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Transcriptional profiling identifies differentially expressed genes in developing turkey skeletal muscle



Skeletal muscle growth and development from embryo to adult consists of a series of carefully regulated changes in gene expression. Understanding these developmental changes in agriculturally important species is essential to the production of high quality meat products. For example, consumer demand for lean, inexpensive meat products has driven the turkey industry to unprecedented production through intensive genetic selection. However, achievements of increased body weight and muscle mass have been countered by an increased incidence of myopathies and meat quality defects. In a previous study, we developed and validated a turkey skeletal muscle-specific microarray as a tool for functional genomics studies. The goals of the current study were to utilize this microarray to elucidate functional pathways of genes responsible for key events in turkey skeletal muscle development and to compare differences in gene expression between two genetic lines of turkeys. To achieve these goals, skeletal muscle samples were collected at three critical stages in muscle development: 18d embryo (hyperplasia), 1d post-hatch (shift from myoblast-mediated growth to satellite cell-modulated growth by hypertrophy), and 16wk (market age) from two genetic lines: a randombred control line (RBC2) maintained without selection pressure, and a line (F) selected from the RBC2 line for increased 16wk body weight. Array hybridizations were performed in two experiments: Experiment 1 directly compared the developmental stages within genetic line, while Experiment 2 directly compared the two lines within each developmental stage.


A total of 3474 genes were differentially expressed (false discovery rate; FDR < 0.001) by overall effect of development, while 16 genes were differentially expressed (FDR < 0.10) by overall effect of genetic line. Ingenuity Pathways Analysis was used to group annotated genes into networks, functions, and canonical pathways. The expression of 28 genes involved in extracellular matrix regulation, cell death/apoptosis, and calcium signaling/muscle function, as well as genes with miscellaneous function was confirmed by qPCR.


The current study identified gene pathways and uncovered novel genes important in turkey muscle growth and development. Future experiments will focus further on several of these candidate genes and the expression and mechanism of action of their protein products.


Hyperplasia and hypertrophy are key processes in myogenesis in the domestic turkey. It is well established that the number of muscle fibers is determined embryonically [1], as myoblasts, originating as somites, migrate to the appropriate site of muscle formation, then proliferate during the process of hyperplasia. These myoblasts then withdraw from the cell cycle, fuse to form multi-nucleated myotubes, and differentiate with commencement of muscle-specific protein expression. After the actual number of muscle fibers is determined during hyperplasia, skeletal muscle stem cells, satellite cells located beneath the basal lamina of the muscle fibers, are activated and fuse with muscle fibers to contribute their nuclei, resulting in a further increase in DNA that directly leads to an increase in protein synthesis. This post-hatch increase in muscle fiber size (hypertrophy) is responsible for the majority of overall muscle mass accretion [2, 3].

All of these events are precisely temporally and spatially regulated by transcription factors, growth factors, and interactions with the extracellular matrix (ECM). The transcription factors Pax3 and Pax7 are responsible early on for determination of cells entering the myogenic program as well as the activation and survival of satellite cells [4, 5]. Myogenic regulatory factors (MRFs), including the four basic helix-loop-helix transcription factors Myf5, myogenin, MRF4, and MyoD, are pivotal in regulating genes involved with commitment of proliferating somatic cells to the myogenic lineage and subsequent differentiation [6]. Myocyte enhancer factors (MEFs) comprise another group of transcription factors that work in conjunction with the MRFs to ensure appropriate expression of muscle-specific proteins during differentiation. Binding sites for MEF2s have been discovered in the promoters of many crucial skeletal muscle structural genes [7]. These groups of transcription factors also regulate each other [6, 7]. Furthermore, the activation, proliferation, and differentiation of satellite cells are regulated by various growth factors, including insulin-like growth factors (IGF), fibroblast growth factor 2 (FGF2), platelet-derived growth factors (PDGF), hepatocyte growth factors, (HGF), epidermal growth factors (EGF), and transforming growth factor-β (TGF-β) [8]. Satellite cell response to the growth factors IGF and FGF2 is different between fast-growing and slow-growing breeds of domestic turkeys [9].

A genetic model has been developed and maintained to study the effects of growth selection in turkeys. This model consists of two lines: a randomly bred control line of turkeys (RBC2), maintained without selection pressure and representing a commercial turkey from 1967 [10], and a unique line genetically derived from the RBC2 birds and selected for over 40 generations solely for 16-wk body weight (F) [11]. The F line turkeys gain body weight faster and yield significantly heavier breast muscles than the RBC2 birds [12]. In addition, satellite cells from F turkeys have higher proliferation and differentiation rates than those from RBC2 turkeys [13]. Growth comparisons between these two lines are not confounded by selection for other characteristics such as disease resistance, reproductive efficiency, or behavioral traits, as are commercial turkeys.

Many gene expression differences between these two lines have been identified in vitro using isolated satellite cells. The MRFs MyoD and myogenin are differentially expressed between F and RBC2 lines in embryonic pectoralis major muscle and cultured satellite cells [14]. In addition, proteoglycans in the extracellular matrix that interact with growth factors important for proliferation and differentiation of satellite cells exhibit differential expression between the two lines [15, 16]. These cell culture studies have been pivotal for understanding how satellite cells contribute to muscle growth.

To build on this work, we developed a microarray approach that enabled the simultaneous analysis of skeletal muscle gene transcripts at specific time points in vivo. Previously, our group created and characterized a skeletal muscle-specific microarray, the Turkey Skeletal Muscle Long Oligonucleotide (TSKMLO) array, with the purpose of screening the skeletal muscle transcriptome for candidate genes critical in growth, proliferation, differentiation, and overall development [17, 18]. Briefly, cDNA libraries were constructed and sequenced using turkey Pectoralis major muscle collected at three stages crucial to development. From these libraries, oligonucleotides representing 5257 putative transcripts as well as oligonucleotides representing unique sequences to control for nonspecific hybridization and template quality were designed and spotted, resulting in the 6K skeletal muscle-specific oligonucleotide microarray. Assessment of this platform using dye-swap experiments, evaluation of control probe signals, and qPCR validation of results established this array as a valid and valuable tool for functional genomics studies. The aims of the current study were to utilize this microarray to elucidate functional pathways of genes responsible for key events in turkey skeletal muscle development and to identify differences in temporal gene expression between two genetic lines.


Animals and Tissue Collection

Animals used in this study were domestic turkeys maintained at the Poultry Research Center at The Ohio Agricultural Research and Development Center located in Wooster, OH under AGACUC protocol #04-AG007. These turkeys were from two genetic lines: RBC2, a randomly bred control line representative of a 1967 commercial turkey [10, 19], and F, a subline genetically selected from the RBC2 line for increased 16wk body weight [11]. The birds were euthanized immediately prior to tissue harvest at one of three developmental stages: 18 d embryo (18de; hyperplasia), 1 d post hatch (1d; shift from myoblast-mediated growth to satellite cell modulated growth by hypertrophy), and 16 wk old birds (16wk; approximate age of commercial slaughter). Pectoralis major muscle was excised [17], snap frozen in liquid nitrogen, and stored at -80°C until shipment on dry ice to Michigan State University (MSU), where samples were stored at -80°C until RNA extraction.

RNA Extraction

Total RNA was isolated from skeletal muscle tissue using TRIReagent (Molecular Research Center, Inc., Cincinnati, OH) as per manufacturer instructions. All samples were treated with DNA-free™ DNase (Ambion, Inc., Austin, TX) to remove any contaminating genomic DNA. Sample integrity was confirmed using an Agilent 2100 Bioanalyzer (Santa Clara, CA) that determined RNA Integrity Number (RIN). All samples used for microarray analysis had an RIN > 8.0.

Microarray Experimental Design

The TSKLMO array was designed and created based on sequences from cDNA libraries constructed at crucial stages in muscle development [18]. Description of this platform can be found on the National Center for Biotechnology Information (NCBI) Gene Expression Omnibus (GEO) database [GEO: GPL9788]. Experiment 1 (Additional File 1, Figure S1a) was designed to directly compare the three developmental stages, 18de vs. 1d or 1d vs. 16wk, for each of the genetic lines. Experiment 2 (Additional File 1, Figure S1b) was designed to directly compare the two genetic lines, F vs. RBC2, at each of the developmental stages. Each Experiment contained 10 arrays per comparison; therefore, Experiment 1 contained 40 arrays, and Experiment 2 contained 30 arrays. Birds were randomly assigned to array, and hybridizations were performed in random order.

RNA Amplification and Microarray Hybridization

Total RNA for microarray analysis was amplified and dye-coupled in preparation for hybridization using the Amino Allyl MessageAmp™ II aRNA Amplification Kit (Ambion, Inc.) per manufacturer instructions. All microarray preparation and hybridization procedures were performed as previously described [17]. Briefly, all microarrays were UV-crosslinked and pre-hybridized prior to hybridization. Fragmented, Cy3-coupled aRNA was mixed with its Cy5-coupled partner, and the mixtures were hybridized to oligonucleotide microarrays for 18 h in a GeneTac Hybridization Station (Genomic Solutions, Ann Arbor, MI). Arrays were then rinsed, dried by centrifugation, and immediately scanned with a GenePix 4000B scanner (Molecular Devices, Sunnyvale, CA). Image analysis was performed using GenePix Pro 6.0 software, and spot intensities were exported as GPR files for statistical analysis. Fluorescence intensity data were not background-corrected in accordance with recent recommendations [20, 21] but were normalized for dye intensity bias using the LOESS procedure of the normalizeWithinArray function of the Bioconductor R software LIMMA [22].

Statistical Analysis

The two sets of experiments were analyzed separately. For the first experiment, in which 1d was directly compared against the other two stages within arrays and within lines, all microarray data were expressed as log2 ratios of each stage with 1d for each array. These log2 ratios were analyzed using a linear mixed model based on an overall intercept, the effect of dye assignment for samples deriving from stage 1d, effects of the other two stages specified as numerator terms in the log2 ratios, effect of line, and the random effects of the animal assigned to stage 1d and its interaction with the other two stages to serve as the experimental error term for stage as each oligonucleotide was spotted twice on an array. For this experiment, the comparisons of interest included all stages against each other within each of the two lines, as well as overall differences between the three stages.

For the second experiment, in which lines were compared directly against each other within arrays and within stages, all data were expressed as log2 ratios of F over RBC2 for each array. These log2 ratios were analyzed using a linear mixed model based on an overall intercept, the dye assignment for samples deriving from line RBC2, stage effects, the effect of line, and the random effect of the animal derived from the RBC2 line. The random effect could have been also arbitrarily chosen as the animal derived from the F line, but, in either case, this specification ensured that replication was based on the number of animals and not on the number of spots per gene per array. In this experiment, the comparisons of interest were overall line differences and line differences within each stage. SAS PROC MIXED was used for both analyses given the linear mixed model specifications for both experiments [23]. Statistical significance was based on the estimated false discovery rates (FDR) [24].

Raw Cy5 intensities, raw Cy3 intensities, LOESS-normalized log2 Cy5:Cy3 ratios, and LOESS-normalized log2 average intensities (A), as well as original GPR files for all arrays, were submitted to the National Center for Biotechnology Information (NCBI)'s Gene Expression Omnibus (GEO) [GSE19585]. Control probes were also evaluated for both Experiments 1 and 2. Results examining the fluorescence intensities of probes designed to contain an increasing number of mismatched bases as well as scrambled sequence oligos that served as negative controls indicated that hybridization was specific in these experiments. These data have been previously presented [17].

Gene annotation and functional analysis

After statistical analysis, genes were sorted by FDR, and the top 200 genes differentially expressed by overall effect of development (Experiment 1) and all genes differentially expressed by overall effect of genetic line (Experiment 2) were investigated by subjecting oligonucleotide sequences to an NCBI BLAST search and choosing best matches for accession number and putative annotation. In addition, the top 30 up-regulated and down-regulated genes in Experiment 1 and all differentially expressed genes in Experiment 2 in each comparison: F 18de:1d, F 1d:16wk, RBC2 18de:1d, and RBC2 1d:16wk were annotated in the same manner. These lists were then probed for patterns in expression using the Ingenuity Pathways Analysis software (IPA; Redwood City, CA).

Quantitative real-time PCR confirmation

Twenty-eight genes were chosen by function of interest and high differential expression by microarray analysis for confirmation of those results by quantitative real-time PCR (qPCR). Primers (Table 1) were designed using Primer Express 3.0 software (Applied Biosystems, Foster City, CA) and synthesized by Operon Inc. (Huntsville, AL). Sample RNAs (2 μg) were reverse transcribed to cDNA using Superscript III (Invitrogen, Carlsbad, CA) and quantified with a Nanodrop ND-1000 spectrophotometer (Thermo Fisher Scientific, Inc., Wilmington, DE). Reactions were run using 10 ng cDNA, 300 nM primer mix, and POWR SYBR Green Master Mix in a 7700 thermocycler system (Applied Biosystems). Data were analyzed by the 2-ΔΔCt method [25] using hypoxanthine phosphoribosyltransferase (HPRT) as a reference gene and the RBC2, 18de stage as the calibrator; i.e., RBC2, 18de expression is set to "1.0," and all other results are shown as a fold change relative to this control. Statistical analysis was performed using a mixed model and Tukey-Kramer test (SAS, Cary, NC).

Table 1 Primer information for genes selected for confirmation by qPCR.


Differential expression of skeletal muscle genes

In Experiment 1, a total of 3474 genes were differentially expressed between at least two developmental stages across both genetic lines (FDR < 0.001; Table 2). Of these, 2544 genes were significantly affected for the RBC2 birds, whereas 2248 were significantly affected for the F birds (Table 2). A greater number of genes were up-regulated in the earlier developmental stage of direct comparisons (i.e., 18de in the 18de:1d comparison or 1d in the 1d:16wk comparison) as compared to those that were down-regulated, and this observation was more pronounced in the RBC2 line than the F line. The top 30 down- and up-regulated genes in each comparison are listed in Additional File 2, Table S1. A much smaller number of genes were significantly affected by genetic line in Experiment 2 (Table 2). Only 16 genes were differentially expressed by overall effect of line at an FDR < 0.10. When considering the effect of line within each developmental stage rather than overall effect across stages, the highest number of genes (63) were affected at the 18de developmental stage (RBC2:F; 39 up-regulated, 24 down-regulated). At 1d post-hatch, 20 genes were differentially expressed (5 up, 10 down), and at 16wk, 8 genes were differentially expressed (4 up, 4 down). The annotations for these genes are detailed in Additional File 3, Table S2.

Table 2 Breakdown of differentially expressed genes as affected by skeletal muscle development (Experiment 1) and by turkey genetic line (Experiment 2).

Functional and pathway analysis

After differentially expressed oligos on the TSKMLO array were annotated, lists of accession numbers were subjected to IPA analysis, and Networks (which involve regulatory relationships), Functions (which involve biological and disease processes), and Canonical Pathways (which involve well-characterized cell signaling and metabolic pathways) were considered when investigating functional groups of genes differentially expressed in turkey skeletal muscle during development. These results for Experiment 1 are shown separately for the RBC2 line and for the F line (Table 3). Experiment 2 results are shown in Table 4; developmental stages were grouped together because of the small number of differentially expressed genes.

Table 3 Top five Networks, Functions, and Canonical Pathways from IPA analysis for Experiment 1 for RBC2 and F lines.
Table 4 Top Networks, Functions, and Canonical Pathways from IPA analysis for Experiment 2.

qPCR confirmation of differentially expressed genes

Genes in the categories of ECM function, cell death, and skeletal muscle development and function, along with several genes with miscellaneous functions, were selected for qPCR confirmation of microarray results. In addition, genes common to both Experiments 1 and 2 were selected for confirmation.

Figure 1 shows results for versican (1A), glypican-1 (1B), syndecan-4 (1C), spondin 2 (1D), fibroblast growth factor 2 (FGF2; 1E), and collagen VI α1 (COL6A1; 1F), which are all involved in ECM regulation. The COL6A1 gene was also common between Experiments 1 and 2. Versican and glypican-1 appeared to be expressed predominantly at the 18de stage when compared to later stages in development. Interestingly, spondin 2 was expressed almost exclusively at the 1d stage, during muscle hypertrophy. Several differences between the RBC2 and F lines were observed by qPCR analysis that were not detected with the significance threshold used for the microarray analysis. Most notably, FGF2 expression at the 18de stage was twice as high in the RBC2 line compared to that of the F line and nearly 3 times greater at the 1d stage in the RBC2 line compared to that of the F line.

Figure 1

Relative expression as determined by quantitative real-time RT-PCR of genes related to extracellular matrix (ECM) function. Different letters (uppercase) represent differences between developmental stages for the RBC2 line; different letters (lowercase) represent differences between developmental stages for the F line (P ≤ 0.05). * represents differences between the two genetic lines, RBC2 and F (P ≤ 0.05); ^ represents differences between the two lines (0.05 < P < 0.10).

Figure 2 shows results for genes involved in cell death/apoptosis as determined by IPA: caspase-3 (2A), growth arrest-specific 2 (GAS2; 2B), death-associated protein (DAP; 2C), β-parvin (2D), platelet-derived growth factor α (PDGFα; 2E), nestin (2F), matrix γ-carboxyglutamic acid (GLA) protein (MGP; 2G), and gelsolin (2H). The gene β-parvin was also common to both Experiments 1 and 2. Caspase-3, GAS2, DAP, and β-parvin all appeared to be down-regulated as muscle develops. Nestin was highly expressed at the 18de stage with greater than 100 times the expression of subsequent developmental stages. The MGP gene, however, was expressed principally at the 1d stage at 80.28 and 55.38 times the 18de expression in RBC2 and F lines, respectively. Gelsolin expression appeared to increase with muscle maturation and peak at the 16wk time point.

Figure 2

Relative expression as determined by quantitative real-time RT-PCR of genes related to cell death/apoptosis. Different letters (uppercase) represent differences between developmental stages for the RBC2 line; different letters (lowercase) represent differences between developmental stages for the F line (P ≤ 0.05). * represents differences between the two genetic lines, RBC2 and F (P ≤ 0.05); ^ represents differences between the two lines (0.05 < P < 0.10).

Genes important to skeletal muscle growth and development and calcium signaling are shown in Figure 3. These are myostatin (3A), Activin IIB receptor (ActIIBR; 3B), calmodulin (3C), calreticulin (3D), and isotypes of troponin: TNNC1 (3E), TNNI1 (3F), TNNT2 (3G), and TNNT3 (3H). Myostatin expression dipped at 1d posthatch, when hypertrophy occurs in muscle; interestingly, its expression was higher in the RBC2 line at 18de but was higher in the F line by 16wk of development. In conjunction, the myostatin receptor ActIIBR was highly down-regulated at 16wk (18de expression was 18.69 and 10.95 times greater in RBC2 and F lines, respectively), when myostatin expression is high. Relative calmodulin and calreticulin expression tended to respond in opposite directions with calmodulin expression highest at the 16wk stage and calreticulin highest at 18de and decreasing as muscle matures. Of the troponins, TNNI1 and TNNT2 exhibited similar profiles with predominant expression at 18de that decreased substantially at the other stages. Interestingly, TNNT3 expression appeared to be regulated in the opposite direction of TNNT2.

Figure 3

Relative expression as determined by quantitative real-time RT-PCR of genes related to calcium regulation/muscle function. Different letters (uppercase) represent differences between developmental stages for the RBC2 line; different letters (lowercase) represent differences between developmental stages for the F line (P ≤ 0.05). * represents differences between the two genetic lines, RBC2 and F (P ≤ 0.05); ^ represents differences between the two lines (0.05 < P < 0.10).

The expression profiles of several other genes that were common to both Experiments 1 and 2 but did not easily fall into a functional category, along with one gene with unknown function, are shown in Figure 4. These genes included: BTBD11 (4A), cMet (4B), plastin3 (4C), 5'-nucleotidase, cytosolic III (NT5C3; 4D), and nebulin-related anchoring protein (NRAP; 4E). In addition, a gene with no known annotation was chosen from the top 40 genes differentially expressed by overall effect of development (FDR < 1.0 × 10-13) and was subsequently coded Unknown (4F). Expression of these genes was variable although line differences were observed at 1d for all genes. Expression of NRAP was dramatically up-regulated at 1d and 16wk when compared to 18de. Expression profiles for these 28 genes confirmed that microarray results were repeatable.

Figure 4

Relative expression as determined by quantitative real-time RT-PCR of genes common to Experiments 1 and 2 and genes without known functions. Unknown = Q3_Reed_1DPH_cDNA_08_B09_130. Different letters (uppercase) represent differences between developmental stages for the RBC2 line; different letters (lowercase) represent differences between developmental stages for the F line (P ≤ 0.05). * represents differences between the two genetic lines, RBC2 and F (P ≤ 0.05); ^ represents differences between the two lines (0.05 < P < 0.10).


Muscle growth and development from the embryonic to the adult stage of an organism consists of a series of exquisitely regulated and orchestrated changes in expression of genes leading to muscle maturation. Genetic selection for body weight and muscle mass is ultimately based on differential expression of genes, and this approach has resulted in dramatic improvements in turkey growth rate, breast muscle mass, and feed efficiency. However, selection for these performance traits has inadvertently led to other undesirable traits including myopathies [26, 27], cardiomyopathies [28, 29], skeletal deficiencies [11, 30], and meat quality defects such as the pale, soft, and exudative (PSE) condition [31, 32] and associated decreased meat protein functionality [33]. The goals in the current study were to exploit the capability of a microarray approach to identify functional pathways of genes and thus characterize molecular events associated with muscle development and between genetic lines of turkeys with different growth rates.

Obvious phenotypic differences exist between RBC2 birds and those from F or commercial lines. The F line turkeys gain body weight faster and yield significantly heavier breast muscles than the RBC2 birds [12]. In addition, satellite cells from the F line have faster proliferation and differentiation rates than those from the RBC2 line [13]. Further, muscle damage with age is significant between lines as birds from the F line display a greater degree of muscle fiber fragmentation and areas of hypercontraction compared to those of the RBC2 [26]. These phenotypic differences are likely the results of differential gene expression throughout development.

This study identified over 3000 genes affected by developmental stage (Experiment 1), but only 16 genes were identified as being differentially expressed by overall effect of genetic line (Experiment 2). When considering effect of line within each developmental stage, the highest number of differences occurred early in development (18de stage). Expression changes in myogenic regulatory factor genes have previously been observed between the F and RBC2 lines at the embryonic stage [14], and satellite cells from F birds have been shown to have increased proliferation rates relative to RBC2 birds in vitro[13]. These results agree with the microarray observations and suggest that phenotypic differences between the two lines may largely be determined embryonically during myogenesis. It is possible that subtle differences in gene expression observed in the current study may be responsible for large phenotypic differences in body and breast muscle weight [12], breast muscle morphology [26], and meat quality characteristics [33] between the RBC2 and F lines at market age.

The Ingenuity Pathway Analysis (IPA) enabled the clustering of differentially expressed genes into functional categories, some of which were expected, while others were novel. Expected differences provided biological validation of the microarray approach, while the novel differences provided new paths to pursue in furthering our understanding of differences in turkey skeletal muscle growth and development. Many genes that may act as master regulators during development appeared in more than one Network, Function, or Canonical Pathway. The identified gene expression differences were grouped by function and discussed, highlighting several individual genes of interest within each group.

Extracellular Matrix Genes

Previous studies have demonstrated that the ECM comprising the connective tissue surrounding muscle can interact with growth factors, regulate cellular signal transduction pathways, and affect growing and developing muscle fibers [3436]. Genes that fell into numerous functions or canonical pathways as well as some genes that were not included in IPA networks were selected for this group. The ECM is composed mainly of collagens and non-fibrous glycoproteins like proteoglycans. The expression of three proteoglycans: versican, glypican-1, and syndecan-4, was quantified in this study. Membrane-associated proteoglycans in the ECM are known to regulate numerous growth factors, the major constituents that regulate activation, proliferation, and differentiation of satellite cells [8]. A predominant example is FGF2, a potent stimulator of muscle fiber proliferation and a strong inhibitor of differentiation [35, 37]. This function would explain the high FGF2 expression at 18de and 1d in the current study, as these are periods of myoblast or satellite cell proliferation. The interaction between FGF2 and the heparan sulfate proteoglycans glypican-1 and syndecan-4 is required for high-affinity binding of FGF2 to its cellular receptor [35]. Differences in expression of syndecan-4 have been observed in vitro between developing RBC2 and F line satellite cells [15], and RBC2 satellite cell expression of syndecan-4 as well as glypican-1 were altered with the addition of FGF2 [38]. Satellite cells from syndecan-4 knockout mice display defective patterns of activation, proliferation, and differentiation [39], indicating a crucial role in muscle development that is also supported for turkeys in the current study. In addition, syndecan-4 and FGF2 appear to have similar expression profiles, especially at 1d. Versican is a chondroitin sulfate proteoglycan that was expressed predominantly at the 18de stage in this study. Fernandez et al. (1991) hypothesized that this protein's high embryonic expression at the time of fiber formation may be involved in fiber spacing, establishing the morphological structure of the muscle in chicks [40]. The space between muscle fibers may play a critical role in the water-holding capacity of mature muscle and may therefore be associated with quality defects like PSE meat. It is therefore possible that characteristics that contribute to meat quality are decided very early in myogenesis.

Dominant negative mutations in the COL6A1 gene, the only collagen that was investigated in the current study, are known to lead to Bethlem myopathy [41] and Ulrich congenital muscle dystrophy [42]; COL6A1 knockout mice exhibit sarcolemmal disorganization [43]. Taken together, it is clear that expression of genes whose proteins are located in the ECM of skeletal muscle likely contribute significantly to myogenesis in RBC2 and F turkeys.

Cell Death/Apoptosis Genes

Cell death and apoptosis are necessary events in muscle differentiation and maintenance. In addition, other reports have shown similarities between mechanisms of apoptosis and myoblast differentiation, suggesting that similar pathways and effectors may be in use [44, 45]. Therefore, it was logical to further evaluate the expression of several differentially expressed genes associated with these functions. For example, caspase-3, an "executioner" cysteine protease in apoptosis [46], is necessary for proper differentiation of C2C12 myoblasts [47]. However, several reports have shown that this role is separate from apoptosis [44, 45] although it employs similar mechanisms, such as DNA strand breakage [48].

A component of the microfilament, GAS2, is a substrate for caspase-3 and is involved in microfilament reorganization, possibly an early event in apoptosis [49]. The protein is expressed in embryonic mouse limbs and involved in apoptosis during interdigital development; GAS2 may also be involved in myogenesis, possibly in the fusion of myoblasts to form myotubules [50]. In addition, GAS2 can regulate p53 action and apoptosis through its inhibition of calpain [51]. Nestin is the initial intermediate filament protein expressed during myogenesis [5254], and phosphorylation of this protein is associated with the disassembly of intermediate filaments during mitosis [53]. Nestin is also associated with increased survival of rat vascular smooth muscle cells under stress [55]. Our results are in agreement as nestin is expressed predominantly at the 18de stage in turkey skeletal muscle when myoblasts are proliferating.

Another intriguing gene was DAP, which was expressed most highly at the 18de stage and decreased throughout development for both RBC2 and F birds. The human homologue of the gene was first identified in surviving HeLa cells treated with an antisense cDNA library and the cytokine interferon-γ to induce apoptosis [56]. Very little is known about this gene other than it seemed to be a candidate for positive mediators of cell death [56, 57] and that it may regulate autophagy in injured planarians [58] and in amino acid-starved HeLa cells [59]. In addition, DAP may play a role as a regulator of turkey skeletal muscle proliferation and differentiation as shown by our group's recent work with satellite cells in vitro (Vellemen et al., manuscript in preparation).

Ca2+ Signaling/Muscle Function Genes

The Ca2+ ion acts as a second messenger in cell signaling and in skeletal muscle contraction. Aberrant Ca2+ signaling postmortem likely plays an important role in the occurrence of meat quality defects that can lead to significant economic losses in the pork and poultry industries. During the postmortem conversion of muscle to meat, increased Ca2+ release from the sarcoplasmic reticulum while the muscle temperature is still high is thought to be responsible for skeletal muscle hypermetabolism that accelerates pH decline, leading to protein denaturation and loss of protein functionality [60, 61]. A point mutation in the "halothane gene" or ryanodine receptor 1 (RYR1), the skeletal muscle sarcoplasmic reticulum Ca2+ release channel, has been identified in the pig [62] and has been associated with porcine stress syndrome (PSS), a sometimes fatal condition of malignant hyperthermia that is triggered by stress and is a major contributor to the development of PSE pork [60]. Genetic selection by pig breeders away from this mutation has not fully resolved the PSE problem. However, RYR1 became a logical candidate for examination in the turkey, a species that has been similarly selected for rapid lean muscle growth and also exhibits meat quality defects such as PSE. Further investigation of this protein in the turkey revealed a higher affinity for ryanodine in heavier commercial turkeys than those from the RBC2 line [63], suggesting a higher open-state probability of the Ca2+ release channel. Multiple alternatively spliced products were later discovered in the avian skeletal muscle ryanodine receptor isoform, αRYR, in RBC2 and commercial turkeys [64], and these alternative splicing sites are clustered in regions of the gene associated with increased frequency of mutations [65]. Recently, alternative splicing and changes in αRYR expression have also been implicated in the occurrence of PSE meat in broiler chickens [66].

Several genes involved in Ca2+ metabolism were identified as differentially expressed during development in this study. Calreticulin functions as a Ca2+ -binding chaperone and aids in maintaining Ca2+ homeostasis in the ER lumen of cells [67]. This protein also appears to be mainly expressed early in murine cardiac development and is essential for proper cardiac development [68]. Calmodulin is another Ca2+ -binding protein that sensitizes RYR1 to activation at nanomolar concentrations of Ca2+ and inhibits RYR1 at micromolar concentrations [69]. However, more recent work suggests that calmodulin is not an essential regulator of RYR1 [70]. Nevertheless, calmodulin plays a central role in calcium signal transduction and the developmentally related changes in gene expression suggest a key role for this protein.

Myostatin is a highly-conserved transforming growth factor-β (TGF-β) family member that strongly inhibits both hyperplasia and hypertrophy. Mutations or knockout of the gene result in an extreme increase in skeletal muscle mass in cattle and in mice [71]. In the current study, a dramatic decrease of myostatin expression was observed at 1d post-hatch, which agrees with our understanding of myostatin function as myofibers are rapidly undergoing hypertrophy at this stage. In addition, line differences at 18de and 16wk were observed, with RBC2 birds expressing myostatin significantly higher than F birds at 18de. This result could imply that F birds are able to undergo a higher degree of hyperplasia and actually produce more mature muscle fibers, leading to greater muscle mass. At 16wk, F-line birds expressed significantly more myostatin, suggesting that the faster growth rate of the heavier birds plateaus sooner than the slower-growing RBC2-line birds. Activin receptor type IIB (ActIIBR) functions as a serine/threonine kinase receptor for myostatin as well as other TGF- β family members, and binding of these ligands to ActIIBR activates the Smad signal transduction pathway to regulate gene expression [72]. Inhibition of myostatin activity by construction of a dominant-negative ActRIIB lacking a kinase domain resulted in increased muscle hyperplasia and hypertrophy in mice, as well as competition with the TGF-β family member follistatin [71]. Treatment of chicken fetal myoblasts with myostatin altered expression of genes involved in myogenic differentiation, cell architecture, energy metabolism, signal transduction and apoptosis [73], suggesting that increased myostatin expression in the current study could lead to similar changes.

Troponins are key proteins that are regulated by changes in intracellular Ca2+ concentrations and are responsible for striated muscle contraction. The three subunits of troponin interact with each other to bind Ca2+ (TNNC), inhibit myosin ATPase activity (TNNI), and to bind tropomyosin (TNNT) [74]. Transcript abundance of the fast/skeletal muscle isoform of TNNT, TNNT3, increased with development in the current study, peaking at 16wk. Interestingly, the cardiac isoform, TNNT2, was chiefly expressed in the embryonic skeletal muscle, and its expression decreased during skeletal muscle development, which is consistent with previous findings in chicken [75, 76]. Expression of another slow-twitch muscle/cardiac isoform of troponin, TNNI1, followed this pattern as well. The expression of all of the troponin isoforms is also in agreement with what is known about myofibrillar protein expression in rat skeletal muscle, as slow/cardiac forms are expressed during the development of myofibrils with a switch to fast/skeletal forms during postnatal growth and muscle regeneration [77]. These genes involved in muscle growth and Ca2+ signaling may be valuable candidates for changes observed in turkey skeletal muscle development.

Miscellaneous/Genes of Unknown Function

One of the goals of the current study was to identify novel genes with unknown or uncertain functions that may play important roles in skeletal muscle development. These genes may play important roles in myogenesis and development even though their annotations and functions have yet to be defined or may not have clear roles in skeletal muscle. In the current study, one gene without known annotation but identified as very highly differentially expressed by microarray analysis was chosen for further confirmation by qPCR along with others that did not easily fit into a functional category. These genes all showed line differences at 1d, indicating a possible important role during muscle hypertrophy that may help explain phenotypic differences between the slow-growing randombred line and the line selected for increased 16-wk body weight.

Several genes identified in this study were first discovered and their activities characterized in tissue types other than skeletal muscle. For example, spondin 2, (also known as mindin), which fell into the ECM group in our study, is expressed in spleen, lymph nodes, and dendritic cells and may be crucial to immune function [78]. In the current study, spondin 2 was expressed at highest levels at 1d post-hatch, over 11 times higher than its 18de expression in both turkey lines. The MGP gene was first cloned in chickens and found in highest levels in bones and relatively low levels in skeletal muscle [79]. Previous studies indicate its role in the inhibition of vascular calcification, as MGP knockout mice die within 2 months due to blood vessel rupture [80]. It may also be important in intracellular calcium homeostasis [81]. While MGP was grouped into the "Cell Death" function by the IPA software, its association with apoptosis is not clear [81]. It was another gene that appeared to be "turned on" at 1d post-hatch, with 80.28 and 55.38 times the 18de expression in RBC2 and F lines, respectively. Thus, this study has begun to uncover novel roles of these genes, which have been characterized in other tissues, in muscle growth and development.

Other interesting findings include the variation in the timing and extent of expression during development. A few stand-out genes were highly expressed at only one stage of development, clearly turned on or off in what appears to be carefully choreographed regulation. During the embryonic stage, when muscle cell hyperplasia is occurring, versican, glypican-1, betaparvin, nestin, TNNI1, and TNNT2 were expressed at least 5 times, and in the case of nestin greater than 100 times, higher than later developmental stages. Spondin 2 and MGP were both highly expressed at 1d posthatch with very little expression at 18de or 16wk. The NT5C3 and TNNT3 genes peaked at 16wk of development.


Taken together, results from the current study demonstrated obvious differences in gene expression between three key developmental stages of turkey skeletal muscle growth. Although differences between the two genetic lines may be more subtle, the TSKMLO microarray platform proved useful in identifying candidate genes responsible for differences in muscle growth and opened the door for future experiments that focus on these candidate genes, their proteins, and their functions in turkey skeletal muscle.


  1. 1.

    Smith JH: Relation of body size to muscle cell size and number in the chicken. Poult Sci. 1963, 42: 283-290.

    Google Scholar 

  2. 2.

    Velleman SG: Muscle development in the embryo and hatchling. Poult Sci. 2007, 86: 1050-1054.

    CAS  PubMed  Google Scholar 

  3. 3.

    Moss FP: The relationship between the dimensions of the fibres and the number of nuclei during normal growth of skeletal muscle in the domestic fowl. Am J Anat. 1968, 12: 555-564. 10.1002/aja.1001220308.

    Google Scholar 

  4. 4.

    Relaix F, Montarras D, Zaffran S, Gayraud-Morel B, Rocancourt D, Tajbakhsh S, Mansouri A, Cumano A, Buckingham M: Pax3 and Pax7 have distinct and overlapping functions in adult muscle progenitor cells. J Cell Biol. 2006, 172 (1): 91-102. 10.1083/jcb.200508044.

    CAS  PubMed  PubMed Central  Google Scholar 

  5. 5.

    Buckingham M, Relaix F: The role of Pax genes in the development of tissues and organs: Pax3 and Pax7 regulate muscle progenitor cell functions. Annu Rev Cell Dev Biol. 2007, 23: 645-673. 10.1146/annurev.cellbio.23.090506.123438.

    CAS  PubMed  Google Scholar 

  6. 6.

    Ludolph DC, Konieczny SF: Transcription factor families: muscling in on the myogenic program. FASEB J. 1995, 9 (15): 1595-1604.

    CAS  PubMed  Google Scholar 

  7. 7.

    Olson EN, Perry M, Schulz RA: Regulation of muscle differentiation by the MEF2 family of MADS box transcription factors. Dev Biol. 1995, 172 (1): 2-14. 10.1006/dbio.1995.0002.

    CAS  PubMed  Google Scholar 

  8. 8.

    McFarland DC: Influence of growth factors on poultry myogenic satellite cells. Poult Sci. 1999, 78 (5): 747-758.

    CAS  PubMed  Google Scholar 

  9. 9.

    McFarland DC, Pesall JE, Gilkerson KK, Ferrin NH: The response to growth factors of cultured satellite cells derived from turkeys having different growth rates. Cytobios. 1995, 82 (331): 229-238.

    CAS  PubMed  Google Scholar 

  10. 10.

    Nestor KE, McCartney MG, Bachev N: Relative contributions of genetics and environment to turkey improvement. Poult Sci. 1969, 48: 1944-1949.

    CAS  PubMed  Google Scholar 

  11. 11.

    Nestor KE: Genetics of growth and reproduction in the turkey. 9. Long-term selection for increased 16-week body weight. Poult Sci. 1984, 63: 2114-2122.

    CAS  PubMed  Google Scholar 

  12. 12.

    Lilburn MS, Nestor KE: Body weight and carcass development in different lines of turkeys. Poult Sci. 1991, 70: 2223-2231.

    CAS  PubMed  Google Scholar 

  13. 13.

    Velleman SG, Liu X, Nestor KE, McFarland DC: Heterogeneity in growth and differentiation characteristics in male and female satellite cells isolated from turkey lines with different growth rates. Comp Biochem Physiol A Mol Integr Physiol. 2000, 125 (4): 503-509. 10.1016/S1095-6433(00)00178-1.

    CAS  PubMed  Google Scholar 

  14. 14.

    Liu C, McFarland DC, Velleman SG: Effect of genetic selection on MyoD and myogenin expression in turkeys with different growth rates. Poult Sci. 2005, 84 (3): 376-384.

    CAS  PubMed  Google Scholar 

  15. 15.

    Liu C, McFarland DC, Nestor KE, Velleman SG: Differential expression of membrane-associated heparan sulfate proteoglycans in the skeletal muscle of turkeys with different growth rates. Poult Sci. 2006, 85: 422-428.

    CAS  PubMed  Google Scholar 

  16. 16.

    Liu X, McFarland DC, Nestor KE, Velleman SG: Developmental regulated expression of syndecan-1 and glypican in pectoralis major muscle in turkeys with different growth rates. Dev Growth Diff. 2004, 46: 37-51. 10.1111/j.1440-169X.2004.00728.x.

    CAS  Google Scholar 

  17. 17.

    Sporer KR, Chiang W, Tempelman RJ, Ernst CW, Reed KM, Velleman SG, Strasburg GM: Characterization of a 6K oligonucleotide turkey skeletal muscle microarray. Anim Genet. 2011, 42 (1): 75-82. 10.1111/j.1365-2052.2010.02085.x.

    CAS  PubMed  Google Scholar 

  18. 18.

    Reed KM, Mendoza KM, Juneja B, Fahrenkrug SC, Velleman S, Chiang W, Strasburg GM: Characterization of expressed sequence tags from turkey skeletal muscle. Anim Genet. 2008, 39 (6): 635-644. 10.1111/j.1365-2052.2008.01787.x.

    CAS  PubMed  Google Scholar 

  19. 19.

    Nestor KE: The stability of two randombred control populations of turkeys. Poult Sci. 1977, 56: 54-57.

    Google Scholar 

  20. 20.

    Kerr KF, Serikawa KA, Wei C, Peters MA, Bumgarner RE: What is the best reference RNA? And other questions regarding the design and analysis of two-color microarray experiments. OMICS. 2007, 11 (2): 152-165. 10.1089/omi.2007.0012.

    CAS  PubMed  Google Scholar 

  21. 21.

    Allison DB, Cui X, Page GP, Sabripour M: Microarray data analysis: from disarray to consolidation and consensus. Nat Rev Genet. 2006, 7 (1): 55-65. 10.1038/nrg1749.

    CAS  PubMed  Google Scholar 

  22. 22.

    Smyth GK: Linear models and empirical Bayes methods for assessing differential expression in microarray experiments. Stat App Genet Mol Biol. 2004, 3 (1): Article 3.

    Google Scholar 

  23. 23.

    Wolfinger RD, Gibson G, Wolfinger ED, Bennett L, Hamadeh H, Bushel P, Afshari C, Paules RS: Assessing gene significance from cDNA microarray expression data via mixed models. J Comput Biol. 2001, 8 (6): 625-637. 10.1089/106652701753307520.

    CAS  PubMed  Google Scholar 

  24. 24.

    Storey JD, Tibshirani R: Statistical methods for identifying differentially expressed genes in DNA microarrays. Methods Mol Biol. 2003, 224: 149-157.

    CAS  PubMed  Google Scholar 

  25. 25.

    Livak KJ, Schmittgen TD: Analysis of relative gene expression data using real-time quantitative PCR and the 2-δδCt method. Methods. 2001, 25: 402-408. 10.1006/meth.2001.1262.

    CAS  Google Scholar 

  26. 26.

    Velleman SG, Anderson JW, Coy CS, Nestor KE: Effect of selection for growth rate on muscle damage during turkey breast muscle development. Poult Sci. 2003, 82: 1069-1074.

    CAS  PubMed  Google Scholar 

  27. 27.

    Wilson BW, Nieberg PS, Buhr RJ, Kelly BJ, Shultz FT: Turkey muscle growth and focal myopathy. Poult Sci. 1990, 69 (9): 1553-1562.

    CAS  PubMed  Google Scholar 

  28. 28.

    Czarnecki CM: Cardiomyopathy in turkeys. Comp Biochem Phys. 1984, 77A (4): 591-598.

    CAS  Google Scholar 

  29. 29.

    Stenzel T, Tykalowski B, Koncicki A: Cardiovascular system diseases in turkeys. Pol J Vet Sci. 2008, 11 (3): 245-250.

    CAS  PubMed  Google Scholar 

  30. 30.

    Julian RJ: Rapid growth problems: ascites and skeletal deformities in broilers. Poult Sci. 1998, 77: 1773-1780.

    CAS  PubMed  Google Scholar 

  31. 31.

    Owens CM, Hirschler EM, McKee SR, Martinez-Dawson R, Sams AR: The characterization and incidence of pale, soft, exudative turkey meat in a commercial plant. Poult Sci. 2000, 79: 553-558.

    CAS  PubMed  Google Scholar 

  32. 32.

    Dransfield E, Sosnicki AA: Relationship between muscle growth and poultry meat quality. Poult Sci. 1999, 78: 743-746.

    CAS  PubMed  Google Scholar 

  33. 33.

    Updike MS, Zerby HN, Sawdy JC, Lilburn MS, Kaletunc G, Wick MP: Turkey breast meat functionality differences among turkeys selected for body weight and/or breast yield. Meat Sci. 2005, 71: 706-712. 10.1016/j.meatsci.2005.05.014.

    CAS  PubMed  Google Scholar 

  34. 34.

    Jenniskens GJ, Veerkamp JH, van Kuppevelt TH: Heparan sulfates in skeletal muscle development and physiology. J Cell Physiol. 2006, 206 (2): 283-294. 10.1002/jcp.20450.

    CAS  PubMed  Google Scholar 

  35. 35.

    Velleman SG: Role of the extracellular matrix in muscle growth and development. J Anim Sci. 2002, 80 (E Suppl 2): E8-E13.

    Google Scholar 

  36. 36.

    Velleman SG, Liu X, Eggen KH, Nestor KE: Developmental regulation of proteoglycan synthesis and decorin expression during turkey embryonic skeletal muscle formation. Poult Sci. 1999, 78 (11): 1619-1626.

    CAS  PubMed  Google Scholar 

  37. 37.

    Velleman SG: The role of the extracellular matrix in skeletal muscle development. Poult Sci. 1999, 78: 778-784.

    CAS  PubMed  Google Scholar 

  38. 38.

    Velleman SG, Li X, Coy CS, McFarland DC: The effect of fibroblast growth factor 2 on the in vitro expression of syndecan-4 and glypican-1 in turkey satellite cells. Poult Sci. 2008, 87: 1834-1840. 10.3382/ps.2008-00029.

    CAS  PubMed  Google Scholar 

  39. 39.

    Cornelison DD, Wilcox-Adelman SA, Goetinck PF, Rauvala H, Rapraeger AC, Olwin BB: Essential and separable roles for Syndecan-3 and Syndecan-4 in skeletal muscle development and regeneration. Genes Dev. 2004, 18 (18): 2231-2236. 10.1101/gad.1214204.

    CAS  PubMed  PubMed Central  Google Scholar 

  40. 40.

    Fernandez MS, Dennis JE, Drushel RF, Carrino DA, Kimata K, Yamagata M, Caplan AI: The dynamics of compartmentalization of embryonic muscle by extracellular matrix molecules. Dev Biol. 1991, 147 (1): 46-61. 10.1016/S0012-1606(05)80006-5.

    CAS  PubMed  Google Scholar 

  41. 41.

    Jobsis GJ, Boers JM, Barth PG, de Visser M: Bethlem myopathy: a slowly progressive congenital muscular dystrophy with contractures. Brain. 1999, 122 (Pt 4): 649-655. 10.1093/brain/122.4.649.

    PubMed  Google Scholar 

  42. 42.

    Camacho Vanegas O, Bertini E, Zhang RZ, Petrini S, Minosse C, Sabatelli P, Giusti B, Chu ML, Pepe G: Ullrich scleroatonic muscular dystrophy is caused by recessive mutations in collagen type VI. Proc Natl Acad Sci USA. 2001, 98 (13): 7516-7521. 10.1073/pnas.121027598.

    CAS  PubMed  Google Scholar 

  43. 43.

    Canato M, Dal Maschio M, Sbrana F, Raiteri R, Reggiani C, Vassanelli S, Megighian A: Mechanical and electrophysiological properties of the sarcolemma of muscle fibers in two murine models of muscle dystrophy: col6a1-/- and mdx. J Biomed Biotechnol. 2010, 2010: 981945-

    CAS  PubMed  PubMed Central  Google Scholar 

  44. 44.

    Ikeda T, Kanazawa T, Otsuka S, Ichii O, Hashimoto Y, Kon Y: Expression of caspase family and muscle- and apoptosis-specific genes during skeletal myogenesis in mouse embryo. J Vet Med Sci. 2009, 71 (9): 1161-1168. 10.1292/jvms.71.1161.

    CAS  PubMed  Google Scholar 

  45. 45.

    Murray TV, McMahon JM, Howley BA, Stanley A, Ritter T, Mohr A, Zwacka R, Fearnhead HO: A non-apoptotic role for caspase-9 in muscle differentiation. J Cell Sci. 2008, 121 (Pt 22): 3786-3793. 10.1242/jcs.024547.

    CAS  PubMed  Google Scholar 

  46. 46.

    Slee EA, Adrain C, Martin SJ: Executioner caspase-3, -6, and -7 perform distinct, non-redundant roles during the demolition phase of apoptosis. J Biol Chem. 2001, 276 (10): 7320-7326. 10.1074/jbc.M008363200.

    CAS  PubMed  Google Scholar 

  47. 47.

    Fernando P, Kelly JF, Balazsi K, Slack RS, Megeney LA: Caspase 3 activity is required for skeletal muscle differentiation. Proc Natl Acad Sci USA. 2002, 99 (17): 11025-11030. 10.1073/pnas.162172899.

    CAS  PubMed  Google Scholar 

  48. 48.

    Larsen BD, Rampalli S, Burns LE, Brunette S, Dilworth FJ, Megeney LA: Caspase 3/caspase-activated DNase promote cell differentiation by inducing DNA strand breaks. Proc Natl Acad Sci USA. 2010, 107 (9): 4230-4235. 10.1073/pnas.0913089107.

    CAS  PubMed  Google Scholar 

  49. 49.

    Sgorbissa A, Benetti R, Marzinotto S, Schneider C, Brancolini C: Caspase-3 and caspase-7 but not caspase-6 cleave Gas2 in vitro: implications for microfilament reorganization during apoptosis. J Cell Sci. 1999, 112 ((Pt 23)): 4475-4482.

    CAS  PubMed  Google Scholar 

  50. 50.

    Lee KK, Tang MK, Yew DT, Chow PH, Yee SP, Schneider C, Brancolini C: gas2 is a multifunctional gene involved in the regulation of apoptosis and chondrogenesis in the developing mouse limb. Dev Biol. 1999, 207 (1): 14-25. 10.1006/dbio.1998.9086.

    CAS  PubMed  Google Scholar 

  51. 51.

    Benetti R, Del Sal G, Monte M, Paroni G, Brancolini C, Schneider C: The death substrate Gas2 binds m-calpain and increases susceptibility to p53-dependent apoptosis. EMBO J. 2001, 20 (11): 2702-2714. 10.1093/emboj/20.11.2702.

    CAS  PubMed  PubMed Central  Google Scholar 

  52. 52.

    Sejersen T, Lendahl U: Transient expression of the intermediate filmament nestin during skeletal muscle development. J Cell Sci. 1993, 106: 1291-1300.

    CAS  PubMed  Google Scholar 

  53. 53.

    Michalczyk K, Ziman M: Nestin structure and predicted function in cellular cytoskeletal organisation. Histol Histopathol. 2005, 20: 665-671.

    CAS  PubMed  Google Scholar 

  54. 54.

    Kachinsky AM, Dominov JA, Miller JB: Myogenesis and the intermediate filament protein, nestin. Dev Biol. 1994, 165 (1): 216-228. 10.1006/dbio.1994.1248.

    CAS  PubMed  Google Scholar 

  55. 55.

    Huang YL, Wu CM, Shi GY, Wu GC, Lee H, Jiang MJ, Wu HL, Yang HY: Nestin serves as a prosurvival determinant that is linked to the cytoprotective effect of epidermal growth factor in rat vascular smooth muscle cells. J Biochem. 2009, 146 (3): 307-315. 10.1093/jb/mvp070.

    CAS  PubMed  Google Scholar 

  56. 56.

    Deiss LP, Feinstein E, Berissi H, Cohen O, Kimchi A: Identification of a novel serine/threonine kinase and a novel 15-kD protein as potential mediators of the gamma interferon-induced cell death. Genes Dev. 1995, 9 (1): 15-30. 10.1101/gad.9.1.15.

    CAS  PubMed  Google Scholar 

  57. 57.

    Levy-Strumpf N, Kimchi A: Death associated proteins (DAPs): from gene identification to the analysis of their apoptotic and tumor suppressive functions. Oncogene. 1998, 17 (25): 3331-3340. 10.1038/sj.onc.1202588.

    PubMed  Google Scholar 

  58. 58.

    Gonzalez-Estevez C, Felix DA, Aboobaker AA, Salo E: Gtdap-1 promotes autophagy and is required for planarian remodeling during regeneration and starvation. Proc Natl Acad Sci USA. 2007, 104 (33): 13373-13378. 10.1073/pnas.0703588104.

    CAS  PubMed  Google Scholar 

  59. 59.

    Koren I, Reem E, Kimchi A: DAP1, a novel substrate of mTOR, negatively regulates autophagy. Curr Biol. 2010, 20 (12): 1093-1098. 10.1016/j.cub.2010.04.041.

    CAS  PubMed  Google Scholar 

  60. 60.

    Barbut S, Sosnicki AA, Lonergan SM, Knapp T, Ciobanu DC, Gatcliffe LJ, Huff-Lonergan E, Wilson EW: Progress in reducing the pale, soft and exudative (PSE) problem in pork and poultry meat. Meat Science. 2008, 79: 46-63. 10.1016/j.meatsci.2007.07.031.

    CAS  PubMed  Google Scholar 

  61. 61.

    Strasburg GM, Chiang W: Pale, soft, exudative turkey - The role of ryanodine receptor variation in meat quality. Poultry Science. 2009, 88: 1497-1505. 10.3382/ps.2009-00181.

    CAS  PubMed  Google Scholar 

  62. 62.

    Fujii J, Otsu K, Zorzato F, de Leon S, Khanna VK, Weiler JE, O'Brien PJ, MacLennan DH: Identification of a mutation in porcine ryanodine receptor associated with malignant hyperthermia. Science. 1991, 253: 448-451. 10.1126/science.1862346.

    CAS  PubMed  Google Scholar 

  63. 63.

    Wang LJ, Byrem TM, Zarosley J, Booren AM, Strasburg GM: Skeletal muscle calcium channel ryanodine binding activity in genetically unimproved and commercial turkey populations. Poult Sci. 1999, 78: 792-797.

    CAS  PubMed  Google Scholar 

  64. 64.

    Chiang W, Allison CP, Linz JE, Strasburg GM: Identification of two αRYR alleles and characterization of αRYR transcript variants in turkey skeletal muscle. Gene. 2004, 330: 177-184.

    CAS  PubMed  Google Scholar 

  65. 65.

    Chiang W, Yoon HJ, Linz JE, Airey JA, Strasburg GM: Divergent mechanisms in generating molecular variations of αRYR and βRYR in turkey skeletal muscle. J Muscle Res Cell Motil. 2007, 28 (6): 343-354. 10.1007/s10974-008-9130-4.

    CAS  PubMed  Google Scholar 

  66. 66.

    Ziober IL, Paiao FG, Marchi DF, Coutinho LL, Binneck E, Nepomuceno AL, Shimokomaki M: Heat and chemical stress modulate the expression of the alpha-RYR gene in broiler chickens. Genet Mol Res. 2010, 9 (2): 1258-1266.

    CAS  PubMed  Google Scholar 

  67. 67.

    Michalak M, Corbett EF, Mesaeli N, Nakamura K, Opas M: Calreticulin: one protein, one gene, many functions. Biochem J. 1999, 344 (Pt 2): 281-292. 10.1042/0264-6021:3440281.

    CAS  PubMed  PubMed Central  Google Scholar 

  68. 68.

    Mesaeli N, Nakamura K, Zvaritch E, Dickie P, Dziak E, Krause KH, Opas M, MacLennan DH, Michalak M: Calreticulin is essential for cardiac development. J Cell Biol. 1999, 144 (5): 857-868. 10.1083/jcb.144.5.857.

    CAS  PubMed  PubMed Central  Google Scholar 

  69. 69.

    Rodney GG, Williams BY, Strasburg GM, Beckingham K, Hamilton SR: Regulation of RYR1 activity by Ca2+ and calmodulin. Biochem. 2000, 39: 7807-7812. 10.1021/bi0005660.

    CAS  Google Scholar 

  70. 70.

    Rodney GG: Calmodulin in adult mammalian skeletal muscle: localization and effect on sarcoplasmic reticulum Ca2+ release. Am J Physiol Cell Physiol. 2008, 294 (5): C1288-1297. 10.1152/ajpcell.00033.2008.

    CAS  PubMed  PubMed Central  Google Scholar 

  71. 71.

    Lee SJ, McPherron AC: Regulation of myostatin activity and muscle growth. Proc Natl Acad Sci USA. 2001, 98 (16): 9306-9311. 10.1073/pnas.151270098.

    CAS  PubMed  Google Scholar 

  72. 72.

    Tsuchida K, Nakatani M, Uezumi A, Murakami T, Cui X: Signal transduction pathway through activin receptors as a therapeutic target of musculoskeletal diseases and cancer. Endocr J. 2008, 55 (1): 11-21. 10.1507/endocrj.KR-110.

    CAS  PubMed  Google Scholar 

  73. 73.

    Yang W, Zhang Y, Ma G, Zhao X, Chen Y, Zhu D: Identification of gene expression modifications in myostatin-stimulated myoblasts. Biochem Biophys Res Comm. 2005, 326: 660-666. 10.1016/j.bbrc.2004.11.096.

    CAS  PubMed  Google Scholar 

  74. 74.

    Gomes AV, Potter JD, Szczesna-Cordary D: The role of troponins in muscle contraction. IUBMB Life. 2002, 54: 323-333. 10.1080/15216540216037.

    CAS  PubMed  Google Scholar 

  75. 75.

    Toyota N, Shimada Y: Differentiation of troponin in cardiac and skeletal muscles in chicken embryos as studied by immunofluorescence microscopy. J Cell Biol. 1981, 91 (2 Pt 1): 497-504. 10.1083/jcb.91.2.497.

    CAS  PubMed  Google Scholar 

  76. 76.

    Ogasawara Y, Komiya T, Obinata T: Identification of two variants of troponin T in the developing chicken heart using a monoclonal antibody. J Biochem. 1987, 102 (1): 25-30.

    CAS  PubMed  Google Scholar 

  77. 77.

    Schiaffino S, Reggiani C: Molecular diversity of myofibrillar proteins: gene regulation and functional significance. Physiol Rev. 1996, 76 (2): 371-423.

    CAS  PubMed  Google Scholar 

  78. 78.

    Li Y, Cao C, Jia W, Yu L, Mo M, Wang Q, Huang Y, Lim JM, Ishihara M, Wells L, et al: Structure of the F-spondin domain of mindin, an integrin ligand and pattern recognition molecule. EMBO J. 2009, 28 (3): 286-297. 10.1038/emboj.2008.288.

    PubMed  PubMed Central  Google Scholar 

  79. 79.

    Wiedemann M, Trueb B, Belluoccio D: Molecular cloning of avian matrix Gla protein. Biochim Biophys Acta. 1998, 1395 (1): 47-49.

    CAS  PubMed  Google Scholar 

  80. 80.

    Luo G, Ducy P, McKee MD, Pinero GJ, Loyer E, Behringer RR, Karsenty G: Spontaneous calcification of arteries and cartilage in mice lacking matrix GLA protein. Nature. 1997, 386 (6620): 78-81. 10.1038/386078a0.

    CAS  PubMed  Google Scholar 

  81. 81.

    Proudfoot D, Shanahan CM: Molecular mechanisms mediating vascular calcification: role of matrix Gla protein. Nephrol. 2006, 11 (5): 455-461. 10.1111/j.1440-1797.2006.00660.x.

    CAS  Google Scholar 

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We would like to gratefully acknowledge the assistance of Ms. Cindy Coy and Mr. Dennis Hartzler (sample collection and maintenance of turkey lines), Dr. Jeff Landgraf (array printing), Ms. Sue Sipkovsky (microarray technical assistance), Ms. Xiaoning Ren (RNA quality checks), and Dr. Hanem Hassan (RNA extraction). This project was supported by National Research Initiative Competitive Grant no. 2005-35604-15628 from the USDA National Institute of Food and Agriculture to G.M.S., C.W.E., K.M.R., S.G.V., and R.J.T.

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Correspondence to Gale M Strasburg.

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KRBS carried out all microarray and qPCR procedures, annotation and pathway analysis, and wrote the manuscript. RJT was involved in experimental design and statistically analyzed all microarray data. CWE, KMR, SGV, and GMS were involved in experimental design and drafting the manuscript. All authors read and approved the final manuscript.

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Sporer, K.R., Tempelman, R.J., Ernst, C.W. et al. Transcriptional profiling identifies differentially expressed genes in developing turkey skeletal muscle. BMC Genomics 12, 143 (2011).

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  • Satellite Cell
  • Ingenuity Pathway Analysis
  • Genetic Line
  • Pectoralis Major Muscle
  • Skeletal Muscle Development