Article | Open | Published:

The multicellularity genes of dictyostelid social amoebas

Nature Communications volume 7, Article number: 12085 (2016) | Download Citation

Abstract

The evolution of multicellularity enabled specialization of cells, but required novel signalling mechanisms for regulating cell differentiation. Early multicellular organisms are mostly extinct and the origins of these mechanisms are unknown. Here using comparative genome and transcriptome analysis across eight uni- and multicellular amoebozoan genomes, we find that 80% of proteins essential for the development of multicellular Dictyostelia are already present in their unicellular relatives. This set is enriched in cytosolic and nuclear proteins, and protein kinases. The remaining 20%, unique to Dictyostelia, mostly consists of extracellularly exposed and secreted proteins, with roles in sensing and recognition, while several genes for synthesis of signals that induce cell-type specialization were acquired by lateral gene transfer. Across Dictyostelia, changes in gene expression correspond more strongly with phenotypic innovation than changes in protein functional domains. We conclude that the transition to multicellularity required novel signals and sensors rather than novel signal processing mechanisms.

Introduction

Multicellularity provided the opportunity for cell-type specialization and the positioning of specialized cells into complex structures. This organization offered an immense gain of function that is reflected in the complex physiology and behaviour of modern animals such as ourselves. To understand how multicellular organisms evolved, it is essential to retrace the origin of the cell–cell communication mechanisms that caused cell-type specialization. While the early ancestors of animals are long extinct, several multicellular eukaryotes still have a unicellular feeding stage, simplifying identification of genes that uniquely regulate multicellular development. The best-studied representative of this group is Dictyostelium discoideum (DD), which forms multicellular structures by aggregation of starving amoebas, which then differentiate into four distinct cell types1. Dictyostelia are members of the mostly unicellular kingdom of Amoebozoa and can be subdivided into two major branches I and II, each containing two major groups2,3. Phenotypic mapping shows that these groups differ in the number of different cell types, the size and shape of multicellular structures, the presence of a freely migrating ‘slug’ stage and light-orientated behaviour. The largest changes occurred at the transition between groups 3 and 4, with group 4 acquiring two novel cell types, cell-type proportioning, the ability to form larger multicellular structures and greater behavioural complexity3,4.

To understand the genetic changes that caused the evolution of multicellularity and the acquisition of multicellular complexity, we completed the set of genomes representing groups 1, 2 and 4 of Dictyostelia5,6,7 with the genome of the group 3 species D. lacteum (DL). The group 1–3 genomes were sequenced to deep coverage. Almost complete assembly was achieved by primer walking, and assisted by detailed fosmid maps of the genomes. In addition to the manually curated DD genome, these high-quality genomes allow accurate assessment of gene gain, modification and loss in the course of Dictyostelid evolution. We used existing8 and novel high-throughput RNA sequencing data to determine differences in gene expression between groups during the entire developmental programme. The genomes of three unicellular amoebozoans are also available: the obligatory parasite Entamoeba histolytica9 and the free-living amoebozoa Acanthamoeba castellani10 and Physarum polycephalum11. The availability of multiple uni- and multicellular amoebozoan genomes enabled us to also assess genetic changes at the transition from uni- to multicellularity.

In the model DD, 385 genes have been recognized by gene disruption to be essential for normal progression through multicellular development. We investigated the presence of these genes across five Dictyostelid and three unicellular Amoebozoan genomes, and identified their closest homologue outside of Amoebozoa. We next assessed changes in gene function by comparing the functional domain architecture of orthologous genes across species and we assessed changes in gene regulation by comparing their transcriptional profiles. We performed gene ontology (GO) enrichment analysis to assess which functional categories of genes were most subjected to change at either the transition from uni- to multicellularity or during the acquisition of multicellular complexity.

Our analysis shows that out of the 385 investigated genes, 305 are conserved throughout Dictyostelia and at least one unicellular amoebozoan. This set is enriched in cytosolic, nuclear and cell cortex proteins, and in protein kinases. The remaining 80 developmentally essential genes (DEGs), unique to Dictyostelia, mostly encode cell surface and secreted proteins, with roles in sensing and cell recognition. These proteins belong to expanded families that show extensive gene gain and loss between individual Dictyostelia and unicellular Amoebozoa. Three enzymes that synthesize signals that induce cell differentiation were acquired from bacteria by lateral gene transfer (LGT). In short, most mechanisms required for signal processing were already present in the unicellular ancestors, while the transition to multicellularity mainly required novel secreted and exposed signals and sensors to detect these signals.

Results

DL genome sequencing

The DL genome was sequenced to 29-fold coverage using the 454 Roche platform. Assembly was assisted by a detailed map of end-sequenced fosmids with average insert sizes of 32.5 kb. Remaining gaps in the scaffolds were closed by primer walking to yield a final assembly of 54 gap-free contigs. The DL genome was at 23.4 Mbp 30% smaller than the DD (group 4), D. purpureum (DP, group 4) Polysphondylium pallidum (PP, group 2) and D. fasciculatum (DF, group 1) genomes, which was due to fewer and smaller introns, smaller intergenic regions and fewer protein-coding genes (Supplementary Table 1). DD has unusual chromosome ends consisting of A/T-rich repeats, as are also present at the extrachromosomal ribosomal DNA palindrome ends5. Both the DF and PP chromosomes and palindromes have normal eukaryote GT-rich telomere repeats, while DL presents an intermediate situation with normal eukaryote chromosome telomeres and DD-like A/T-rich palindrome ends (Supplementary Fig. 1).

Comparative analysis of DEGs

DEGs are defined as DD genes for which deletion causes defects in multicellular development. Around 385 DEGs were retrieved from Dictybase12. The DEGs were subdivided in sets, according to the developmental stage where the defect was first evident: growth, aggregation, mound/tip formation, slug formation and migration, culmination, pre(stalk) and pre(spore) differentiation. The genes are listed in Supplementary Data 1 together with their null mutant phenotype, their orthologues/homologues in DP, DL, PP and DF, and in the Amoebozoa Physarum polycephalum (PhyP), Acanthamoeba castellani (AC) and Entamoeba histolytica (EH), as well as their closest homologue outside Amoebozoa, determined as described below.

Homologues of the DD genes were retrieved by BLASTp, and orthology was first assessed from the probability (E) values of best bidirectional hits (BBHs), and second from the node structure and branch lengths of trees generated by Bayesian inference of aligned protein sequences. In general, if the node structure of the protein tree follows that of the genome-based Amoebozoan phylogeny (Fig. 1a)3, genes were considered to be orthologous. Such correspondence with the Amoebozoan phylogeny is exemplified by the AcrA tree (Fig. 1c). If the homologues group more closely with genes of more distantly related species, or with different DD genes, they were likely to be paralogues. This is evident for the PadA tree (Fig. 1c). Conservation of protein length and functional domain architecture further assists the assignment of orthology, as does conservation of developmental regulation (Fig. 1c). However, changes in protein function and gene regulation may also highlight genetic changes in orthologous genes that have given rise to phenotypic innovation across Dictyostelid evolution (see, for example, Fig. 1b). They therefore carry less weight in orthology assessment, but are of considerable interest for evolutionary comparative studies.

Figure 1: Dictyostelid phylogeny with life cycles and selected annotated gene trees.
Figure 1

(a) Phylogenetic tree of dictyostelid and unicellular amoebozoan species with sequenced genomes, as inferred from 30 concatenated proteins by Bayesian inference3. (b) Schematic of life cycle complexity of the Dictyostelid test species. DF, PP and DL form multiple fruiting bodies directly from the aggregate. All cells first differentiate into prespore cells and then form the stalk by dedifferentiation of prespore cells at the tip. DD and DP form single fruiting bodies from aggregates and display an intermediate migratory ‘slug’ in which cells pre-differentiate into prestalk and prespore cells. During fruiting body formation, two more cell types emerge that support the stalk and spore mass3,4. 1: aggregate, 2: early sorogen (slug), 3: migrating slug, 4: mid-culminant, 5: fruiting body. Light red: prespore; dark red: spore; light blue: prestalk; dark blue: stalk; green: basal disc or supporter; yellow: upper and lower cup. (c) Annotated gene trees. Examples of trees, based on the amino-acid sequence of homologues of DD DEG, annotated with protein functional domains and developmental expression profiles and inferred by Bayesian inference (see Methods for procedures). The AcrA tree follows the amoebozoan tree topology, identifying all amoebozoan homologs as orthologues. The PadA tree does not, identifying PPL_02565 and DLA_06544 as paralogues of DD padA.

To compare developmental gene expression profiles, published time series of high-throughput RNA expression data for DD and DP8 were expressed as percentage of maximal expression and stage-matched to new RNA expression data for DL, PP and DF. The latter three species do not complete development with the same timing as DD and DP, and we therefore isolated RNAs at the defined stages of growth, early and late aggregation, tipped mound, slug, early culmination and completed fruiting bodies. The developmental programme of DL, PP and DF is also less synchronous than that of DD and DP resulting in quenching of gene expression peaks. With this in mind, we only considered a gene to be differentially regulated between species when its expression profile clearly differed from profiles of at least two other species. All trees, annotated with protein functional domain architectures and transcription profile schematics, are listed in Supplementary Data 2.

A summary of the conservation of all DEGs, their functional domain architectures and expression profiles is presented in Fig. 2. Cursory observation shows that the greater majority of DEG is conserved in Dictyostelia, inclusive of their domain architecture and expression, and this is confirmed by quantitation of the number of orthologues, genes with conserved domains and genes with conserved expression profiles (Fig. 3). Seventy-three per cent of DEGs have orthologues in all five Dictyostelid genomes, while 5% of DEGs are present only in DD. For 55% of DEG, domain architecture is conserved across Dictyostelia, and for 45% the expression profile is conserved across Dictyostelia (Fig. 3a). The DEGs that regulate different developmental stages show no large differences in these aspects (Supplementary Table 2). Among unicellular amoebozoa, 76% of DD DEG have homologues in PhyP, followed by 46% in AC and 19% in EH (Fig. 3c). Despite these low levels of conservation in AC and EH, most (72%) DD DEGs have homologues outside of Amoebozoa, indicating that some amoebozoan taxa underwent considerable gene loss. We compared conservation of DD DEGs with a set of genes without known function (Supplementary Fig. 2). Of the latter set, only 31% are conserved as orthologues throughout Dictyostelia, with 33% unique to DD. PhyP, AC and EH genomes contained 63, 15 and 1% homologues, respectively, of DD genes with no known roles (Fig. 3b,d). The observation that 73% of DEGs were conserved in Dictyostelia, compared with 31% of genes with unknown function, indicates that genes with proven roles are more likely to be conserved.

Figure 2: Conservation of 385 D. discoideum developmentally essential genes across and outside of Amoebozoa.
Figure 2

The presence of validated orthologues and homologues of 385 DD DEGs is plotted over the amoebozoan phylogeny and the kingdom outside Amoebozoa with their closest homologue. DEGs are grouped according to the stage, where their null mutant defect is first evident. Box fill colours denote orthology/homology and functional domain conservation. Black and red borders for Dictyostelid orthologues and homologues, respectively, mark genes with developmental expression different from majority (when n≥3, all differ from each other). Coloured borders for outgroup species denote kingdom of origin.

Figure 3: Quantification of conserved features.
Figure 3

(a) Using the data in Supplementary Data 2, percentages of DD DEGs were determined which had orthologues, homologues with conserved domains or homologues with conserved expression over 1 (DD only) or 2–5 Dictyostelid genomes. (b) For 72 unnamed genes (no known function) at 0.4-Mb intervals along the genome, percentages of orthologues and homologues, only, were determined over 1–5 Dictyostelid genomes. Percentages of homologues and homologues with conserved domains of DD DEG (c) and unbiased genes (d) in each of the three amoebozoan genomes (PhyP, AC and EH) and the non-amoebozoan outgroup. Red: orthologues; light blue: homologues; dark blue: homologues with conserved domains; green: homologues with conserved gene expression.

GO term enrichment of DD DEGs that are unique to Dictyostelia

A total of 80 DD DEGs are absent from unicellular Amoebozoa and are therefore potential ‘multicellularity’ genes. We compared enrichment of GO terms between these multi-only DEGs and the remaining 305 uni+multi DEGs (Supplementary Data 3). Not surprisingly, both sets are enriched in development-associated biological process terms, but multi-only has more proteins involved in cell recognition and glucose homeostasis (Fig. 4a). Protein kinases and nucleotide-binding proteins are less prevalent in multi-only, while G-protein-coupled receptors and sensor histidine kinase-associated terms are highly enriched (Fig. 4b). The multi-only set also has less cytoplasmic and nuclear proteins than the uni+multi set, and is enriched in integral plasma membrane, spore wall and external proteins (Fig. 4c). Enrichment of transmembrane and external proteins in the multi-only set is substantiated by computational prediction of signal peptide and transmembrane domains (Fig. 4d; Supplementary Data 4). In multi-only, 58% of proteins have transmembrane domains, signal peptides or both, while for uni+multi this is only 27%. Strikingly, while there are six times more soluble than membrane-associated protein kinases in the uni+multi set, the few protein kinases in the multi-only set are mostly membrane-associated (Fig. 4e).

Figure 4: GO enrichment, signal peptides (SigP) and transmembrane (TM) domains.
Figure 4

(a-c) Enrichment of GO terms in the categories ‘biological process’ (a), ‘molecular function (b) and ‘cellular component’ (c). The sets of 305 and 80 DEGs, which are respectively with and without homologues in unicellular amoebozoa, were analysed for GO term enrichment (Supplementary Data 3). The 10 terms with lowest P values in each set are compared with the same terms in the other set. The enrichment factor (frequency in set/frequency in genome) for each term is shown. Note that for GO terms that are very abundant in the genome (numbers on right axis) low-enrichment factors are still associated with very low P values. (d) SigP and TM domains. Proteins in the 305 and 80 sets, as well as 37 proteins with limited conservation within Dictyostelia (green) were analysed with Phobius63 for transmembrane domains and signal peptides (Supplementary Data 4). Percentages of proteins with either SigP or TM domains, or with both are presented. (e) Protein kinase localization. All protein kinases in the 305 and 80 sets (S/T/Y, histidine and alpha kinases) were analysed with Phobius (Supplementary Data 4) and numbers of proteins in each set without SigP or TM domains (soluble) and with either TM or SigP domains are presented.

Overall, it appears that signalling or sensing processes at the plasma membrane are enriched in DEGs, unique to Dictyostelia, while intracellular signal transduction proteins are shared with unicellular Amoebozoa.

Distribution of conserved features and outgroup homologues

Between Dictyostelia, gene expression profiles were generally conserved, with 69 being different in one species (Fig. 5a), 41 being different in group 4 and only 26 being different between the early diverging branches I and II (Fig. 1a). The prevalence of divergent gene regulation in group 4 is correlated with the major phenotypic innovation that occurred in this group3,4 (Fig. 1b). Functional domain architecture is also well conserved, but when different, the affected genes are more scattered across the phylogeny, suggesting no obvious links between domain change and phenotypic change (Fig. 5b).

Figure 5: Phylogenetic distribution of conserved features and outgroup homologues.
Figure 5

(a) Gene expression. Phylogenetic distribution of numbers of DEG with different patterns of conservation of gene expression. (4)(123) signifies that developmental expression was different between groups 4 and 1–3, while (I)(II) signifies different expression between branches I and II (Fig. 1a). (b) Protein domain architecture. Phylogenetic distribution of DEG with different patterns of functional domain conservation. (c) Origin of outgroup homologues. Numbers of DEG (out of 385) without no homologues outside Amoebozoa, or with outgroup homologues in each of the eukaryote kingdoms or in prokaryota. Inset; the same out of 72 unnamed genes.

For DD DEGs with homologues outside Amoebozoa, the sister kingdom Opisthokonta provided 152 outgroup homologues (Fig. 5c), while the remaining 122 were about equally distributed over other eukaryote kingdoms and prokaryotes. Eleven DD DEG (acgA, cadA, chlA, dgcA, dhkA, dhkB, dhkC, dokA, iptA, phyA and ppk1) have closest homologues in prokaryotes, but none in unicellular amoebozoa, suggesting acquisition by LGT. To validate these putative cases of LGT, we combined bidirectional searches with phylogenetic inference to assess whether the DD gene was indeed more closely related to its prokaryote homologue than to any eukaryote gene outside of Dictyostelia. The results of these analyses are listed in Supplementary Data 5 and summarized in Table 1.

Table 1: Analysis of candidate genes for lateral gene transfer.

For acgA, dhkA, dhkB, dhkC, phyA and ppk1, LGT appeared to have occurred more deeply in the eukaryote lineage, while for cadA, its homologue cadC is the more likely candidate for LGT. DgcA is very prevalent in bacteria and therefore a common contaminant of eukaryote genome sequences. However, in such cases, the LGT candidates are neither transcribed nor present in close relatives of the eukaryote host. The Dictyostelid dgcAs are present in all Dictyostelid genomes and were shown to have a biological role in DD13. ChlA, dokA and iptA also appeared to be genuine cases of LGT. For iptA, this was already proposed previously5. DgcA, chlA and iptA encode the enzymes that respectively synthesize c-di-GMP, DIF-1 and discadenine (Table 2), which, with cyclic AMP (cAMP) and 4-Methyl-5-pentylbenzene-1,3-diol (MBPD), represent all known differentiation-inducing signals in DD that are not of peptide origin1,14.

Table 2: Dictyostelium DEGs with closest homologues in prokaryotes.

Non-conserved DEGs

Genes that have a proven function in DD, but limited conservation in other Dictyostelia are of interest, since their appearance in the course of Dictyostelid evolution may have caused group-specific phenotypic innovation. Table 3 summarizes 37 DD DEGs that are unique to DD, to group 4 (DD+DP) or to branch II (DD+DP+DL). Twenty-six of these proteins contain a signal peptide or single transmembrane domain, indicating they are either secreted or exposed exteriorly. High enrichment of exteriorly exposed proteins was also evident for DD DEGs that are unique to Dictyostelia, indicating that this class of proteins is most frequently subjected to gain, loss and/or major modification in the course of multicellular evolution. Among them are four spore coat proteins (CotA, B, C and E), five matrix proteins with CTDC domains and three Tgr adhesion proteins. These three types of exposed proteins belong to large variable families that are present in all Dictyostelia, PhyP and for Tgrs also AC (Table 4). Binding of compatible Tgr variants mediates kin recognition, excluding unrelated cells from participating in the same fruiting body15,16. In aggregative multicellularity, this is an important feature, since unrelated cells entering the aggregate can cheat by forming predominantly spores and not stalk cells. In case of obligate cheaters, lack of stalk cell differentiation could lead to the collapse of multicellularity17,18. The mutual adhesiveness of cells with compatible Tgr proteins not only keeps them together in one aggregate, but also triggers signalling pathways that are required for post-aggregative development19. Obviously, for these proteins species specificity is essential for their function. Among the matrix proteins with CTDC domains, four (pdiA, psiA, psiF and psiN) also act as signals or signal regulators.

Table 3: Molecular functions of DD DEGs with limited conservation.
Table 4: Amoebozoan families of exposed and secreted proteins.

Among the other exposed DEGs are the two countin proteins, CtnB and CtnC, which are unique to group 4. With CtnA, these proteins are components of the counting factor complex of secreted proteins that regulates aggregate size20. Interestingly, SmlA and SslA1, two proteins that regulate secretion or processing of counting factors21,22 are also unique to group 4, suggesting that size regulation by counting factor complex was elaborated in this group. The remaining exposed/secreted proteins, ChtC, RtoA and SrsA, have roles in social cooperation23, cell-type proportioning24 and timely aggregation25, respectively, while two others, DDB_G0279727 and DDB_G0 268314, are needed for normal fruiting body formation26. None of these proteins have orthologues outside group 4, and their roles must also be recent.

Three intracellular proteins, DtfA, PonA and ManH, which are required for tip formation27, efficient chemotaxis28 and normal growth and development26, respectively, are unique to DD. Another intracellular protein, IptA, which synthesizes the spore germination inhibitor discadenine29, is unique to group 4. This agrees with the absence of discadenine from non-group 4 species30. CatB, a catalase required for H2O2 resistance of spores31, is an innovation of branch II.

Some transmembrane proteins involved in signal processing also show limited conservation. They are the cAMP phosphodiesterase Pde4, which is only present in branch II and is required for normal late development32, the ABC transporters TagB and TagD, which duplicated from TagC in DD only. TagB is with TagC required for prestalk differentiation33. The cAMP receptors CarB, CarC and CarD are also unique to group 4, with only CarA orthologues being present in groups 1–3, as evident from gene synteny and phylogenetic inference34,35. However, single and double gene duplications of CarA occurred in groups 2 and 1, respectively (Supplementary Data 2). DD CarB is essential for development beyond the mound stage36, while CarC and CarD have opposite effects on prespore/prestalk patterning by activating and inhibiting GSK3, respectively37,38. The duplicated CarA genes in PP have overlapping roles in fruiting body morphogenesis and induction of prespore differentiation by cAMP34,35, indicating that the roles of cARs B,C and D are novel to group 4. Zak1 and Zak2, two tyrosine kinases with overlapping roles in mediating CarC activation of GSK3 (refs 39, 40), are also unique to DD (Supplementary Data 2), as is the nuclear factor PslA. CarC, Zak1, Zak2, GSK3 and PslA are all proposed to mediate cAMP-induced prespore gene expression37,39,41,42, a process that also occurs in PP34, but evidently without CarC, Zak1, Zak2 or PslA. One study found no requirement for GSK3 in cAMP-induced prespore gene expression in DD43, while another excluded an essential role for CarC44. This evidence, together with the lack of most pathway components in non-group 4 species, encourages further study of this central pathway for Dictyostelid survival. The essential role of CarB in post-aggregative morphogenesis in DD is also enigmatic. To test whether its role may have been erroneously assigned, we recreated a carb null mutant in two different parent strains AX2 and AX3. Supplementary Figure 3 shows that both the AX2 and AX3 carb null mutants develop normally to fruiting bodies, indicating that carB is not of major importance for DD development. Evidently, essential central roles assigned to poorly conserved genes require careful scrutiny.

Discussion

The DL genome completes the set of high-quality genome sequences representative of the four major groups of Dictyostelia. Earlier comparative genome analyses have focussed on conservation and change in gene families, of which at least some members have established functions in biological processes. These analyses provided global information on differences in protein-coding potential between Dictyostelium taxon groups, and between Dictyostelia and other eukaryotes5,6,7. We seek to understand the genetic changes that caused the evolution of multicellularity and cell-type specialization, combining results from comparative genome analysis with detailed comparative phenotypic mapping of Dictyostelia3,4. In this work, we therefore investigated genes that have an established role in multicellular development of DD, and compared their conservation and change across the group-representative Dictyostelid genomes and three genomes of unicellular Amoebozoa. Not all genes in this set of 385 DEGs will control development directly in a regulatory manner. Many genes have unknown molecular functions; several, such as the spore coat genes, define the phenotype of the differentiated cells; others, such as cytoskeletal components, enable cellular movements that cause morphogenesis. However, since the boundaries between these categories are not clearly defined, we cannot meaningfully use them to assign subsets. We have however excluded all genes that are essential for growth, although the 385 set contains 66 DEGs that in addition to their developmental defects also show mild growth defects, when deleted.

A major outcome of the work is that a large percentage (73%) of DD DEGs is conserved as orthologues across all Dictyostelid taxon groups, while 76% of DEGs have orthologues or homologues in Physarum, the closest unicellular relative of Dictyostelia. This finding indicates that most of the genes required for multicellular development were already present in the last common unicellular ancestor to Dictyostelia. The conserved DEG have mostly similar transcription profiles across species, but for those which have not, differences occur more frequently between groups 4 and 1–3 than between the more distantly related branch I (groups 1 and 2) and branch II (groups 3 and 4). Phenotypic mapping revealed that group 4 is also phenotypically most different from groups 1–3 (refs 3, 4). The 41 genes with different regulation in group 4 therefore deserve deeper study into possible involvement in the phenotypic innovation in this group. For one gene, carA, this role was already established. This gene, encoding the chemotactic cAMP receptor, is expressed both during and after aggregation in group 4, but only after aggregation in groups 1–3 (ref. 35). Pre-aggregative expression of carA in group 4 is associated with the use of cAMP as chemoattractant for aggregation in this group3,34.

Changes in gene function may also cause phenotypic innovation, and such changes could be evident from changes in the functional domain architecture of proteins. However, in this case, only 10 architectures were different between group 4 and 1–3, and an equal number between branch I and II. Many more (51) diverging architectures were scattered across the Dictyostelid phylogeny, suggesting that the change in gene function, assessed by this metric, is not correlated with the phenotypic change. It therefore appears that in Dictyostelia, the phenotypic change is more closely correlated with the changes in gene regulation than the changes in gene function. Morphological evolution in metazoa was proposed to be caused more frequently by the changes in gene expression rather than gene function and several instances of the former were reported45.

Among the genes with limited conservation within Dictyostelia, 70% encode secreted or exposed proteins with roles in cell recognition, adhesion or signalling. Many of the remaining genes cause only minor aberrations when deleted, while among the set of poorly conserved genes with essential roles, there may be some for which this role was assigned in error. By repeating a gene knockout experiment for the group 4 specific gene carB, we show that the essential role of carB in post-aggregative development was overstated.

For most DD DEGs, the closest homologues outside Amoebozoa are found in Opisthokonta, the sister group to Amoebozoa, with the remaining homologues being about equally distributed among each of the other eukaryote divisions and prokaryotes. Four genes that are present in Dictyostelia, but not in unicellular Amoebozoa, entered Dictyostelia by LGT from prokaryotes. Three of these genes, dgcA, chlA and iptA, encode enzymes that synthesize three out of the five known non-peptide signals in DD that induce cell differentiation.

The set of 80 DEGs that are present in Dictyostelia, but not in unicellular Amoebozoa, is strongly enriched in proteins that are either secreted or exposed to the cell exterior and have roles in cell adhesion, sensing and cell–cell recognition. In contrast, the set of DEGs that are also present in unicellular Amoebozoa is enriched in cytosolic and nuclear proteins, with roles in nucleotide binding and protein kinase activity. The enrichment of secreted or exteriorly exposed proteins in DEGs unique to Dictyostelia suggests that the transition from uni- to multicellularity mostly required novel genes that mediate cell–cell interactions, while the intracellular machinery for processing these interactions was already present in the unicellular ancestor. Similar findings were also reported for distinctions between the multicellular metazoa and their unicellular holozoan relatives. Intracellular signal transduction components are generally well conserved in holozoa, while externally exposed proteins and sensors are much more diversified in the metazoa46,47,48. This distinction is particularly striking for the tyrosine kinases, where the cytosolic kinases, but not the receptor tyrosine kinases, are mostly conserved in holozoa48. Also in Amoebozoa, the few protein kinases that are unique to the multicellular Dictyostelia are mostly membrane associated (Fig. 4e).

Many of the secreted and exposed proteins that are unique to Dictyostelia or taxon groups within Dictyostelia are members of large families of adhesion and matrix proteins, which also have members in unicellular Amoebozoa. In the unicellular forms, they have likely roles in adhesion to substrata, mates and prey. We propose that these families are the reservoirs from which primordial multicellularity genes, mediating cell–cell adhesion, were recruited. For the next step, cell-type specialization, Dictyostelia converted some matrix/adhesion proteins, such as PsiA, PsiF, PsiN, TgrB and TgrC into signal molecules, but additionally acquired some genes to synthesize differentiation-inducing signals by LGT from their bacterial prey.

The importance of matrix proteins for the evolution of multicellularity is also demonstrated by experiments showing that under simple gravity selection, unicellular yeast and green algae evolve into multicellular agglomerates within months, accompanied by increased adhesion for yeast and matrix deposition for algae49,50. We show here that most genes required for multicellular development were already present in unicellular relatives or were recruited from existing matrix/adhesion protein families. Combined, these separate approaches show that the major evolutionary transition from uni- to multicellularity depended more on environmental pressures than massive genetic change.

Methods

Genome sequencing and assembly

DL cells, grown in association with Escherichia coli, were freed from bacteria and starved for 6 h. For genomic DNA isolation, 108 cells were resuspended in 0.5 ml 10 mM K-phosphate, pH 6.5, and cells were lysed by slowly adding the suspension to 3 ml ice-cold LB (0.32 M sucrose, 5 mM MgCl2, 1% Triton X-100 in 10 mM Tris (pH 7.5)). Nuclei were precipitated by centrifugation for 10 min at 7,500g, washed once and resuspended in 50 μl LB. The suspension was successively mixed with 0.5 ml of 10 μg ml−1 RNAseA and 10 mM EDTA in 10 mM Tris (pH 7.5), and 0.5 ml of 200 μg ml−1 proteinase K and 0.7% SDS in 10 mM Tris (pH 7.5), and incubated for 1 h at 65 °C and 1 h at 37 °C. After addition of 21 μl 5 M NaCl, the suspension was extracted with 1 ml 1:1 phenol/chloroform and once more with chloroform. DNA was precipitated by addition of 3.5 ml absolute ethanol to the supernatant fraction. DNA libraries for 454 Roche sequencing were prepared according to the manufacturer’s protocols. Libraries were sequenced, using a Roche flx platform, yielding 1.5 million raw reads, which added up to a genome coverage of 29 × . Initial assembly was performed with the Newbler assembler51 and contigs >500 bases were entered in the Staden assembly package52, including the Newbler-derived quality values. Fosmid libraries with average insert sizes of 32.5 kb in vector pCC2FOS were prepared according to the manufacturer’s instructions (Epicentre Biotechnologies). Fosmid ends were sequenced using the ABI BigDye kit, and standard forward primer 5′-GTACAACGACACCTAGAC-3′ and reverse primer 5′-CAGGAAACAGCCTAGGAA-3′. Pre-assembly trimming of sequences was performed with Phred53. The fosmid reads were mapped to the genome assembly using BLAT54. The fosmid end sequence information was used to assemble the contigs into scaffolds. Gaps in the scaffolds were closed by primer walking. The assembly and gap closure procedure resulted in 54 gap-free contigs spanning 23.4 Mb.

Chromosome structure analysis

The consensus sequences of the telomere repeats were used to search for contigs and single reads containing these repeats using BLASTn in the whole DL genome. The assembly of all contigs with such repeats was checked manually for wrongly assembled reads, since repetitive sequences tend to cause faulty assembly. Consensus sequences of the DD repetitive elements were used as query to find similar sequences in the genomes of the other social amoebae. Regions adjacent to telomeres were searched for other repeated sequence motifs. Detected repeat units were used next as query to find additional identical sequences throughout the genome.

Gene model prediction

Protein-coding genes were predicted using Augustus55 after training with DL transcript data obtained by Illumina sequencing (Supplementary Data 6). Specifically, single transcript reads were aligned to the reference genome sequence using BLAT54 and the resulting aligned positions were filtered against spurious hits. Intron–exon boundaries were extracted from the resulting alignments and used as a training set for Augustus. In addition, coding sequences from defined orthologues covered by transcript reads were used as a training set to define coding sequence features. The gene models used for comparative analysis in this manuscript were manually curated when alignment with orthologues indicated the presence of non-conserved indels.

Identification of orthologues of DEGs across species

DEGs are defined as DD genes, for which deletion causes defects in multicellular development. Around 385 DEGs were retrieved from Dictybase12. To identify orthologues of DD DEGs in other Dictyostelium species, unicellular Amoebozoa and other kingdoms, we first used Blastp to identify BBHs by query of Genbank for AC, EH and non-amoebozoan proteins, and query of locally generated libraries for DP, DL, PP, DF and PhyP proteins. The DP protein sequences were downloaded from Dictybase (http://dictybase.org/) and the Physarum library was derived from the translated Physarum reference transcriptome11. When proteins were missing in a single species, the query was repeated with a tBlastn query of genome sequence to retrieve coding sequences that had escaped computational gene model prediction.

The BBH approach cannot distinguish between orthologues and paralogues with full confidence, particularly when genes are members of larger families. We therefore used Bayesian phylogenetic inference (see below) to determine relatedness between protein sequences, and assessed orthology from the node structure and branch lengths of the inferred phylogenies. Genes were validated as orthologues, when their phylogenetic position and branch length relative to that of the DD DEG mirrored that of the amoebozoan species tree, constructed from 30 concatenated protein sequences3. The term homologue comprises both paralogues and orthologues that could not be validated because tree nodes were not well resolved or genes had undergone recent duplications. The phylogenies were annotated with the functional domain architectures of the proteins using SMART56, which provided additional evidence for evaluation of orthology.

Protein phylogenies

Protein sequences were aligned using Clustal Omega with five combined iterations57. Poorly aligned sections were deleted and phylogenetic relationships were determined using MrBayes v3.1.2 (ref. 58) after model selection in Topali59. Analyses were run for 1 million generations or until the standard deviation (SD) of split frequencies <0.01. Trees were midpoint rooted using Figtree v1.4.2 (ref. 60).

Comparative transcriptomics

For the group 4 species, DD and DP, replicate gene expression profiles that cover the 24 h developmental programme, as well as genes expressed in purified prestalk and prespore cells, were prepared by others8. The development of DL, PP and DF mostly takes longer than 24 h and is less synchronous than in group 4. RNAs were therefore isolated at specific stages of development, rather than at regular time intervals. Cells were cultured on one-fifth SM agar in association with E. coli, collected and distributed at 5 × 105 cells per cm2 on non-nutrient agar. Plates were incubated at 22 °C with charcoal pellets in the lids to improve synchronous development. RNA was isolated before plating cells (growth), at early and completed aggregation, tipped mound and slug stages, and at early and completed fruiting body formation. For PP, RNAs were also isolated from purified spores and stalks. First, unencapsulated cells from fruiting bodies were lysed with 0.1% Triton X-100 and next spores were separated from stalks by sieving though a 10-μm mesh. RNAs of amoeboid cells were isolated using the Qiagen RNAeasy kit. Fruiting bodies, spore and stalk samples were additionally vortexed for 15 min with glass beads in the first cell lysis step to break the cell walls. Poly-A RNA was isolated from 1 μg total RNA, and reverse-transcribed into complementary DNA (cDNA) using a random priming cDNA Synthesis kit (Roche).The cDNA was converted into a sequencing library for 454 sequencing using the GS FLX Titanium Rapid Library Preparation kit and sequenced on the Roche 454 platform. The resulting sequencing reads were mapped to the genome using BLAT54, and realigned with Exalign61 to determine the intron/exon boundaries. The expression levels were normalized by dividing the matching reads by the total number of reads obtained for each sample, multiplied by two times the average read length. The results are listed in Supplementary Data 6. Replicate developmental time series of PP, DL and DF were prepared in the same manner, but sequenced using the Illumina HiSeq platform. The results of these experiments are listed in Supplementary Data 6.

To compare developmental gene expression profiles between species, published expression data for DD and DP8 were stage-matched to new RNA expression data for DL, PP and DF. Normalized read counts from the individual time series were expressed as percentage of the maximum read count in the series. Normalized read counts for purified prestalk and prespore cells (DD and DP) or purified stalks and spores (PP) were expressed as percentage of the sum of the (pre)stalk and (pre)spore counts. For presentation, these percentages were converted into heatmaps as shown in Fig. 1c and Supplementary Data 2.

Validation of LGT

To validate putative instances of LGT, we used the criteria that Dictyostelid genes should first have prokaryote genes as BBHs and second should have prokaryote genes as closest sister group in phylogenies constructed from the closest prokaryote and eukaryote homologues. To identify BBHs, we first used the DD protein sequence as bait to query all non-redundant genes in Genbank, with the exclusion of Dictyostelia. When the best hits of the search were prokaryotes, the top prokaryote hit was used to query all non-redundant eukaryote genes. The first 10–20 eukaryotes hits were then aligned with the DD protein and the top hits from the first query as described above for protein phylogenies. The alignment was subjected to phylogenetic inference using MrBayes v3.1.2 (ref. 58) after model selection in Topali59. Analysis were run for 1 million generations or until the SD of split frequencies <0.01. Trees were also inferred using RAXML in Topali59 with 100 bootstrap replicates after model selection. All BlastP output files and the unrooted trees are shown in Supplementary Data 5.

CarB knockout

A 1.25-kB carB fragment was amplified from genomic DNA using primers carB sense (5′-AATTAAAAAATGACTATTATGTCAGAT-3′) and carB antisense (5′-TTATCACTTTTAAA TCATATCATTTTT-3′) and cloned blunt-end into a TOPO pCR2.1 plasmid vector. The actin15 blasticidin resistance cassette was obtained by digestion of pUCBsrΔBam62 with BamHI and HindIII, filled in with Klenow and blunt-end cloned into the filled in unique NdeI site of the carB fragment. For gene disruption, a knockout construct with the Bsr cassette in reverse orientation was amplified using the carB sense and carB antisense primers and transfected into DD AX2 and AX3 cells by electroporation. Gene disruption was confirmed by PCR with test primer carB-out (5′-AAAAAAACATCCCGAACA-3′) outside the knockout construct and primer Bsr2 (5′-AGCATTGTAATCTTCTCTGTCGCTACTTCTACT-3′) inside the blasticidin resistance cassette (Supplementary Fig. 3).

Data availability

The DL genome can be browsed in SACGB (http://sacgb.fli-leibniz.de/cgi/index.pl). The whole DL genome shotgun project has been deposited at DDBJ/EMBL/GenBank under the accession LODT01000000.1

Additional information

How to cite this article: Glöckner, G. et al. The multicellularity genes of dictyostelid social amoebas. Nat. Commun. 7:12085 doi: 10.1038/ncomms12085 (2016).

Accessions

GenBank/EMBL/DDBJ

References

  1. 1.

    Cell signaling during development of Dictyostelium. Dev. Biol. 391, 1–16 (2014).

  2. 2.

    et al. Molecular phylogeny and evolution of morphology in the social amoebas. Science 314, 661–663 (2006).

  3. 3.

    et al. Analysis of phenotypic evolution in Dictyostelia highlights developmental plasticity as a likely consequence of colonial multicellularity. Proc. Biol. Sci. 280, 20130976 (2013).

  4. 4.

    , & Evolutionary reconstruction of pattern formation in 98 Dictyostelium species reveals that cell-type specialization by lateral inhibition is a derived trait. EvoDevo 5, 34 (2014).

  5. 5.

    et al. The genome of the social amoeba Dictyostelium discoideum. Nature 435, 43–57 (2005).

  6. 6.

    et al. Phylogeny-wide analysis of social amoeba genomes highlights ancient origins for complex intercellular communication. Genome Res. 21, 1882–1891 (2011).

  7. 7.

    et al. Comparative genomics of the social amoebae Dictyostelium discoideum and Dictyostelium purpureum. Genome Biol. 12, R20 (2011).

  8. 8.

    et al. Conserved developmental transcriptomes in evolutionarily divergent species. Genome Biol. 11, R35 (2010).

  9. 9.

    et al. The genome of the protist parasite Entamoeba histolytica. Nature 433, 865–868 (2005).

  10. 10.

    et al. Genome of Acanthamoeba castellanii highlights extensive lateral gene transfer and early evolution of tyrosine kinase signaling. Genome Biol. 14, R11 (2013).

  11. 11.

    et al. The Physarum polycephalum genome reveals extensive use of prokaryotic two-component and metazoan-type tyrosine kinase signaling. Genome Biol. Evol. 8, 109–125 (2016).

  12. 12.

    , , , & Expanding data and annotations in a new software environment. Genesis 53, 523–534 (2015) .

  13. 13.

    & The prokaryote messenger c-di-GMP triggers stalk cell differentiation in Dictyostelium. Nature 488, 680–683 (2012).

  14. 14.

    , , , & The evolution of aggregative multicellularity and cell-cell communication in the Dictyostelia. J. Mol. Biol. 427, 3722–3733 (2015).

  15. 15.

    , , , & Self-recognition in social amoebae is mediated by allelic pairs of tiger genes. Science 333, 467–470 (2011).

  16. 16.

    , , & Kin recognition protects cooperators against cheaters. Curr. Biol. 23, 1590–1595 (2013).

  17. 17.

    , , & High relatedness is necessary and sufficient to maintain multicellularity in Dictyostelium. Science 334, 1548–1551 (2011).

  18. 18.

    & Evolution of cooperation and control of cheating in a social microbe. Proc. Natl Acad. Sci. USA 108, 10855–10862 (2011).

  19. 19.

    , , , & Allorecognition, via TgrB1 and TgrC1, mediates the transition from unicellularity to multicellularity in the social amoeba Dictyostelium discoideum. Development 142, 3561–3570 (2015).

  20. 20.

    , & Cell density sensing and size determination. Dev. Growth Differ. 53, 482–494 (2011).

  21. 21.

    et al. A cell number-counting factor regulates levels of a novel protein, SslA, as part of a group size regulation mechanism in Dictyostelium. Eukaryot. Cell 6, 1538–1551 (2007).

  22. 22.

    et al. A Dictyostelium mutant with defective aggregate size determination. Development 122, 2569–2578 (1996).

  23. 23.

    et al. Cheater-resistance is not futile. Nature 461, 980–982 (2009).

  24. 24.

    et al. RtoA links initial cell type choice to the cell cycle in Dictyostelium. Development 122, 3677–3685 (1996).

  25. 25.

    et al. An immediate-early gene, srsA: its involvement in the starvation response that initiates differentiation of Dictyostelium cells. Differentiation 76, 1093–1103 (2008).

  26. 26.

    , , & High-throughput analysis of spatio-temporal dynamics in Dictyostelium. Genome Biol. 8, R144 (2008).

  27. 27.

    , , , & A novel Dictyostelium cell surface protein important for both sell adhesion and cell sorting. Development 125, 3343–3352 (1998).

  28. 28.

    et al. Ponticulin plays a role in the positional stabilization of pseudopods. J. Cell Biol. 131, 1495–1506 (1995).

  29. 29.

    & Cytokinins induce sporulation in Dictyostelium. Development 135, 819–827 (2008).

  30. 30.

    , & Discadenine distribution in cellular slime molds and its inhibitory activity on spore germination. Agric. Biol. Chem. 45, 1295–1296 (1981).

  31. 31.

    , , , & The Dictyostelium discoideum prespore-specific catalase B functions to control late development and to protect spore viability. Biochim. Biophys. Acta. 1641, 55–64 (2003).

  32. 32.

    , , & DdPDE4, a novel cAMP-specific phosphodiesterase at the surface of Dictyostelium cells. J. Biol. Chem. 281, 20018–20026 (2006).

  33. 33.

    , & A multidrug resistance transporter/serine protease gene is required for prestalk specialization in Dictyostelium. Genes Dev. 9, 1111–1122 (1995).

  34. 34.

    et al. Activated cAMP receptors switch encystation into sporulation. Proc. Natl Acad. Sci. USA 106, 7089–7094 (2009).

  35. 35.

    et al. Evolutionary origin of cAMP-based chemoattraction in the social amoebae. Proc. Natl Acad. Sci. USA 102, 6385–6390 (2005).

  36. 36.

    et al. CAR2, a prestalk cAMP receptor required for normal tip formation and late development of Dictyostelium discoideum. Genes Dev. 7, 262–272 (1993).

  37. 37.

    , , & Glycogen synthase kinase-3 (GSK-3) is regulated during Dictyostelium development via the serpentine receptor cAR3. Development 126, 325–333 (1999).

  38. 38.

    , & The cAMP receptor CAR4 regulates axial patterning and cellular differentiation during late development of Dictyostelium. Genes Dev. 8, 2086–2096 (1994).

  39. 39.

    , & The novel tyrosine kinase ZAK1 activates GSK3 to direct cell fate specification. Cell 99, 399–408 (1999).

  40. 40.

    et al. Combinatorial cell-specific regulation of GSK3 directs cell differentiation and polarity in Dictyostelium. Development 138, 421–430 (2011).

  41. 41.

    , , , & Glycogen synthase kinase 3 regulates cell fate in Dictyostelium. Cell 80, 139–148 (1995).

  42. 42.

    , & Identification and analysis of a gene that is essential for morphogenesis and prespore cell differentiation in Dictyostelium. Development 125, 2565–2576 (1998).

  43. 43.

    , , , & GSK3 is a multifunctional regulator of Dictyostelium development. Development 131, 4555–4565 (2004).

  44. 44.

    , , , & Functional promiscuity of gene regulation by serpentine receptors in Dictyostelium discoideum. Mol. Cell. Biol. 18, 5744–5749 (1998).

  45. 45.

    & Changes in cis-regulatory elements during morphological evolution. Biology (Basel) 1, 557–574 (2012).

  46. 46.

    , , , & Unexpected repertoire of metazoan transcription factors in the unicellular holozoan Capsaspora owczarzaki. Mol. Biol. Evol. 28, 1241–1254 (2011).

  47. 47.

    et al. The Capsaspora genome reveals a complex unicellular prehistory of animals. Nat. Commun. 4, 2325 (2013).

  48. 48.

    et al. Genomic survey of premetazoans shows deep conservation of cytoplasmic tyrosine kinases and multiple radiations of receptor tyrosine kinases. Sci. Signal. 5, ra35 (2012).

  49. 49.

    , , & Experimental evolution of multicellularity. Proc. Natl Acad. Sci. USA 109, 1595–1600 (2012).

  50. 50.

    et al. Experimental evolution of an alternating uni- and multicellular life cycle in Chlamydomonas reinhardtii. Nat. Commun. 4, 2742 (2013).

  51. 51.

    , & Assembly algorithms for next-generation sequencing data. Genomics 95, 315–327 (2010).

  52. 52.

    , & A new DNA sequence assembly program. Nucleic Acids Res. 23, 4992–4999 (1995).

  53. 53.

    , , & Base-calling of automated sequencer traces using phred. I. Accuracy assessment. Genome Res. 8, 175–185 (1998).

  54. 54.

    BLAT--the BLAST-like alignment tool. Genome Res. 12, 656–664 (2002).

  55. 55.

    & AUGUSTUS: a web server for gene prediction in eukaryotes that allows user-defined constraints. Nucleic Acids Res. 33, W465–W467 (2005).

  56. 56.

    , , & SMART, a simple modular architecture research tool: identification of signaling domains. Proc. Natl Acad. Sci. USA 95, 5857–5864 (1998).

  57. 57.

    & Clustal omega, accurate alignment of very large numbers of sequences. Methods Mol. Biol. 1079, 105–116 (2014).

  58. 58.

    & MrBayes 3: Bayesian phylogenetic inference under mixed models. Bioinformatics 19, 1572–1574 (2003).

  59. 59.

    et al. TOPALi v2: a rich graphical interface for evolutionary analyses of multiple alignments on HPC clusters and multi-core desktops. Bioinformatics 25, 126–127 (2009).

  60. 60.

    Figtree. Available at (2006).

  61. 61.

    , , & Exalign: a new method for comparative analysis of exon–intron gene structures. Nucleic Acids Res. 36, e47–e47 (2008).

  62. 62.

    , , , & Isolation of Dictyostelium discoideum cytokinesis mutants by restriction enzyme-mediated integration of the blasticidin S resistance marker. Biochem. Biophys. Res. Commun. 205, 1808–1814 (1994).

  63. 63.

    , & Advantages of combined transmembrane topology and signal peptide prediction--the Phobius web server. Nucleic Acids Res. 35, W429–W432 (2007).

  64. 64.

    , & A flavin-dependent halogenase catalyzes the chlorination step in the biosynthesis of Dictyostelium differentiation-inducing factor 1. Proc. Natl Acad. Sci. USA 107, 5798–5803 (2010).

  65. 65.

    , & DIF-1 induces the basal disc of the Dictyostelium fruiting body. Dev. Biol. 317, 444–453 (2008).

  66. 66.

    , , , & The hybrid histidine kinase DokA is part of the osmotic response system of Dictyostelium. EMBO J. 15, 3880–3889 (1996).

  67. 67.

    , , & Structure of discadenine, a spore germination inhibitor from the cellular slime mold. Tetrahedron Lett. 17, 3807–3810 (1976).

  68. 68.

    et al. InterProScan 5: genome-scale protein function classification. Bioinformatics 30, 1236–1240 (2014).

Download references

Acknowledgements

This work was supported by BBSRC project grants BB/E016308, BB/K000799/1 and BB/G020426/1, and Wellcome Trust Senior Investigator Award 100293/Z/12/Z to P.S.

Author information

Affiliations

  1. Institute of Biochemistry I, Medical Faculty, University of Cologne, Cologne D-50931, Germany

    • Gernot Glöckner
  2. Leibniz Institute of Freshwater Ecology and Inland Fisheries (IGB), Müggelseedamm 301, Berlin D-12587, Germany

    • Gernot Glöckner
  3. Division of Cell and Developmental Biology, School of Life Sciences, University of Dundee, Dundee DD15EH, UK

    • Hajara M. Lawal
    • , Reema Singh
    • , Gail Singer
    • , Cornelis J. Weijer
    •  & Pauline Schaap
  4. Leibniz Institute on Aging, Beutenbergstr.11, Jena D-07745, Germany

    • Marius Felder

Authors

  1. Search for Gernot Glöckner in:

  2. Search for Hajara M. Lawal in:

  3. Search for Marius Felder in:

  4. Search for Reema Singh in:

  5. Search for Gail Singer in:

  6. Search for Cornelis J. Weijer in:

  7. Search for Pauline Schaap in:

Contributions

G.G. prepared genome and cDNA libraries, sequenced and assembled the DL genome, performed gene model prediction, and sequenced transcriptomes. H.M.L. performed fosmid sequencing, primer walking and most bioinformatic analysis. R.S. performed bioinformatics. G.S. and C.J.W. analysed carB knockouts. P.S. designed the study and wrote the manuscript.

Competing interests

The authors declare no competing financial interests.

Corresponding author

Correspondence to Pauline Schaap.

Supplementary information

PDF files

  1. 1.

    Supplementary Information

    Supplementary Figures 1-3, Supplementary Tables 1-2 and Supplementary References

  2. 2.

    Supplementary Data 2

    Phylogenies of D. discoideum developmentally essential genes and their homologs, annotated with domain architectures and developmental expression profiles

Excel files

  1. 1.

    Supplementary Data 1

    Spreadsheet listing all D. discoideum genes analysed in this work with their knock-out phenotypes, protein function and homologs in Amoebozoa

  2. 2.

    Supplementary Data 3

    Spreadsheet listing gene ontology terms that are enriched in the set of developmentally essential genes that are present in both unicellular Amoebozoa and Dictyostelia and the set that is only present in Dictyostelia

  3. 3.

    Supplementary Data 4

    Spreadsheet listing the presence of transmembrane domains and signal peptides in four subsets of D. discoideum developmentally essential genes

  4. 4.

    Supplementary Data 5

    Spreadsheet listing the BLASTp queries and phylogenetic trees that provide the evidence in favour or against instances of lateral gene transfer for 11 D. discoideum genes

  5. 5.

    Supplementary Data 6

    Sequencing statistics and read counts for high throughput RNA sequencing of P. pallidum, D. fasciculatum and D. lacteum developmental time courses

About this article

Publication history

Received

Accepted

Published

DOI

https://doi.org/10.1038/ncomms12085

Further reading

Comments

By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.