- Open Access
Myofibril-Inducing RNA (MIR) is essential for tropomyosin expression and myofibrillogenesis in axolotl hearts
© Zhang et al; licensee BioMed Central Ltd. 2009
- Received: 8 May 2009
- Accepted: 3 September 2009
- Published: 3 September 2009
The Mexican axolotl, Ambystoma mexicanum, carries the naturally-occurring recessive mutant gene 'c' that results in a failure of homozygous (c/c) embryos to form hearts that beat because of an absence of organized myofibrils. Our previous studies have shown that a noncoding RNA, M yofibril-I nducing R NA (MIR), is capable of promoting myofibrillogenesis and heart beating in the mutant (c/c) axolotls. The present study demonstrates that the MIR gene is essential for tropomyosin (TM) expression in axolotl hearts during development. Gene expression studies show that mRNA expression of various tropomyosin isoforms in untreated mutant hearts and in normal hearts knocked down with double-stranded MIR (dsMIR) are similar to untreated normal. However, at the protein level, selected tropomyosin isoforms are significantly reduced in mutant and dsMIR treated normal hearts. These results suggest that MIR is involved in controlling the translation or post-translation of various TM isoforms and subsequently of regulating cardiac contractility.
- Embryonic Heart
- Heart Tube
- Mutant Heart
- Ambystoma Mexicanum
- Tropomyosin Isoforms
The Mexican axolotl, Ambystoma mexicanum, has proven to be a unique animal model in the study of cardiac development. The axolotl (a neotenous salamander) carries a naturally occurring recessive mutation, gene c, first discovered and characterized by Humphrey , which results in abnormal cardiac development in homozygous recessive "c/c" embryos. The mutant embryonic hearts develop, but fail to beat, making them distinguishable from normal embryonic hearts which start to beat at stage 35. The myocytes of the mutant hearts fail to form organized myofibrils and the embryos survive only to stage 42, the hatching stage, due to a lack of circulation.
Among the various myofibril structural proteins, tropomyosin has been shown by SDS-PAGE , radio-immunoassay , 2D gel electrophoresis  and confocal microscopy of whole hearts to be drastically reduced in the mutants [5–7]. Interestingly, other myofibril structural proteins such as actin, myosin and myosin binding protein C, however, were found to be at or near normal levels in the mutant hearts [8–10].
Using this animal model, M yofibril-I nducing R NA (MIR), a small bioactive RNA, was shown in previous studies to be able to restore tropomyosin protein synthesis, promote myofibrillogenesis, and initiate heartbeat in the mutant embryonic hearts in organ culture . The MIR appears to function through its unique secondary structure since it is a non-coding RNA [7, 11].
In mammals, birds and amphibians, altogether four different types of tropomyosin genes have been identified: alpha gene (TPM1), beta gene (TPM2), gamma gene (TPM3) and TM4 type gene (TPM4) . More recently, TM4, a cytoskeletal tropomyosin, also has been associated with growth and regeneration in response to injury, disease state and stress in skeletal muscle of mouse and humans . Moreover, in zebrafish embryos, a heart specific isoform of TM4 is essential for normal myofibril formation and developing a heartbeat . In addition, it has been found recently that tropomyosin is likely necessary for actin filament formation in motile cells that employ lamellipodia and filopodia for locomotion . Thus, tropomyosin appears to play a major role in actin filament modulation and contractility in both muscle and nonmuscle contractile systems. Striated muscle-specific alpha-tropomyosin is the predominant isoform in cardiac muscle, with low levels of beta-tropomyosin expressed during fetal development in the mouse heart . In amphibian models, such as Xenopus, the cardiac muscle tropomyosins are synthesized from the alpha-TM and TM-4 genes . In all of these animal models, the alpha-tropomyosin gene is the major contributor to the tropomyosin proteins in the cardiac myofibril structures.
There are at least three striated muscle isoforms of tropomyosin present in the axolotl. Two isoforms of tropomyosin cDNA have been identified which apparently are derived from the single alpha-tropomyosin gene (TPM1) through alternative splicing . Spinner et al.  cloned another tropomyosin cDNA which is the product of a TM4 type tropomyosin gene from axolotl heart. Our results from the axolotl model of heart development are consistent with the findings in Xenopus in that both alpha (ATmC-1 and ATmC-2) and TM4 type (ATmC-3) tropomyosin transcripts are expressed in axolotl hearts [18, 19].
In the present studies, we conducted a series of experiments to further understand the role of MIR in the expression of tropomyosin and myofibrillogenesis using our mutant axolotl heart model. First, we have cloned the full-length cDNA sequence of MIR. Sequence analyses suggest that MIR is a noncoding RNA molecule. However, functional studies indicate that the MIR is essential for tropomyosin expression as well as myofibrillogenesis in axolotl hearts during development at the level of translation or post-translation.
Procurement of animal tissues
The embryos used in the study were derived from adult animals maintained in our colony. We followed NIH Guidelines for the Care and Use of Laboratory Animals and all animal protocols were approved by the Institutional Animal Care and Use Committee. Embryos at stages 35-38 were collected and dissected in Steinberg's solution (SS) as described previously . The inner thoracic cavities were exposed and the hearts removed and used in the various bioassays.
Bioassays with cationic liposome transfection and confocal microscopy
Liposome reagents (0.1-0.16 μg/μl) and MIR sense (500 nt) (0.022 μg/μl), antisense RNA (500 nt) (0.022 μg/μl) or dsRNA (500 bp, 0.002 μg/μl) were diluted in SS without antibiotics for 30-45 minutes at room temperature (RT). The two solutions were mixed and drops of transfection solution were prepared. The hearts are transferred with SS into drops containing the transfection solution for a total volume of 20 μl and appropriate concentrations of RNAs (7 ng/μl) or double-stranded RNA (4 ng/μl), and lipofectin. 10× of SS was added to the transfection medium to dilute the liposome reagents after 24 hours and the hearts were cultured for an additional 2 days (for mutant hearts + MIR RNA) or an additional 9 days (for normal hearts + dsRNA) in a 17°C incubator. The hearts were stained for immunofluorescent observation and analyzed by confocal microscopy following our previously published procedures [7, 21, 22].
Synthesis of double-stranded MIR
Sense and antisense MIR are synthesized in vitro using T7 RNA polymerase (Ambion, TX) on PCR generated MIR cDNA templates with T7 promoter added to either 5' or 3' end sequences. 20 μg of both sense and antisense RNA are mixed in annealing buffer (pH 7.4) and denatured at 68°C for 5 minutes. Sense and antisense RNAs are annealed to each other to form dsRNA by gradually reducing the temperature to 25°C. The products were run on 1.5% agarose gels and the dsRNA was recovered from the gels. FITC-labeled dsRNA was synthesized as described above but using 1:3 FITC-conjugated UTP and unlabeled UTP for single-stranded RNA transcription.
Primers used for different genes in real time RT-PCR experiments.
Cloning of exon 1b sequence for axolotl alpha-TM
We have cloned exon 1b of the axolotl alpha-TM. 5'RACE experiments using primers designed from the exon 3 sequence of the axolotl alpha-TM (ATmC1-exon3-rev-1: 5'-CCAGACGCTCCTGAGCACGATCC; ATmC1-exon3-rev-2:5'-CCAGCTGGATACGCCTGT TC) and a 5' adaptor sequence revealed both PCR bands corresponding to the ATmC-1 sequence and a shorter PCR band after agarose gel electrophoresis. The shorter band was cloned into a pGEM-T easy vector (Promega, WI) and sequenced. The sequence shows high homology to the 5' ends of alpha-TM5a or 5b from other vertebrates. The sequence is: 5'-GTACTGTTGAGGCATCCACGTCTTCACTATTACTGGGGCATTTGTAGTCCCTTGGAATTTGAG CTGACCTTATCGCTACTCGCCTCATATGATAGAGGCGCCACACCTACCTGCGAGTGTTCCGTT CCCCGGCCCTCAGCATG TCTGGGGGCACCTCCCTGGAAGCGGTGCGGCGGAAGATCCGCGC CCTGCAGGAGCAGGCGGACTCCGCTGAAGCCCGGGCGTGTAGCCTGCAGCGGGAACGAGAC GCTGAGCGGCAGCTGCGAGAGGCGGCTGAGAGTGATGTAGCCTCCCTGAACAGGCGTATCCA GCTGGTTGAGGAAGAGTTGGAT CGTGCTCAGGAGCGTCTGG. The bolded ATG represents a putative translation start site. The cloned sequence corresponding to exon 3 shows 100% identity to alpha-TM but with variations to axolotl ATmC-3, demonstrating the origin of this fragment from axolotl alpha-TM. We have named this isoform ATm5.
Two-dimensional gel electrophoresis and Western blotting
The immobilized pH gradient (IPG) gel strips (pH range 3-6, 11 cm, Bio-Rad, CA) were rehydrated in 200 μl ReadyPrep Rehydration/Sample Buffer that contained heart samples for 12 hours. Isoelectric focusing (IEF) was performed on the rehydrated IPGs at 20°C in three steps: 250 volts for 20 minutes, 8,000 volts for 2.5 hours, and then 20,000 Volts/hour using Protean IEF Cell system (Bio-Rad, CA).
After isoelectrical focusing was completed, IPG strips were prepared for SDS-PAGE using 12% Bis-Tris precast gels (Bio-Rad, CA). The strips were then rinsed with electrophoresis running buffer (pH7.7) and laid into the two-dimensional well of 12% precast gels and were run at 200 V for 1 hour following the manufacturer's protocol (ReadyPrep™ 2-D Starter Kit; Bio-Rad, CA.).
The two-dimensional SDS-PAGE gels were transferred to nitrocellulose membranes and processed for hybridization. The membranes were incubated with CH1 monoclonal antibody (1:5000) (from Developmental Studies Hybridoma Bank, University of Iowa) at a 1:2000 dilution for 1 hour at RT. After two washings for 5 minutes each, they were hybridized with horseradish peroxidase-conjugated mouse antihuman IgG (Amersham-Pharmacia Biosciences) at 1:5000 dilution for 1 hour at RT and the blots were washed and exposed to X-ray film and developed with an ECL chemiluminescence system .
Cloning the full length cDNA of the myofibril-inducing RNA (MIR) gene
We have previously published the nucleotide sequence of the 166 nt long bioactive MIR  and showed that the artificially synthesized 166 nt RNA can promote myofibril formation and initiate beating of the mutant hearts in organ culture studies .
Full length MIR promotes tropomyosin protein expression in cardiac nonfunction mutant embryonic hearts
MIR-promoted tropomyosin protein expression in the mutant hearts is not due to increased transcription levels or splicing pattern changes of tropomyosin genes
To determine whether MIR-promoted tropomyosin protein expression in the mutant heart is due to regulation at the transcriptional levels or changes in the splicing patterns of the TM transcripts, we proposed two hypotheses. We tested those hypotheses by performing a series of real-time RT-PCR experiments.
Our second hypothesis proposes that the MIR regulates splicing of tropomyosin transcripts to produce correct isoforms in the cardiac muscle cells. For these real time RT-PCR studies, we designed specific primer pairs based on representative alternative spliced exons of the alpha-tropomyosin gene. From our previous studies, we found that both ATmC-1 and ATmC-2 cDNAs are expressed from the same alpha-tropomyosin gene but differ in exon 2, with ATmC-1 containing a striated muscle specific exon 2b while ATmC-2 contains a smooth muscle isoform specific exon 2a (Fig. 3A). We have shown previously that both ATmC-1 and ATmC-2 can be incorporated into cardiac muscle fibers . Alpha-TM has been reported also to produce fibroblast tropomyosin isoforms with smaller molecular weights, such as TM5a and TM5b, both of which can be incorporated into myofibrils . Isoforms TM5a and 5b are produced by using an internal promoter located between exon 2b and exon 1b thus skipping exon 2a and exon 2b and conjoining exon 1b and exon 3 directly together . To determine whether MIR can regulate the expression pattern of tropomyosin by selectively favoring the use of exon 1b, 2a or 2b, we have cloned exon 1b of the axolotl alpha-TM to study the A xolotl Tm5 gene (ATm5). 5' RACE experiments using primers designed from the exon 3 sequence of axolotl alpha-TM and a 5' adaptor sequence revealed PCR bands corresponding to the ATmC-1 sequence and a shorter PCR band by agarose gel electrophoresis. The shorter PCR band was gel purified and cloned into T-vectors (Promega, WI). Sequencing results demonstrated a highly conserved sequence of axolotl alpha-TM exon 1 compared to other vertebrates (Fig. 3C). We then designed different primer pairs based on the alpha-TM exon 1b, 2a and 2b sequences (Fig. 3A). Real-time RT-PCR was performed on normal, mutant, MIR sense and antisense RNA-treated mutant embryonic hearts using these primer pairs to compare alpha-TM splicing patterns. Results from these experiments did not support our second hypothesis. That is, the alpha-TM splicing pattern at the 5' end is not regulated by the MIR. Neither ATmC-1 (exon 2b included) nor ATmC-2 (exon 2a included) type splicing is altered with MIR treatment (Fig. 4B1, B2). Similar quantities of splicing products also were observed for fibroblast type tropomyosin with direct exons 1b and 3 conjunctions in all normal, mutant, MIR sense and antisense RNA treated hearts (Fig. 4B3).
Thus these studies reiterate that MIR-promoted tropomyosin expression in the mutant hearts is not due to increased transcription levels or splicing pattern changes in the tropomyosin genes.
Knockdown of MIR expression decreases sarcomeric tropomyosin protein resulting in the failure of myofibril formation in normal hearts
Percentage of beating hearts at different time points after ds RNA transfection.
Day 0 (0 hr)
Day 4 (96 hrs)
Day 9 (216 hrs)
dsRNA treated group
RNase-pretreated dsRNA treated group
Steinberg's solution only group
The dissected normal hearts with mock transfection (no RNA) showed abundant tropomyosin expression and organized myofibrils easily detectable by confocal microscopy even after 9 days in culture (Fig. 6A). Most double-stranded MIR-transfected hearts (22 out of 30 total hearts at stage 37) when dissected stopped beating after 4 days in culture. Careful observation of these hearts under an inverted microscope (× 200) revealed sporadic contractions in portions of the heart tube indicating that these hearts have live tissue. We evaluated the viability of the cells in the organ-cultured hearts by staining the whole hearts with Trypan Blue. Interestingly, 9 out of the 22 ds MIR-transfected hearts that had stopped beating, resumed contraction activity after 6 days in culture although at a decreased beating rate and strength, while the rest remained quiescent for the duration of the experiment (9 days). Confocal microscopy on these hearts that stopped beating and never regained their contractility after 9 days in culture showed a significant disarray in the myofibril structures and decreased levels of tropomyosin protein expression (Fig. 6B), similar to the untreated mutant hearts [7, 21]. No rescuing effect was observed in the mutant hearts transfected by ds RNA and also they showed a negative staining pattern for tropomyosin expression (Fig. 6C). A mock-transfected (no RNA) normal heart showed numerous cells positively stained by tropomyosin antibody, CH-1 (Fig. 6D). Fig. 6E shows a normal heart treated with double-stranded MIR. It clearly showed significantly lower tropomyosin expression than normal levels in the whole heart tube except for the conus region, which showed a few positively stained cells. Results are reminiscent of a similar staining pattern for mutant hearts in our previously published study , with negative staining for tropomyosin in the ventricle but positive staining in the conus region. Since ds RNA could be degraded by Nuclease S1 , we also included a control group of normal hearts transfected with dsRNA predigested with Nuclease S1 (Promega, WI) in our experiments, to determine whether degraded double-stranded RNA has any effect on normal heart beating. Interestingly, after transfection with the degraded double-stranded RNA, these hearts stopped beating temporarily (possibly due to the damaging effects of RNases remaining in the medium) but regained normal beating activity after an additional 3 days in culture. Confocal microscopy showed numerous positively-stained cells in these hearts which appeared similar to untreated normal hearts after 9 days in culture.
In the double-stranded MIR RNA treated normal hearts that stopped beating after 3 or 4 days but regained contractions after 9 days, confocal microscopy studies still revealed decreased staining of tropomyosin protein (Fig. 6F) compared to mock transfected cells (Fig. 6G). Organized myofibrils with tropomyosin staining could be found in a few sparsely distributed cells in the heart although the overall numbers of stained cells were dramatically decreased in the dsRNA-treated hearts (Fig. 6E) compared to the control normal hearts without dsRNA treatment (Fig. 6D). Since our whole-mount heart specimens are usually 150-200 μm in thickness, we used epifluorescence microscopy to view the fluorescence image of the whole heart. Thus we were able to clearly observe the groups of cells that show positive staining in the dsRNA-treated whole hearts (Fig. 6F, G).
These findings strongly suggest that the MIR gene is essential for myofibrillogenesis and heart development in normal embryonic hearts.
The transcription levels of ATmC-1 and 2 (alpha-TM) and ATmC-3 (TM4) genes are not altered by short term but decrease after long term MIR knockdown following double-stranded RNA treatment
However, after collecting RNA samples from hearts organ-cultured for 9 days with either dsRNA or the no RNA controls, we found that both the alpha-tropomyosin and TM4 type tropomyosin decreased in mRNA levels in our real-time RT-PCR assays (Fig. 8). No significant changes in the tropomyosin expression levels were observed in dsRNA-treated hearts compared to the mock-transfected normal hearts (no dsRNA) in alpha-tropomyosin (ATmC-1 and ATmC-2) and TM4 type tropomyosin total RNA transcripts at either 36 hours or 84 hours post-transcription. A confirmation of the effect of double-stranded RNA transfection was shown by down regulation of the endogenous MIR to 1/4th (36 hours) to 1/5th (84 hours) dsRNA transfection (Fig. 8A). Decreased expression levels for both types of tropomyosin have also been detected in the 9-day-cultured hearts compared to the hearts cultured for only 36 or 84 hours.
These results indicate that MIR possibly influences tropomyosin gene expression by an indirect regulatory mechanism. We also showed that decreasing the tropomyosin protein level in normal hearts after double-stranded MIR treatment is not due to changes of alpha-tropomyosin (ATmC-1 and 2) or TM4 tropomyosin (ATmC-3) mRNAs, but rather due to a failed translational or posttranslational control.
The reduced expression of tropomyosin may be related to the differential regulation of MIR of various tropomyosin isoforms in normal and mutant hearts
As shown in Fig. 9, we have observed an isoform switch between embryonic hearts at stage 36 (Fig. 9D) and stage 42 (Fig. 9G). The stage 36 hearts predominantly express isoform 1 while the stage 42 hearts express isoforms 2 and 5. To further confirm the active translational activity for tropomyosin proteins in mutant hearts, we have treated the mutant hearts with the cysteine-protease inhibitor, N-acetyl-leucine-leucine-norleucinal (LLnL, Calbiochem, San Diego, CA). The LLnL is a membrane-permeable proteinase inhibitor that inhibits Calpain and proteosome and has been reported to affect tropomyosin turnover in other cell culture systems . All tropomyosin isoforms, except for No. 1, show significant increases in both normal and mutant hearts after incubating with LLnL for 10 hours. Using another lyosomal cysteine proteinase inhibitor, E-64d (Sigma, St. Louis, WA), which inhibits Calpain but not proteosome, interestingly showed increased expression of all isoforms including No.1 (Fig. 9I). These results suggest that different tropomyosin isoforms are degraded by different proteinases.
To confirm the increased expression level of tropomyosin protein after sense MIR treatment of mutant hearts, we conducted 2D Western blotting experiments using protein samples from mutant hearts treated with sense or antisense MIR for 4 days. (Fig. 9D, H and 9J), show that antisense MIR treatment decreases the amount of tropomyosin isoform 1 in mutant hearts without altering isoforms 3, 4 and 5. A significant increase of isoform 2, one of the major isoforms of tropomyosin in the embryonic heart at stage 42, is also detected. However, an unexpected loss of isoform 5 is observed in the sense MIR-treated mutant heart sample. These results unequivocally prove that MIR post-transcriptionally controls tropomyosin expression in embryonic hearts. In normal and mutant heart samples, irrespective of stage or MIR treatment, isoform 4 is always detectable with negligible alteration in expression, indicating that it probably has a housekeeping function.
MIR promotes expression of myofibril structural protein genes
In summary, there are three categories of myofibril structural genes that respond to the treatment of MIR differently at their mRNA level: 1) genes that can be quickly (36 hours) up-regulated in transcription by MIR sense RNA treatment (α-MHC, C-protein, cTnT and α-syntrophin); 2) genes that can be slowly (72 hours) up-regulated by MIR sense RNA treatment (p53 and Msx-1); and 3) genes that are not affected by MIR treatment (cardiac actin, β-syntrophin and ATmC-1, -2 and -3).
Our research on the MIR gene has been the first to demonstrate that a small RNA is involved in the regulation of embryonic heart development in the cardiac mutant (gene c) of Ambystoma mexicanum. In the case of the MIR gene, since we now know that the MIR is a polyadenylated RNA, there is reason to believe that it may function through its unique secondary structure to promote myofibrillogenesis in the mutant hearts. We favor this hypothesis for the following reasons: First, the RNA used for rescuing experiments (either 650 nt full length or 166 nt clone #4 RNA) was not processed for translation by capping or polyadenylation before it was added to the heart cultures implying that it lacked necessary machinery for translation inside the cells. The possibility that the active RNA rescues mutant hearts by providing mRNA that is translated is unlikely. Second, although there are several small open reading frames (ORF) predicted for the full length gene (the longest ORF is shown in Fig. 1), the shortest RNA we have shown to preserve bioactivity (140 nt with 26 nt deleted from the 3' end of 166 nt Clone #4 sequence shown with an underline in Fig. 1) does not cover the whole ORF . Thus, the chance of this RNA being translated in the cells is virtually nonexistent.
Recently, there have been numerous tissue-specific and embryonic stem cell-expressed microRNAs cloned from mouse, some of which are heart specific [34, 35]. Prior to our finding on the MIR [7, 11] there had been no previously reported non-coding RNAs important for heart development). In fact, the MIR gene appears to be the first non-coding RNA that has been reported to be involved in the process of anterior endoderm inducing precardiac mesoderm to form functional cardiac muscle tissue . Further characterization is underway to rule out the possibility of MIR as being a typical miRNA and/or consider as a piRNA [37–39] or some other unique regulatory RNA molecule.
One of the long term objectives of our studies is to find the mammalian homolog of the MIR gene and study related pathways in mammals, including human. Although some of the noncoding RNAs, such as some micro RNAs, are conserved between species, there are others that have many variations . Based on sequence similarity, we have not yet identified the mammalian MIR homolog gene from a database search although we have preliminary data indicating that both sheep heart  and human heart (our unpublished data) contain functional MIR homologs which are able to promote myofibrillogenesis and rescue the mutant axolotl hearts. Recently, Mummery et al.  have indicated that there exists a very similar, probably identical, induction mechanism for mouse heart development from signals secreted from cultured mouse visceral endoderm-like cells. This factor has been found to be capable of promoting beating cardiomyocyte differentiation and beating in human embryonic stem cell cultures, indicating a non-protein factor secreted from mouse visceral endoderm cells, possibly the mouse homolog of our MIR gene. Thus, these results and findings from our studies in the animal model, Ambystoma mexicanum, suggest that the relationship between endoderm and heart induction is genetically conserved across the vertebrate species.
We have previously demonstrated that the MIR (166 nt core sequence) can bind to more than one protein. The MIR gene and its binding proteins are apparently involved in the regulation of tropomyosin expression . Prior to current studies, it was not clear whether the failure of tropomyosin expression in mutant hearts takes place at the transcriptional level or the translational level and which isoform(s) of tropomyosin is/are significantly reduced in the mutant embryonic hearts. Our results in this study prove unequivocally that the MIR and, perhaps, its binding protein(s) work together to regulate tropomyosin expression translationally or posttranslationally in the mutant hearts since our studies did not detect transcriptional or splicing pattern differences in tropomyosin genes between normal and mutant embryonic hearts. Moreover, sequencing of the full-length cDNAs of both alpha-tropomyosin and ATmC-3 from the embryonic hearts of both normal and mutant axolotls showed no differences reiterating the possible non-existence of splice variants of these genes in mutant hearts.
In addition to its significance for studying the basic mechanisms of myofibrillogenesis, irregularities in tropomyosin expression have also been shown to have clinical significance. There have been a number of reports indicating that familial cardiomyopathy can be caused by mutations in the tropomyosin gene itself [42–44]. Homozygous alpha-TM knockout mice are embryonic lethal . Therefore, the cardiac mutant axolotl, with its deficiency in tropomyosin and its ability to be corrected, is potentially a very important model system for studying regulation of tropomyosin isoforms. It is clear from our analyses of the cardiac lethal mutant axolotl, that gene 'c' does not control early heart morphogenesis since the heart appears to form normally at pre-heartbeat stages . However, the expression of tropomyosin is significantly reduced at the heartbeat stage (stage 35) . Moreover, fewer isoforms of tropomyosin are detectable in embryonic mutant hearts by two-dimensional gel electrophoresis as compared to normal hearts . This tropomyosin deficiency is intriguing given the current understanding of tropomyosin genetics and expression [16, 17, 25, 44, 48]. Despite these numerous studies, the mechanisms of tropomyosin gene regulation in cardiac tissues are not completely understood.
In addition to the identification of tissue specific transcription factors that regulate different tropomyosin gene transcription and specific intron/exon splicing regulatory sequences and factors that control alternative splicing, there are numerous recent findings that show both translational and posttranslational (sorting and protein turnover) control on tropomyosin proteins. For example, Rethinasamy et al.  have shown that translational regulation plays a major role in tropomyosin expression. In heterozygous knockout mouse hearts with a 50% reduction in cardiac muscle α-TM mRNA, no compensatory increase in transcript levels were found for striated muscle β-TM or TM-30 isoforms. However, normal amounts of striated muscle α-TM protein are produced and integrated into the myofibril, suggesting a mechanism for adjusting translational levels in functioning mouse hearts.
Besides the sorting mechanism for specific tropomyosin isoform subcellular localization, proteinase degradation is another important regulatory mechanism in the posttranslational control of tropomyosin. In non-muscle normal rat kidney (NRK) cells, it has been reported that large molecular weight tropomyosin proteins are degraded faster than smaller molecular weight tropomyosin proteins indicating different proteinases are involved in their proteolysis . The stress fiber component tropomyosin degradation in normal cells or under growth factor treatment can be blocked by LLnL, a proteinase inhibitor to lysosomal cathepsins B and L, cytoplasmic calpains I and II  and proteasomes. However, using inhibitors that block calpains but not proteasomes does not block TM degradation . These results indicate that striated muscle myofibril structural tropomyosins, stress-fiber high molecular weight tropomyosins and small molecular weight non-muscle tropomyosins are degraded by different proteinases within the cell. In our studies using axolotl heart tissue, we have also shown that LLnL can prevent degradation of some striated muscle tropomyosin proteins (CH1 antibody recognizable) but not all, especially isoform number 1 that has increased expression along with heart development but has not been protected from the degradation by LLnL. Another Proteinase inhibitor, E-64d, inhibits Calpain activities but not proteosome activites and thus protects a different subset of tropomyosin isoforms including isoform number 1 in the embryonic hearts.
In our mutant axolotl system, the decreased translational level of tropomyosin protein, abnormal tropomyosin sorting and significantly higher rates of protein degradation of the tropomyosin protein could all exist as a potential foundation for this mutant phenotype. However, recent studies on mutant hearts with normal ATmC-1, ATmC-2 and ATmC-3 tropomyosin cDNA transfected constructs, clearly show reorganization of myofibril structures, indicating the possible existence of a sorting mechanism in mutant cardiomyocytes [20, 51].
A mechanism whereby the MIR enters the mutant heart cells, is transported into the nucleus, perhaps together with its binding protein(s) , and promotes gene transcription of the various myofibril components. The MIR could as well regulate RNA splicing processes for these genes as indicated in our studies on cardiac troponin T . The myofibrillogenesis is thus promoted with increased expression of building blocks of myofibrillar proteins. While the nascent myofibrillar structures may incorporate tropomyosin proteins and protect them from being degraded in MIR treated hearts, it is possible that those proteins, existing in unprotected monomer form in the untreated hearts, get degraded by unknown proteinase(s).
A second possibility might be that MIR and its binding proteins promote gene expression followed by translation of protein products that facilitate the translation of the mRNA of tropomyosin and possibly others, thus providing the essential building blocks for myofibrillogenesis. It is very unlikely that MIR and its binding proteins directly promote tropomyosin translation, since it takes 3-4 days after MIR transfection before increased tropomyosin expression and myofibril formation is observed in the mutant heart cells.
Recent studies show that short double-stranded RNA duplexes trigger post-transcriptional gene silencing and can also induce epigenetic silencing of genes at the level of transcription . They can also interact at promoter regions and can activate or repress gene expression  or affect translation without affecting transcription .
While studies on siRNAs and miRNAs were extensively conducted in a wide variety of systems, comparatively, no remarkable studies were reported on small RNAs especially those that are similar to MIR. Recently, Makarev et al.  identified several miRNAs and small RNAs from adult newt eye, 42 of which have no similarity with known miRNAs or piRNAs. Our studies also clearly suggest that our MIR has no sequence homology with any of these known RNAs. Furthermore, none of the known small RNAs, to our knowledge, have been shown to regulate myofibrillogenesis similar to MIR. However, miRNAs on the other hand have been implicated as regulators of transcription as well as translation in a wide variety of systems [54, 56].
Although such reports indicate the regulatory role of different small RNAs at the transcription and/or translational levels, the underlying molecular mechanisms, however, are still poorly understood. Whatever the final mechanism of action of MIR turns out to be, it is very clear that MIR promotes tropomyosin synthesis and myofibrillogenesis in the mutant hearts and is essential for tropomyosin expression and myofibrillogenesis in normal hearts. We are conducting several experiments to isolate functional mouse/human homologues of MIR for further characterization. We assume also that MIR, or an MIR-type functional homologue, is involved in cardiomyocyte precursor cell differentiation in all vertebrate species.
This study was supported by NIH grant HL061246 and by a Christine E. Lynn American Heart Association Grant-in-Aid to L.F.L. Some of the embryos used for this study were purchased from the Axolotl Colony at the University of Kentucky (NSF-DBI-0443496).
The content of this publication is solely the responsibility of the authors and does not necessarily represent the official views of the National Heart, Lung and Blood Institute or the National Institutes of Health.
- Humphrey RR: Genetic and experimental studies on a mutant gene (c) determining absence of heart action in embryos of the Mexican axolotl (Ambystoma mexicanum). Dev Biol. 1972, 27: 365-375. 10.1016/0012-1606(72)90175-3.View ArticlePubMedGoogle Scholar
- Lemanski LF: Role of tropomyosin in actin filament formation in embryonic salamander heart cells. J Cell Biol. 1979, 82: 227-238. 10.1083/jcb.82.1.227.View ArticlePubMedGoogle Scholar
- Moore PB, Lemanski LF: Quantitation of tropomyosin by radioimmunoassay in hearts of cardiac mutant axolotls, Ambystoma mexicanum. J Musc Res And Cell Motil. 1982, 3: 161-167. 10.1007/BF00711940.View ArticleGoogle Scholar
- Starr CM, Diaz JG, Lemanski LF: Analysis of actin and tropomyosin in hearts of cardiac mutant axolotls by two-dimensional gel electrophoresis, western blots, and immunofluorescent microscopy. J Morphol. 1989, 201: 1-10. 10.1002/jmor.1052010102.View ArticlePubMedGoogle Scholar
- LaFrance SM, Lemanski LF: Imunofluorescent confocal analysis of tropomyosin in developing hearts of normal and cardiac mutant axolotls. Int J Devel Biol. 1994, 38: 695-700.Google Scholar
- Zajdel RW, Zhu Y, Fransen ME, Lemanski LF: A primary cell culture model for defective cardiac myofibrillogenesis in Mexican axolotl embryos. In Vitro Cell Dev Biol Anim. 1997, 33: 677-680. 10.1007/s11626-997-0124-0.View ArticlePubMedGoogle Scholar
- Zhang C, Dube DK, Huang X, Zajdel RW, Bhatia R, Foster D, Lemanski SL, Lemanski LF: A point mutation in bioactive RNA results in the failure of mutant heart correction in Mexican axolotls. Anat Embryol. 2003, 206: 495-506.PubMedGoogle Scholar
- Lemanski LF, Mooseker MS, Peachey LD, Iyengar MR: Studies of muscle proteins in embryonic myocardial cells of cardiac lethal mutant mexican axolotls (Ambystoma mexicanum) by use of heavy meromyosin binding and sodium dodecyl sulfate polyacrylamide gel electrophoresis. J Cell Biol. 1976, 68: 375-388. 10.1083/jcb.68.2.375.View ArticlePubMedGoogle Scholar
- Erginel-Unaltuna N, Dube DK, Lemanski LF: Protein synthesis during heart development in normal and cardiac mutant axolotls. Axol Newsletter. 1994, 23: 48-60.Google Scholar
- Ward SM, Dube DK, Fransen ME, Lemanski LF: Differential expression of C-protein isoforms in the developing heart of normal and cardiac lethal mutant axolotls (Ambystoma mexicanum). Dev Dyn. 1996, 205: 93-103. 10.1002/(SICI)1097-0177(199602)205:2<93::AID-AJA1>3.0.CO;2-Z.View ArticlePubMedGoogle Scholar
- Lemanski LF, Nakatsugawa M, Bhatia R, Erginel-Unaltuna N, Spinner BJ, Dube DK: A specific synthetic RNA promotes cardiac myofibrillogenesis in the Mexican axolotl. Biochem Biophys Res Commun. 1996, 229: 974-981. 10.1006/bbrc.1996.1910.View ArticlePubMedGoogle Scholar
- Hook J, Lemckert F, Qin H, Schevzov G, Gunning P: Gamma tropomyosin gene products are required for embryonic development. Mol Cell Biol. 2004, 24: 2318-2323. 10.1128/MCB.24.6.2318-2323.2004.PubMed CentralView ArticlePubMedGoogle Scholar
- Vlahovich N, Schevzov G, Nair-Shaliker V, Ilkovski B, Artap ST, Joya JE, Kee AJ, North KN, Gunning PW, Hardeman EC: Tropomyosin 4 defines novel filaments in skeletal muscle associated with muscle remodeling/regeneration in normal and diseased muscle. Cell Motil Cytoskeleton. 2008, 65: 73-85. 10.1002/cm.20245.View ArticlePubMedGoogle Scholar
- Zhao L, Zhao X, Tian T, Lu Q, Skrbo-Larssen N, Wu D, Kuang Z, Zheng X, Han Y, Yang S, Zhang C, Meng A: Heart-specific isoform of tropomyosin4 is essential for heartbeat in zebrafish embryos. Cardiovasc Res. 2008, 80: 200-208. 10.1093/cvr/cvn177.View ArticlePubMedGoogle Scholar
- Grenklo S, Hillberg L, Rathje LZ, Pinaev G, Schutt CE, Lindberg U: Tropomyosin assembly intermediates in the control of microfilament system turnover. Eur J Cell Biol. 2008, 87: 905-920. 10.1016/j.ejcb.2008.06.006.View ArticlePubMedGoogle Scholar
- Muthuchamy M, Boivin GP, Grupp IL, Wieczorek DF: Beta-tropomyosin overexpression induces severe cardiac abnormalities. J Mol Cell Cardiol. 1998, 30: 1545-1557. 10.1006/jmcc.1998.0720.View ArticlePubMedGoogle Scholar
- Hardy S, Theze N, Lepetit D, Allo MR, Thiebaud P: The Xenopus laevis TM-4 gene encodes non-muscle and cardiac tropomyosin isoforms through alternative splicing. Gene. 1995, 156: 265-270. 10.1016/0378-1119(94)00929-M.View ArticlePubMedGoogle Scholar
- Luque EA, Spinner BJ, Dube S, Dube DK, Lemanski LF: Differential expression of a novel isoform of alpha-tropomyosin in cardiac and skeletal muscle of the Mexican axolotl (Ambystoma mexicanum). Gene. 1997, 185: 175-180. 10.1016/S0378-1119(96)00606-3.View ArticlePubMedGoogle Scholar
- Spinner BJ, Zajdel RW, McLean MD, Denz CR, Dube S, Mehta S, Choudhury A, Nakatsugawa M, Dobbins N, Lemanski LF, Dube DK: Characterization of a TM-4 type tropomyosin that is essential for myofibrillogenesis and contractile activity in embryonic hearts of the Mexican axolotl. J Cell Biochem. 2002, 85: 747-761. 10.1002/jcb.10178.View ArticlePubMedGoogle Scholar
- Zajdel RW, McLean MD, Lemanski SL, Muthuchamy M, Wieczorek DF, Lemanski LF, Dube DK: Ectopic expression of tropomyosin promotes myofibrillogenesis in mutant axolotl hearts. Dev Dyn. 1998, 213: 412-420. 10.1002/(SICI)1097-0177(199812)213:4<412::AID-AJA6>3.0.CO;2-C.View ArticlePubMedGoogle Scholar
- Zajdel RW, McLean MD, Isitmangil G, Lemanski LF, Wieczorek DF, Dube DK: Alternation of cardiac myofibrillogenesis by liposome-mediated delivery of exogenous proteins and nucleic acids into whole embryonic hearts. Anat Embryol. 2000, 201: 217-228. 10.1007/s004290050312.View ArticlePubMedGoogle Scholar
- Jia P, Zhang C, Huang XP, Poda M, Akbas F, Lemanski SL, Erginel-Unaltuna N, Lemanski LF: A novel protein involoved in heart development in Ambystoma Mexicanum is localized in endoplasmic reticulum. J Biomed Sci. 2008, 15: 789-799. 10.1007/s11373-008-9262-y.View ArticlePubMedGoogle Scholar
- Sferrazza GF, Zhang C, Jia P, Athauda G, Dube S, Lemanski SL, Dube DK, Lemanski LF: Role of Myofibril-Inducing RNA in cardiac TnT expression in developing Mexican axolotl. Biochem Biophys Res Com. 2007, 357: 32-37. 10.1016/j.bbrc.2007.03.064.PubMed CentralView ArticlePubMedGoogle Scholar
- Cho YJ, Hitchcock-DeGregori SE: Relationship between alternatively spliced exons and functional domains in tropomyosin. Proc Natl Acad Sci USA. 1991, 88: 10153-10157. 10.1073/pnas.88.22.10153.PubMed CentralView ArticlePubMedGoogle Scholar
- Helfman DM, Berthier C, Grossman J, Leu M, Ehler E, Perriard E, Perriard JC: Non-muscle tropomyosin-4 requires coexpression with other low molecular weight isoforms for binding to thin filaments in cardiomyocytes. J Cell Sci. 1999, 112: 371-380.PubMedGoogle Scholar
- Goodwin LO, Lees-Miller JP, Leonard MA, Cheley SB, Helfman DM: Four fibroblast tropomyosin isoforms are expressed from the rat alpha-tropomyosin gene via alternative RNA splicing and the use of two promoters. J Biol Chem. 1991, 266: 8408-8415.PubMedGoogle Scholar
- Lin JJ, Chou CS, Lin JL: Monoclonal antibodies against chicken tropomyosin isoforms: production, characterization, and application. Hybridoma. 1985, 4: 223-242. 10.1089/hyb.1985.4.223.View ArticlePubMedGoogle Scholar
- Vogt VM: Purification and further properties of single-strand-specific nuclease from Aspergillus oryzae. Eur J Biochem. 1973, 33: 192-200. 10.1111/j.1432-1033.1973.tb02669.x.View ArticlePubMedGoogle Scholar
- Fransen MF, Lemanski LF: Epicardial development in the axolotl, Ambystoma mexicanum. Anat Rec. 1990, 226: 228-236. 10.1002/ar.1092260212.View ArticlePubMedGoogle Scholar
- Lin JJ, Lin JL: Assembly of different isoforms of actin and tropomyosin into the skeletal tropomyosin-enriched microfilaments during differentiation of muscle cells in vitro. J Cell Biol. 1986, 103: 2173-2183. 10.1083/jcb.103.6.2173.View ArticlePubMedGoogle Scholar
- Warren RH: TGF-alpha-induced breakdown of stress fibers and degradation of tropomyosin in NRK cells is blocked by a proteasome inhibitor. Exp Cell Res. 1997, 236: 294-303. 10.1006/excr.1997.3728.View ArticlePubMedGoogle Scholar
- Ujfalusi Z, Vig A, Hild G, Nyitrai M: The effect of topomyosin on formin-bound actin filaments. Biophys J. 2009, 96: 162-168. 10.1529/biophysj.108.138420.PubMed CentralView ArticlePubMedGoogle Scholar
- Lemanski LF, Zajdel RW, Nakasugawa M, Bhatia R, Spinner BJ, Fransen ME, Gaur AF, McLean MD, Lemanski SL, Dube DK: Molecular biology of heart development in the Mexican axolotl, Ambystoma mexicanum. Tsitologiia. 1997, 39: 918-927.PubMedGoogle Scholar
- Lagos-Quintana M, Rauhut R, Yalcin A, Meyer J, Lendeckel W, Tuschl T: Identification of tissue-specific microRNAs from mouse. Curr Biol. 2002, 12: 735-739. 10.1016/S0960-9822(02)00809-6.View ArticlePubMedGoogle Scholar
- Houbaviy HB, Murray MF, Sharp PA: Embryonic stem cell-specific MicroRNAs. Dev Cell. 2003, 5: 351-358. 10.1016/S1534-5807(03)00227-2.View ArticlePubMedGoogle Scholar
- Thum T, Catalucci D, Bauersachs J: MicroRNAs: novel regulators in cardiac development and disease. Cardiovasc Res. 2008, 79: 562-570. 10.1093/cvr/cvn137.View ArticlePubMedGoogle Scholar
- Zucker M: Mfold web server for nucleic acid folding and hybridization prediction. Nucleic Acids Res. 2003, 31: 3406-3415. 10.1093/nar/gkg595.View ArticleGoogle Scholar
- Grivna ST, Beyret E, Wang Z, Lin H: A novel class of small RNAs in mouse spermatogenic cells. Genes Dev. 2006, 20: 1709-1714. 10.1101/gad.1434406.PubMed CentralView ArticlePubMedGoogle Scholar
- O'Donnell KA, Boeke JD: Mighty piwis defend the germline against genome intruders. Cell. 2007, 129: 37-44. 10.1016/j.cell.2007.03.028.PubMed CentralView ArticlePubMedGoogle Scholar
- Sempere LF, Sokol NS, Dubrovsky EB, Berger EM, Ambros V: Temporal regulation of microRNA expression in Drosophila melanogaster mediated by hormonal signals and broad-Complex gene activity. Dev Biol. 2003, 259: 9-18. 10.1016/S0012-1606(03)00208-2.View ArticlePubMedGoogle Scholar
- Mummery C, Oostwaard DW, Doevendans P, Spijker R, Brink van den S, Hassink R, Heyden van der M, Opthof T, Pera M, de la Riviere AB, Passier R, Tertoolen L: Differentiation of human embryonic stem cells to cardiomyocytes: role of coculture with visceral endoderm-like cells. Circulation. 2003, 107: 2733-2740. 10.1161/01.CIR.0000068356.38592.68.View ArticlePubMedGoogle Scholar
- Watkins H, Anan R, Coviello DA, Spirito P, Seidman JG, Seidman CE: A de novo mutation in alpha-tropomyosin that causes hypertrophic cardiomyopathy. Circulation. 1995, 91: 2302-2305.View ArticlePubMedGoogle Scholar
- Bing W, Redwood CS, Purcell IF, Esposito G, Watkins H, Marston SB: Effects of two hypertrophic cardiomyopathy mutations in alpha-tropomyosin, Asp175Asn and Glu180Gly, on Ca2+ regulation of thin filament motility. Biochem Biophys Res Commun. 1997, 236: 760-764. 10.1006/bbrc.1997.7045.View ArticlePubMedGoogle Scholar
- Prabhakar R, Boivin GP, Grupp IL, Hoit B, Arteaga G, Solaro JR, Wieczorek DF: A familial hypertrophic cardiomyopathy alpha-tropomyosin mutation causes severe cardiac hypertrophy and death in mice. J Mol Cell Cardiol. 2001, 33: 1815-1828. 10.1006/jmcc.2001.1445.View ArticlePubMedGoogle Scholar
- Rethinasamy PM, Muthuchamy M, Hewett T, Arteaga G, Solaro JR, Wieczorek DF: Molecular and physiological effects of alpha-tropomyosin ablation in the mouse. Circ Res. 1998, 82: 116-123.View ArticlePubMedGoogle Scholar
- Fransen MF, Lemanski LF: Myocardial cell relationships during morphogenesis in normal and cardiac lethal mutant axolotls, Ambystoma mexicanum. Am J Anat. 1988, 183: 245-257. 10.1002/aja.1001830307.View ArticlePubMedGoogle Scholar
- Lemanski LF, LaFrance SM, Erginel-Unaltuna N, Luque EA, Ward SM, Fransen ME, Mangiacapra FJ, Nakatsugawa M, Lemanski SL, Capone RB, Goggins KJ, Nash BP, Bhatia R, Dube A, Gaur A, Zajdel RW, Zhu Y, Spinner BJ, Pietras KM, Lemanski SF, Kovacs CP, VanArsdale X, Lemanski JL, Dube DK: The cardiac mutant gene c in axolotls: cellular, developmental, and molecular studies. Cell Mol Biol Res. 1995, 41: 293-305.PubMedGoogle Scholar
- Gromak N, Rideau A, Southby J, Scadden AD, Gooding C, Hüttelmaier S, Singer RH, Smith CW: The PTB interacting protein raver1 regulates alpha-tropomyosin alternative splicing. EMBO J. 2003, 22: 6356-6364. 10.1093/emboj/cdg609.PubMed CentralView ArticlePubMedGoogle Scholar
- Sasaki T, Kishi M, Saito M, Tanaka T, Higuchi N, Kominami E, Katunuma N, Murachi T: Inhibitory effect of di- and tripeptidyl aldehydes on calpains and cathepsins. J Enzyme Inhib. 1990, 3: 195-201. 10.3109/14756369009035837.View ArticlePubMedGoogle Scholar
- Rock KL, Gramm C, Rothstein L, Clark K, Stein R, Dick L, Hwang D, Goldberg AL: Inhibitors of the proteasome block the degradation of most cell proteins and the generation of peptides presented on MHC class I molecules. Cell. 1994, 78: 761-771. 10.1016/S0092-8674(94)90462-6.View ArticlePubMedGoogle Scholar
- Denz CR, Narshi A, Zajdel RW, Dube DK: Expression of a novel cardiac-specific tropomyosin isoform in humans. Biochem Biophys Res Commun. 2004, 320: 1291-1297. 10.1016/j.bbrc.2004.06.084.View ArticlePubMedGoogle Scholar
- Papenfort K, Vogel J: Multiple target regulation by small noncoding RNAs rewires gene expression at the post-transcriptional level. Res Microbiol. 2009, 160: 278-287. 10.1016/j.resmic.2009.03.004.View ArticlePubMedGoogle Scholar
- Janowski BA, Younger ST, Hardy DB, Ram R, Huffman KE, Corey DR: Activating gene expression in mammalian cells with promoter-targeted duplex RNAs. Nature Chem Biol. 2007, 3: 166-173. 10.1038/nchembio860.View ArticleGoogle Scholar
- Zhu S, Si M, Wu H, Mo Y: MicroRNA-21 Targets the Tumor Suppressor Gene Tropomyosin 1 (TPM1). J Biol Chem. 2007, 282: 14328-14336. 10.1074/jbc.M611393200.View ArticlePubMedGoogle Scholar
- Makarev E, Spence JR, Del Rio-Tsonis K, Tsonis PA: Identification of microRNAs and other small RNAs from the adult newt eye. Mol Vision. 2006, 12: 1386-1391.Google Scholar
- Luo X, Lin H, Pan Z, Xiao J, Zhang Y, Lu Y, Yang B, Wang Z: Down-regulation of miR-1/miR-133 Contributes to Re-expression of Pacemaker Channel Genes HCN2 and HCN4 in Hypertrophic Heart. J Biol Chem. 2008, 283: 20045-20052. 10.1074/jbc.M801035200.View ArticlePubMedGoogle Scholar
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