Cloning, Sequencing, and the Expression of the Elusive Sarcomeric TPM4<i>α</i> Isoform in Humans

Dube, Dipak K.; Dube, Syamalima; Abbott, Lynn; Alshiekh-Nasany, Ruham; Mitschow, Charles; Poiesz, Bernard J.

doi:https://doi.org/10.1155/2016/3105478

Molecular Biology International

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Research Article | Open Access

Volume 2016 | Article ID 3105478 | https://doi.org/10.1155/2016/3105478

Cloning, Sequencing, and the Expression of the Elusive Sarcomeric TPM4α Isoform in Humans

Dipak K. Dube,¹Syamalima Dube,¹Lynn Abbott,¹Ruham Alshiekh-Nasany,¹Charles Mitschow,¹and Bernard J. Poiesz¹

Academic Editor: József Szeberényi

Received31 May 2016

Revised22 Jul 2016

Accepted10 Aug 2016

Published15 Sept 2016

Abstract

In mammals, tropomyosin is encoded by four known TPM genes (TPM1, TPM2, TPM3, and TPM4) each of which can generate a number of TPM isoforms via alternative splicing and/or using alternate promoters. In humans, the sarcomeric isoform(s) of each of the TPM genes, except for the TPM4, have been known for a long time. Recently, on the basis of computational analyses of the human genome sequence, the predicted sequence of TPM4α has been posted in GenBank. We designed primer-pairs for RT-PCR and showed the expression of the transcripts of TPM4α and a novel isoform TPM4δ in human heart and skeletal muscle. qRT-PCR shows that the relative expression of TPM4α and TPM4δ is higher in human cardiac muscle. Western blot analyses using CH1 monoclonal antibodies show the absence of the expression of TPM4δ protein (~28 kDa) in human heart muscle. 2D western blot analyses with the same antibody show the expression of at least nine distinct tropomyosin molecules with a mass ~32 kD and above in adult heart. By Mass spectrometry, we determined the amino acid sequences of the extracted proteins from these spots. Spot “G” reveals the putative expression of TPM4α along with TPM1α protein in human adult heart.

1. Introduction

Tropomyosin (TPM) is a coiled-coil dimer protein that plays important role(s) in regulating muscle contraction in conjunction with other sarcomeric proteins like actin, troponins, tropomodulin, and so forth. TPM also provides structural stability to actin filaments, thereby modulating cytoskeleton function. In vertebrates, there are four TPM genes, designated as TPM1, TPM2, TPM3, and TPM4, except for zebrafish where six TPM genes are present [1–10]. Each of the four genes generates a large number of TPM isoforms via alternative splicing and/or using different promoters. In mammals, the exon and intron organization of TPM genes are very similar, if not identical [6]. The rodent TPM4 gene has lost the use of exons 1a and 2; the high molecular weight isoforms encoding 284 amino acid residues such as TPM4α and TPM4β are not expressed as they are in nonmammalian species. It was speculated for a long time that the TPM4 gene in humans as in rodents does not encode sarcomeric isoform with exon 9a/b [2, 3]. The first report on the expression of a high molecular weight TPM4 protein was reported in human ovary tumor tissues in 2004 (accession number AK023385). This isoform, defined as TPM4β, contains exons 1a, 2, 3, 4, 5, 6, 7, 8, and 9d (Figure 1), which differs from the sarcomeric TPM4α isoform containing exon 9a/b instead of 9d. It is to be noted that exon 9a but not 9d encodes the peptide that is essential for binding TPM with troponins [2, 3], essential components of thin filament. Recently, two predicted sequences (derived from a genomic sequence) of the two different isoforms of the human TPM4 gene containing exon 9a have been reported in GenBank (on March 12, 2015). One of the predicted isoforms is TPM4α (as in avian and amphibians) containing exons 1a, 2, 3, 4, 5, 6b, 7, 8, and 9a/b encoding 284 amino acids (accession number XM_006722865). The other one may encode a low molecular weight novel protein with 248 amino acids consisting of exons 1b, 3, 4, 5, 6, 7, 8, and 9a/b (accession number XM_005260042.2). In this study, for the first time we confirmed the expression of these two new transcripts, viz TPM4α (or Tpm4.3 (8)) and TPM4δ (Tpm 4.4 (8)) by RT-PCR with the RNA from human adult heart, fetal heart, and skeletal muscle using two primer-pairs designed from the predicted nucleotide sequences. We confirmed the sequences of both the isoforms by cloning and sequencing of the amplified products. We also determined the relative expression of the two transcripts by qRT-PCR with RNA from human adult heart, fetal heart, and skeletal muscle using isoform specific primer-pairs. For protein expression, we performed 1D and 2D western blot analyses with the extract from adult human heart using the exon 9a-specific monoclonal antibody, CH1. We found nine spots on western blot and the protein was extracted from the spots for mass spectrometry (LC-MS/MS) analyses. The results suggest that spot G may have TPM4α along with TPM1α protein. To the best of our knowledge, this is the first report of TPM4α protein expression in humans.

Figure 1

Alternative splicing pattern of the TPM4 gene in humans. Exon composition of the TPM4 gene is derived from the published documents (top) and the recently submitted data in GenBank. Although the splice variants TPM4β (NM_001145160) and TPM4γ (NM-003290.2) are known for some time, the cartoons of the splice variants of TPM4α and TPM4δ are generated with the information of the recently submitted sequences of the corresponding predicted isoforms in GenBank as well as the results from the present study. Exon locations of primers P1(+), P2(−), and P3(+) are shown.

2. Materials and Methods

Human adult and fetal cardiac tissue RNA were obtained from Zyagen (San Diego, CA); adult human heart protein samples were obtained from Imgenex (San Diego, CA).

2.1. Conventional RT-PCR

All PCR and post-PCR experiments were done by different personnel in in different buildings using separate equipment and separate ventilation so as to avoid carryover contamination. For RT-PCR, 0.5 μg of RNA in a total volume of 40 μL was used to synthesize cDNA with SuperScript® II (Life Technologies, Grand Island, NY) and oligo-dT primers following the manufacturer’s specifications. For each PCR 3 μL of cDNA was used and TPM4α and TPM4δ RNA were amplified as previously described [11, 12]. The nucleotide sequences of the primer-pairs for amplification of TPM4α and TPM4δ are given in Table 1. It is to be noted that the negative primer for amplification of TPM4α and TPM4δ is the same. The positive primers for TPM4α and TPM4d are from exon 1a and exon 1b, respectively. The PCR amplified DNAs were run in an agarose gel and the ethidium bromide stained bands were excised from the gel and DNA was extracted from the excised bands using a MinElute Gel extraction kit from Qiagen (Valencia, CA) following the manufacturer’s direction. Part of the DNA was used for sequencing and part of the gel extracted DNAs was ligated and cloned into the T/A cloning vector (Life Technologies) following our published protocol [11, 12]. Positive clones were identified by PCR using the above-mentioned specific primer-pairs previously described. Vectors or constructs were grown in E. coli, and the DNA was extracted using Qiagen Miniprep kit (Valencia, CA). The isolated DNA was sequenced (Cornell University Life Science Core Laboratories Center, Ithaca, NY). Each clone was sequenced twice in both directions. It is to be noted that the primer-pair we have used for TPM4α and TPM4δ is very specific for the respective isoform.

2.2. Real-Time Quantitative RT-PCR

qRT-PCR analysis of cDNA template was performed using the LightCycler 480 Real-Time PCR System. Reactions were carried out in a 384-well plate using the LightCycler 480 SYBR Green I Master kit (Roche). Briefly, each well contained a total volume of 10 μL reaction solution, of which 2 μL was.

cDNA template and 8 μL were SYBR green mix (5 μL 1x SYBR green master mix, 2.8 μL of PCR-grade water, and 0.2 μL of 10 μM primer-pair). Primers for real-time PCR for TPM4α and TPM4δ are listed in Table 1.

In this case cDNA was made with an oligonucleotide from exon 9a/b (5′-CACCATGTGAGAAGGACAGA-3′) that allowed us to make a gene specific cDNA corresponding to the mRNA containing exon 9/b as in TPM4α and TPM4δ and would avoid any subsequent nonspecific PCR amplification. For the amplification of TPM4α and TPM4δ, we have employed the positive primers from exon 1a and exon 1b, respectively, and the same negative primer located in exon 3. Amplification in the absence of cDNA template was also evaluated to insure a lack of signal due to primer dimerization and extension or carryover. All samples and controls were performed in triplicate. Data were analyzed using delta-delta CT (sample delta CT minus comparator delta CT) methods [13–15]. Efficiencies (E) of PCR amplification were determined using dilution series of plasmids and/or human heart cDNAs generated with gene specific primer-pairs as described by Nan et al. [16]. As a result, the primer-pair we have used from each of the isoforms is very specific and does not amplify other isoforms generated from the TPM4 or any other TPM gene.

2.3. Western Blot

10 μg of protein from each sample (human adult and fetal heart) was used for western blot analyses following our published protocol [17]. Primary antibodies included TM311 (Sigma-Aldrich, St. Louis, MO) and CH1 antisarcomeric tropomyosin (DSHB, University of Iowa, Iowa). Secondary antibody was sheep antimouse immunoglobulin HRP (GE Healthcare Bio-Sciences, Pittsburgh, PA).

2.4. 2D Western Blot and Mass Spectrometry

2D (two-dimensional) western blot analyses of the commercial human adult heart extract obtained from Zyagen (San Diego, CA) were performed for us by Kendrick Labs, Inc. (Madison, WI). Two-dimensional electrophoresis was performed according to the carrier ampholine method of isoelectric focusing [18, 19] by Kendrick Labs, Inc. (Madison, WI) as described by Wang et al. [20]. The key to 2D Gel loading and sample preparation is given in Table 2. The Coomassie blue-stained PVDF membrane was desktop scanned, destained in 100% methanol, rinsed briefly in Tween-20 Tris-buffered saline (TTBS), and blocked for two hours in 5% nonfat dry milk (NFDM) in TTBS. The blot was incubated in primary antibody (Anti-Tropomyosin-Clone CH1 (Developmental Studies Hybridoma Bank) diluted 1 : 10,000 in 2% NFDM TTBS) overnight and rinsed 3 × 10 minutes in TTBS. The blot was placed in secondary antibody (antimouse IgG-HRP (GE Healthcare, Cat number NA931V, Lot number 9621358) diluted 1 : 2,000 in 2% NFDM TTBS) for two hours, rinsed as above, treated with ECL, and exposed to X-ray film. For the developed X-ray film when superimposed on the Coomassie stained human adult heart protein gel, 9 spots (A–I) were exhibited (as in Figure 7(a)). Nine gel spots were excised, washed, and trypsinized following the published protocols [21–23]. The resulting peptides were extracted twice with 5% formic acid/50 mM ammonium bicarbonate/50% acetonitrile and once with 100% acetonitrile under moderate shaking. The peptide mixture was then dried in SpeedVac, solubilized in 20 μL of 0.1% formic acid/2% acetonitrile.

2.5. LC-MS/MS

The peptides mixture was analyzed by reverse phase liquid chromatography (LC) and MS (LC-MS/MS) using a nanoACQUITY UPLC (Micromass/Waters, Milford, MA) coupled to a Q-TOF Ultima API MS (Micromass/Waters, Milford, MA), according to published procedures [22–24]. Briefly, the peptides were loaded onto a 100 μm × 10 mm nanoACQUITY BEH130 C18 1.7 μm UPLC column (Waters, Milford, MA) and eluted over a 150-minute gradient of 2–80% organic solvent (ACN containing 0.1% FA) at a flow rate of 400 nL/min. The aqueous solvent was 0.1% FA in HPLC water. The column was coupled to a PicoTip Emitter SilicaTip nanoelectrospray needle (New Objective, Woburn, MA). MS data acquisition involved survey MS scans and automatic data dependent analysis (DDA) of the top three ions with the highest intensity ions with the charge of 2+, 3+, or 4+ ions. The MS/MS was triggered when the MS signal intensity exceeded 10 counts/second. In survey MS scans, the three most intense peaks were selected for collision-induced dissociation (CID) and fragmented until the total MS/MS ion counts reached 10,000 or for up to 6 seconds each. The entire procedure used was previously described [22–24]. Calibration was performed for both precursor and product ions using 1 pmol GluFib (Glu1-Fibrinopeptide B) standard peptide with the sequence EGVNDNEEGFFSAR and the monoisotopic doubly charged peak with of 785.84.

2.6. Data Processing and Protein Identification

The raw data were processed using ProteinLynx Global Server (PLGS, version 2.4) software as previously described by Darie et al. [22].

3. Results

3.1. Detection of RNA Expression by RT-PCR and Cloning and Sequencing of TPM4α and TPM4δ cDNAs

In order to detect the expression of TPM4α and TPM4δ in human striated muscles, we used conventional RT-PCR with the RNA from adult human heart and skeletal muscles. The primer-pairs were designed from the predicted sequences as reported in the GenBank (accession number XM_006722865.1 for TPM4α and XM_005260042.2 for TPM4δ). The nucleotide sequences of the primer-pairs designed are presented in Table 1.

Conventional RT-PCR results presented in Figure 2(a) show that TPM4δ is expressed in both fetal (lane 1) and adult human heart (lane 2).

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(b)

Figure 2

Expression of TPM4 isoforms with exon 9a/b in human heart and skeletal muscle by conventional RT-PCR. (a) Expression of TPM4α and TPMδ in human fetal and adult hearts as determined. TPM4δ amplified with primer 1(+) and primer 2(−) as shown in Figure 1 and Table 1. The size of the amplified DNA is ~747 bp. Lane 1: adult heart; lane 2: fetal heart; lane 3: primer control. TPM4α amplified with primer 1(+) and primer 2(−) as shown in Figure 1 and Table 1. The size of the amplified DNA is ~855 bp. Lane 4: adult heart; lane 5: fetal heart; lane 6: primer control. (b) Expression of TPM4α in human fetal heart, adult heart, and adult skeletal muscle. TPM4α amplified with primer 1(+) and primer 2(−) as shown in Figure 1 and Table 1. The size of the amplified DNA is ~855 bp. Lane 1: fetal heart; lane 2: adult heart; lane 3: adult skeletal muscle (source 1); lane 4: adult skeletal muscle (source 2); lane 5: primer control.

Also, the TPM4α is expressed in both fetal and adult heart as depicted in lanes 4 and 5, respectively. Again, TPM4a is expressed in fetal heart (lane 1, Figure 2(b)), adult heart (lane 2, Figure 2(b)), and also skeletal muscle (lanes 3 and 4 representing two different sources of adult human skeletal muscle RNA).

The amplified DNA from the ethidium stained band(s) on agarose gel was extracted and purified using a gel extraction kit from Ambion, Inc. Gel extracted DNA was used subsequently for nucleotide sequence determination as well as cloning into T/A cloning vector (Invitrogen). Direct DNA sequence analyses confirmed the expression of TPM4α and TPM4δ in both heart and skeletal muscle. DNA sequencing was also performed with the cDNA of each TPM4 isoform cloned in T/A cloning vector. Figures 3 and 4 depict the nucleotide as well as deduced amino acid sequences of TPM4α and TPM4δ. The sequences are identical with the predicted sequences as submitted in GenBank. When the amino acid sequences of TPM4α and TPM1α (Acc number NP_001018005) are compared, there are 96.127 percent similarity and 88.028 percent identity between the two sarcomeric isoforms (best fit results not shown). To the best of our knowledge this is the first report on the expression of TPM4α and TPM4δ in human striated muscles. Comparisons of the amino acid sequences of TPM4δ and the known TPM4γ indicate that both isoforms encode a 248-amino acid polypeptide with identical sequences except for exon 9. The exon compositions of TPM4γ and TPM4δ are given in Figure 1. TPM4γ contains exons 1b, 3, 4, 5, 6b, 7, 8, and 9d while TPM4δ contains exon 9a instead of 9d.

3.2. qRT-PCR Analyses to Determine the Relative Expression of TPM4α and TPM4δ in Human Fetal Heart, Adult Heart, and Adult Skeletal Muscle

The results depicted in Figures 5 and 2(b) confirm that TPM4α is expressed in human hearts and skeletal muscle. Interestingly, the expression level of both isoforms is the least in skeletal muscle. However, the relative expression of TPM4α and TPM4δ is higher in fetal heart compared to adult heart and adult skeletal muscle. The results also indicate that the relative expression of TPM4α is much higher compared to TPM4δ in all the tissues tested. Please note the difference in scale for TPM4α and TPM4δ shown in Figure 5.

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(b)

3.3. Western Blot Analyses with the Total Protein Extracts of Human Adult Heart

In order to explore whether or not TPM4α and TPM4δ proteins are expressed in human striated muscles, we have employed western blot analyses with the CH1 monoclonal antibody that recognizes an epitope in exon 9a. In other words, CH1 monoclonal antibody recognizes all known sarcomeric TPM isoforms (TPM1α, TPM1κ, TPM2α, TPM3α, and TPM4α) and the nonsarcomeric TPM4δ having a peptide encoded by exon 9a at the C-terminus end. Each of these sarcomeric isoforms contains 284 amino acids and is considered as high molecular wt tropomyosin. Although TPM4δ encodes 248 amino acids and has different exon 1, exon 9 is identical to TPM4α. Hence, if TPM4δ protein is expressed, one should observe a signal at the ~28 kDa region in the western blot. We have employed another monoclonal antitropomyosin antibody TM311, which recognizes all high molecular wt tropomyosin molecules (~32 kDa and above) containing exon 1a. As TPM4δ, unlike TPM4α, contains exon 1b instead of exon 1a, one should not observe any ~28 kDa signal with TM311 antibodies. The results depicted in Figure 6 (staining with CH1 monoclonal antibodies) show strong signal(s) at ~39 kDa region. The results show the presence of most likely several sarcomeric isoforms, for example, TPM1α, TPM1κ, TPM2α, and TPM3α, in human hearts. Without using a TPM4 specific antibody one cannot infer that the signal(s) at the ~39 kDa region indicates the presence of TPM4α protein in human cardiac muscles. In addition, we did not detect the presence of low molecular wt tropomyosin like TPM4δ. If it was expressed in detectable quantity, we should have picked up a signal. Western blot analyses with TM311 confirm the expression of high molecular wt sarcomeric and nonsarcomeric TPM isoforms in adult and fetal heart tissues. TM311 should not recognize low molecular wt TPM4δ, which contains exon 1b rather than exon 1a region [6].

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(b)

(c)

Figure 6

Western blot analysis of protein extracts from human adult and fetal hearts with CH1 and TPM311 antitropomyosin antibodies. (a) Ponceau-stained blot: lane 1: extract of adult heart; lane 2: extract of fetal heart; lane M: molecular weight markers. (b) Blots stained with CH1 monoclonal antibodies that recognize all sarcomeric TPM isoforms as well as TPM4δ with exon 9a C-terminus end. (c) Blot stained with TM311 monoclonal antibodies that recognize all high molecular wt TPM isoforms with exon 1a at the N-terminus end. However, it does not recognize TPM4δ with exon 1b at the N-terminus end.

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(b)

(c)

(d)

(e)

Figure 7

2D gels of commercially available extracts of human adult heart. (a) The Coomassie stained human adult heart protein across the gel. Seven spots A, B, C, D, E, F, and G were identified, which are not visible clearly. (b) This panel represents the enlarged portion of the gel in (a) and shows clearly A–E spots. (c) The PVDF filter was stained with CH1 monoclonal antibody followed by treatment with secondary antibody as mentioned under Materials and Methods and subsequently treated with ECL and exposed to X-ray film. (d) Developed X-ray film was merged on the top of the Coomassie stained blot. (e) Enlarged nine spots (A–I) were marked on the PVDF filter (as in (a) and (b)) and on the duplicate gel. All the spots were marked and excised and were used for extraction of protein for subsequent mass spectrometric analyses. Extracted peptides from spots E, F, and G were analyzed for mass spectrometry as described in the method section.

3.4. 2D Western Blot Analyses with Protein Extracts of Adult Human Heart with CH1 Monoclonal Antibody That Recognizes All Sarcomeric Tropomyosin Isoforms including TPM4a and the Newly Found TPM4δ with Exon 9α Polypeptide at the C-Terminus End

Two-dimensional western blot analyses were performed with commercially available human heart extract with antisarcomeric antitropomyosin (CH1) antibodies. Figure 7(a) shows the Coomassie blue-stained PVDF membrane before western blotting and Figure 7(b) depicts the signals on the X-ray film exposed on the blot after being treated with ECL (see the method section). Figure 7(d) represents the developed X-ray film superimposed on the top of the Coomassie blue-stained PVDF membrane (as in Figures 7(a) and 7(b)). Nine spots were identified and marked as A, B, C, D, E, F, G, H, and I (Figures 7(a) and 7(b)). The results indicate that there are at least nine detectable CH1 positive tropomyosin molecules present in the extract from adult human hearts. It is to be noted that each of these spots represents high molecular wt (32 kD and above) tropomyosin protein. However, we have failed to detect the presence of a low molecular wt CH1-positive tropomyosin protein with a molecular mass ~28 kDa like TPM4δ in adult human heart.

In the next step, each of the protein spots that were separated by 2D PAGE and stained by Coomassie dye was excised and washed and the proteins from the gel were treated/processed according to the published protocol (please see the method section) for LS-MS/MS analyses using nanoACQUITY UPLC (Micromass/Waters, Milford, MA) coupled to a Q-TOF Ultima API MS (Micromass/Waters, Milford, MA). The raw data were processed using ProteinLynx Global Server (PLGS, version 2.4) software. Mascot and PLGS database search provided a list of proteins for each gel band. To eliminate false positive results, for the proteins identified by either one peptide or a mascot score lower than 25, we verified the MS/MS spectra that led to identification of a protein. In spot G, a total of 53 peptide sequences were identified. As shown in Figure 8, the identified peptides cover 76% of TPM1α (accession number gi/63252898) and 38% of TPM4α protein (accession number GI: 578833543; PREDICTED: tropomyosin alpha-4 chain isoform X1; Homo sapiens). It is to be noted that there are not very many differences between TPM1α and TPM4α. In this study, we found three peptides, containing a total of three amino acid residues, that are specific for TPM4α and eight peptides containing eighteen amino acids that are specific for TPM1α. The remainders of the identified peptides are identical in both isoforms. For TPM1α, peptide in exons 1a, 2, 3, 4, 5, 6, 7, 8, and 9a was identified. For TPM4α, peptides in exons 1a, 8, and 9a were identified. Some amino acid changes found in the striated muscle TPM4α are also found in skeletal muscle TPM2α (gi I 42476296 isoform, which is also expressed in heart). One of such changes is L19I. Again, ²⁵²T is also present in TPM2α. However, the peptide of the TPM4α that we have sequenced is quite different from TPM2a peptide. This is true for ²⁸⁴L. The peptide containing ²⁸⁴L residue from TPM4α that we have sequenced (as marked with red color) is different from human TPM2α (gi I42476296). The results indicate the potential expression of TPM4α protein in human cardiac tissues.

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(b)

Figure 8

Identification of amino acid sequences from the peptides extracted from spot G after 2D western blot analyses of adult heart extracts with CH1 antibodies. Red color letters indicate the isolated peptides that have been sequenced by mass spectrometry. (a) TPM1α and (b) TPM4α. Three amino acid residues in exons 1a, 8, and 9a are different in TPM4α marked as bold. In case of TPM1α 76% (red marked) of the total 284 amino acid residues are being identified. For TPM4α it is 38%. It is to be noted that peptide SIDDLEDELYAQKLK in TPM1α was identified by two precursor ions with of 594.07 (3+) and 890.06 (2+) ions. On the other hand, peptide TIDDLEDELYAQKLK in TPM4α was identified by one precursor ion with of 888.06 (2+).

4. Discussion

In this study, we have cloned and sequenced cDNAs of two novel TPM4 isoforms using RNA from human hearts (Figures 1–3); one is the sarcomeric isoform TPM4α that encodes a protein with 284 amino acids and the other known as TPM4 encodes a protein with 248 amino acids (Figures 1 and 4). The transcripts of these two isoforms are expressed in fetal heart, adult heart, and skeletal muscle. The expression level is somewhat higher in hearts compared to skeletal muscle (Figures 2 and 5). We were unable to detect the expression of TPM4δ (a ~28 kD protein) in either adult or fetal hearts by western blot analyses using CH1 monoclonal antibody that recognizes an epitope in exon 9a. However, CH1 antibody detected the expression of high molecular weight TPM proteins (~32 kDa and above) in adult and fetal hearts (Figure 6). One of the limitations in tropomyosin research is the unavailability of isoform specific antibodies. Without them, it is practically impossible to pinpoint whether the TPM4α protein is present in the cluster of signals at the high molecular wt region (32–40 kDa) as depicted in Figure 6. In order to gain further insight, we have performed 2D western blot analyses with CH1 antibody. The gel extracted proteins from various spots with positive signal were analyzed by LS-MS/MS. The results indicate that the spot G contains TPM4α protein along with TPM1α. It is to be noted that we have also found the expression of TPM1κ, TPM2α, and TPM3α in other spots (data not shown). Our future plan is to further confirm the expression of TPM4α protein in human striated muscles in healthy and diseased ones. We have compared the expression level of TPM4α transcripts in fetal and adult human hearts and are planning to compare the corresponding protein expression level in fetal and adult human hearts as well. The fact that we found more peptides specific to TPM1a than TPM4a in spot G is consistent with our bias that there is more of the former than the latter in human cardiomyocytes.

Although the expression of multiple isoforms of tropomyosin has long been known in vertebrates including humans, the precise function of each of the isoforms generated by various TPM genes is not well understood. For example, the expressions of TPM1α (the sarcomeric isoform of the TPM1 gene) and TPM2α (sarcomeric isoform of the TPM2 gene) in human hearts have been known for a long time. However, the precise role(s) of the two sarcomeric TPM proteins in cardiac muscle contraction have not been elucidated. More recent published results suggest that TPM1 makes up about 90% of the total sarcomeric TPM protein in human hearts. TPM2α and TPM1κ (another sarcomeric isoform of the TPM1 gene) may constitute the remaining 10 percent of the TPM protein. Peng et al. [25] using top-down mass spectrometry confirmed that TPM1α constitutes 90% of the total sarcomeric tropomyosin in human hearts. They also detected a low amount of TPM2α and TPM1κ expression in human hearts. There was no mention about the expression of TPM4α in this paper. Marston et al. also reported the expression of TPM3α in human heart [26]. These authors reported that the level of expression of TPM1α and TPM1κ was 95% and 4%, respectively, of the total sarcomeric tropomyosin in human hearts. In addition, a low level of expression of TPM2α, TPM3α, and TPM1β (smooth muscle type tropomyosin) was also detected. Again, there was no mention about the expression of TPM4α.

Researchers from different laboratories using transgenic mouse models have delineated the tentative function of TPM1α and TPM2α in mammalian hearts [27–29]. In the adult healthy mouse heart the protein expression level of TPM2α is less than 2%. When there was 55–60% of TPM2α present in the myocardium of transgenic mouse heart, the time of relaxation, maximum rate of relaxation, and sensitivity to calcium changed significantly. Further altering of TPM2α to an even higher level in the heart of transgenic mice will cause postnatal death in between 10 and 14 days [27–29]. TPM3α is not expressed in mouse hearts [4]. High ectopic expression level of TPM3α (40–60%) can lead to hyperdynamic effect on systolic and diastolic function and decreased calcium sensitivity [30]. As TPM3α is not expressed in mouse heart, it is not possible to perform knockout/knockdown experiments for TPM3α. Again, overexpression of TPM1κ in a cardiac-specific manner in transgenic mouse leads to a dilated cardiomyopathy (DCM) like syndrome. Interestingly, the expression level of TPM1κ protein has been found to be significantly higher in hearts from DCM and heart failure patients. The functional analysis of TPM1κ provides a possible mechanism for the consequences of the TPM isoform switch observed in DCM and heart failure patients [31].

The functional aspect of TPM3α in human cardiac tissues is not known yet. Our finding of the potential expression of TPM4α in human heart muscles makes the situation more complicated. The most important, as well as most difficult, question yet to be addressed is whether minute expression of the sarcomeric TPM proteins such as TPM1κ, TPM2α, TPM3α, and TPM4α plays any significant role in cardiac contractility and/or cardiac function.

As rodents with truncated TPM4 genes are not capable of producing sarcomeric TPM4α protein, the in vivo function of TPM4α using knockdown/knockout technology is not possible. However, one can generate transgenic mouse ectopically overexpressing human TPM4α protein in a cardiac specific manner and find out whether ectopic expression is altering the cardiac morphology and/or cardiac contractility. Another approach researchers have used for assigning the function of a protein is to look for its association with any human disease(s). For example, various TPM1 and TPM2 mutations have been implicated in hypertrophic cardiomyopathy (HCM) including familial hypertrophic cardiomyopathy (FHC) in humans [31]. Similarly, several missense mutations in TPM2 and TPM3 have been implicated in nemaline myopathy that suggest the functional importance of these genes or particular isoform in cellular function. To the best of our knowledge no mutation in TPM4 gene has been implicated in any diseases of striated muscles in humans. However, one cannot rule out that this possibility was not considered before because of the belief that the TPM4 gene in humans, as in rodents, does not produce the sarcomeric isoform TPM4α.

Competing Interests

The authors declare that there is no conflict of interests regarding the publication of this paper.

Acknowledgments

The work was supported by a grant from the Department of Medicine and Barbara Kopp Cancer Research Fund to Bernard J. Poiesz. The authors would like to thank Dr. Costal C. Darie, Associate Professor, Clarkson University, Potsdam, New York, for his kind help in explaining the details of LC-MS/MS analysis. Authors are thankful to Ms. Lori Spicer for her assistance for the preparation of the manuscript.

References

P. Gunning, G. O'Neill, and E. Hardeman, “Tropomyosin-based regulation of the actin cytoskeleton in time and space,” Physiological Reviews, vol. 88, no. 1, pp. 1–35, 2008.
View at: Publisher Site | Google Scholar
J. P. Lees-Miller and D. M. Helfman, “The molecular basis for tropomyosin isoform diversity,” BioEssays, vol. 13, no. 9, pp. 429–437, 1991.
View at: Publisher Site | Google Scholar
S. V. Perry, “Vertebrate tropomyosin: distribution, properties and function,” Journal of Muscle Research and Cell Motility, vol. 22, no. 1, pp. 5–49, 2001.
View at: Publisher Site | Google Scholar
K. Pieples and D. F. Wieczorek, “Tropomyosin 3 increases striated muscle isoform diversity,” Biochemistry, vol. 39, no. 28, pp. 8291–8297, 2000.
View at: Publisher Site | Google Scholar
M. F. Pittenger, J. A. Kazzaz, and D. M. Helfman, “Functional properties of non-muscle tropomyosin isoforms,” Current Opinion in Cell Biology, vol. 6, no. 1, pp. 96–104, 1994.
View at: Publisher Site | Google Scholar
G. Schevzov, S. P. Whittaker, T. Fath, J. J.-C. Lin, and P. W. Gunning, “Tropomyosin isoforms and reagents,” BioArchitecture, vol. 1, no. 4, pp. 135–164, 2011.
View at: Publisher Site | Google Scholar
M. A. Geeves, S. E. Hitchcock-DeGregori, and P. W. Gunning, “A systematic nomenclature for mammalian tropomyosin isoforms,” Journal of Muscle Research and Cell Motility, vol. 36, no. 2, pp. 147–153, 2015.
View at: Publisher Site | Google Scholar
D. E. Fleenor, K. H. Hickman, G. J. Lindquester, and R. B. Devlin, “Avian cardiac tropomyosin gene produces tissue-specific isoforms through alternative RNA splicing,” Journal of Muscle Research and Cell Motility, vol. 13, no. 1, pp. 55–63, 1992.
View at: Publisher Site | Google Scholar
S. Hardy, N. Thézé, D. Lepetit, M.-R. Allo, and P. Thiebaud, “The Xenopus laevis TM-4 gene encodes non-muscle and cardiac tropomyosin isoforms through alternative splicing,” Gene, vol. 156, no. 2, pp. 265–270, 1995.
View at: Publisher Site | Google Scholar
B. J. Spinner, R. W. Zajdel, M. D. McLean et al., “Characterization of a TM-4 type Tropomyosin that is essential for myofibrillogenesis and contractile activity in embryonic hearts of the Mexican axolotl,” Journal of Cellular Biochemistry, vol. 85, no. 4, pp. 747–761, 2002.
View at: Publisher Site | Google Scholar
A. Thomas, S. Rajan, H. L. Thurston et al., “Expression of a novel tropomyosin isoform in axolotl heart and skeletal muscle,” Journal of Cellular Biochemistry, vol. 110, no. 4, pp. 875–881, 2010.
View at: Publisher Site | Google Scholar
H. L. Thurston, S. Prayaga, A. Thomas et al., “Expression of Nkx2.5 in wild type, cardiac mutant, and thyroxine-induced metamorphosed hearts of the mexican axolotl,” Cardiovascular Toxicology, vol. 9, no. 1, pp. 13–20, 2009.
View at: Publisher Site | Google Scholar
M. W. Pfaffl, “A new mathematical model for relative quantification in real-time RT-PCR,” Nucleic Acids Research, vol. 29, no. 9, article e45, pp. 2002–2007, 2001.
View at: Publisher Site | Google Scholar
K. J. Livak and T. D. Schmittgen, “Analysis of relative gene expression data using real-time quantitative PCR and the $2^{- Δ Δ C_{T}}$ method,” Methods, vol. 25, no. 4, pp. 402–408, 2001.
View at: Publisher Site | Google Scholar
J. S. Yuan, A. Reed, F. Chen, and C. N. Stewart Jr., “Statistical analysis of real-time PCR data,” BMC Bioinformatics, vol. 7, article 85, 2006.
View at: Publisher Site | Google Scholar
C. Nan, S. Dube, A. Matoq et al., “Expression of sarcomeric tropomyosin in striated muscles in axolotl treated with Shz-1, a small cardiogenic molecule,” Cardiovascular Toxicology, vol. 15, no. 1, pp. 29–40, 2015.
View at: Publisher Site | Google Scholar
S. Dube, L. Panebianco, A. A. Matoq et al., “Expression of TPM1κ, a novel sarcomeric isoform of the TPM1 gene, in mouse heart and skeletal muscle,” Molecular Biology International, vol. 2014, Article ID 896068, 9 pages, 2014.
View at: Publisher Site | Google Scholar
P. H. O'Farrell, “High resolution two-dimensional electrophoresis of proteins,” The Journal of Biological Chemistry, vol. 250, no. 10, pp. 4007–4021, 1975.
View at: Google Scholar
A. Burgess-Cassler, J. J. Johansen, D. A. Santek, J. R. Ide, and N. C. Kendrick, “Computerized quantitative analysis of coomassie-blue-stained serum proteins separated by two-dimensional electrophoresis,” Clinical Chemistry, vol. 35, no. 12, pp. 2297–2304, 1989.
View at: Google Scholar
J. Wang, D. K. Dube, J. White, Y. Fan, J. M. Sanger, and J. W. Sanger, “Clock is not a component of Z-bands,” Cytoskeleton, vol. 69, no. 12, pp. 1021–1031, 2012.
View at: Publisher Site | Google Scholar
A. Shevchenko, M. Wilm, O. Vorm, and M. Mann, “Mass spectrometric sequencing of proteins from silver-stained polyacrylamide gels,” Analytical Chemistry, vol. 68, no. 5, pp. 850–858, 1996.
View at: Publisher Site | Google Scholar
C. C. Darie, K. Deinhardt, G. Zhang, H. S. Cardasis, M. V. Chao, and T. A. Neubert, “Identifying transient protein-protein interactions in EphB2 signaling by blue native PAGE and mass spectrometry,” Proteomics, vol. 11, no. 23, pp. 4514–4528, 2011.
View at: Publisher Site | Google Scholar
I. Sokolowska, A. G. Woods, M. A. Gawinowicz, U. Roy, and C. C. Darie, “Identification of potential tumor differentiation factor (TDF) receptor from steroid-responsive and steroid-resistant breast cancer cells,” The Journal of Biological Chemistry, vol. 287, no. 3, pp. 1719–1733, 2012.
View at: Publisher Site | Google Scholar
D. S. Spellman, K. Deinhardt, C. C. Darie, M. V. Chao, and T. A. Neuebrt, “Stable isotopic labeling by amino acids in cultured primary neurons: application to brain-derived neurotrophic factor-dependent phosphotyrosine-associated signaling,” Molecular and Cellular Proteomics, vol. 7, no. 6, pp. 1067–1076, 2008.
View at: Publisher Site | Google Scholar
Y. Peng, D. Yu, Z. Gregorich et al., “In-depth proteomic analysis of human tropomyosin by top-down mass spectrometry,” Journal of Muscle Research and Cell Motility, vol. 34, no. 3, pp. 199–210, 2013.
View at: Publisher Site | Google Scholar
S. B. Marston, O. Copeland, A. E. Messer et al., “Tropomyosin isoform expression and phosphorylation in the human heart in health and disease,” Journal of Muscle Research and Cell Motility, vol. 34, no. 3-4, pp. 189–197, 2013.
View at: Publisher Site | Google Scholar
M. Muthuchamy, I. L. Grupp, G. Grupp et al., “Molecular and physiological effects of overexpressing striated muscle β-tropomyosin in the adult murine heart,” The Journal of Biological Chemistry, vol. 270, no. 51, pp. 30593–30603, 1995.
View at: Publisher Site | Google Scholar
M. Muthuchamy, L. Pajak, P. Howles, T. Doetschman, and D. F. Wieczorek, “Developmental analysis of tropomyosin gene expression in embryonic stem cells and mouse embryos,” Molecular and Cellular Biology, vol. 13, no. 6, pp. 3311–3323, 1993.
View at: Publisher Site | Google Scholar
M. Muthuchamy, P. Rethinasamy, and D. F. Wieczorek, “Tropomyosin structure and function: new insights,” Trends in Cardiovascular Medicine, vol. 7, no. 4, pp. 124–128, 1997.
View at: Publisher Site | Google Scholar
K. Pieples, G. Arteaga, R. John Solaro et al., “Tropomyosin 3 expression leads to hypercontractility and attenuates myofilament length-dependent Ca²⁺ activation,” American Journal of Physiology—Heart and Circulatory Physiology, vol. 283, no. 4, pp. H1344–H1353, 2002.
View at: Publisher Site | Google Scholar
S. Rajan, G. Jagatheesan, C. N. Karam et al., “Molecular and functional characterization of a novel cardiac-specific human tropomyosin isoform,” Circulation, vol. 121, no. 3, pp. 410–418, 2010.
View at: Publisher Site | Google Scholar

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Copyright © 2016 Dipak K. Dube et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

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