Ancestral and derived attributes of the dlx gene repertoire, cluster structure and expression patterns in an African cichlid fish
© Renz et al; licensee BioMed Central Ltd. 2011
Received: 18 June 2010
Accepted: 4 January 2011
Published: 4 January 2011
Cichlid fishes have undergone rapid, expansive evolutionary radiations that are manifested in the diversification of their trophic morphologies, tooth patterning and coloration. Understanding the molecular mechanisms that underlie the cichlids' unique patterns of evolution requires a thorough examination of genes that pattern the neural crest, from which these diverse phenotypes are derived. Among those genes, the homeobox-containing Dlx gene family is of particular interest since it is involved in the patterning of the brain, jaws and teeth.
In this study, we characterized the dlx genes of an African cichlid fish, Astatotilapia burtoni, to provide a baseline to later allow cross-species comparison within Cichlidae. We identified seven dlx paralogs (dlx1a, -2a, -4a, -3b, -4b, -5a and -6a), whose orthologies were validated with molecular phylogenetic trees. The intergenic regions of three dlx gene clusters (dlx1a-2a, dlx3b-4b, and dlx5a-6a) were amplified with long PCR. Intensive cross-species comparison revealed a number of conserved non-coding elements (CNEs) that are shared with other percomorph fishes. This analysis highlighted additional lineage-specific gains/losses of CNEs in different teleost fish lineages and a novel CNE that had previously not been identified. Our gene expression analyses revealed overlapping but distinct expression of dlx orthologs in the developing brain and pharyngeal arches. Notably, four of the seven A. burtoni dlx genes, dlx2a, dlx3b, dlx4a and dlx5a, were expressed in the developing pharyngeal teeth.
This comparative study of the dlx genes of A. burtoni has deepened our knowledge of the diversity of the Dlx gene family, in terms of gene repertoire, expression patterns and non-coding elements. We have identified possible cichlid lineage-specific changes, including losses of a subset of dlx expression domains in the pharyngeal teeth, which will be the targets of future functional studies.
Cichlid fishes are amongst the premier models of evolution, as they have undergone rapid adaptive radiation to fill a multitude of ecological niches. This has been made possible, in part, by their striking diversity of jaw and tooth morphologies [1–5]. It has been hypothesized that one of the central factors that has permitted the cichlids' dramatic trophic radiation is their unique pharyngeal jaw apparatus, or 'throat jaws' [6, 7]. These modified gill arches have taken on the role of food processing, freeing up the oral jaws for more specialized forms of food acquisition such as algal scraping . An understanding of the genetic basis of cichlid craniofacial diversity first requires thorough dissections of the genes responsible for neural crest patterning. This knowledge can then be used to compare neural crest patterning between cichlid species, as this forms the basis for their highly variable oral and pharyngeal jaws [8–10].
Cichlid craniofacial specification and morphogenesis are beginning to be characterized at the molecular level. In the Nile tilapia, Hox paralog group 2 gene is expressed in the neural crest that populates the pharyngeal arches in a similar pattern to that of striped bass and zebrafish [11, 12]. Later in development, numerous haplochromine cichlids express Hox genes in the dental mesenchyme directly surrounding the tooth germs in the lower pharyngeal jaw . Albertson et al. identified bmp4 as a putative candidate for craniofacial diversity in a QTL study that compared cichlids with different jaw shapes . Lastly, Kobayashi et al. identified myofibril-associated glycoprotein 4 gene (magp4) as a potentially important gene for cichlid craniofacial diversification as it is differentially expressed in the jaws of Haplochromis chilotes and Haplochromis sp."rockkribensis" .
The Dlx genes have a significant role in patterning the brain, jaw and teeth among amniotes , and represent excellent candidates to further characterize cichlid cranial morphogenesis. The Dlx genes are the vertebrate homologs of the distal-less (dll) gene first identified in Drosophila, which is known to be required for distal limb development . Dlx and dll both belong to the homeobox-containing superfamily of transcription factors (reviewed in ). Six Dlx genes have been identified in mammals - they are likely to be derived from a tandem gene duplication event followed by chromosomal duplications . This scheme also seems to hold in the leopard shark . In contrast, in lampreys, although six Dlx genes have also been documented, their orthology relationships to the six dlx genes of gnathostomes (jawed vertebrates) are not fully resolved [19, 20]. Previous studies have reported conserved non-coding elements in the Dlx clusters, suggesting that these intergenic elements contribute to the maintenance of syntenic relationships for sequential pairs of dlx genes within clusters [21–23].
Combinatorial expression patterns of mouse Dlx genes in the mandibular and hyoid arches were reported to be indispensable for establishing dorsoventral polarity between upper and lower jaw elements ('Dlx code') [24, 25]. In the chicken, although Dlx gene expression fundamentally resembles that of mouse, Dlx4 was found to be pseudogenized . In addition, the Dlx1-Dlx2 cluster has not been identified in its genome assembly even though the expression patterns of these individual genes have been reported [26, 27]. In the zebrafish, it was shown that dorsoventral patterning of pharyngeal arches is achieved by regulatory genes including dlx genes [28–30]. This indicates that the Dlx-dependent patterning is derived from the common ancestor of at least all extant bony vertebrates. An analysis of a distantly-related teleost fish will provide clues that will help to reconstruct the ancestral state and infer secondary changes.
Among the teleost fishes, dlx gene functions have been well studied so far in zebrafish [28–31] and medaka . Because of the teleost-specific genome duplication (TSGD), they possess more genes than tetrapods [33, 34]. In cichlid fishes, only dlx2 (more precisely dlx2a) has been characterized so far [8, 13]. In light of the nested expression patterns seen in the Dlx code [24, 33], it is crucial to analyze the entire dlx gene repertoire of a single species. This is a challenge in species such as cichlid fishes where craniofacial morphology shows such unique features.
In this study, as a baseline to later explore the intra-Cichlidae variation, we provide comparative analysis of molecular phylogeny, genomic linkage and expression patterns of dlx genes between a selected cichlid species and non-cichlids. We identified seven dlx genes in an African cichlid fish, Astatotilapia burtoni, and analyzed their molecular phylogenies and their embryonic expression patterns. Intergenic regions of the three dlx gene clusters were also sequenced and subjected to searches for conserved non-coding elements (CNEs). Our intensive cross-species comparison revealed a relatively high level of conservation of CNEs among ray-finned fishes (Acanthopterygii) and additional lineage-specific gains/losses of CNEs amongst the teleost fishes as well as conservation of previously unidentified CNEs outside the dlx gene clusters. We detected differential expression of dlx genes particularly in the first and second pharyngeal arches, as previously characterized in zebrafish. In the developing pharyngeal teeth, we show that four of the seven identified dlx genes are expressed. Comparisons with other teleost fishes revealed possible losses of a subset of dlx expression in the pharyngeal teeth which to the best of our knowledge could be a unique feature of cichlid fishes.
Identification of A. burtoni dlx genes
Through RT-PCR, we obtained sequences for seven dlx transcripts from Astatotilapia burtoni, each of which contained full-length protein-coding regions (see Materials and Methods). In the multiple alignment of the deduced amino acid sequences, all genes showed strong similarity to members of the Dlx subfamily of homeobox-containing genes, as they contain the characteristic amino acid residues of the dlx homeobox, TQTQVKIWFQN (Additional file 1). Based on sequence similarity to, and subsequent phylogenetic analyses with homologs from other teleost fishes, these seven cDNA sequences were inferred to be derived from orthologs of dlx1a, -2a, -3b, -4a, -4b, -5a, and -6a, and were designated accordingly. Although we performed in silico surveys of expressed sequence tags (ESTs) and partial genomic sequences from cichlid fishes currently available in NCBI dbEST http://www.ncbi.nlm.nih.gov/projects/dbEST/, no additional Dlx paralogs were found.
Molecular phylogenetic analyses
In our molecular phylogenetic trees, all Dlx genes except Dlx4, (for which mammalian members show extremely long branches ), exhibited a dichotomy between teleost fishes and tetrapods, supported strongly by both the neighbor-joining (NJ) and maximum-likelihood (ML) methods (Figure 1D). The newly identified A. burtoni genes always grouped with homologs of other acanthomorpha species (Figure 1), consistent with previous studies on the phylogenetic relationships of teleost fishes [37–40]. Overall, our phylogenetic trees supported their orthologies and accordingly these A. burtoni dlx genes were named dlx1a, dlx2a, dlx3b, dlx4a, dlx4b, dlx5a, and dlx6a.
We observed relatively long branches at the base of teleost fishes for dlx1a, -5a and -6a (Figure 1A, E, F), suggesting an elevation of evolutionary rates for these genes. Moreover, dlx2b and -3a exhibited markedly longer branch lengths compared with their paralogs generated in the TSGD  (Figure 1B, C). This phylogenetic analysis also highlighted possible lineage-specific losses of dlx genes. Second teleost duplicates, generated by the TSGD, which we tentatively call dlx1b, dlx5b and dlx6b in the hypothetical common ancestor, are absent from all teleost fish genome sequences currently available. The absence of these putative duplicates implies that they were lost following their duplication in the stem lineage leading to teleosts. We also noted that the absence of dlx3a appears to be unique to Cypriniformes including the zebrafish, and that the absence of dlx2b appears to be unique to the percomorphs including pufferfishes, stickleback, medaka and cichlids (Figure 1B, C). These lineage-specific gene losses were also proposed by a previous report . In our extended study, the absence of an A. burtoni dlx3a ortholog as well as a medaka dlx4a ortholog suggests additional gene losses.
In addition to the A. burtoni genes, we identified EST sequences in NCBI, encoding dlx genes of diverse teleost fishes, covering, for example, Salmoniformes, Siluriformes and Characiformes, including representatives of teleosts without sequenced genomes. After assembly of these previously unidentified dlx-encoding ESTs, we constructed molecular phylogenetic trees including them (Additional file 2; see also Materials and methods). According to the data available so far, none of these lineages have retained the dlx paralogs that should have existed just after the TSGD (namely dlx1b, -5b and -6b). All previously identified teleost-specific paralogs (dlx1a, -2a, -3a, -3b, -4a, -4b, -5a, and -6a) were retained by representative species from Salmoniformes, while only four of these (dlx2a, -2b, -3a, and -5a), including information in GenBank (dlx2a and -2b of Synodontis multipunctatus), were found in species from Siluriformes (Additional file 2B, C, E). Taken together, even though taxon and sequence sampling is obviously not complete, the loss of dlx3a (as seen in the zebrafish) at most dates back to the split of Cypriniformes from other otocephalan lineages (for example, Characiformes and Siluriformes) (Additional file 2C). On the other hand, since the presence of dlx2b is confined to the otocephalan representatives (Cypriniformes, Siluriformes and Characiformes) (Additional file 2B), this suggests that its ortholog was lost only in the basal lineage of Percomorpha (including stickleback, pufferfishes and medaka) at the latest. This gene loss might date back to the origin of Euteleostei before the split of Salmoniformes from others.
dlx clusters: detection of putative cis-regulatory elements
Throughout the three A. burtoni dlx clusters, we did not detect the loss of any CNEs shared by other species, with one exception: a CNE tentatively named I12.3b (see Materials and methods for this naming). Notably, we identified CNEs shared by only a subset of teleost fishes. Most of them (for example, I12.7, I34.1, I34.2, I34.4, I34.5, I34.6, I56.6a and I56.7) were shared only between A. burtoni, medaka, stickleback and pufferfishes, excluding zebrafish, consistent with their phylogenetic relationships  (Figure 2). This type of conservation pattern was also frequently observed for flanking regions (Additional file 3A, B, C). One lineage-specific CNE I12.3ab was conserved only in medaka, A. burtoni and stickleback (Figure 2). Our comparison also revealed conservation of the previously characterized CNEs, I12.4, I12.5, I56.3, and I56.4 (I12b, I12a, I56ii and I56i, respectively; ) in a wider range of species, including A. burtoni, medaka, Tetraodon nigroviridis and anole lizard Anolis carolinensis (Figure 2). We also detected losses of CNEs in the zebrafish lineage (for example, I56.5) (Figure 2). In the flanking region of the dlx5a-dlx6a cluster, we detected an uncharacterized CNE, F56.9, which is conserved among all analyzed species, except the anole lizard where the corresponding region is not completely sequenced (Additional file 3).
We performed Blastn searches, using the identified CNE sequences of A. burtoni (for those in the intergenic regions) and stickleback (for those in the flanking regions) as queries, in currently available sea lamprey Petromyzon marinus and elephant shark Callorhinchus milii genome assemblies. In an elephant shark genome sequence (AAVX01041446 in GenBank), we identified a match for only the CNE I12.5, which is conserved in all osteichthyans surveyed in the present study (Additional file 4;also see ). In P. marinus, we could not find any homologous sequences to CNEs that we identified in this study. This should be reexamined with the anticipated whole genome sequences of this species and other cyclostomes.
dlx gene expression analysis
Embryonic expression domains of A. burtoni dlx genes.
7, 8 and 10 dpf
++ (I and II)
- (III and IV)
+ (V and VI)
- (7 dpf)
- (10 dpf)
- (13 dpf)
++ (I and II)
+ (III and IV)
++ (V and VI)
+ (7 dpf)
+ (8 dpf)
- (10 dpf)
+ (18 dpf)
++ (7 dpf)
+ (8 dpf)
++ (10 dpf)
++ (13 dpf)
+ (18 dpf)
++ (7 dpf)
++ (8 dpf)
++ (10 dpf)
++ (13 dpf)
- (7 dpf)
- (10 dpf)
- (13 dpf)
+ (18 dpf)
++ (7 dpf)
++ (8 dpf)
++ (10 dpf)
- (7 dpf)
- (10 dpf)
At 5 dpf, intense expression was detected in the ventrolateral region of the ectomesenchyme in the developing pharyngeal arches (PAs) for all seven A. burtoni dlx genes (Figure 4). In parallel, we performed whole-mount in situ hybridization of hoxa2a gene, which is known to be expressed in the second and more posterior arches [12, 42, 43]. In PA1, which is marked by the absence of hoxa2a expression (Figure 4A, B), we detected expression of all analyzed dlx genes (Figure 4C-P). Of these, along the dorsoventral (DV) axis, dlx2a expression is distributed more broadly within PA1 (Figure 4F), while expression of at least dlx3b was more restricted (Figure 4J). In addition, the ventral-most areas of the anterior pharyngeal arches are devoid of dlx4a expression (Figure 4G). In contrast, expression of dlx5a and -6a extended further towards the ventral midline than the other dlx genes (Figure 4M, O). In the anterior part of the PA1 immediately behind the eye, no expression of dlx4a, -3b and -5a was observed (Figure 4H, J, N). We observed weaker expression of dlx1a and dlx2a in PA3 and PA4 than in other PAs (Figure 4C, E). Expression signals of dlx1a, -3b, -4a, -4b and -5a persisted until 10 dpf (data not shown). At 7 and 10 dpf, we observed only weak expression signals for dlx2a, while no clear signal of dlx6a expression was detected (data not shown).
Other expression domains
We also detected A. burtoni dlx expression in other tissues. This includes expression of dlx2a, -3b, and -5a in the otic vesicle (Table 1). Intense signals of dlx3b, dlx4b and dlx5a were detected in the caudal fin rays at 7 dpf, 9 dpf and 10 dpf (Table 1). In the pectoral fin, we detected expression signals of dlx5a at 10 dpf (Additional file 5). Expression signals of dlx3b and -4b were also detected in the circular smooth muscles (csm) of the esophagus, posterior to the pharyngeal jaw, at 13 dpf (Additional file 6).
The evolution of dlx gene repertoires in teleosts
The canonical genomic organization of the vertebrate dlx repertoire comprises three conserved bi-gene clusters . One example violating this dogma is the pseudogenization of Dlx4 in chicken . Based on our analysis, the anole lizard Anolis carolinensis retains an only partially annotated, but intact Dlx4 gene (Ensembl ID: ENSACAG00000005126), which is confirmed by the presence of its transcript in the NCBI EST Database (Accession ID: FG754683). We propose that the pseudogenization of the chicken Dlx4 might be a bird- or archosaurian lineage-specific event, and we can regard the '3 × 2 state' as the plesiomorphic condition of Dlx cluster architecture at least for jawed vertebrates. As observed previously for other genes , the identification of dlx genes in zebrafish  suggested an altered scheme for teleost fishes due to the additional whole genome duplication (TSGD, [33, 34]). A more recent study on medaka dlx genes also produced a similar conclusion supporting the duplicated gene repertoires as well as its subsequent differentiation between teleost fish lineages .
Stepwise establishment of putative cis-regulatory elements
Our comparison of the intergenic regions of dlx clusters, including tetrapods, provided an overall picture of their putative cis-regulatory elements. Many gains of non-coding elements are deduced from the phylogenetic tracing even during the relatively recent evolution of teleost fishes (Figure 6). Additionally, we found a match of I12.5 in the elephant shark C. milii. This element has also been found in a BAC clone sequence containing Dlx2, thus providing the first evidence of a putative cis-regulatory element in Dlx clusters outside Osteichthyes (Additional file 4). Our comparison also identified already functionally characterized CNEs in a wider range of vertebrates (see Results). At the same time, an element I12.3b, which has not been functionally characterized to date, was found to have been lost specifically in the cichlid lineage (Figure 6). In contrast, identification of cichlid-specific gains of CNE by means of phylogenetic footprinting  requires the addition of at least one more species that is sufficiently distant from A. burtoni.
The gains of the elements I12.3ab, I56.2 and F56.10 would support a closer phylogenetic relationship of stickleback to medaka/cichlid than to pufferfishes (Figure 6). The phylogenetic relationship among these percomorph fishes has not yet reached a consensus based on available molecular data [37, 38, 40, 47]. These so-called 'rare genomic changes'  might serve as genomic synapomorphies for a stickleback-medaka-cichlid grouping.
Dlx code in teleost fishes
A. burtoni dlx expression patterns in the brain closely resemble that of the mouse (Figure 3; ). Therefore, our riboprobes are regarded as specific enough to discern spatiotemporal regulation of dlx genes throughout embryogenesis. In light of the differential expression patterns of this group of genes observed in mouse and zebrafish ([24, 28–30]; see also Introduction), we assessed dorsoventral (or proximodistal) distribution of A. burtoni dlx transcripts particularly in the PA1 and PA2. Our examination revealed the expression of all analyzed A. burtoni dlx genes in the PA1, the Hox-negative region, and in the hoxa2a-positive PA2 (Figure 4). At least dlx2a transcripts showed slightly wider distribution along the DV axis in the PA1 and PA2 than those of other dlx genes (Figure 4F). The broadest expression of Dlx2 homolog resembles the situation in zebrafish [28–30] and mouse , suggesting the conservation since the osteichthyan ancestor. Although not as distinct as the dlx2a expression, relatively broad expression of dlx5a along the DV axis is also described in zebrafish [28, 30, 31]. Our analysis on A. burtoni dlx5a, however, did not yield a similar pattern (Figure 4N). Including dlx5a, all the analyzed dlx genes except for dlx2a seemed to be expressed in a similar manner to each other in the PA1 and PA2 (Figure 4D, H, J, L, N and 4P), except that expression particularly of dlx3/4 genes did not protrude ventrally towards the midline (Figure 4G, I and 4K), as seen in zebrafish . In summary, our analysis on A. burtoni supported the common ancestry of differential dlx expression patterns in the PA1/2 among teleost fishes, and also among osteichthyans. Equivalence of functional properties of Dlx code in cichlid fish could be tested by loss-of-function experiments as demonstrated in mouse and zebrafish [24, 29].
Possible roles for dlx genes in dentition: novelty in cichlids?
We performed an intensive analysis of A. burtoni dlx expression in pharyngeal teeth (Figure 5). Previously, dlx expression in teeth was described for zebrafish and medaka [31, 32]. For cichlids, expression of dlx2a (designated 'Dlx2' there) has been described in the teeth (oral, pharyngeal or both) for Lake Malawi species (Tramitichromis intermedius, Labeotropheus fuelleborni, Dimidiochromis compressiceps and Metriaclima zebra[8, 13]). In A. burtoni, the dlx2a expression in the pharyngeal teeth was detected in a highly restricted manner both spatially and temporally (Figure 5B, C; see also Results). This restricted dlx2a expression was also documented in medaka and zebrafish [31, 32]. dlx5a expression also exhibited striking dynamism in that its intense expression at the tooth base shifted from the dental epithelium to the mesenchyme in the course of tooth development (Figure 5H and 5I). As similar expression patterns are described in medaka and zebrafish [31, 32], these dynamic expressions of dlx2a and dlx5a, as well as the most intense expression of dlx3b (see Results; [31, 32]), are recognized as conserved features shared among the major lineages of Teleostei. dlx3a, which we could not identify in A. burtoni, has not been observed in the pharyngeal teeth in medaka . dlx4a, the other gene on the same ancient bi-gene cluster as dlx3a, has not been identified in medaka . Interestingly, in A. burtoni, we identified a dlx4a ortholog, and detected its relatively weak expression in pharyngeal teeth (Figure 5G), as well as in zebrafish . We did not detect dlx1a, dlx4b, and dlx6a expressions in the pharyngeal teeth in the developmental stages we analyzed, while we detected expression signals of these genes in other tissues (Table 1). Of these, the absence of dlx1a expression in the pharyngeal teeth is documented also in medaka, while they express dlx4b and dlx6a. Thus, it is possible that, in the lineage leading to cichlids after the split of the medaka lineage, pharyngeal tooth expression of dlx4b and dlx6a was secondarily lost. Further study would be required to determine whether the absence of those gene expressions is the result of our incomplete selection of stages or if they represent a genuine diversification of dlx functions after the split of the cichlid lineage from others. To confirm the cichlid lineage-specific changes, careful analyses of their expression in intermediate fish lineages (Pomacentridae and Embiotocidae; ) may also be necessary.
Overall, inclusion of teleost fishes in the framework of vertebrate Dlx study and inclusion of a cichlid fish in that of teleost dlx study allowed us to highlight stepwise gains and losses of putative cis-regulatory elements as well as dlx family members at a higher resolution. Especially, in the lineage leading to an African cichlid A. burtoni, we discovered 1) a possible loss of dlx3a and 2) loss of the CNE I12.3b in the intergenic region of the dlx1-dlx2 cluster. We also detected possible loss of dlx4b and dlx6a expression in the developing pharyngeal teeth.
Materials and methods
An inbred Astatotilapia burtoni line, originally provided by Hans Hoffmann (University of Texas, Austin, TX, USA), was kept at 24°C. Broods of up to 80 eggs were fertilized naturally and kept in the mothers' mouth until elicitation. For in situ hybridization, embryos were either fixed in 4% paraformaldehyde (PFA) in phosphate-buffered saline (PBS), dehydrated and stored in 100% methanol, or fixed in Serra's fixative (60% ethanol, 30% formaldehyde, 10% acetic acid) and kept in 100% ethanol at -20°C. The chorion and yolk were removed for embryos up to 6 dpf.
Isolation and sequencing of cDNAs
Total RNA was extracted from whole embryos at 13 dpf using TRIzol reagent (Invitrogen, Carlsbad, CA, USA), and reverse transcribed into cDNA using a 3'RACE System (Invitrogen). The cDNA was used as a template in the following PCR amplification with the FastStart High Fidelity PCR System (Roche, Basel, Switzerland). Degenerate primers were designed based on the multiple alignment of major vertebrate dlx genes: 5'-GCG CAR ACN CAR GTN AAR ATH TGG TT-3' and 5'- GCG CAR GTN AAR ATH TGG TTY CAR AA-3' for the conserved amino acid stretches TQTQVKIWF and TQVKIWFQN, respectively. Nested 3'RACE PCRs were performed using the two degenerate primers, with universal primers that were designed to the 3' end of the oligo(dT) used for making cDNA. We amplified 3' cDNA fragments of dlx3b, dlx5a, dlx4a and dlx4b from this PCR. To isolate dlx1a, dlx2a and dlx6a, we designed forward gene specific primers based on partial exonic sequences of their putative orthologs in Malawi Lake cichlid fishes identified from genome shotgun reads available at Joint Genome Institute  (Additional file 7). These were used with the universal primers in 3'RACE reactions. 5' upstream sequences of the isolated cDNA fragments were amplified and sequenced with a 5'RACE System (Invitrogen). Details of PCR conditions and following procedures for cloning and sequencing were described previously . cDNA sequences for A. burtoni dlx genes were deposited under accession numbers (EMBL: FN667596 to FN667602). The cDNA template for hoxa2a riboprobe was amplified using gene specific primers designed based on the A. burtoni hoxa2a genome sequence in GenBank (EF594313).
Genomic DNA sequencing
Genomic DNA was extracted from a whole embryo of A. burtoni using the traditional phenol-chloroform protocol . For long PCR against this genomic DNA, we designed primers specific to the 3' UTR of each isolated dlx gene. PCRs were performed using either a Long Range PCR System (Roche) or Long PCR Enzyme (Fermentas, St. Leon-Rot, Germany). Amplified DNA fragments were purified with the MinElute PCR Purification kit (Qiagen, Hilden, Germany), and cloned with the TOPO-XL Cloning kit (Invitrogen). Sequencing was performed through primer walking or random sequencing with EZ-Tn Kit (Epicentre, Madison, WI, USA). Genomic DNA sequences for A. burtoni dlx intergenic regions were deposited under accession numbers (EMBL: FN668537 to FN668539).
Comparison of intergenic sequences
By using Genscan  and Augustus , we confirmed that there is no additional protein-coding sequence in the intergenic regions of the A. burtoni dlx clusters. Cross-specific comparison of intergenic sequences was performed using mVISTA  with the newly determined A. burtoni sequences as well as dlx clusters of model teleost fishes available in the Ensembl Genome Browser (; version 54). Searches of the partial sea lamprey (version PMAR3) and elephant shark genome assemblies were performed using Blastn to detect local similarities, because no intact Dlx bi-gene cluster was contained in the genome assemblies. To detect CNEs, we were based on a criterion of 70% similarity in a 100 bp sequence stretch. See Additional file 8 for the naming of CNEs with 'a' and 'b' (for example, I12.3b). It should be noted that there could be functional cis-regulatory elements that are less similar or shorter than our criterion. A potential complication of pairwise comparisons arises when non-overlapping regions (tentatively named CNE a and CNE b in the present study) of a single CNE (CNE ab) are conserved between the query and each of the aligned sequences (Additional file 8).
Molecular phylogenetic analyses
By using deduced amino acid sequences of the newly isolated sequences as queries, Blastp searches were performed to collect available homologous peptide sequences from Ensembl , and Genpept . A multiple alignment was constructed using the alignment editor Xced where the alignment algorithm MAFFT is implemented . Preliminary neighbor-joining trees were inferred on the Xced. Final trees were inferred using PhyML , assuming the JTT + I + Γ4 model. Bayesian posterior probabilities were calculated using MrBayes . To confirm presence and absence of particular dlx genes in diverse teleost fish lineages, we ran an original Perl script to automatically detect orthologous sequences in assembled expressed sequence tags (ESTs) downloaded from NCBI dbEST . Sequences found by this procedure were also included in molecular phylogenetic trees in Additional file 2.
Whole-mount in situ hybridization
Digoxigenin (DIG)-labeled antisense and sense riboprobes were synthesized according to the manufacturer's instructions (Invitrogen) using SP6, T7 or T3 polymerase, according to the orientation of inserted template cDNA in the plasmid. After rehydration of fixed embryos and washing in PBTw (PBS containing 0.1% Tween 20), the embryos were post-fixed in 4% PFA/PBS for 20 minutes. Digestion with proteinase K (5 μg/ml, Roche) was adapted for cichlid embryos: 5 minutes at room temperature for embryos 5 dpf, 8 minutes for embryos 7, 8, 10 and 13 dpf and 10 minutes for embryos 18 dpf. After another post-fixation step, embryos were washed with DEPC-PBT, immersed in 50% formamide and prehybridized in hybridization buffer (50% formamide, 5× SSC, 1 mg/ml total yeast RNA, 50 μg/ml heparin, 0.1% Tween 20, in DEPC) for 3 h at 68°C. The specimens were then incubated in hybridization buffer with DIG-labeled RNA probes overnight at 68°C. After hybridization, the specimens were washed with 100% formamide solution (containing 50% formamide, 5× SSC, 0.1% Tween20 and 9 mM Citric acid in DEPC-water), 75%, 50% and 25% of this solution in 2% SSCTw (saline sodium citrate buffer containing 0.1% Tween 20) and in 2× SSCTw and 0.2× SSCTw at 68°C, each for 15 minutes. Then embryos were washed for each 10 minutes in 75%, 50% and 25% SSCTw in PBTw and finally in pure PBTw at room temperature. The specimens were soaked in 0.5% Blocking reagent (Roche) in PBTw for 30 minutes and subsequently the reagent was replaced by a 1:2000 dilution of anti-DIG-AP antibody in 0.5% Blocking solution and gently agitated at 4°C o/n. After incubation, the embryos were washed extensively in PBTw at room temperature, and hybridization was detected by incubation with NBT and BCIP (Roche). For histological observation in Figure 5, the stained embryos were dehydrated with a series of methanol, and embedded and sectioned as described below. Prepared sections were aligned on glass slides and deparaffinized for microscopic observation.
Section in situ hybridization
Embryos were embedded in Paraplast (Carl Roth, Karlsruhe, Germany) and transverse sectioned with a microtome at a thickness of 8 μm. Detailed procedures were reported previously .
Sectioned specimens were deparaffinized with three five-minute washes in xylene and were stepped into 70% ethanol. Staining in Mayer's Hematoxylin (Fluka, Buchs, Switzerland) was conducted for 20 minutes, and the slides were washed with running tap water for 5 to 10 minutes. Slides were incubated in 80% ethanol and stained with 0.25% EosinY (Fluka) in 80% ethanol for three to five minutes. They were quickly washed twice with 100% ethanol and twice in xylene. Sections were mounted with Eukitt (Fluka) for microscopic observation.
conserved non-coding element
teleost-specific genome duplication.
This study was supported by grants of the German Research Foundation (DFG) to AM. We thank Nils Offen, Nicola Blum, Silke Pittlik, Elke Hespeler, Philippe Reuter, Konrad Bergen, Wei-Jen Chen, Dave Gerrard, Nathalie Feiner and Ursula Topel for technical support in cDNA cloning, sequencing and in situ hybridization, and Sven Boekhoff for bioinformatic assistance. We are also grateful to two anonymous reviewers for their constructive comments. The sea lamprey genomic data were produced by the Genome Center at Washington University School of Medicine in St Louis and they can be obtained from ftp://genome.wustl.edu/pub/organism/Other_Vertebrates/Petromyzon_marinus/.
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