# Profiling of Age-Related Changes in theTibialis Anterior Muscle Proteome of the mdx Mouse Model of Dystrophinopathy

Authors: Steven Carberry; Margit Zweyer; Dieter Swandulla; Kay Ohlendieck
Journal: Journal of Biomedicine and Biotechnology
 (2012)

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## Abstract

X-linked muscular dystrophy is a highly progressive disease of childhood and characterized by primary genetic abnormalities in the dystrophin gene. Senescent mdx specimens were used for a large-scale survey of potential age-related alterations in the dystrophic phenotype, because the established mdx animal model of dystrophinopathy exhibits progressive deterioration of muscle tissue with age. Since the mdxtibialis anterior muscle is a frequently used model system in muscular dystrophy research, we employed this particular muscle to determine global changes in the dystrophic skeletal muscle proteome. The comparison of mdx mice aged 8 weeks versus 22 months by mass-spectrometry-based proteomics revealed altered expression levels in 8 distinct protein species. Increased levels were shown for carbonic anhydrase, aldolase, and electron transferring flavoprotein, while the expressions of pyruvate kinase, myosin, tropomyosin, and the small heat shock protein Hsp27 were found to be reduced in aged muscle. Immunoblotting confirmed age-dependent changes in the density of key muscle proteins in mdx muscle. Thus, segmental necrosis in mdx tibialis anterior muscle appears to trigger age-related protein perturbations due to dystrophin deficiency. The identification of novel indicators of progressive muscular dystrophy might be useful for the establishment of a muscle subtype-specific biomarker signature of dystrophinopathy.


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## Body

## 1. Introduction

Voluntary muscle fibres are one of the most abundant cellular units in the body. Skeletal muscle tissues are responsible for the provision of postural control, the coordination of excitation-contraction-relaxation cycles for voluntary movements, the integration of key metabolic and biochemical pathways, and the regulation of heat homeostasis. Under normal physiological conditions, these highly complex cellular tasks require a large and diverse number of protein interactions. Hence, supramolecular protein complexes with specialized functions, structures, and connections represent a major biochemical feature of muscle fibres. An excellent example of a large protein assembly present in skeletal muscle is the dystrophin-glycoprotein complex of the sarcolemma [1–5]. The crucial importance of the dystrophin-associated protein complex is exemplified by the pathophysiological fact that primary genetic abnormalities in the dystrophin gene result in progressive muscle wasting diseases, such as Duchenne or Becker muscular dystrophy [6–8]. In normal muscle, the dystrophin-glycoprotein complex provides a trans-sarcolemmal linkage between the actin membrane cytoskeleton and the extracellular matrix component laminin [2]. The subsarcolemmal dystrophin matrix and the molecular connection between the basal lamina structure and the muscle interior is believed to prevent damage to the muscle surface from potential membrane-distorting forces during contraction-relaxation cycles [5].In X-linked muscular dystrophy, dystrophin deficiency results in a drastic reduction of sarcolemmal glycoproteins that triggers a loss of plasmalemmal integrity [9]. Dystrophic muscle fibres are more susceptible to contraction-induced injury [10] and their lateral transmission of force is impaired [11]. Cycles of sarcolemmal microrupturing and natural membrane repair mechanisms appear to cause the introduction of Ca2+-leak channels [12] that in turn elevate cytosolic Ca2+-levels [13] and disturb Ca2+-fluxes through the sarcoplasmic reticulum in dystrophic fibres [14–16]. Interestingly, a recent study on the therapeutic effect of upregulating the intramuscular heat shock protein Hsp72 to ameliorate the dystrophic phenotype revealed that the SERCA-type Ca2+-ATPase is dysfunctional in severely dystrophic muscle [17]. These findings strongly indicate that impaired Ca2+-homeostasis plays a key role in X-linked muscular dystrophy. However, it is not well understood how many molecular and cellular factors are involved in the overall process leading to the highly complex pathology of dystrophinopathy. Thus, in order to determine the hierarchy of secondary pathobiochemical effects that render a dystrophic muscle more susceptible to necrosis, it is crucial to elucidate global alterations due to the disintegration of the dystrophin-glycoprotein complex [18]. Mass-spectrometry-based proteomics suggests itself as a suitable analytical tool for such large-scale and high-throughput approaches to study the effects of dystrophin deficiency.In contrast to hypothesis-based and targeted bioresearch, proteomics can be considered an unbiased and technology-driven approach for the comprehensive cataloging of entire protein complements [19–21]. Skeletal muscle proteomics in particular is concerned with the global identification and detailed cataloguing of the protein constituents of voluntary contractile fibres in health and disease [22–24]. In the long term, comparative proteomics promises to be instrumental for the establishment of comprehensive biomarker signatures of myogenesis, muscle repair mechanisms, physiological adaptations and pathological changes [25], as well as the natural aging process [26]. Most gel electrophoresis-based proteomic studies use high-resolution two-dimensional gel electrophoresis in combination with advanced mass spectrometric analysis for the unequivocal identification of muscle proteins of interest [27–29]. In the case of X-linked muscular dystrophy, a variety of mass spectrometric investigations have attempted to determine proteome-wide changes in dystrophin-deficient muscle tissue in order to establish a dystrophy-specific biomarker signature [30, 31].Large-scale proteomic profiling studies have included investigations of serum [32, 33], cardiac muscle [34, 35], and various skeletal muscle tissues [16, 36–43] from the mdx mouse model of Duchenne muscular dystrophy, as well as a proteomic analysis of dystrophic GRMD dog skeletal muscle [44]. Although the findings from individual studies do not agree on the exact number and extent of protein alterations within the dystrophic muscle proteome, all investigations concur that dystrophin-deficient fibres exhibit a generally perturbed protein expression pattern [30]. Previous gel electrophoresis-based proteomic profiling studies of dystrophic samples have focused on the cytosolic fraction from 1, 3, and 6 months old hind limb muscle covering a pI range of 4–7 and using Coomassie and silver-staining methods [36, 37], crude extracts from gastrocnemius muscle from 9 weeks old hind limb tissue covering a pI range of 3–10 and using Stains-All labeling [16], preparations from 6 weeks old gastrocnemius muscle covering a pI range of 3–10 and using fluorescence 2D-DIGE labeling [38], crude extracts from 9 weeks old diaphragm tissue covering a pI range of 3–10 and using hot Coomassie staining [39], crude extracts from 9 weeks old diaphragm muscle covering a pI range of 3–10 and using fluorescence 2D-DIGE labeling [40], crude extracts from 10 weeks old antisense oligomer-treated diaphragm tissue covering a pIrange of 3–10 and using 2D-DIGE labeling [41], crude extracts from 9 weeks old extraocular muscle covering a pI range of 3–10 and using fluorescence 2D-DIGE labeling [42], and crude extracts from aged diaphragm muscle covering a pIrange of 3–10 and using fluorescence RuBPs labeling [43].In analogy to the above-outlined proteomic studies, this report has focused on aged tibialis anterior muscle from dystrophic mdx mice. The tibialis anterior is one of the most active lower leg muscles [45], which exhibits a relatively high degree of resistance to fatigue during periods of intense running [46], making it an interesting contractile system to study with respect to secondary effects of dystrophinopathy. In addition, previous experimental gene therapy studies have focused on mdx tibialis anterior muscle [47]. Labeling of proteins with fluorescent dyes has been extensively applied in proteomic investigations [48] and we have used here fluorescent RuBPs staining [49] for a comparative proteomic survey of dystrophic leg muscle from 8 weeks, 12 months, and 22 months old mdx mice. The densitometric analysis of two-dimensional gels, covering a pI range of 3–10, in combination with mass spectrometry identified significant age-related changes in carbonic anhydrase, aldolase, electron transferring flavoprotein, pyruvate kinase, myosin, tropomyosin, and the small heat shock protein Hsp27 in dystrophic mdx tibialis anterior muscle.


## 2. Materials and Methods

### 2.1. Materials

Materials and electrophoresis-grade chemicals for the proteomic analysis of muscle proteins were purchased from Amersham Biosciences/GE Healthcare, Little Chalfont, Buckinghamshire, UK. For protein digestion, sequencing grade-modified trypsin was obtained from Promega (Madison, WI, USA). Chemiluminescence substrate and protease inhibitors were from Roche Diagnostics (Mannheim, Germany). Primary antibodies were obtained from Vision Biosystems Novocastra, Newcastle upon Tyne, UK (mAb NCL-b-DG to the dystrophin-associated glycoproteinβ-dystroglycan) and Abcam, Cambridge, UK (ab54913 to the CA3 isoform of carbonic anhydrase; and ab12351 to the small heat shock protein Hsp27). Secondary antibodies were purchased from Chemicon International (Temecula, CA). All other chemicals used were of analytical grade and purchased from Sigma Chemical Company, Dorset, UK.


### 2.2. Dystrophic mdx Animal Model

The mdx mouse is an established model system of X-linked muscular dystrophy and widely used in basic research and for the evaluation of novel therapeutic options to treat diseases of progressive skeletal muscle wasting [50]. The mdx mouse is a naturally occurring mutant [51] that is missing the Dp427 protein isoform of the membrane cytoskeletal protein dystrophin due to a point mutation in the dmd gene [52]. In analogy to the etiology of patients suffering from Duchenne muscular dystrophy [9], deficiency in full-length dystrophin results in a drastic reduction of all dystrophin-associated glycoproteins in mdx skeletal muscle [53], making it a suitable animal model for studying secondary pathobiochemical changes due to dystrophin deficiency. Dystrophic tibialis anterior muscle from 8 weeks, 12 months, and 22 months old mdx mice and normal tissues from age-matched C57 mice were obtained from the bioresource unit of the University of Bonn [54]. Mice were kept under standard conditions and all procedures were performed in accordance with German guidelines on the use of animals for scientific experiments. Animals were sacrificed by cervical dislocation and muscle tissues quickly removed and quick-frozen in liquid nitrogen.


### 2.3. Preparation of Skeletal Muscle Extracts from Aged mdx Mice

For the mass spectrometry-based proteomic survey of aged mdx skeletal muscle tissue, tibialis anterior specimens were shipped to Ireland on dry ice and stored at −80°C prior to usage. In order to obtain muscle protein extracts, 4 dystrophic muscle specimens from each age group were pulverized by grinding tissue pieces in liquid nitrogen using a mortar and pestle. Ground muscle powder was solubilized in lysis buffer with the ratio of 100 mg wet weight to 1 mL lysis buffer (7 M urea, 2 M thiourea, 4% CHAPS, 2% IPG buffer pH 3–10, 2% (w/v) DTT). To prevent excess protein degradation, the lysis buffer was supplemented with a freshly prepared protease inhibitor cocktail [35]. Following gentle rocking for 30 minutes, suspensions were centrifuged at 4°C for 20 min at 20,000 ×g and the protein concentration determined [55].


### 2.4. Two-Dimensional Fluorescence Gel Electrophoretic Analysis

For the separation of muscle proteins, standard two-dimensional gel electrophoresis was carried out by previously optimized methodology using first dimension isoelectric focusing with pH 3–10 strips, and second dimension slab gel electrophoresis with 500μg protein per gel [55]. Twelve slab gels were run in parallel at 0.5 W/gel for 60 min and then 15 W/gel until the blue dye front had disappeared from the bottom of the gel. Postelectrophoretic staining for the total protein profile was performed with the fluorescent dye ruthenium II tris bathophenanthroline disulfonate (RuBPs). As described previously by Rabilloud and colleagues [56], a stock solution of RuBPs dye was prepared. Following washing twice for 5 min, gels were stained for 6 hours in 20% (v/v) ethanol containing 200 nM of ruthenium chelate. Gels were re-equilibrated twice for 10 min in distilled water prior to imaging [57]. Fluorescently labelled proteins from aged mdx tibialis anterior muscle were visualised using a Typhoon Trio variable mode imager. Gel analysis was performed with Progenesis 2D analysis software and protein spots with significantly altered expression levels were identified by mass spectrometry.


### 2.5. Mass Spectrometric Identification of Proteins

Protein identification was performed with 2D protein spots from Coomassie-stained pick gels, following counter-staining of RuBPs-labelled analytical gels. Excised protein spots were treated by standardized in-gel tryptic digestion for the generation of representative peptide mixtures. Excision, washing, destaining, and treatment with sequencing-grade trypsin were performed by a previously optimized method [55]. Peptide populations were harvested by removing supernatants from digested gel plugs after centrifugation. Further recovery was achieved by adding 30% acetonitrile/0.2% trifluoroacetic acid to the gel plugs for 10 min at 37°C with gentle agitation. Resulting supernatants were pooled with the initially recovered peptides following trypsin digestion. Samples were dried through vacuum centrifugation and concentrated peptide fractions were then suspended in mass spectrometry-grade distilled water and 0.1% formic acid, spun down through spin filters and added to LC-MS vials for identification by ion trap LC-MS analysis. The mass spectrometric analysis of peptides was carried out with a Model 6340 Ion Trap LC/MS apparatus from Agilent Technologies (Santa Clara, CA, USA). Separation of peptides was performed with a nanoflow Aglient 1200 series system equipped with a Zorbax 300SB C18 analytical reversed phase column using HPLC-Chip technology. Mobile phases used were A: 0.1% formic acid, B: 50% acetonitrile and 0.1% formic acid. Samples were loaded into the enrichment part of the chip at a capillary flow rate set to 4 μL/min with a mix of solvent A and solvent B at a ratio of 19 : 1. Tryptic digests were eluted with a linear gradient of 5% to 70% solvent B over 6 min, 70% to 100% solvent B over 1 min, 100% to 5% over 1 min. A 5 min post-time of solvent A was used to remove any potential carry over. The capillary voltage was set to 2000 V. The flow and temperature of the drying gas were 4L/min and 300°C, respectively. Database searches were carried out with Mascot MS/MS ion search (Matrix Science, London, UK; NCBI database, release 20100212). All searches used “Mus musculus” as taxonomic category and the following parameters: (1) two missed cleavages by trypsin, (2) mass tolerance of precursor ions ±2.5 Da and product ions ±0.7 Da, (3) carboxymethylated cysteins fixed modification, (4) oxidation of methionine as variable modifiaction, (5) percentage coverage was set at over 10%, and (6) at least 2 matched distinct peptides. Mascot scores over 50 are listed in Tables 1 and 2. All pI-values and molecular masses of identified proteins were compared to the relative position of their corresponding 2D spots on analytical slab gels.Table 1
List of unchanged landmark 2D protein spots from normal mouse tibialis anterior muscle.
Spot No.
Protein name
Accession No.
Isoelectric point (pI)
Molecular mass (Da)
Number of peptides
Coverage
Mascot score
(%)
1
Mitochondrial ATP synthase
AAH37127
5.24
56,632
23
64
456
2
Unnamed protein [Mus musculus]
BAC34145
5.75
70,730
12
21
230
3
Pyruvate kinase, isozymes M1/M2
NP_001240812
6.69
58,461
25
51
1149
4
Enolase, beta, isoform 1
NP_031959
6.73
47,337
21
56
450
5
Creatine Kinase, M-type
NP_031736
6.58
43,250
23
47
509
6
Actin, beta
CAA27396
5.78
39,446
12
41
103
7
Tropomyosin, beta chain
NP_033442
4.66
32,931
22
59
395
8
Tropomyosin, beta chain
NP_033442
4.66
32,933
32
15
241
9
Malate dehydrogenase, cytosolic
AAA37423
6.16
36,625
9
36
190
10
Aldolase A, isoform 2
NP_031464
8.31
39,795
24
75
498
11
Glyceraldehyde-3-phosphate dehydrogenase
NP_032110
8.44
36,072
14
57
238
12
Carbonic anhydrase CA3
NP_031632
6.89
29,638
12
43
431
13
Triosephosphate isomerase
AAB48543
5.62
22,720
11
62
248
14
Triosephosphate isomerase
AAB48543
5.62
22,720
11
68
638
15
Troponin TnI, fast skeletal muscle
NP_033431
8.65
21,515
5
20
150
16
Adenylate kinase, isoenzyme 1
NP_067490
5.7
23,330
14
70
184
17
Myosin light chain MLC1/3
NP_067260
4.98
20,697
17
79
426
18
Myosin light chain MLC2
NP_058034
4.82
19,057
15
61
216
19
Myosin light chain MLC2
NP_058034
4.82
19,059
19
81
391
20
Myosin light chain MLC3
AAH59087
4.63
18,968
11
60
222
21
Parvalbumin, alpha
NP_038673
5.02
11,923
12
89
622
22
Myoglobin
NP_038621
7.07
17,116
5
37
98Table 2
List of identified proteins that exhibit a drastic change in abundance during aging of the dystrophic mdx tibialis anterior muscle.
Spot No.
Protein name
Accession No.
Isoelectric point (pI)
Molecular mass (Da)
Number of peptides
Coverage
Mascot
Fold change 8w-22 m
(%)
Score
1
Carbonic anhydrase CA3
NP031632
6.89
29,638
4
26
181
2.9
2
Aldolase A isoform 2
NP031464
8.31
39,795
2
14
85
2.3
3
Electron transferring flavoprotein, beta
EDL22660
8.50
29,177
13
42
190
1.9
4
Carbonic anhydrase CA3
NP031632
6.89
29,638
12
53
182
1.7
5
Pyruvate kinase
NP035229
7.18
58,388
7
18
440
0.7
6
Myosin 3
NP001078847
5.62
224,755
9
5
141
0.7
7
Tropomyosin, beta chain
NP033442
4.66
32,933
3
14
126
0.6
8
Heat shock protein Hsp27
AAA18335
6.45
22,945
2
15
55
0.5


### 2.6. Immunoblot Analysis

One-dimensional immunoblotting was employed to verify key findings from the proteomic profiling of aged mdxtibialis anterior muscle. Gel electrophoretic separation and transfer was carried out with a Mini-Protean II electrophoresis and transfer system from BioRad Laboratories (Hemel-Hempstead, Herts, UK). Muscle proteins were transferred to nitrocellulose for 70 minutes at 100 V and at 4°C. Blocking of membranes was achieved with a milk protein solution (5% (w/v) fat-free milk powder in 0.9% (w/v) NaCl, 50 mM sodium phosphate, pH 7.4) for 1 hour. Incubation with sufficiently diluted primary antibody was carried out overnight with gentle agitation. Nitrocellulose sheets were washed and then incubated for 1 hour with secondary peroxidase-conjugated antibodies, diluted in blocking solution [55]. Immunodecorated bands were visualized using chemiluminescence substrate (Roche Diagnostics, Mannheim, Germany). Densitometric scanning of immunoblots was performed using ImageJ (NIH, USA) software.


## 2.1. Materials

Materials and electrophoresis-grade chemicals for the proteomic analysis of muscle proteins were purchased from Amersham Biosciences/GE Healthcare, Little Chalfont, Buckinghamshire, UK. For protein digestion, sequencing grade-modified trypsin was obtained from Promega (Madison, WI, USA). Chemiluminescence substrate and protease inhibitors were from Roche Diagnostics (Mannheim, Germany). Primary antibodies were obtained from Vision Biosystems Novocastra, Newcastle upon Tyne, UK (mAb NCL-b-DG to the dystrophin-associated glycoproteinβ-dystroglycan) and Abcam, Cambridge, UK (ab54913 to the CA3 isoform of carbonic anhydrase; and ab12351 to the small heat shock protein Hsp27). Secondary antibodies were purchased from Chemicon International (Temecula, CA). All other chemicals used were of analytical grade and purchased from Sigma Chemical Company, Dorset, UK.


## 2.2. Dystrophic mdx Animal Model

The mdx mouse is an established model system of X-linked muscular dystrophy and widely used in basic research and for the evaluation of novel therapeutic options to treat diseases of progressive skeletal muscle wasting [50]. The mdx mouse is a naturally occurring mutant [51] that is missing the Dp427 protein isoform of the membrane cytoskeletal protein dystrophin due to a point mutation in the dmd gene [52]. In analogy to the etiology of patients suffering from Duchenne muscular dystrophy [9], deficiency in full-length dystrophin results in a drastic reduction of all dystrophin-associated glycoproteins in mdx skeletal muscle [53], making it a suitable animal model for studying secondary pathobiochemical changes due to dystrophin deficiency. Dystrophic tibialis anterior muscle from 8 weeks, 12 months, and 22 months old mdx mice and normal tissues from age-matched C57 mice were obtained from the bioresource unit of the University of Bonn [54]. Mice were kept under standard conditions and all procedures were performed in accordance with German guidelines on the use of animals for scientific experiments. Animals were sacrificed by cervical dislocation and muscle tissues quickly removed and quick-frozen in liquid nitrogen.


## 2.3. Preparation of Skeletal Muscle Extracts from Aged mdx Mice

For the mass spectrometry-based proteomic survey of aged mdx skeletal muscle tissue, tibialis anterior specimens were shipped to Ireland on dry ice and stored at −80°C prior to usage. In order to obtain muscle protein extracts, 4 dystrophic muscle specimens from each age group were pulverized by grinding tissue pieces in liquid nitrogen using a mortar and pestle. Ground muscle powder was solubilized in lysis buffer with the ratio of 100 mg wet weight to 1 mL lysis buffer (7 M urea, 2 M thiourea, 4% CHAPS, 2% IPG buffer pH 3–10, 2% (w/v) DTT). To prevent excess protein degradation, the lysis buffer was supplemented with a freshly prepared protease inhibitor cocktail [35]. Following gentle rocking for 30 minutes, suspensions were centrifuged at 4°C for 20 min at 20,000 ×g and the protein concentration determined [55].


## 2.4. Two-Dimensional Fluorescence Gel Electrophoretic Analysis

For the separation of muscle proteins, standard two-dimensional gel electrophoresis was carried out by previously optimized methodology using first dimension isoelectric focusing with pH 3–10 strips, and second dimension slab gel electrophoresis with 500μg protein per gel [55]. Twelve slab gels were run in parallel at 0.5 W/gel for 60 min and then 15 W/gel until the blue dye front had disappeared from the bottom of the gel. Postelectrophoretic staining for the total protein profile was performed with the fluorescent dye ruthenium II tris bathophenanthroline disulfonate (RuBPs). As described previously by Rabilloud and colleagues [56], a stock solution of RuBPs dye was prepared. Following washing twice for 5 min, gels were stained for 6 hours in 20% (v/v) ethanol containing 200 nM of ruthenium chelate. Gels were re-equilibrated twice for 10 min in distilled water prior to imaging [57]. Fluorescently labelled proteins from aged mdx tibialis anterior muscle were visualised using a Typhoon Trio variable mode imager. Gel analysis was performed with Progenesis 2D analysis software and protein spots with significantly altered expression levels were identified by mass spectrometry.


## 2.5. Mass Spectrometric Identification of Proteins

Protein identification was performed with 2D protein spots from Coomassie-stained pick gels, following counter-staining of RuBPs-labelled analytical gels. Excised protein spots were treated by standardized in-gel tryptic digestion for the generation of representative peptide mixtures. Excision, washing, destaining, and treatment with sequencing-grade trypsin were performed by a previously optimized method [55]. Peptide populations were harvested by removing supernatants from digested gel plugs after centrifugation. Further recovery was achieved by adding 30% acetonitrile/0.2% trifluoroacetic acid to the gel plugs for 10 min at 37°C with gentle agitation. Resulting supernatants were pooled with the initially recovered peptides following trypsin digestion. Samples were dried through vacuum centrifugation and concentrated peptide fractions were then suspended in mass spectrometry-grade distilled water and 0.1% formic acid, spun down through spin filters and added to LC-MS vials for identification by ion trap LC-MS analysis. The mass spectrometric analysis of peptides was carried out with a Model 6340 Ion Trap LC/MS apparatus from Agilent Technologies (Santa Clara, CA, USA). Separation of peptides was performed with a nanoflow Aglient 1200 series system equipped with a Zorbax 300SB C18 analytical reversed phase column using HPLC-Chip technology. Mobile phases used were A: 0.1% formic acid, B: 50% acetonitrile and 0.1% formic acid. Samples were loaded into the enrichment part of the chip at a capillary flow rate set to 4 μL/min with a mix of solvent A and solvent B at a ratio of 19 : 1. Tryptic digests were eluted with a linear gradient of 5% to 70% solvent B over 6 min, 70% to 100% solvent B over 1 min, 100% to 5% over 1 min. A 5 min post-time of solvent A was used to remove any potential carry over. The capillary voltage was set to 2000 V. The flow and temperature of the drying gas were 4L/min and 300°C, respectively. Database searches were carried out with Mascot MS/MS ion search (Matrix Science, London, UK; NCBI database, release 20100212). All searches used “Mus musculus” as taxonomic category and the following parameters: (1) two missed cleavages by trypsin, (2) mass tolerance of precursor ions ±2.5 Da and product ions ±0.7 Da, (3) carboxymethylated cysteins fixed modification, (4) oxidation of methionine as variable modifiaction, (5) percentage coverage was set at over 10%, and (6) at least 2 matched distinct peptides. Mascot scores over 50 are listed in Tables 1 and 2. All pI-values and molecular masses of identified proteins were compared to the relative position of their corresponding 2D spots on analytical slab gels.Table 1
List of unchanged landmark 2D protein spots from normal mouse tibialis anterior muscle.
Spot No.
Protein name
Accession No.
Isoelectric point (pI)
Molecular mass (Da)
Number of peptides
Coverage
Mascot score
(%)
1
Mitochondrial ATP synthase
AAH37127
5.24
56,632
23
64
456
2
Unnamed protein [Mus musculus]
BAC34145
5.75
70,730
12
21
230
3
Pyruvate kinase, isozymes M1/M2
NP_001240812
6.69
58,461
25
51
1149
4
Enolase, beta, isoform 1
NP_031959
6.73
47,337
21
56
450
5
Creatine Kinase, M-type
NP_031736
6.58
43,250
23
47
509
6
Actin, beta
CAA27396
5.78
39,446
12
41
103
7
Tropomyosin, beta chain
NP_033442
4.66
32,931
22
59
395
8
Tropomyosin, beta chain
NP_033442
4.66
32,933
32
15
241
9
Malate dehydrogenase, cytosolic
AAA37423
6.16
36,625
9
36
190
10
Aldolase A, isoform 2
NP_031464
8.31
39,795
24
75
498
11
Glyceraldehyde-3-phosphate dehydrogenase
NP_032110
8.44
36,072
14
57
238
12
Carbonic anhydrase CA3
NP_031632
6.89
29,638
12
43
431
13
Triosephosphate isomerase
AAB48543
5.62
22,720
11
62
248
14
Triosephosphate isomerase
AAB48543
5.62
22,720
11
68
638
15
Troponin TnI, fast skeletal muscle
NP_033431
8.65
21,515
5
20
150
16
Adenylate kinase, isoenzyme 1
NP_067490
5.7
23,330
14
70
184
17
Myosin light chain MLC1/3
NP_067260
4.98
20,697
17
79
426
18
Myosin light chain MLC2
NP_058034
4.82
19,057
15
61
216
19
Myosin light chain MLC2
NP_058034
4.82
19,059
19
81
391
20
Myosin light chain MLC3
AAH59087
4.63
18,968
11
60
222
21
Parvalbumin, alpha
NP_038673
5.02
11,923
12
89
622
22
Myoglobin
NP_038621
7.07
17,116
5
37
98Table 2
List of identified proteins that exhibit a drastic change in abundance during aging of the dystrophic mdx tibialis anterior muscle.
Spot No.
Protein name
Accession No.
Isoelectric point (pI)
Molecular mass (Da)
Number of peptides
Coverage
Mascot
Fold change 8w-22 m
(%)
Score
1
Carbonic anhydrase CA3
NP031632
6.89
29,638
4
26
181
2.9
2
Aldolase A isoform 2
NP031464
8.31
39,795
2
14
85
2.3
3
Electron transferring flavoprotein, beta
EDL22660
8.50
29,177
13
42
190
1.9
4
Carbonic anhydrase CA3
NP031632
6.89
29,638
12
53
182
1.7
5
Pyruvate kinase
NP035229
7.18
58,388
7
18
440
0.7
6
Myosin 3
NP001078847
5.62
224,755
9
5
141
0.7
7
Tropomyosin, beta chain
NP033442
4.66
32,933
3
14
126
0.6
8
Heat shock protein Hsp27
AAA18335
6.45
22,945
2
15
55
0.5


## 2.6. Immunoblot Analysis

One-dimensional immunoblotting was employed to verify key findings from the proteomic profiling of aged mdxtibialis anterior muscle. Gel electrophoretic separation and transfer was carried out with a Mini-Protean II electrophoresis and transfer system from BioRad Laboratories (Hemel-Hempstead, Herts, UK). Muscle proteins were transferred to nitrocellulose for 70 minutes at 100 V and at 4°C. Blocking of membranes was achieved with a milk protein solution (5% (w/v) fat-free milk powder in 0.9% (w/v) NaCl, 50 mM sodium phosphate, pH 7.4) for 1 hour. Incubation with sufficiently diluted primary antibody was carried out overnight with gentle agitation. Nitrocellulose sheets were washed and then incubated for 1 hour with secondary peroxidase-conjugated antibodies, diluted in blocking solution [55]. Immunodecorated bands were visualized using chemiluminescence substrate (Roche Diagnostics, Mannheim, Germany). Densitometric scanning of immunoblots was performed using ImageJ (NIH, USA) software.


## 3. Results

### 3.1. Proteomic Profiling ofTibialis Anterior Muscle

Prior to the proteomic analysis of differently aged dystrophic tibialis anterior muscle preparations, the protein complement from extracts of normal muscle samples was gel electrophoretically separated and key proteins identified by mass spectrometry. This procedure established a select number of reliable landmark protein spots of a typical proteomic muscle map for control purposes. Figure1 shows a representative fluorescent RuBPs-labelled gel with the electrophoretically separated protein spot pattern of normal mouse tibialis anterior muscle. Major 2D protein spots were treated by in-gel digestion and the most abundant constituent of this area of the gel identified by mass spectrometry. Table 1 lists the names of identified muscle marker proteins, their international accession number, pI-values, their relative molecular masses, number of matched peptide sequences, percentage sequence coverage, and Mascot scores. Identified proteins ranged in molecular mass from 17.1 kDa (spot 22, myoglobin) to 70.7 kDa (spot 2, unknown protein), and covered a pI-range from pI 4.6 (spot 20, myosin light chain MLC3) to pI 8.7 (spot 15, fast troponin subunit TnI). Spots 1 to 22 represent major muscle-associated protein species with apparent molecular mass to isoelectric point ratios of 57 kDa/pI 5.2, 71 kDa/pI 5.8, 59 kDa/pI 6.7, 47 kDa/pI 6.7, 43 kDa/pI 6.6, 40 kDa/pI 5.8, 33 kDa/pI 4.7, 33 kDa/pI 4.7, 37 kDa/pI 6.2, 40 kDa/pI 8.3, 36 kDa/pI 8.4, 30 kDa/pI 6.9, 23 kDa/pI 5.6, 23 kDa/pI 5.6, 22 kDa/pI 8.7, 23 kDa/pI 5.7, 21 kDa/pI 5.0, 19 kDa/pI 4.8, 19 kDa/pI 4.8, 19 kDa/pI 4.6, 12 kDa/pI 5.0, and 17 kDa/pI 7.1, respectively (Figure 1). Electrospray ionization mass spectrometry identified these marker proteins as isoforms of mitochondrial ATP synthase, pyruvate kinase, enolase, creatine kinase, actin, tropomyosin, malate dehydrogenase, aldolase, glyceraldehyde-3-phosphate dehydrogenase, carbonic anhydrase, triosephosphate isomerase, troponin, adenylate kinase, parvalbumin, myoglobin, and various myosin light chains (Table 1).Figure 1
Two-dimensional gel electrophoretic analysis of normal mousetibialis anterior muscle. Shown is a fluorescent RuBPs-stained gel of total extracts from 8 weeks old tibialis anterior muscle. Major protein spots are marked by circles and are numbered 1 to 22. See Table 1 for the mass spectrometric identification of 2D landmark proteins that do not change during aging of the mdx animal model of Duchenne muscular dystrophy. The pH values of the first dimension gel system and molecular mass standards of the second dimension are indicated on the top and on the left of the panels, respectively.


### 3.2. Proteomic Analysis of DystrophicTibialis Anterior Muscle during Aging

Following the optimization and initial mass spectrometric identification of muscle marker proteins in normal mouse tibialis anterior muscle, fluorescence high-resolution two-dimensional gel electrophoresis was employed to detect potential differences in aging-related protein expression patterns in mdxtibialis anterior muscle. Figure 2 summarizes analytical gels with 4 biological repeats of 8 weeks, 12 months, and 22 months old total mdx muscle extracts. Panels TA MDX 1 to 4, TA MDX 5 to 8 and TA MDX 9 to 12 represent 8 weeks, 12 months, and 22 months old muscle preparations, respectively. Since the overall 2D spot patterns of normal versus dystrophic tibialis anterior muscle were relatively comparable, a detailed denitometric analysis was carried out in order to evaluate potential differences in individual protein species. Densitometric scanning was performed with a Typhoon Trio variable imager and Progenesis 2D analysis software was used to establish differential expression patterns during muscle aging. The detailed proteomic survey of dystrophic tibialis anterior revealed distinct age-related changes in 8 muscle protein species between 8 weeks and 22 months old total mdx muscle preparations.Figure 2
Two-dimensional gel electrophoretic analysis of aging mdxtibialis anterior muscle. Shown are RuBPs-stained gels of total extracts from 8 weeks (TA MDX 1 to 4), 12 months (TA MDX 5 to 8), and 22 months (TA MDX 9 to 12) old tibialis anterior muscle. Fluorescent images are shown for the pH 3–10 range.


### 3.3. Mass Spectrometric Identification of Protein Alterations in Aged mdxTibialis Anterior Muscle

A representative fluorescent 2D master gel of mdx tibialis anterior muscle is shown in Figure3. As compared to a recent study on senescent mdx diaphragm muscle, which showed drastic age-dependent changes in 11 proteins in this severely necrotic tissue [43], the more mildly affected mdx tibialis anterior muscle showed less pronounced proteome-wide changes during the aging process. This finding agrees with the differing pathology of mdx leg muscle versus mdx diaphragm muscle. Skeletal muscle proteins that exhibited significant alterations in expression levels are marked by circles and are numbered 1 to 8 in the 2D gel representing the urea-soluble proteome from mdx tibialis anterior muscle. The mass spectrometric identification of these altered protein species is listed in Table 2. Besides listing the names of identified proteins, their accession number, pI-values, their relative molecular masses, the number of matched peptide sequences, percentage sequence coverage, and MS/MS scores, this table also shows the fold change of individual proteins affected in dystrophin-deficient mdx tibialis anterior muscle during aging. Proteins species with a changed concentration in mdx tibialis anterior muscle ranged in molecular mass from 23 kDa (heat shock protein Hsp27) to 224 kDa (myosin 3) and covered a pI-range from pI 4.7 (tropomyosin) to pI 8.5 (electron transferring flavoprotein). An increased abundance was shown for the CA3 isoform of carbonic anhydrase (spots 1 and 4), the glycolytic enzyme aldolase (spot 2), and electron transferring flavoprotein (spot 3). The key cytosolic enzyme pyruvate kinase (spot 5), myosin 3 (spot 6), tropomyosin (spot 7), and the molecular chaperone Hsp27 (spot 8) were found to be decreased in mdx tissue.Figure 3
Fluorescence gel electrophoretic analysis of aged mdxtibialis anterior muscle. Shown is a representative RuBPs-labelled master gel of crude tissue extracts from mdx tibialis anterior muscle. Protein spots with an age-related change in expression levels are marked by circles and are numbered 1 to 8. See Table 2 for the mass spectrometric identification of individual muscle-associated proteins. The pH values of the first dimension gel system and molecular mass standards of the second dimension are indicated on the top and on the left of the panels, respectively.


### 3.4. Immunoblot Analysis of Novel Proteomic Markers of Muscular Dystrophy

Following the mass spectrometric establishment of age-related changes in the urea-soluble mdxtibialis anterior muscle proteome, immunoblotting was used to investigate the concentration of the two most extensively changed new markers CA3 and Hsp27 in normal versus dystrophic preparations. Antibodies to the dystrophin-associated glycoprotein β-dystroglycan (β-DG), which forms the main trans-sarcolemmal linker between the extracellular matrix and the cortical actin cytoskeleton in the fibre periphery, were employed to verify the dystrophic status of mdx tissue samples during aging. Figure 4(a) illustrates the drastic reduction of β-DG in both 8 weeks and 22 months old mdx tibialis anterior muscle, which is characteristic of dystrophinopathy. Equal loading of lanes was ensured by silver staining of gel electrophoretically separated protein preparations (not shown). Immunoblotting of young versus old muscle samples with antibodies to the CA3 isoform of carbonic anhydrase (Figure 4(b)) and the molecular chaperone Hsp27 (Figure 4(c)) showed an increased abundance of the metabolic enzyme and a decreased concentration of the small heat shock protein in dystrophin-deficient muscle. Thus, both the fibre type-specific protein CA3 and the stress protein Hsp27 represent suitable candidate biomarkers of the dystrophic phenotype.Immunoblot analysis of novel marker proteins in normal versus mdxtibialis anterior muscle during aging. Shown are representative immunoblots with expanded views of antibody-decorated protein bands. Panels (a, b, c) were labeled with antibodies to the dystrophin-associated glycoprotein β-dystroglycan (β-DG), the CA3 isoform of the fibre type-specific enzyme carbonic anhydrase, and the molecular chaperone Hsp27, respectively. Lanes 1 and 2, and lanes 3 and 4, represent 8 weeks versus 22 months old normal wild type versus dystrophic mdx tibialis anterior muscle, respectively. Immuno-decorated protein bands are indicated by arrowheads.
(a)
Marker of dystrophinopathy
(b)
Increased proteomic marker
(c)
Decreased proteomic marker


## 3.1. Proteomic Profiling ofTibialis Anterior Muscle

Prior to the proteomic analysis of differently aged dystrophic tibialis anterior muscle preparations, the protein complement from extracts of normal muscle samples was gel electrophoretically separated and key proteins identified by mass spectrometry. This procedure established a select number of reliable landmark protein spots of a typical proteomic muscle map for control purposes. Figure1 shows a representative fluorescent RuBPs-labelled gel with the electrophoretically separated protein spot pattern of normal mouse tibialis anterior muscle. Major 2D protein spots were treated by in-gel digestion and the most abundant constituent of this area of the gel identified by mass spectrometry. Table 1 lists the names of identified muscle marker proteins, their international accession number, pI-values, their relative molecular masses, number of matched peptide sequences, percentage sequence coverage, and Mascot scores. Identified proteins ranged in molecular mass from 17.1 kDa (spot 22, myoglobin) to 70.7 kDa (spot 2, unknown protein), and covered a pI-range from pI 4.6 (spot 20, myosin light chain MLC3) to pI 8.7 (spot 15, fast troponin subunit TnI). Spots 1 to 22 represent major muscle-associated protein species with apparent molecular mass to isoelectric point ratios of 57 kDa/pI 5.2, 71 kDa/pI 5.8, 59 kDa/pI 6.7, 47 kDa/pI 6.7, 43 kDa/pI 6.6, 40 kDa/pI 5.8, 33 kDa/pI 4.7, 33 kDa/pI 4.7, 37 kDa/pI 6.2, 40 kDa/pI 8.3, 36 kDa/pI 8.4, 30 kDa/pI 6.9, 23 kDa/pI 5.6, 23 kDa/pI 5.6, 22 kDa/pI 8.7, 23 kDa/pI 5.7, 21 kDa/pI 5.0, 19 kDa/pI 4.8, 19 kDa/pI 4.8, 19 kDa/pI 4.6, 12 kDa/pI 5.0, and 17 kDa/pI 7.1, respectively (Figure 1). Electrospray ionization mass spectrometry identified these marker proteins as isoforms of mitochondrial ATP synthase, pyruvate kinase, enolase, creatine kinase, actin, tropomyosin, malate dehydrogenase, aldolase, glyceraldehyde-3-phosphate dehydrogenase, carbonic anhydrase, triosephosphate isomerase, troponin, adenylate kinase, parvalbumin, myoglobin, and various myosin light chains (Table 1).Figure 1
Two-dimensional gel electrophoretic analysis of normal mousetibialis anterior muscle. Shown is a fluorescent RuBPs-stained gel of total extracts from 8 weeks old tibialis anterior muscle. Major protein spots are marked by circles and are numbered 1 to 22. See Table 1 for the mass spectrometric identification of 2D landmark proteins that do not change during aging of the mdx animal model of Duchenne muscular dystrophy. The pH values of the first dimension gel system and molecular mass standards of the second dimension are indicated on the top and on the left of the panels, respectively.


## 3.2. Proteomic Analysis of DystrophicTibialis Anterior Muscle during Aging

Following the optimization and initial mass spectrometric identification of muscle marker proteins in normal mouse tibialis anterior muscle, fluorescence high-resolution two-dimensional gel electrophoresis was employed to detect potential differences in aging-related protein expression patterns in mdxtibialis anterior muscle. Figure 2 summarizes analytical gels with 4 biological repeats of 8 weeks, 12 months, and 22 months old total mdx muscle extracts. Panels TA MDX 1 to 4, TA MDX 5 to 8 and TA MDX 9 to 12 represent 8 weeks, 12 months, and 22 months old muscle preparations, respectively. Since the overall 2D spot patterns of normal versus dystrophic tibialis anterior muscle were relatively comparable, a detailed denitometric analysis was carried out in order to evaluate potential differences in individual protein species. Densitometric scanning was performed with a Typhoon Trio variable imager and Progenesis 2D analysis software was used to establish differential expression patterns during muscle aging. The detailed proteomic survey of dystrophic tibialis anterior revealed distinct age-related changes in 8 muscle protein species between 8 weeks and 22 months old total mdx muscle preparations.Figure 2
Two-dimensional gel electrophoretic analysis of aging mdxtibialis anterior muscle. Shown are RuBPs-stained gels of total extracts from 8 weeks (TA MDX 1 to 4), 12 months (TA MDX 5 to 8), and 22 months (TA MDX 9 to 12) old tibialis anterior muscle. Fluorescent images are shown for the pH 3–10 range.


## 3.3. Mass Spectrometric Identification of Protein Alterations in Aged mdxTibialis Anterior Muscle

A representative fluorescent 2D master gel of mdx tibialis anterior muscle is shown in Figure3. As compared to a recent study on senescent mdx diaphragm muscle, which showed drastic age-dependent changes in 11 proteins in this severely necrotic tissue [43], the more mildly affected mdx tibialis anterior muscle showed less pronounced proteome-wide changes during the aging process. This finding agrees with the differing pathology of mdx leg muscle versus mdx diaphragm muscle. Skeletal muscle proteins that exhibited significant alterations in expression levels are marked by circles and are numbered 1 to 8 in the 2D gel representing the urea-soluble proteome from mdx tibialis anterior muscle. The mass spectrometric identification of these altered protein species is listed in Table 2. Besides listing the names of identified proteins, their accession number, pI-values, their relative molecular masses, the number of matched peptide sequences, percentage sequence coverage, and MS/MS scores, this table also shows the fold change of individual proteins affected in dystrophin-deficient mdx tibialis anterior muscle during aging. Proteins species with a changed concentration in mdx tibialis anterior muscle ranged in molecular mass from 23 kDa (heat shock protein Hsp27) to 224 kDa (myosin 3) and covered a pI-range from pI 4.7 (tropomyosin) to pI 8.5 (electron transferring flavoprotein). An increased abundance was shown for the CA3 isoform of carbonic anhydrase (spots 1 and 4), the glycolytic enzyme aldolase (spot 2), and electron transferring flavoprotein (spot 3). The key cytosolic enzyme pyruvate kinase (spot 5), myosin 3 (spot 6), tropomyosin (spot 7), and the molecular chaperone Hsp27 (spot 8) were found to be decreased in mdx tissue.Figure 3
Fluorescence gel electrophoretic analysis of aged mdxtibialis anterior muscle. Shown is a representative RuBPs-labelled master gel of crude tissue extracts from mdx tibialis anterior muscle. Protein spots with an age-related change in expression levels are marked by circles and are numbered 1 to 8. See Table 2 for the mass spectrometric identification of individual muscle-associated proteins. The pH values of the first dimension gel system and molecular mass standards of the second dimension are indicated on the top and on the left of the panels, respectively.


## 3.4. Immunoblot Analysis of Novel Proteomic Markers of Muscular Dystrophy

Following the mass spectrometric establishment of age-related changes in the urea-soluble mdxtibialis anterior muscle proteome, immunoblotting was used to investigate the concentration of the two most extensively changed new markers CA3 and Hsp27 in normal versus dystrophic preparations. Antibodies to the dystrophin-associated glycoprotein β-dystroglycan (β-DG), which forms the main trans-sarcolemmal linker between the extracellular matrix and the cortical actin cytoskeleton in the fibre periphery, were employed to verify the dystrophic status of mdx tissue samples during aging. Figure 4(a) illustrates the drastic reduction of β-DG in both 8 weeks and 22 months old mdx tibialis anterior muscle, which is characteristic of dystrophinopathy. Equal loading of lanes was ensured by silver staining of gel electrophoretically separated protein preparations (not shown). Immunoblotting of young versus old muscle samples with antibodies to the CA3 isoform of carbonic anhydrase (Figure 4(b)) and the molecular chaperone Hsp27 (Figure 4(c)) showed an increased abundance of the metabolic enzyme and a decreased concentration of the small heat shock protein in dystrophin-deficient muscle. Thus, both the fibre type-specific protein CA3 and the stress protein Hsp27 represent suitable candidate biomarkers of the dystrophic phenotype.Immunoblot analysis of novel marker proteins in normal versus mdxtibialis anterior muscle during aging. Shown are representative immunoblots with expanded views of antibody-decorated protein bands. Panels (a, b, c) were labeled with antibodies to the dystrophin-associated glycoprotein β-dystroglycan (β-DG), the CA3 isoform of the fibre type-specific enzyme carbonic anhydrase, and the molecular chaperone Hsp27, respectively. Lanes 1 and 2, and lanes 3 and 4, represent 8 weeks versus 22 months old normal wild type versus dystrophic mdx tibialis anterior muscle, respectively. Immuno-decorated protein bands are indicated by arrowheads.
(a)
Marker of dystrophinopathy
(b)
Increased proteomic marker
(c)
Decreased proteomic marker


## 4. Discussion

Duchenne muscular dystrophy is one of the most crippling neuromuscular disorders of childhood [58], therefore warranting detailed large-scale studies into the establishment of comprehensive biomarker signatures of dystrophinopathy [30, 31]. In dystrophinopathy, the almost complete absence of the Dp427 isoform of the membrane cytoskeletal protein dystrophin causes a drastic reduction of a large number of surface glycoproteins that in turn triggers a loss of sarcolemmal integrity. The mdx mouse is a widely used model system for the evaluation of novel treatment options to counter-act the symptoms of X-linked muscular dystrophy [59] and basic biomedical research promises to provide the basis of evidence for the development of novel treatment regimes, such as stem cell therapy, myoblast transfer, or exon skipping therapy [60]. Previous proteomic studies have established a considerable number of novel biomarkers of secondary changes in dystrophin-deficient organisms [30]. Besides the cataloging of generally perturbed protein expression patterns, individual proteomic surveys of mdx muscles of differing subtype and age have demonstrated a drastically altered abundance of adenylate kinase isoform AK1 [36], the luminal Ca2+-binding protein calsequestrin of the terminal cisternae [16, 41], the cytosolic Ca2+-buffering element regucalcin [39], mitochondrial isocitrate dehydrogenase [38], and the muscle-specific molecular chaperone cvHsp [40, 41]. A recent aging study of the severely dystrophic mdx diaphragm has demonstrated a drastic increase in the extracellular matrix proteins collagen and dermatopontin, the molecular chaperone αB-crystallin, and the intermediate filament protein vimentin, suggesting increased accumulation of connective tissue, an enhanced cellular stress response and compensatory stabilization of the weakened membrane cytoskeleton in severely dystrophic muscle tissue [43].In the present report, proteomic profiling showed that during the natural aging of the moderately dystrophictibialis anterior muscle a number of key skeletal muscle proteins change in abundance. We have studied aged mdx muscle, because dystrophic mouse muscle tissue progressively deteriorates with age and thus more closely resembles the neuromuscular pathology seen in Duchenne patients [61]. The age-related pathogenesis of mdx muscle is characterized by a drastic loss of myofibres and concomitant replacement by connective tissue [62–64], progressive motor weakness [65], the presence of branched fibres that trigger mechanical weakening of the muscle periphery [66], a reduced life span and increased susceptibility to spontaneous rhabdomyosarcoma [67], a decline in regenerative potential and alterations in the crucial mTOR signaling pathway [68], and impaired functional and structural recovery after injury [54]. Hence, senescent mdx muscle represents a suitable dystrophic phenotype for determining potential global changes in the protein complement during aging. This report has summarized the findings of a comparative proteomic analysis of mildly affected mdx tibialis anterior muscle from 8 weeks versus 22 months old mice. The identification of aldolase, pyruvate kinase, carbonic anhydrase, tropomyosin, myosin, electron transferring flavoprotein and small heat shock protein Hsp27 as new indicators of progressive muscular dystrophy might be useful for the establishment of a more comprehensive biomarker signature of dystrophinopathy.The protein with the highest age-related increase was identified as carbonic anhydrase isoform CA3 [69]. In general, carbonic anhydrases catalyze the reversible hydration of CO2 and are widely distributed throughout the body [70]. Skeletal muscles express several isoforms of this crucial metabolic enzyme in a fibre-type-specific manner. The predominant CA3 isoform is mostly present in the cytosolic fraction of type I and IIa fibers [69]. Interestingly, metabolic adaptations, altered neuromuscular activity patterns, stretch-induced hypertrophy, and disuse atrophy greatly influence the expression of muscle carbonic anhydrases [71–73]. The higher concentration of the CA3 isoform of carbonic anhydrase in aged mdx muscle, as shown here by mass spectrometry-based proteomics, could be an indication of an increased demand for efficient CO2 removal during mdx fibre aging. On the other hand, since the CA3 isoform is predominantly located in slower-twitching fibre populations, its altered density could also be due to age-related fibre-type shifting in the mdx tibialis anterior muscle. This would agree with the findings of a recent proteomic survey of middle aged versus aged vastus lateralis muscle, which revealed increased levels of CA3 in senescent human skeletal muscle [74].The greatest reduction in a muscle-associated protein during aging of the mdxtibialis anterior was shown to be the small heat shock protein Hsp27. This indicates a potentially blunted cellular stress response in dystrophic tibialis anterior fibres and demonstrates that marked differences exist with respect to expression levels of small heat shock proteins in moderately affected hind limb muscles versus severely dystrophic diaphragm muscle in the mdx model of dystrophinopathy [40, 41]. While changes in elements of the contractile apparatus suggest downstream effects of dystrophin deficiency on myosin and tropomyosin organization, altered expression levels in electron transferring flavoprotein and glycolytic enzymes indicate perturbed mdx muscle metabolism. The beta-polypeptide chain of the electron transferring flavoprotein is involved in mitochondrial fatty acid and amino acid catabolism and mediates the shuttling of electrons between flavoprotein dehydrogenases [75]. The enzymes aldolase and pyruvate kinase catalyze the reversible break-down of fructose-1,6-biphosphate into dihydroxyacetone phosphate and glyceraldehyde-3-phosphate and the critical oxidoreduction-phosphorylation step that converts ADP and phosphoenolpyruvate to ATP and pyruvate, respectively [76]. Alterations in glycolytic enzymes and mitochondrial proteins in mdx tibialis anterior muscle indicate altered flux rates through key metabolic pathway. With respect to the glycolytic pathway, the activity of four muscle proteins is central to its regulation on the enzymatic level, i.e. the metabolic flux through hexokinase, phosphofructokinase, glycogen phosphorylase, and pyruvate kinase, whereby metabolic silencing of muscle glycolysis is probably mediated by the inactivation of pyruvate kinase [76]. This central role of pyruvate kinase in muscle metabolism makes its changed abundance in the mdx tibialis anterior muscle a crucial finding. Pyruvate kinase was previously shown to be a suitable biomarker of the general aging process in skeletal muscle tissues [77, 78]. Interestingly, the change of metabolic enzymes in aged mdx tibialis anterior muscle, such as pyruvate kinase and aldolase, agrees with the proteomic analysis of golden retriever muscular dystrophy. In the grmd dog model of dystrophinopathy, targets of the transcriptional control factor of energy metabolism PGC-1α, that is, various glycolytic and oxidative enzymes, were found to be reduced [44].In conclusion, the comparative proteomic survey of dystrophic tibialis anterior muscle from 8 weeks versus 22 months old mdx mice has revealed altered expression levels in a number of critical proteins during skeletal muscle aging. However, the degree of concentration changes was less pronounced in the moderately dystrophic tibialis anterior muscle as compared to the recently analyzed aged mdx diaphragm [43]. These differing proteomic findings agree with the pathophysiological concept that the aged mdx diaphragm muscle is more severely affected as compared to moderately necrotic mdx hind limb muscle. In the long-term, the proteomic identification of new biomarkers of dystrophinopathy might be useful for the establishment of a comprehensive and muscle subtype-specific signature of Duchenne muscular dystrophy. This would be useful for improving diagnostic procedures, monitor disease progression, identify novel therapeutic targets and aid in the evaluation of novel treatments, such as exon-skipping therapy or stem cell therapy.



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*Source: 691641-2012-10-03.xml*