|Home | About | Journals | Submit | Contact Us | Français|
Transcription factors from the MADS-box family play a relevant role in cell differentiation and development and include the animal SRF (serum response factor) and MEF2 (myocyte enhancer factor 2) proteins. The social amoeba Dictyostelium discoideum contains four genes coding for MADS-box transcription factors, two of these genes code for proteins that are more similar to SRF, and the other two code for proteins that are more similar to MEF2 animal factors.
The biological function of one of the two genes that codes for MEF2-related proteins, a gene known as mef2A, is described in this article. This gene is expressed under the transcriptional control of two alternative promoters in growing cells, and its expression is induced during development in prespore cells. Mutant strains where the mef2A gene has been partially deleted were generated to study its biological function. The mutant strains showed reduced growth when feeding on bacteria and were able to develop and form fruiting bodies, but spore production was significantly reduced. A study of developmental markers showed that prespore cells differentiation was impaired in the mutant strains. When mutant and wild-type cells were set to develop in chimeras, mutant spores were underrepresented in the fruiting bodies. The mutant cells were also unable to form spores in vitro. In addition, mutant cells also showed a poor contribution to the formation of the tip-organizer and the upper region of slugs and culminant structures. In agreement with these observations, a comparison of the genes transcribed by mutant and wild-type strains during development indicated that prestalk gene expression was enhanced, while prespore gene expression decreased in the mef2A- strain.
Our data shows that mef2A plays a role in cell differentiation in D. discoideum and modulates the expression of prespore and prestalk genes.
Mef-2-related transcription factors belong to a family of proteins that are present in all eukaryotic organisms [1,2]. These proteins share a very conserved DNA-binding and protein-dimerization domain, the MADS-box, named after the transcription factors MCM1 (from yeast), Agamous, Deficiens (from plants) and SRF (from animals) [3,4]. Two subfamilies of MADS-box transcription factors have been defined according to the MADS-box sequence: type I and type II . Plants have a large number of types I and II MADS-box proteins while other organisms, such as fungi and animals, usually have one or more proteins of each subfamily . Animals, for example, have only one type I protein (serum response factor [SRF]) and four type II proteins (myocyte enhancer factor 2 A-D [Mef2 A-D]). The two types of factors recognize different A/T rich binding sites. SRF and related factors recognize the consensus sequence CC(A/T)6GG [7,8], while Mef-2-related factors recognize the CTA(A/T)4TAG consensus sequence .
MADS-box transcription factors accomplish various biological functions. In plants, they are critically involved in floral formation and development . In yeasts, MCM1 participates in the regulation of pheromone expression, metabolism  and DNA replication . In animals, these transcription factors are mainly involved in the regulation of cell-differentiation processes. SRF deletion is lethal in mice because cells are impaired in cell adhesion and migration , and the embryo cannot complete gastrulation . Tissue-specific deletion has shown that SRF is also required for terminal differentiation of skeletal, cardiac and smooth muscle cells and for neural cell migration . Additional studies have demonstrated that SRF regulates the expression of a large number of genes coding for actin-cytoskeleton-related proteins [15,16].
Mef-2 proteins are involved in regulating the expression of muscle-specific genes, both in Drosophila and in mammals , in collaboration with MyoD-related transcription factors . In mammals, there are four genes coding for very similar Mef-2 factors that appear to functionally complement each other, at least partially (Mef2A-D) . However, Mef2C-null mice die early in their development due to cardiovascular abnormalities , and Mef2A-null mice die perinatally from heart defects . In addition, numerous studies have shown that Mef-2 factors are also involved in the differentiation of several other cell types, such as neural crest cells, endothelial cells, chondrocytes, neurons and lymphocytes [23,24].
Our group has approached the functional study of MADS-box transcription factors in the social amoeba Dictyostelium discoideum. These unicellular organisms live in forest soils, feeding on bacteria and other microorganisms and are able to develop as multicellular organisms under starvation conditions. In such conditions, up to 105 individual amoebas aggregate to form a fruiting body composed of a basal disk, stalk and sorus where up to 80% of the original amoeba differentiate into resistant forms called spores [25-27]. The initial step is the aggregation of the cells towards cAMP-secreting centers to form a mound. Cells within the aggregates initiate a differentiation process to form two main cell types: prestalk and prespore. Prestalk cells migrate to the top of the mound, emerging as a tip. A culmination process is later initiated by the migration of prestalk cells from the tip towards the substrate through the mass of prespore cells, piling up and terminally differentiating to form the stalk. The mass of prespore cells remains attached to the top of the forming stalk, rising from the substrate until culmination is completed. Migratory structures, called slugs, can be formed before culmination under adverse environmental conditions. In this case, the slugs migrate towards warmer and lighter places for culmination to facilitate the dissemination of the spores. By the end of culmination, prespore cells differentiate inside the sorus to form mature spores.
Analysis of the D. discoideum genome has shown that it contains four genes coding for MADS-box transcription factors, namely srfA, B, C and D. Previous studies in our laboratory have shown that srfA is required for the proper development of the fruiting body, including the slug migration and culmination steps, and is essential for spore terminal differentiation [28,29]. The srfB gene is expressed earlier than srfA during development, and the encoded protein is involved in the initiation of the developmental process, cell migration and the initiation of culmination . The functional study of the srfC gene is described in this article. We present evidence demonstrating that srfC is more similar to animal Mef-2 genes and propose naming it mef2A. By analyzing the phenotype of mutant strains and gene expression levels during development, we clearly show that this protein is involved in D. discoideum development and, in particular, in the differentiation of prespore cells and one group of prestalk cells.
The analysis of the D. discoideum genome identified four genes coding for proteins with regions similar to the MADS-box domain. These genes were named srfA, B, C and D. The putative MADS-box region of the proteins encoded by these genes was analyzed in more detail and compared to that of vertebrates (H. sapiens, G. gallus, X. laevis), invertebrates (D. melanogaster, A. franciscana), amoeba (E. histolytica) and fungi (S. cerevisiae) type I (SRF, MCM1, ARG1) and type II (Mef2) proteins. Amino acid sequences were aligned using the ClustalW and ClustalX programs (Additional file 1: Figure S1). The multiple alignments were used to calculate the phylogenetic tree shown in Figure1. The results indicate that the D. discoideum genes srfA and srfB code for proteins that are more similar to type I genes, such as the animal SRF gene, than to type II genes, such as Mef2. D. discoideum SrfA and SrfB appear to form a monophyletic group that more closely resembles to animal proteins than to fungi proteins. In contrast, the proteins encoded by D. discoideum srfC and srfD are more similar to animal MEF2 than to SRF proteins. In this case, the protein encoded by srfC is more closely related to that of the amoeba E. histolytica and is also more similar to animal Mef2 proteins than to SrfD. In fact, SrfD appears to have diverged significantly from the other type II proteins analyzed. The results of this analysis centered our attention on srfC, which we propose to rename as mef2A, a name that we will use throughout the rest of the article.
The expression of mef2A during vegetative growth and development was analyzed by RT-PCR, and the results are shown in Figure2A. Expression was detected in growing cells (time 0 in Figure2A), but a large induction was observed at 4 hours of development, an induction that was maintained at later developmental stages. The promoter region of the gene was characterized to further determine the temporal and spatial patterns of expression. Primer-extension experiments were performed using the RACE (rapid amplification of cDNA ends) technique. The data indicated the existence of one intron in the 5′ UTR and two regions of transcription initiation (Additional file 1: Figure S2) [GenBank:KC852901]. The gene structure diagram, which includes the 5′ untranslated region (UTR) and the transcription initiation sites, is shown in Figure2B. The more upstream transcription initiation sites of each region are located at nucleotides −144 and −814, respectively. The first intron is located in the 5′ UTR of one of the two transcribed mRNAs (nucleotides −536 to −371, in relation to the A of the initiation codon). The data obtained from the experiments also enabled us to define the limits of the second intron, located between the first (A) and second nucleotide (T) of the translation initiation codon.
The transcriptional activity of both promoters was analyzed by the use of reporter vectors where Promoter 1 (Pr1), Promoter 2 (Pr2) or the complete promoter region (cPr) were cloned, thereby driving lacZ expression. Pools of transformed cells obtained for each promoter were analyzed for β-galactosidase activity. Promoter 1 drove lacZ expression in scattered cells at the mound and finger stages of development, but its activity markedly increased in the prespore region of slug, Mexican-hat and culminant structures (Figure2C). Promoter 2 was active in scattered cells of aggregates and fingers, but the activity decreased almost completely at later developmental stages, except for a few cells in the basal disk of culminant structures. The activity of the complete promoter showed the sum of Pr1 and Pr2 and was maximal in the prespore region of developing structures.
The study of the biological function of mef2A was approached through the generation of mutant strains where the gene was partially deleted by homologous recombination. The deleted region included the first two exons, coding for the 5′ untranslated region of the gene, and the third exon, coding for the N-terminal region of the protein, including the MADS-box domain (Figure2B). Several mutant clones were isolated on two different backgrounds, the AX2 and AX4 D. discoideum axenic strains. Figure3A shows the RT-PCR analyses demonstrating mef2A gene deletion in one AX4-derived clone (37) and two AX2-derived clones (2, 3). Later results show no evidence of any transcription of the remaining coding DNA of this gene (Gene Expression profile of mef2A mutant cells Subsection). The mef2A- deleted strains grew more slowly than the wild type strains when feeding on bacteria (Figure3B), although no difference in growth was observed in the axenic culture (data not shown).
The mutant strains completed development under starvation conditions at the same time as the wild-type strains, but several differences were observed during the process, as shown in Figure3C. Both the mutant and wild-type strains formed streams during aggregation, but the streams of the mutant strain appeared more fragmented than those of the wild-type strains, forming more heterogeneous and smaller mounds. Subsequently, the mutant strains formed fewer slugs, which were smaller and migrated shorter distances than those formed by the wild-type strains. Finally, the mutant strains formed more culminant structures that were more heterogeneous in size than those of the wild-type strains. The number of spores formed by each strain was quantified, and the mutant strains produced about half the number of spores formed by the wild-type strains (Table1). However, the viability of the mature spores was similar for the mutant and wild-type strains.
The developmental phenotype of the mutant was further characterized by studying the expression of cell-type specific marker genes. AX4 and mef2A- mutant cells were transfected with reporter vectors that drive lacZ expression under the control of the ecmA and ecmB prestalk gene promoters or the pspA prespore gene promoter. The lacZ expression was analyzed at the finger, slug and mid-culminant stages of development (Figure4). The ecmA gene promoter is active in the anterior, prestalk region of finger and slug structures (PstA region) and in the stalk, upper and lower cups and basal disk of wild-type structures. The activity was detected in the same regions in mef2A- mutants, but the anterior prestalk region was larger in the fingers. A quantification of the relative size of the PstA prestalk region indicated that it represented 23.45% (standard deviation: 5.27%) of the finger length in AX4 structures and 31.16% (SD 6.62%) in the mef2A- mutants, difference that is statistically significant (p<0,001 according to the student’s test). In addition, ecmA promoter activity was more extended and diffuse in the mutant slugs. ecmB promoter activity in the anterior prestalk region of mound and slug structures is more restricted than that of the ecmA promoter and is mainly located in the tip organizer region, as well as in a number of cells scattered around the posterior regions, i.e., the anterior-like cells . In culminant structures, the ecmB promoter is active in the stalk. The mutant strains showed an extended region of ecmB promoter activity in the finger structures. In the slug structures, ecmB-expressing cells were more disperse in the mutant strains, and no well-defined tip organizer region was observed. The pspA prespore promoter presented a pattern of activity opposite to that of the ecmA promoter. In the fingers, the pspA promoter was active in the posterior, prespore region. The quantification of the pspA prespore region indicated that it is shorter in mef2A- mutants (61.32%, SD 9.2%) than in AX4 structures (70.92%, SD 7.52%)(p<0,001). In the culminant structures, pspA was active in the sorus. The mef2A mutants showed reduced pspA promoter activity, especially in the slugs where no well-defined prespore region was observed (Figure4). In the culminant structures, the mutant sori were thinner than the wild-type sori.
The differences observed could be due to the participation of Mef2A in the process of prespore differentiation but could also be due to defective inter-cellular signaling in the mutant structures. We designed a developmental analysis of mixtures of the mutant and wild-type cells to discriminate between these two possibilities. In these experiments, we transfected wild-type and mutant cells with a reporter vector that would express lacZ upon differentiation of the cells to prestalk (ecmB::lacZ) or prespore (pspA::lacZ) cells. The transfected cells were mixed with non-transfected cells in a 1:4 proportion and allowed to develop. If the mef2A- mutant cells were defective in generating the intercellular signals required for cell differentiation, their mixture with wild-type cells would provide the defective signal and induce correct differentiation of the mutant cells. Alternatively, if the mef2A- mutant cells were defective in the process of cell differentiation, the presence of wild-type cells would not compensate for their differentiation defect. Therefore, wild-type and mutant cells expressing lacZ from the prestalk-specific ecmB promoter or the prespore-specific pspA promoter were mixed with unlabeled cells and allowed to develop. The slugs and early culminant structures were analyzed for lacZ expression, the results of which are shown in Figure5. The expected distribution of ecmB-expressing cells can be observed in the AX4/AX4-lacZ samples. The ecmB-expressing cells are located in the tip-organizer region of the slugs, as well as scattered in their posterior region. In culminant structures, ecmB is expressed in the stalk (including the tip) and in the upper and lower- cup regions. The mixture of mef2A- mutant labeled and unlabeled cells showed a staining pattern similar to that shown in Figure4 for ecmB::lacZ-expressing mutant cells. When the ecmB-expressing mef2A- cells were mixed with the wild-type cells, no lacZ expression was detected in the tip organizer region in the slugs or in the tip of the culminant structures, indicating that the mef2A- cells were excluded from these regions. As expected, AX4-ecmB::lacZ cells were found in these regions when mixed with mef2A- cells, indicating that mef2A might be required for prestalk cell differentiation at the tip-organizer region.
The results obtained using pspA::lacZ as a cell marker are shown in the lower panel of Figure5. Homogeneous mixtures of AX4/AX4 and mef2A- mutant/mef2A- mutant cells presented the same pattern of staining shown in Figure4. In the case of the mutant cells, a reduced population of lacZ-expressing cells was also observed in the slugs and, to a lesser extent, the culminant structures. The mixture of pspA-labeled mef2A- mutant cells with wild-type unlabeled cells showed that very few mutant cells differentiated as prespore cells, and the cells that expressed pspA were found at the rear region of the slugs and the lower part of the sorus in the culminating structures. In contrast, intense lacZ staining was observed when pspA-expressing AX4 cells were mixed with mef2A- mutant cells.
Mixing experiments were also employed to study spore formation in chimeras. In this case, the cells were labeled (Cell-tracker, see MM) and mixed in a 1:1 proportion with unlabeled cells. Cells mixtures were set to develop and allowed to differentiate for 24 hours. Spores were collected, and the percentage of fluorescent spores was determined. Table2 shows that homogeneous mixtures of wild-type (AX4 or AX2) or mef2A- mutant cells yielded the expected proportion of approximately 50% fluorescent spores. However, the mixture of labeled wild-type cells with unlabeled mef2A- mutant cells produced more than 90% fluorescent spores. In perfect agreement with this result, when labeled mef2A- cells were mixed with unlabeled wild-type cells, less than 10% of the spores showed fluorescence.
We also analyzed spore formation by in vitro differentiation. In these experiments, starved cells were induced to differentiate into spores by incubation with 8-Br-cAMP . After 30 hours, the presence of differentiated spores was determined by the morphological changes observed under the microscope (Figure6). Incubation of AX4 cells induced the differentiation of more that 90% of the cells into ellipsoid, highly refringent spores. However, when the mef2A- mutant cells were treated, the majority of the cells appeared rounded and flattened and very few (less than 5%) refringent spores were observed (lower panel of Figure6). Similar results were obtained for AX2 wild-type and mutant cells (data not shown).
We analyzed the differences in gene expression between AX4 and mef2A- strains after 16 hours of development (at the finger stage) when the difference in cell-type marker expression is greatest (see Figure4). Poly(A)+RNAs were isolated, converted to cDNA and sequenced using an Illumina massive sequencing machine. A total of 14,847,781 alignable sequences were obtained for the AX4 RNA and 11,809,110 for the mef2A- RNA, corresponding to approximately 13,500 different genes. The sequences obtained were aligned over the AX4 genome sequence, and the number of sequences obtained for each gene was determined. The genes that presented a significant difference in the number of reads between wild-type and mef2A- mutant strains were finally determined. Given that only one RNA sample was analyzed for each strain, stringent filters were used to determine the genes that were differentially expressed: more than 3 times in the number of reads, with an adjusted p value of less than 0.01. Seventy-seven genes showed significant differences with these criteria. Thirty two of these 77 genes showed higher expression in the wild-type strain, and 45 showed higher expression in the mef2A- mutant strain. As a control, the mef2A transcript was sequenced 73 times in the AX4 sample and none in the mutant sample. Table3 shows the more significant genes that were found coding for known proteins or for proteins with a number of conserved domains. The largest group of genes code for small proteins that are expressed in prestalk cells and that are generally expressed to higher levels in the mef2A- mutant structures. A number of these genes showed similarity to the hssA gene . A second group of genes coded for 57–59 amino acid long proteins that do not show significant similarity to hssA but are also expressed in prestalk cells. Three genes coding for small proteins (69–72 amino acid long) that were expressed in prespore cells showed lower expression in the mef2A- mutant structures. Other genes that are important for prestalk development and that were expressed at higher levels in the mef2A- mutant structures include Pks32, which codes for a polyketide synthase and could be involved in the synthesis of prestalk differentiation factors, and mybC, which codes for a transcription factor involved in the response to prestalk differentiation factors . A number of genes coding for proteins possibly involved in transcription regulation were identified. Their expression appears to be dependent on mef2A because the expression is significantly decreased in mutant structures.
To confirm and extend the data obtained, we performed quantitative RT-PCR experiments on new mRNAs isolated from structures collected after every two hours of development. The expression levels of 11 of the genes listed in Table3 were determined by quantitative RT-PCR, and the results are shown in Figure7. The genes selected were representative of the main categories identified in Table3 and include two hssA-related genes (hssA, G0283503) and one gene coding for a small protein that was expressed at higher levels in the wild-type strain (G0285863). The other analyzed genes coded for proteins involved in prestalk differentiation (Pks32, mybC), for proteins possibly involved in transcription regulation (G0290847, G0271438, mybC), for spore-inducing factors (psiI) and for membrane proteins possibly involved in extracellular signaling or cell adhesion (tgrF1, tgrC5, G0285697). The results for these genes are in complete agreement with the mRNA sequencing data and show that the majority of these genes are similarly dependent on mef2A for all developmental times analyzed. The only exception was psiI, which was expressed at later developmental stages in the mef2A- mutant structures than in the wild-type structures (16 hours vs. 6 hours). The expression of several of the genes studied (G0285863, G0290847, G0271438, G0285697) was almost completely dependent on mef2A for all developmental stages analyzed.
The study of the biological function of the mef2A gene was approached by generating deletion mutants in D. discoideum. Several mutants were generated in the AX2 and AX4 strains, and similar phenotypes were observed for all strains, as shown in Figure3 and Tables1 and and2.2. Over-expression of mef2A caused developmental defects that were morphologically similar to those observed in the mutants. Pools of mef2A over-expressing cells were similar to the mutant strains in the formation of more structures, more heterogeneous in size, and fewer slugs with reduced migration (data not shown), which prevented mutant complementation studies. Similar results were obtained when mef2A was expressed from integrative vectors using the constitutive Act15 promoter or the endogenous, prespore-specific mef2A promoter. A possible explanation for these results might be that over-expressed MefA proteins bind to co-factors or activating molecules outside the chromatin environment, thus impairing their regulatory function on DNA-bound Mef2A molecules.
The results indicate that mef2A is involved in the determination or differentiation of prespore cells and of a group of prestalk cells in D. discoideum. Mutant cells do not differentiate to spores in vitro and, in vivo, produce approximately half the number of spores than wild-type cells produce. These defects are cell-autonomous because the presence of wild-type cells is not able to induce differentiation of the mef2A- mutant cells. The proposed role would represent a conserved function for Mef2 proteins during evolution, given that plant and animal homologous proteins also play important roles in cell differentiation, as mentioned in the Introduction. Mef2A mutants also show impaired growth when feeding on bacteria. This defect does not appear to be due to a reduced phagocytic capacity, as determined by incubation with fluorescent microspheres (Fluoresbrite, PolySciences, data not shown). Differences in cell motility could also explain the smaller size of the colonies, but these possibilities have not been further studied. However, mef2A (srfC) has been previously identified as one of the genes whose expression is regulated depending on the growth substrate of the D. discoideum cells, bacteria or axenic media .
As mentioned above, mef2A appears to be involved in the determination or differentiation of a population of prestalk cells located at the tip of the culminant structures and at the anterior-most region of the slugs. These cells express the ecmB gene and include the tip-organizer cells that regulate the culmination of the structures . The evidence for this function is that mef2A- mutant cells expressing ecmB::lacZ do not participate in the formation of the tip in mixed developmental processes (Figure5). In addition, mef2A mutant cells differentiate poorly to ecmB-expressing prestalk cells in vitro in the presence of DIF and cAMP  (data not shown). However, we have not detected mef2A expression in these cells. The cell-autonomous function of mef2A during differentiation may be due to a cell-type determination process taking place at the previous mound stage of development where mef2A is expressed (Figure2). Alternatively, the expression of mef2A in ecmB-expressing prestalk cells might be too low to be detected by gene reporter expression analyses.
Other populations of prestalk cells, however, are enlarged in mutant structures, as shown in Figure4. Differences in cell type specification could explain the phenotypes observed. For example, the existence of a larger number of prestalk cells that adhere more strongly to each other might contribute to the breakage of the streams. In addition, a number of the genes that are misregulated in mef2A mutants, such as the tgr family of genes (tgrF1, tgrC5), are involved in cell adhesion . However, no differences in Ca-dependent cell adhesion could be determined experimentally using the method described by Parkinsons et al.  (data not shown). The slug structures also showed a highly altered proportion and distribution of prestalk and prespore cells (Figure4), which could explain their smaller size and limited motility.
Despite the developmental defects discussed above, it seems clear that mef2A is not absolutely required for D. discoideum development given that a large number of fruiting bodies and spores are formed in the mutant strains. We would like to suggest that mef2A participates in a network of transcription factors that regulate cell differentiation and that could compensate, at least partially, for the absence of mef2A. For example, mutations of histone deacetylases  and chromatin-binding proteins  affect prespore differentiation or cell-type patterning. In addition, the expression of several genes coding for putative transcriptional regulators is regulated by mef2A. For example, comH codes for a GATA-binding transcription factor expressed in prespore cells. G0288967 codes for a putative β-sandwich domain transcription factor, and G0290847, G0290855 and G0271438 code for proteins containing domains possibly involved in DNA binding and transcription regulation. rblA, a retinoblastoma homolog, also controls the preference of the cells for stalk or spore differentiation . This gene is expressed in the prespore region, and, in chimera with wild-type cells, rblA mutant cells show a strong preference for stalk differentiation, as was also demonstrated here for mef2A mutants.
Mef2A might play a cell-autonomous regulatory role in cell differentiation in response to extracellular signals analogous to those described in other biological systems. The activity of vertebrate Mef2 transcription factors is tightly regulated by extracellular signals. One of the best-known regulatory pathways involves the regulated association of Mef2 with class II histone deacetylases in a process mediated by protein phosphorylation . Mef2 can also be directly phosphorylated through MAP kinase pathways, regulating its transcriptional activity . In this respect, the D. discoideum MAP kinase ErkB is required for spore differentiation [44,45]. It would be of interest to determine whether mef2A participates in this ErkB-mediated spore differentiation pathway, especially given that Mef2A presents three consensus ERK phosphorylation sites.
The main regulatory pathway described as inducing prespore cell differentiation is initiated by extracellular cAMP and requires protein kinase A (PKA) activation . The in vitro spore differentiation study shown in Figure6 was induced by Br-cAMP treatment, resulting in direct PKA activation. The mef2A- mutant cells were unable to differentiate under these conditions. This result indicates that Mef2A regulation takes place downstream of PKA. In fact, a PKA consensus phosphorylation site is present close to the C-terminal end of Mef-2, indicating the possibility that this protein might be a substrate for PKA.
Massive-sequencing analyses of gene expression indicate that Mef2A can play a role in cell differentiation through the regulation of gene expression. There are 32 genes whose expression decreases in mef2A mutants, and many of these genes are specifically expressed in prespore cells, as determined by the mRNA expression analysis available at Dictybase (DictyExpress ) and by the in situ hybridization analysis . A number of prespore specific proteins, often used as prespore markers, also showed differences in expression between AX4 and the mef2A mutant strain but did not reach the filter requirements set up in the analysis of the sequencing data (more than 3 times the difference in the expression level and a p-value smaller than 0.01). For example, cotA was expressed 2.12 more times in AX4 than in the mutant, cotC was expressed 2.02 times, cotD 1.48 times, pspD 1.95 times, pspB 2.52 times and pspA 1.39 times. In contrast, many of the genes that are over-expressed in the mef2A mutant have been identified as prestalk-specific, as shown in Table3. The prestalk-specific gene ecmA was also expressed at higher levels in the mutant (1.51 times). However, ecmB was expressed 1.53 times more in AX4, in agreement with the reduced and more disorganized distribution of ecmB-expressing cells in the mutant at 16 hours of development (Figure4).
Further studies are required to determine the mechanism involved in the transcriptional regulation of the genes whose expression is altered in mef2A mutants. Several of the genes that are under-expressed in mef2A mutants appear to be almost completely dependent on this transcription factor for their expression. The regulation of the expression of these genes could be mediated by the direct binding of Mef2A to their regulatory regions. The DNA binding site of Mef2-related factors has been conserved through evolution and corresponds to the consensus sequence CTA(A/T)4ATG. We looked for the presence of this sequence on the 1000 nucleotide-long fragments located upstream of the 21 genes down-regulated in the mutant using the oPOSSUM program . As shown in Table3, 6 of these genes contained this consensus sequence in the region analyzed. Thirteen additional genes contained related sequences that differed in the C or the G nucleotides. In addition, 4 genes presented the consensus binding site of a related MADS-box transcription factor (ARG80 from S. cerevisiae) . These data indicate that a number of these genes could be direct regulatory targets of Mef2A. Alternatively, mef2A could regulate the expression of other transcription factors controlling the expression of these genes.
The initial analysis of the structure of the mef2A gene detected the existence of alternative promoters that drive the expression of the gene at different times of development and in distinct structures. It is remarkable that the related srfA and srfB genes are also transcribed from alternative promoters, specific for different cell types and developmental stages [30,51]. Other developmental regulatory genes are also transcribed from alternative promoters in D. discoideum, such as pdsA (extracellular phosphodiesterase) carA (cAMP receptor)  and acaA (adenylyl cyclase A) . The existence of alternative promoters might have been an evolutionary adaptation that regulates the expression of a gene under different conditions of growth and/or different developmental processes.
mef2A, which codes for a protein homologous to myocyte enhancer factor 2 transcription factors, is required for several of the steps of the D. discoideum biological cycle, including growth on bacteria and multicellular development. In particular, mef2A is involved in the regulation of the determination or differentiation of prespore cells and a group of prestalk cells during the developmental process of fruiting body formation.
D. discoideum cells were cultured axenically in HL5. Transformation by electroporation was performed as described previously . Transformed cells were selected by treatment with blasticidin  or neomycin (G418). Filter development was induced by spreading 1–2×107 cells (0.6-1.2×106 cells/cm2) on nitrocellulose filters (Millipore Co., Bradford, MA, USA) . The phosphate-based PDF buffer was used to obtain finger, Mexican-hat and culminant structures. Slug structures were obtained by conducting the development in water-soaked filters under directional light. Submerged development was induced by incubation of the cells in 2 ml of PDF phosphate-based buffer on 37-mm diameter cell-culture dishes at 5×105 cells/ml.
The amino acid sequences of MADS-box regions from various organisms were obtained from public databases and compared to those of the four D. discoideum proteins containing MADS-box-related sequences, obtained from DictyBase (http://www.dictybase.org). Amino acid sequences were compared using the ClustalW program at the online Biology Workbench facilities from the San Diego Supercomputer Center (http://workbench.sdsc.edu) and the ClustalX program . Phylogenetic trees were determined using the neighbor-joining method . A random generator seed of 111 and 1000 bootstrap trials were calculated. Trees were drawn using the NJplot program.
RNA was isolated from AX4 cells at 8 hours of multi-cellular development on nitrocellulose filters. The SMART™ cDNA amplification kit from Clontech (Clontech Laboratories, Inc, Mountain View, CA, USA) was used for the amplification of the 5′ untranslated region of mef2A mRNA according to the manufacturer’s instructions. The oligonucleotide TGTTGCCTGTCTATTTCTTTCATTAG, complementary to nucleotides 145 to 164 of the gene, was used as the primer. Amplification products were cloned in the pGEM®-T Easy Vector System (Promega Co, Madison, WI, USA), and the insert of at least 10 different colonies of each product were sequenced.
RNA was isolated from 2×107 cells, either during growth or after development on nitrocellulose filters for 2 to 24 hours, using the TRI reagent (Sigma-Aldrich Inc., St. Louis, MO, USA) according to the manufacturer’s instructions. RNA was further purified using the RNeasy Mini Kit (Quiagen). cDNAs were generated from 2 μg of total RNA using gene-specific oligonucleotides as primer. cDNAs were used as substrates for PCR reactions using as primers the oligonucleotides used for cDNA synthesis and upstream oligonucleotides designed from the coding region of the transcripts. The oligonucleotides GGACTAGTTTCCATTGAACCAATTGGGTGAGCG and CTGATAATACAGATAATACTCGC were used for mef2A cDNA synthesis. The large mitochondrial rRNA was amplified as a control, using oligonucleotides GGGTAGTTTGACTGGGGCGG and CACTTTAATGGGTGAACACC.
Flanking regions of the mef2A gene, including nucleotides −4069 to −2692 and 596 to 1298, in relation to the A of the translation initiation codon were generated by PCR and cloned on both sides of the blasticidin resistance gene in the pLPBLP plasmid vector . The ligonucleotides GGCCGCGGCCATTCCCAGCAACGCTGGTAATC, GGTCTAGACCTGGAAAACTGGAAAACCAATTG, GGATCGATCCACCCACACTAACACACACC and GGGTCGACGGTGGTGGTGATTGGTGCTG were used for these amplifications. The oligonucleotides TGGGAAGGAATAAAATTACAATTGAAAAG and GCGAGTATTATCTGTATTATCAG were used to test for the deletion in AX4 strains, and GTTGCCTGTCTATTTCTTTC and CACTCACTTACATATCACACACC were used in AX2 strains.
The two mef2A promoter regions were amplified by PCR from D. discoideum genomic DNA and cloned in the reporter vector PsA-ialphaGal  in substitution of the XbaI/BglII pspA promoter fragment. The oligonucleotides GGTCTAGAGCACAAGATTATACTTGCCA and GGAGATCTCATGGTGTGTGATATGTAAGTGAGTG were used to amplify the −2201 to −489 region of the gene, corresponding to Promoter 1. The oligonucleotides GGTCTAGACACTCACTTACATATCACACACC and GGAGATCTTGTTGCCTGTCTATTTCTTTCATTAG were used to amplify the −511 to 164 region, corresponding to Promoter 2. The complete promoter region (−2201 to 164) was amplified using the first and last oligonucleotides described above. Previously described lacZ reporter vectors were used to determine the expression of the developmental markers pspA, ecmA and ecmB.
The mef2A gene was expressed using the pDV-CGFP-CTAP vector , under control of the Actin15 promoter. The region coding amino acids 4 to 1046 of the protein, including the third intronic region of the gene, was amplified from genomic DNA using the Pfx DNA Polymerase (Invitrogene™). Two overlapping fragments were obtained using the oligonucleotide pairs GGATCCAGGAATAAAATTACAATTGAAAAG/GGAGATTGATGCTGTGGTTG and CAACAACAAAGCGCCAATCC/ACTAGTAGGTTCCATTGATTTTCTTTTTCGG. The two fragments were joined together using the overlapping HaeII restriction site and the resultant fragment cloned between the BamHI and SpeI restriction sites of the vector. A second expression vector where mef2A was expressed under control of his own promoter was constructed by substituting the Actin15 promoter of the pDV-CGFP-CTAP/mef2A vector by the mef2A promoter. The Actin15 promoter was excised by SalI and BamHI digestion and replaced by the complete mef2A promoter previously cloned in the PsA-ialphaGal vector, as described above. The mef2A promoter was isolated by XbaI/BglII digestion. The SalI end of the vector and the XbaI end of the promoter were converted to blunt ends before ligation.
Cells transformed with the different reporter vectors were allowed to develop on nitrocellulose filters for the time periods indicated in each experiment. The structures were fixed and permeabilized, and β-galactosidase activity was detected by hydrolysis of X-gal (5-Bromo-4-chloro-3-indolyl β-D-galactopyranoside), as previously described .
Growing cells were collected by centrifugation and resuspended in phosphate-based PDF buffer containing 5 μl/ml of 100 mM CellTracker™ Blue CMHC (4-chloromethyl-7-hydroxycoumarin) (Invitrogen, Eugene, Oregon, USA) or a vehicle (DMSO) and incubated for 1 hour in shaking cultures. Cells were then washed, resuspended in free PDF buffer and mixed in a 1:1 proportion. A total of 6.6×106 cells from each mixture were spread out on nitrocellulose filters for 24–36 hours, after which several sori from each mixture were harvested and dissociated in water. Spores were visualized in a Zeiss Axiophot fluorescence microscope and counted.
RNA was isolated from 2×107 cells, either during growth or after development on nitrocellulose filters for the times indicated in each experiment, using the TRI reagent (Sigma-Aldrich Inc., St. Louis, MO, USA) according to the manufacturer’s instructions. RNA was further purified using the RNeasy Mini kit (Quiagen). cDNAs were generated from 2 μg of total purified RNA using random primers (Promega Co., Madison, WI, USA). cDNAs were used as substrate for quantitative real-time PCR reactions using the following gene-specific oligonucleotides: hssA gene (DDB_G0280999) GTGCTATTACCTCAATTTCAAG and GGCAACCACATGAACCACTTG; DDB_G0283503 gene CAAATCATTACAATCAATCACAAGTG and GGGCTACAGCAGCAACTG; prS1 gene (DDB_G0285863) CCAATAATTCTTTGAAGGCCC and CAATAGCTTGGCCCATAGTAGC; tgrF1 gene (DDB_G0292732) CCCACCATTTACTCCAATACTC and GTAGAGATGGTGTTGATGGAG; tgrC5 gene (DDB_G0281407) GCTGGCTTAGCACTTTCATCAG and GAGACCAACGGCAGCGACAC; pks32 gene (DDB_G0292732) CAACTCCAGTCACAACTATAGC and GATTATCATGAATGTGGAATGCTG; mybC gene (DDB_G0281563) GGTGGAGGTAAAACTGGTGC and CATCCATCCAACTAATATCACG; DDB_G0290847 gene CAGTACTGAACAAGCATTATCAAG and GTTAACATAACCTTGTTGAGAATC; DDB_G0271438 gene GTCATGAAATTGGAGATCGAAG and CATGAGATGATGTTGATTTGG; psiI gene (DDB_G0288919) GGTTGTACACTTGTACCACG and GAGGTGCTTCAAAGAGAGC; DDB_G0285697 gene GGTAAGGCAGTTGTCAATGC and GCCTACCAGCTGAGACTTCAGC. A region of the large mitochondrial ribosomal RNA was amplified as a loading control using the oligonucleotides CACTTTAATGGGTGAACACC (used as a reverse oligonucleotide) and GGGTAGTTTGACTGGGGCGG (used as a forward oligonucleotide). The StepOnePlus Real-Time PCR System (Life Technologies Co., Applied Biosystems, Carlsbad, CA, USA) was used in these experiments. PCR products were labeled with SYBR Green using the Power SYBR® Green PCR Master Mix reaction mix (Applied Biosystems) following the manufacturer’s instructions. The final volume of the reaction was 20 μl, using a 0.2 μM concentration of each primer. PCR conditions were as follows: 95°C, 10 m; (95°C, 15 s; 45°C, 30 s; 62° 1 m)×30–40 cycles.
Exponentially growing cells were washed in KK2 buffer (16.5 mM KH2PO4, 3.9 mM K2HPO4, 2 mM MgSO4, pH 6.2), plated on culture dishes at a concentration of 106 cells/ml in spore buffer (10 mM MOPS, 20 mM KCl, 20 mM NaCl, 1 mM CaCl2, 1 mM MgCl2, pH 6.2) and supplemented with 12.5 mM 8-Br-cyclic-AMP and 20 μM CdCl2[32,65]. Cells were incubated in the dark for 30 hours and then observed under a TS100 Eclipse Nikon microscope (Nikon, Tokyo, Japan). Pictures were taken with a Leica DFC420 camera (Leica Microsystems, Wetzlar, Germany).
RNA was isolated from structures developed on nitrocellulose filters for 16 hours using the TriReagent and purified with an RNeasy Mini kit, as described previously. Poly(A)-containing RNA was isolated and converted to cDNA. The cDNA was fragmented, amplified by PCR and the nucleotide sequences determined using an Illumina Genome Analyzer IIx massive sequencer at the Parque Científico de Madrid. Sequencing data were analyzed at Sistemas Genómicos, S.L. (Valencia, Spain). The generated sequences were mapped to the D. discoideum genome using the TopHat v1.1.3 software . Transcripts were identified and quantified using the Cufflinks v1.0.3 program. The total number of reads per gene was determined using the HTSeq package (http://www-huber.embl.de). Statistical analyses of the results was performed using the DESeq package , using an FDR of 0.01. A minimal difference of three times in expression levels was considered.
The authors declare that they have no competing interest in the publication of this manuscript.
MG-C performed the experiments on gene expression and the characterization of the mutant strain and participated in the draft of the manuscript. IF-A characterized the promoter region and generated the mutant strains. TS performed the in vitro differentiation experiments and participated in the draft of the manuscript. LS conceived the study and participated in its design and coordination, as well as the drafting of the manuscript. All authors read and approved the final manuscript.
Comparative study of the amino acid sequences of the D. discoideum MADS-boxcontaining proteins. Panel A. The functional and structural domains present in the D. discoideum SrfC (Mef2A) protein are schematically shown. M: MADS-box; m: Mef2-conserved domain; N: Polyasparagine tract; Q: Polyglutamine tract. Panel B. The amino acid sequences of the MADS-box domains (amino acids 1 to 60 of the SrfC sequence) and the contiguous SRF- or Mef2-specific domains (amino acids 61 to 86) of the species indicated on the left are aligned in relation to the D. discoideum SrfC (Mef2A) sequence using the Clustal W program. Darker boxes indicate the presence of 8 or more identical amino acids. Lighter boxes indicate the existence of 8 or more amino acids with similar chemo-physical characteristics. Figure S2. Analysis of the structure of the 5′ region of the mef2A gene and determination of the transcription start sites. The sequence of the 5′ region of the mef2A mRNA was determined by primer extension using the rapid amplification of the cDNA ends (RACE) technique. The sequences obtained were aligned with the genomic DNA sequence to determine the intron/exon structure of this region of the gene and the transcription initiation sites [GenBank:KC852901]. Exon regions are indicated in black capital letters while intron sequences are indicated in blue small letters. Consensus splicing sites are underlined. The sequence is numbered from the Adenine of the translation initiation codon, shown in bold characters. Transcription initiation sites, as determined by RACE, are indicated with red asterisks over the nucleotide sequence. The complete sequence of the third intron of the gene and the sequence of the large fourth exon, coding for the C-terminal region of the protein, are not shown but are schematically indicated on Figure2.
The authors are indebted to the Dictybase organization for information and reagents. The collaboration of the Parque Cientifico de Madrid with RNA sequencing experiments is also acknowledged. LS was funded by grant BFU2008-02249 from the Spanish Ministry of Science and Innovation (Ministerio de Ciencia e Innovacion). MGC was supported by a JAE predoctoral fellowship from the High Council on Scientific Research (Consejo Superior de Investigaciones Cientificas). We acknowledge the financial support for publication by the CSIC Open Access Publication Support Initiative through its Research Information Resources Unit (URICI).