen fibers in endomysium. *Deposition of collagen fibers in polarized light.
Intramuscular collagen deposition
Gastrocnemius and tibial anterior muscle morphometry of collagen fibers deposition showed similar features. The percentage area of intramuscular collagen fibers deposition of the mdxNT group (4.26±3.3) was higher than the mdxT (1.75±0.9) and WT (1.13±1.1) (P=0.025) groups to gastrocnemius muscle. Tibial anterior muscle percentage area was also higher in the mdxNT group (0.70±0.2) than mdxT (0.31±0.1) and WT (0.30±0.1) (P=0.000). No significant difference could be observed between mean values of mdxT and WT groups for gastrocnemius (P=1) or tibial anterior (P=1) analysis (Fig. 3).
Effect of low-intensity training on the percentage of intramuscular collagen fibers deposition. Morphometric analysis of the percentage of intramuscular collagen fiber deposition in tibial anterior and gastrocnemius muscles. TA, tibial anterior; GASTROC, gastrocnemius; WT, wild-type; mdxT, trained mdx animals; mdxNT, untrained mdx animals. *Significant difference between groups (analysis of variance one-way with post hoc Bonferroni test, n=21).
Markers of oxidative stress analysis
Concentration of oxidative stress markers (thiobarbituric reactive substances and carbonyl derivatives in proteins) were higher in the mdxT group when compared to mdxNT or WT groups for gastrocnemius and tibial anterior muscles.
Mean values of thiobarbituric reactive substances on tibial anterior and gastrocnemius muscles were higher in the mdxT group (1.24±0.2 and 1.36±0.4) than the mdxNT group (0.83±0.0 and 0.75±0.1) (P=0.005 for gastrocnemius and P=0.013 for tibial anterior), respectively. Carbonyl derivatives in proteins concentration in gastrocnemius and tibial anterior were higher in the mdxT group (1.66±0.3 and 1.40±0.6) than mdxNT (0.85±0.1 and 1.40±0.6) (P=0.004 for gastrocnemius and P=0.019 for tibial anterior analysis) (Fig. 4, Table 1).
Effect of low-intensity training on markers of oxidative damage in muscles. Concentration of malondialdehyde in tibial anterior and gastrocnemius muscles. Concentration of carbonyl compounds in the tibial anterior and gastrocnemius muscles. TA, tibial anterior; GASTROC, gastrocnemius; mdxT, trained mdx animals; mdxNT, untrained mdx animals. *Significant difference between groups (independent t-test or Mann–Whitney U-test, n=21).
Concentration ratio of muscle damage markers of dystrophic animals normalized by wild-type
Antioxidant enzyme system analysis
Superoxide dismutase activity was similar to gastrocnemius muscle in both mdx groups (P=0.306), with mdxT group (1.10± 0.4) presenting 28.8% higher activity than mdxNT group (0.81±0.1). At tibial anterior muscle superoxide dismutase activity was higher in the mdxT group (0.98±0.1) than the mdxNT group (0.65±0.0) (P=0.003).
Catalase presented no difference between the studied muscles or animal groups. Even though its activity was 47.4% higher on the mdxT group (1.20±0.9) than the mdxNT group (0.72±0.3), there was no significant difference between them with regard to gastrocnemius muscle (P=0.323). Regarding tibial anterior muscle analysis, catalase activity was 15.6% higher in the mdxT group (0.95±0.3) when compared to mdxNT (0.81±0.3) (P=0.527).
Total antioxidant capacity of the gastrocnemius muscle was similar to mdxT (1.45±0.4) and mdxNT groups (1.09±0.1) (P=0.110), with the trained group presenting 35.9% more antioxidant capacity than the untrained group. For the tibial anterior muscle this activity was significantly higher in the trained group (0.90±0.0) than the mdxNT group (0.74±0.1) (P=0.024), as shown in (Fig. 5).
Effect of low-intensity training on the antioxidant defense of muscles. Activity of the superoxide dismutase (SOD), catalase (CAT), and ferric reducing ability of plasma (FRAP) in tibial anterior and gastrocnemius muscles. TA, tibial anterior; GASTROC, gastrocnemius; mdxT, trained mdx animals; mdxNT, untrained mdx animals. *Significant difference between groups (independent t-test or Mann–Whitney U-test, n=21).
Table 2 shows that the activity of superoxide dismutase and total antioxidant capacity were perceptually higher in the trained group compared to the untrained one.
Concentration ratio of antioxidants of dystrophic animals normalized by wild-type
Antioxidant system x collagen fiber deposition correlation
The correlation between antioxidant system values and collagen fiber deposition showed values that are considered weak with no statistical significance. Values of the correlation and r2 are shown in (Fig. 6). Even then, it is possible to observe that the correlation was always negative showing that there is an inverse proportion among these analyzed variables.
Correlation between deposition of collagen fibers and antioxidants after low-intensity training. Analysis of the correlation between collagen fiber deposition and superoxide dismutase (SOD), catalase (CAT), and ferric reducing ability of plasma (FRAP) on tibial anterior and gastrocnemius muscles. The value of r 2 Linear is expressed at the figure. TA, tibial anterior; GASTROC, gastrocnemius.
DISCUSSION
The muscle groups of mdx mice are differently affected by the absence of dystrophin: hindlimb muscles show more necrosis than diaphragm but little fibrosis after the regeneration process. For this reason, it is recommended to investigate more than one single muscle to understand the effects of an intervention (Hyzewicz et al., 2015a).
Gastrocnemius and tibial anterior are both hindlimb muscles, but they present different fiber type distribution (Grounds et al., 2008; Qaisar et al., 2016) and function on the biomechanics of the gait (Baltgalvis et al., 2012), which impacts on their response to injury induced by exercise. In general, gastrocnemius is affected in horizontal treadmill training as it has more type II fiber (Hyzewicz et al., 2015b) and slow-twitch oxidative (type I) muscle fibers demonstrating a higher antioxidant capacity than fast-twitch (type II) fibers (Gomez-Cabrera et al., 2009). Low-intensity training provoked the same adaptation in the deposition of collagen fibers in the anterior tibial and gastrocnemius muscle of the mdx mice, but presented higher mean values of connective tissue infiltration in the gastrocnemius muscle. Although the studied muscles had a greater amount of type II fibers, the tibial anterior muscle had a better performance of antioxidant defenses than the gastrocnemius muscle which is probably due to its gait function.
According to Chapman et al. (2015) and Smith et al. (2016), the accumulation of collagen fibers on the extracellular matrix results in fibrosis. It is a significant clinical problem as it has an impact on the normal cellular function, strength transmission among muscle fibers and inhibits the process of repair and regeneration, perpetuating the chronic damage due to the absence of dystrophin.
The histopathological analysis of both muscles had their features confirmed by the morphometric analysis of the intramuscular collagen fiber deposition. Low-intensity training decreased intramuscular collagen fiber deposition on the trained dystrophic animals with values getting near to the ones of the control animals.
The fibrosis deposition reflects the final step of an aberrant repair of the dystrophic skeletal muscle (Hardy et al., 2016; Mann et al., 2011), and training protocols that increase the fibrosis deposition are considered deleterious to dystrophic muscles as in the case of Barreto et al. (2012) who employed the high intensity training protocol of 30 min/day, every day for 4 weeks at a speed of 12 m/min.
Hyzewicz et al. (2015a) stated that the formation of fibrosis occurs after the tenth week of age of the mdx mice. The low intensity protocol employed here initiated when the animals were eleven weeks old which seems that the training reduced the fibrosis deposition, positively repairing the extracellular matrix as the trained group presented lower collagen fiber deposition when compared to the untrained ones which means that this training intensity and modality had a positive impact on muscle function.
The level of activity is highly related to the physiological features of skeletal muscle. Hourdé et al. (2013) showed that the inactivity promoted by hindlimb immobilization had worsened the muscle strength and increased the susceptibility of contraction-induced injury in the mdx mice. They conclude that it can be improved through activity. This subtle threshold among activity and inactivity is still under investigation in preclinical models (Hyzewicz et al., 2015a) and humans DMD (Gianola et al., 2013).
The intensity of the exercise is an important point that influences the response of ROS. The increase of hydrogen peroxide is a signalization to stimulate the antioxidant enzymes synthesis. Due to the effects of ROS on positive regulation of antioxidant defense, moderate exercise can be seen as an antioxidant, even in muscular dystrophies (Gomez-Cabrera et al., 2009).
Existing publications of exercise and status redox on DMD usually focus on one single marker of the status redox. In order to make an inference about the ROS response on gastrocnemius and tibial anterior muscles of the mdx mice submitted to low-intensity training, we have here analyzed catalase, superoxide dismutase, total antioxidant capacity to reflect the activity of antioxidant defense, thiobarbituric reactive substances (lipid peroxidation) and oxidation of proteins to reflect the concentration of the oxidative damage.
The increased level of MDA, final product of the lipid peroxidation, can be associated with the increased necrosis tissue which, according to Manning and O’Malley (2015), is observed after 12 and 48 hr of voluntary exercise.
To Kozakowska et al. (2015), skeletal muscle cells have a sophisticated antioxidant enzymatic system which makes it extremely flexible to answer to the status redox alterations. Gastrocnemius and tibial anterior muscles showed a similar response of the antioxidant enzyme system (superoxide dismutase, catalase and total antioxidant capacity) to the low intensity training. This increased activity of antioxidant enzymes is expected in response to a training protocol in a health muscle (Espinosa et al., 2016) as it induces a positive regulation of this antioxidant system, but little is known about the answer to the same system on dystrophic muscle.
The superoxide dismutase presents 28.8% higher activity on the tibial anterior muscle of trained animals when compared to untrained ones, but this increase of activity was not statistically significant. This same behavior was observed in a study of Kaczor et al. (2007) that investigated a low intensity training of 8 weeks on mdx mice where superoxide dismutase activity on the gastrocnemius muscle was not modified with training. Superoxide dismutase activity is expected to increase in muscle tissue after exercise while catalase tends to remain unchanged (Moulin and Ferreiro, 2017).
According to Fontana et al. (2015), the low intensity resistance exercise can significantly recover superoxide dismutase levels in mdx muscles suggesting that a specific training protocol can contribute to skeletal muscle repair promoting protection against oxidative stress.
Our muscle tissue collection was made 24 hr after the last training protocol and, according to Kozakowska et al. (2015), the increase of catalase expression is usually late and has a peak of activity on day 2 after injury, which can explain the absence of change in this antioxidant enzyme.
The total antioxidant capacity was higher on the tibial anterior muscle of the trained animals. On the gastrocnemius muscle of trained animals this activity was 35.9% higher (but not significant) than the untrained animals. This increase in antioxidant enzymes was not sufficient in preventing lipidic peroxidation during the first 24 hr after the protocol but their joint action can sustain the attenuation of intramuscular collagen fibers deposition on trained animals after 8 weeks of training.
A transitory oxidative stress on injured muscle cells is considered necessary to activate multiple signal transduction pathways relevant to complete muscle restoration. Prolonged oxidative stress can unbalance long-term intracellular antioxidant homeostasis of muscle cells (Barbieri and Sestili, 2012). Inflammatory process is intrinsically related to oxidative stress which is modified by exercise and seems to ameliorate status redox (Kostek and Gordon, 2018). Sies (2015) report it is still necessary to add new know on the relation of oxidative stress and inflammatory responses.
The trained mdx animals had a decreased intramuscular collagen fibers deposition influenced by low intensity training, and muscular damage seems to have been lessened by the antioxidants that presented an increase in their activity. Treadmill low intensity training is beneficial to the hindlimb dystrophic muscle as it improved the status redox through the increased activity of antioxidant defense and reduction of collagen fibers deposition of the mdx model.
Notes
CONFLICT OF INTEREST
No potential conflict of interest relevant to this article was reported.
ACKNOWLEDGMENTS
The authors thank to FAPEMIG (Minas Gerais State Agency for Research and Development) by the financial support of the process number APQ-01971-12.