ABSTRACT

Myostatin is a major factor involved in the regulation of skeletal muscle protein mass. High myostatin levels have been associated with an increase in myotube shrinkage. Enhanced myostatin expression is caused by pro-catabolic reactions involving compounds such as tumor necrosis factor (TNF)-α. The present study investigated the effects of agaro-oligosaccharides (AOSs) on hypercatabolism of myotubes exposed to TNF-α. C2C12 myotubes exposed to TNF-α in the presence or absence of AOSs. Myotube exposure to TNF-α resulted in a reduction in the amount of myosin heavy chain (MyHC) protein and a decrease in myotube diameter, which was associated with increased myostatin mRNA expression. AOSs prevented TNF-α-induced MyHC protein loss and restored normal myostatin mRNA levels, with agarobiose and agarotetraose effectively suppressing the hyperexpression of the mRNA. In addition, expression levels of the known myostatin inhibitors, latent transforming growth factor beta binding protein 3 (Ltbp3) and growth and differentiation factor-associated serum protein 1 (Gasp1) mRNAs, decreased more in TNF-α-induced myotubes than in the TNF-α-free control, possibly resulting in myostatin upregulation. However, AOSs restored nearly normal expression levels of Ltbp3 and Gasp1 mRNA, potentially suppressing myostatin expression. These findings suggest that AOSs could prevent myotube shrinkage induced by TNF-α.

Keywords:

Agaro-Oligosaccharides, Myotubes, Myosin Heavy Chain, Myostatin

1. Introduction

Skeletal muscle is the most abundant tissue in the human body and is critical for locomotion and metabolic adaptation. It comprises approximately 40% - 50% of the human body by weight and is mainly maintained by a balance between protein synthesis and degradation. Exercise, nutrients, and exogenous stimuli increase the rate of protein synthesis and increase muscle mass (hypertrophy), whereas starvation, immobilization, aging, and diseases increase the rate of protein degradation and markedly reduce muscle mass (atrophy) [1] . Muscle atrophy is defined as a decrease in the size of tissue or organ due to myotube shrinkage caused by the loss of organelles, cytoplasm, and proteins [2] .

Many recent findings have highlighted a complex scenario whereby an intricate network of signalling pathways regulates the size of myotubes. Four major pathways (IGF1-Akt-FoxO, myostatin, NFκB and glucocorticoids) relate and modulate one another at different levels, coordinating protein synthesis and degradation simultaneously during muscle atrophy [2] . Myostatin, a member of the transforming growth factor-β (TGF-β) superfamily, is a potent negative regulator of skeletal muscle growth. Myostatin overexpression may cause muscle atrophy, whereas its inactivation can induce skeletal muscle hypertrophy [3] . Myostatin inhibits fast myosin heavy chain (MyHC) expression during myogenic differentiation in mouse [4] . Inversely, loss-of-function mutations of the myostatin gene lead to a hypertrophic phenotype in mammals [5] [6] , and similar mutation in the human myostatin gene induces increased muscle mass [7] .

Agar extracted from red seaweed has been used as a food substance in Japan for nearly 400 years. Agarose, the main component of the polysaccharide in agar, is a linear sugar chain consisting of alternating galactose (3-O-linked β-D-galactopyranose) and anhydrogalactose (4-O-linked 3,6-anhydro-α-L-galactopyranose) residues. The α-1,3 linkage of agarose is easily hydrolysed under acidic conditions, yielding agaro-oligosaccharides (AOSs) consisting of repeating agarobiose (Abi) units with galactose at the non-reducing end and anhydrogalactose at the reducing end (Abi, agarotetraose (Ate), agarohexaose (Ahe) and agarooctaose (Aoc); Figure 1). Recent studies have demonstrated the versatile biological activities of AOSs. Enoki et al. reported that AOSs can suppress the production of pro-inflammatory cytokines and the expression of inducible nitric oxide (NO) synthase (iNOS), an enzyme associated with the production of NO [8] . Higashimura et al. demonstrated that AOSs suppress high fat diet-induced dysbiosis, change microbial community function, and prevent colonic tumorigenesis in a mouse model [9] . Therefore, AOSs have potential as highly safe functional ingredients in food, drink, and/or pharmaceuticals.

AOSs exhibit high antioxidant activity [10] , and several antioxidants, such as epigallocatechin-3-gallate [11] , resveratrol [12] , and flavones [13] are known to attenuate shrinkage in C2C12 myotubes. In the present study, we investigated the inhibitory effects of AOSs on protein degradation and gene expressions related to myotube shrinkage induced by tumor necrosis factor (TNF)-α.

2. Materials and Methods

2.1. Materials

Dulbecco’s modified Eagle’s medium (DMEM, High Glucose, with L-Glutamine, Phenol Red and HEPES), penicillin-streptomycin solution (×100), Isogen, and GeneAce SYBR^Ò qPCR Mix α were purchased from Wako Pure Chemical Industries (Osaka, Japan). TNF-α and antibody against hypoxanthine phosphoribosyltransferase 1 (Hprt1) were from Sigma-Aldrich Co. LLC (St. Louis, MO, USA). Fetal bovine serum (FBS) and horse serum (HS) were from Thermo Fisher Scientific Inc. (Waltham, MA, USA). Monoclonal anti-MyHC antibody as a primary antibody, donkey anti-sheep, goat anti-rabbit and goat anti-mouse peroxidase-conjugated IgG as secondary antibodies were from R&D Systems, Inc (Minneapolis, MN, USA). All chemicals used in this study were of the highest analytical grade commercially available.

2.2. Preparation of AOSs Mixture and Isolation of Each AOS

AOSs mixture was prepared, and each AOS (i.e., Abi, Ate, Ahe and Aoc) was isolated as described by Enoki et al. [8] . The composition of Abi, Ate, Ahe and Aoc present in the AOSs mixture was 41.8%, 41.0%, 14.5% and 2.7%, respectively, as measured by high performance liquid chromatography [14] .

2.3. Cell Cultures

C2C12 skeletal myoblasts, a murine skeletal muscle cell line (DS Pharma Biomedical Co., Ltd., Osaka, Japan), were grown in DMEM supplemented with 10% FBS, and maintained at 37˚C in a humidified atmosphere of 5% CO₂ in air. For the experiments, cells were seeded at 35,000 cells/cm² to obtain full confluence 2 d later. Differentiation to myotubes was induced by shifting confluent cultures to DMEM supplemented with 2% HS. The medium was changed every second day, and within 3 d most of the cells had fused to form myotubes. On day 4, the cultures were treated with TNF-α (100 ng/ml), AOSs mixture, or both in combination, and cells were collected after 24 h for mRNA assay or after 48 h for protein assay.

2.4. Cell Proliferation Assay

Cells in 96-well plates were plated at 50% confluence and synchronized in serum-free medium at 37˚C for 24 h. Then, cells were incubated in medium containing 10% FBS, treated with AOSs mixture and incubated for a further 24 h. A CellTiter 96^Ò Aqueous One Solution kit (Promega, Madison, WI, USA) was used to measure cell viabilities. The optical density at 490 nm was determined using a microplate reader (Beckman Coulter, Inc., Brea, CA, USA).

2.5. Preparation of Total RNA and Real-Time Reverse Transcription (RT)-Polymerase Chain Reaction (PCR)

The total RNA from cells was extracted as described previously [15] . Real-time RT-PCR was conducted using a Mx3000P Real-Time PCR System (Agilent Technologies, Santa Clara, CA, USA) and GeneAce SYBR^Ò qPCR Mix α. The primers for amplifying myogenin, myosin light chain 3f (Mlc3f), myostatin, latent transforming growth factor beta binding protein 3 (Ltbp3), growth and differentiation factor-associated serum protein 1 (Gasp1), and Hprt1 were designed using Probe Finder (Roche Diagnostics GmbH, Penzberg, Germany) and the probes were purchased from Hokkaido System Science (Hokkaido, Japan). Sequences of the specific primers are shown in Table 1. The real-time RT-PCR reaction involved 40 cycles at 95˚C for 5 s and 60˚C for 30 s. The relative amount of each mRNA was normalized using Hprt1 expression as an internal control. An expression index was calculated from the normalized relative amount in the absence of TNF-α to the normalized relative amount in the presence of TNF-α. These analyses were carried out in at least triplicate, and representative results are presented.

2.6. Myotube Diameter Measurements

Images of myotubes exposed to TNF-α for 48 h were visualized at ×40 magnification using an inverted light microscope and images were captured with a camera (Olympus, Tokyo, Japan). Using a slight modification of the method described by Williamson et al. [16] , diameters of myotubes were measured from randomly selected six microscope fields from three different wells (35 mm) of control and treated conditions, and 50 myotubes per well (total 150 myotubes)

were measured using ImageJ software (NIH, Frederick, MD, USA).

2.7. Western Blot Analysis

Myotubes were washed three times with ice-cold phosphate-buffered saline buffer (PBS), solubilized in lysis buffer (150 mM NaCl, 0.1% Triton X-100, 0.5% sodium deoxycholate, 0.1% sodium dodecyl sulphate (SDS), 50 mM Tris-HCl (pH 8.0) and protease inhibitors (Sigma-Aldrich)), centrifuged at 15,000 × g for 10 min at 4˚C and the supernatant was collected. Protein concentration was assayed according to Sedmak and Grossberg [17] using bovine serum albumin as the working standard. Equal amounts of protein (10 μg) were heat-denatured in sample-loading buffer (62.5 mM Tris-HCl (pH 6.8), 5% 2-mercaptoethanol, 2% SDS, 0.002% bromophenol blue, 10% glycerol), resolved on a SDS-polyacrylamide gel electrophoresis (PAGE), and transferred for 2 h to nitrocellulose membranes (Bio-Rad, Hercules, CA). The membranes were then blocked with Tris-buffered saline (TBS) containing 0.05% Tween (TBS-T) and 5% non-fat dry milk. The membranes were incubated overnight with a monoclonal anti-MyHC antibody (1:20,000) or a polyclonal anti-Hprt1 antibody (1:2500) in TBS-T at 4˚C, then incubated with HRP-conjugated secondary antibody (1:20,000 for MyHC and 1:2000 for Hprt1) in TBS-T at 25˚C for 1 h. The membrane-bound immune complexes were detected by chemiluminescence using an Immuno Star LD (Wako Pure Chemical Industries) on photon-sensitive film (BioMax Light-1 film; Carestream Health, Inc., Rochester, NY, USA). Bands were quantified by densitometric analysis with ImageJ software.

2.8. Statistical Analysis

Data are expressed as the mean ± standard error of mean (SEM). Differences were assessed using Student’s t-test. Dunnett’s multiple comparison test as post-hoc test after one-way analysis of variance. Details of each statistical analysis used are provided in the figure legends. Differences were considered significant when P-values were less than 0.05.

3. Results

3.1. Effects of AOSs on Cell Number and Differentiation

Figure 2(A) shows the effects of AOSs on cell number and viability quantified by visually counting cells and by a cell proliferation assay, respectively. Neither the cell number nor the titer of cells treated with AOSs mixture (at 0.625, 2.5 and 10 µg/ml) was significantly different from the control. Figure 2(B) shows the expression levels of myogenic markers [18] , i.e., myogenin and Mlc3f mRNA. The expression levels of both mRNAs were not significantly different compared to the control.

3.2. Effect of AOSs on Diameters of TNF-α-Exposed Myotubes

Figure 3(A) shows the effects of AOSs on the diameters of myotubes exposed to

TNF-α. The diameters of myotubes exposed to TNF-α (TNF-α-added control) were significantly decreased compared to the TNF-α-free control. However, the diameters of myotubes exposed to TNF-α and treated with AOSs mixture (at 2.5 and 10 µg/ml) were significantly (P = 0.0328 at 2.5 µg/ml and P = 0.0113 at 10 µg/ml) increased compared to that of the TNF-α-added control. Figure 3(B) shows microscopic images of the myotubes subjected to each treatment (TNF-α-free control, left; TNF-α-added control, center; AOSs mixture-treated (at 10 µg/ml), right).

3.3. Effect of AOSs on MyHC Protein Levels in TNF-α-Exposed Myotubes

Figure 4 shows the effects of AOSs on the amount of MyHC protein in myotubes exposed to TNF-α. The amount of MyHC protein in myotubes exposed to TNF-α (TNF-α-added control) was significantly decreased compared to the TNF-α-free control. However, the amount of MyHC protein in myotubes exposed to TNF-α and treated with AOSs mixture (at 0.625, 2.5 and 10 µg/ml) increased significantly in a dose-dependent manner compared to that of the TNF-α-added control.

3.4. Effect of AOSs on mRNA Expression in TNF-α-Exposed Myotubes

Figure 5 shows the effects of AOSs on myostatin, Ltbp3 and Gasp1 mRNA expression levels following the exposure of myotubes to TNF-α. The level of myostatin mRNA expression in myotubes exposed to TNF-α (TNF-α-added control) was significantly greater than that of the TNF-α-free control. However, the level of myostatin mRNA expression in myotubes exposed to TNF-α and treated with AOSs mixture (at 0.625, 2.5 and 10 µg/ml) was significantly lower than that of the TNF-α-added control and decreased in a dose-dependent manner. In contrast, the level of Ltbp3 and Gasp1 mRNA expression in the

TNF-α-added control was significantly lower than that of the TNF-α-free control. However, the mRNA expressions of both Ltbp3 and Gasp1 in myotubes exposed to TNF-α and treated with AOSs mixture (at 2.5 and 10 µg/ml for Ltbp3, and 10 µg/ml for Gasp1) were significantly greater than that of the TNF-α-added control.

3.5. Effect of Each AOS on Myostatin mRNA Expression in TNF-α-Exposed Myotubes

Figure 6 shows the effects of each AOS (i.e., Abi, Ate, Ahe and Aoc) on the myostatin mRNA expression level in myotubes exposed to TNF-α. Abi and Ate (both at 10 µM) significantly reduced the level of myostatin mRNA expression, and Ahe had a slightly lesser effect, compared to the TNF-α-added control. Aoc had no effect.

4. Discussions

This study reports that AOSs derived from agar had inhibitory effects toward myotube shrinkage, and these effects were associated with a down-regulation of myostatin expression.

We first examined whether AOSs had any cytotoxic or proliferative effects on the cells, even though AOSs (at 1 mg/ml) were reported to exhibit no cytotoxic effects on mammalian cells [19] . In the present study, neither the number nor the titer of cells treated with AOSs mixture (at 0.625, 2.5 and 10 µg/ml) was significantly different from the AOSs mixture-free control (Figure 2(A)). In addition, we investigated whether AOSs had any effect on the differentiation of the

cells. The expression levels of myogenic marker mRNAs, i.e., myogenin and Mlc3f mRNAs, were not significantly different compared to that of the AOSs mixture-free control (Figure 2(B)). Zammit et al. reported that myogenin and Mlc3f mRNAs are markers of myotube composition [18] . Our results indicate that AOSs may have little effect on the cell viability and differentiation.

We next examined whether AOSs prevented a TNF-α-induced decrease in myotube size and increase in myotube protein degradation. Exposure of myotubes to TNF-α reduced the diameters by 20% - 25% (Figure 3) and stimulated MyHC protein degradation by approximately 20% (Figure 4). Importantly, both the TNF-α-induced increase in myotube shrinkage and MyHC protein degradation were prevented by AOSs mixture. These results suggest that AOSs influence the increase in MyHC protein amount in the myotubes exposed to TNF-α, thereby preventing myotube shrinkage. Moreover, the level of MyHC protein in the myotubes exposed to TNF-α and treated with AOSs mixture (at 10 µg/ml) was significantly increased compared to that of the TNF-α-free control (Figure 4, P = 0.00074). This result indicates that AOSs might affect the accumulation of MyHC.

It is known that cytokines are involved in the onset of myotube protein degradation [20] , but little is known about the specific targets of these mediators for activating proteolysis. Enhanced expressions of myostatin in TNF-α-exposed myotubes have been reported [21] . In the present study, the level of myostatin mRNA expression in myotubes exposed to TNF-α was significantly greater than that of the TNF-α-free control. However, the level of myostatin mRNA expression in TNF-α-exposed myotubes treated with AOSs mixture was significantly greater than that of the AOSs mixture-free control (Figure 5). These results indicate that the preventative effect of AOSs on MyHC protein degradation may be due to the suppression of myostatin mRNA expression.

Myostatin is known to be regulated by at least four different inhibitors. The mechanism of myostatin inhibition remains elusive, and crosstalk between the different intrinsic inhibitors similarly remains unclear [22] . One inhibitor, Ltbp3, binds directly to myostatin to form an inactive myostatin/LTBP3 complex [23] . Another inhibitor, Gasp1, can also bind to myostatin and may regulate the activation of myostatin through proteolytic cleavage [24] . In the present study, the levels of Ltbp3 and Gasp1 mRNA expression in TNF-α-exposed myotubes were significantly lower than that of the TNF-α-free control (Figure 5), suggesting that the level of myostatin function might be upregulated in TNF-α-exposed myotubes. However, the levels of Ltbp3 and Gasp1 mRNA expression in TNF-α-exposed myotubes treated with AOSs mixture (at 2.5 and 10 µg/ml for Ltbp3, and 10 µg/ml for Gasp1) were significantly greater than that of the TNF-α-added control, indicating that AOSs might suppress myostatin function by upregulating the expressions of the myostatin inhibitors.

AOSs such as Abi, Ate and Ahe have been reported to inhibit nitrite production in lipopolysaccharide-stimulated RAW264.7 murine macrophages, and 3,6-anhydro-L-galactose, the reducing end of these AOSs, may play a crucial role in this inhibition [8] . It was also reported that an accumulation of nitrite may be related to myostatin expression in myotubes [25] . In the present study, Abi and Ate (at 10 µM both) significantly reduced the level of myostatin mRNA expression, and Ahe had a slightly lesser effect, compared to the TNF-α-added control (Figure 6). The concentration of 10 µM of Abi was 3.24 µg/ml, and that of Ate was 6.30 µg/ml. The level of myostatin mRNA expression in myotubes exposed to TNF-α and treated with AOSs mixture (at 0.625, 2.5 and 10 µg/ml) was significantly lower than that of the TNF-α-added control (Figure 4). These results suggested that Abi and Ate in the AOSs were effectively suppressed the expression level of myostatin mRNA, and indicate that the preventive effects of AOSs toward the myotube shrinkage induced by TNF-α might be due to the action of 3,6-anhydro-L-galactose suppressing the accumulation of nitrite in the myotubes.

5. Conclusion

The present study demonstrated the inhibitory effect of AOSs on TNF-α induced C2C12 myotube shrinkage via the regulation of myostatin expression. Consequently, AOSs may be important regulatory oligosaccharides in maintaining myotube mass and tone, and therefore be advantageous for maintaining a healthy status.

Cite this paper

Shirai, I., Sakai, T., Shiba, K., Uzuhashi, Y. and Karasawa, K. (2018) Agaro-Oligosaccharides Prevent Myostatin Hyperexpression and Myosin Heavy Chain Protein Degradation in C2C12 Myotubes Induced by Tumor Necrosis Factor-α. CellBio, 6, 23-34. https://doi.org/10.4236/cellbio.2018.72003

References