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High-throughput genome sequencing of lichenizing fungi to assess gene loss in the ammonium transporter/ammonia permease gene family

BMC Genomics volume 14, Article number: 225 (2013) Cite this article

Abstract

Background

Horizontal gene transfer has shaped the evolution of the ammonium transporter/ammonia permease gene family. Horizontal transfers of ammonium transporter/ammonia permease genes into the fungi include one transfer from archaea to the filamentous ascomycetes associated with the adaptive radiation of the leotiomyceta. The horizontally transferred gene has subsequently been lost in most of the group but has been selectively retained in lichenizing fungi. However, some groups of lichens appear to have secondarily lost the archaeal ammonium transporter. Definitive assessment of gene loss can only be made via whole genome sequencing.

Results

Ammonium transporter/ammonia permease gene sequences were recovered from the assembled genomes of eight lichenizing fungi in key clades including the Caliciales, the Peltigerales, the Ostropomycetidae, the Acarosporomycetidae, the Verrucariales, the Arthoniomycetidae and the Lichinales. The genes recovered were included in a refined phylogenetic analysis. The hypothesis that lichens symbiotic with a nitrogen-fixing cyanobacterium as a primary photobiont or lichens living in high nitrogen environments lose the plant-like ammonium transporters was upheld, but did not account for additional losses of ammonium transporters/ammonia permeases in the lichens from the Acarosporomycetidae, Chaetotheriomycetes and Arthoniomycetes. In addition, the four ammonium transporter/ammonia permease genes from Cladonia grayi were shown to be functional by expressing the lichen genes in a strain of Saccharomyces cerevisiae in which all three native ammonium transporters were deleted, and assaying for growth on limiting ammonia as a sole nitrogen source.

Conclusions

Given sufficient coverage, next-generation sequencing technology can definitively address the loss of a gene in a genome when using environmental DNA isolated from lichen thalli collected from their natural habitats. Lichen-forming fungi have been losing ammonium transporters/ammonia permease genes at a slower rate than the most closely related non-lichenized lineages. These horizontally transferred genes in the Cladonia grayi genome encode functional ammonium transporters/ammonia permeases.

Background

Lichens are symbioses between a fungus and a photosynthesizing partner such as a green alga, a cyanobacterium, or both. About one-fifth of all known fungi lichenize, and for these fungi the symbiosis is, with few exceptions, obligate. Unlike mycorrhizal or rhizobial symbioses, lichen symbioses are not well understood. This is mainly because lichens grow very slowly (≤1 cm a year), it is very difficult to grow the fungus and the alga separately and, moreover, it is not yet possible to resynthesize the mature symbiosis in the laboratory from the fungal and photobiont partners isolated in axenic culture [1–4]. Also, it is not yet possible to delete genes, nor has any transformation method been established to introduce genes into the genomes of any lichenizing fungus or alga. However, the lack of genetic tools for these intractable organisms has been partially compensated for by the advent of high-throughput genome sequencing.

Previously, the genomes of the model lichen Cladonia grayi, made up of the lichenizing fungus Cladonia grayi for which the association is named, and its green algal partner Asterochloris sp., were sequenced at Duke University [5, 6]. We searched the genome sequences for evidence of horizontal gene transfer [7–9] between the lichen symbionts; that is, whether there were genes of algal origin in the fungal genome or genes of fungal origin in the algal genome. A thorough homology search of all the genes in each genome revealed that two genes in the fungal genome appeared to have been horizontally transferred, although not from green algae. Both genes encoded ammonium transporters [10].

Ammonium transporters/ammonia permeases (AMTPs) are highly conserved proteins found in most organisms, including prokaryotes and eukaryotes. These proteins are composed of 11 transmembrane helices that fold to form a pore through which ammonia or ammonium moves [11, 12]. In their native conformation they trimerize, forming a tripartite pore [13]. While some AMTPs have been shown to transport ammonium (NH4+), notably those proteins in the AMT2 family of land plants [14, 15], most AMTPs have been shown to transport ammonia (NH3) [16–22]. Proteins in the related Rh family [23] have 12 transmembrane domains and have been shown to conduct ammonia and in some cases CO2[24–26].

The evolutionary history of this family of genes is complex, involving lineage-specific gene family expansions, contractions, and losses as well as ancient and recent horizontal gene transfer events. Fungal AMTPs are in a phylogenetic clade by themselves that includes both low-affinity [27–30] and high-affinity [31–35] AMTPs (MEP γ clade [10]). The history of these genes in the fungi is particularly complicated, appearing to commence with an ancient horizontal gene transfer event of high-affinity AMTPs of prokaryotic origin during the early evolution of the fungi, followed by several lineage-specific gene-family expansions, as well as a duplication and neofunctionalization event in the early evolution of the Dikarya that lead to the evolution of low-affinity AMTPs [10].

In addition to these events, a second horizontal gene transfer event of high-affinity AMTPs occurred in the early evolution of filamentous ascomycetes (associated with a putative adaptive radiation of the leotiomyceta [10, 36, 37]). These horizontally transferred AMTPs are distinct from the fungal high- and low-affinity AMTPs of the MEP γ clade, and in fact are most closely related to AMTPs from land plants in the AMT2 family e.g. [12, 15, 35, 38–41] and to transporters from mostly hyperacidophilic chemoautolithotrophic prokaryotes inhabiting deep sea thermal vents [42], volcanic hotsprings and thermal vents [43–48], acid mine drainages [49–55], and similar extreme environments (MEP α clade) [10].

Interestingly, only a subset of the leotiomyceta, most of which are symbiotic with green algae in lichen symbioses, have representatives of this new clade of AMTPs in their genomes. In fact, lichenizing fungi in three different taxonomic classes of fungi, including the Lecanoromycetes, the Eurotiomycetes and the Dothideomycetes [36, 56, 57], have actually duplicated these genes. By contrast, as of 2012 only four non-lichenizing fungi in two genera (Penicillium with Talaromyces teleomorphs, Fusarium with Gibberella teleomorphs) out of more than 200 publicly available sequenced fungal genomes have representatives of this new clade of AMTPs in their genomes, and these transporters are not duplicated. This result suggests that lichenized fungi have preferentially retained the MEP α gene after the initial horizontal gene transfer event during the early evolution of the filamentous ascomycetes, while non-lichenized fungi have lost this gene [10].

The MEP α gene was not found in all lichens surveyed. In particular, the MEP α gene was never recovered from the two orders of lichens most closely related to the order in which the original discovery was made. In one of these two orders, the Peltigerales [58], the lichens are symbiotic with nitrogen-fixing cyanobacteria. In the other order, the Teloschistales [59], many lichens inhabit high-nitrogen niches, like bird perching sites. The availability of nitrogen sources from the environment or from a symbiont, coupled with the failure to identify the AMTP gene by PCR suggests that lichens in these two orders may no longer need the MEP α AMTP and may have shed it from their genomes.

Here, we further characterize this new clade of fungal AMTPs. We sequence the genomes of eight lichenizing fungi in key lineages that may have shed the AMTPs and search the genomes for the horizontally-transferred AMTPs. We correlate the presence of the AMTPs of the new clade with nitrogen lifestyle by surveying lichen fungi that are closely related to the main lineages previously examined but that tolerate high-nitrogen habitats, or that employ nitrogen-fixing cyanobacteria rather than green algae as the primary symbionts. We also characterize the function of the AMTPs from one lichen, Cladonia grayi, by assaying for growth on ammonium as a sole nitrogen source. We present a phylogeny of fungal AMTPs to contextualize this clade.

Results

Genome assembly completeness

There is no way to definitively assess the absence of a gene from a genome except the sequencing of the whole genome. Even then, however, it could be argued that the gene is in fact present in the genome but is not found simply because the assembly is incomplete. In order to test completeness of the assemblies, the CEGMA (Core Eukaryotic Genes Mapping Approach) pipeline [60, 61] was used. CEGMA queries against a core group of 248 highly conserved eukaryotic genes (CEGs). Completeness scores (Table 1) varied from 92-96% complete, and 97-98% partial detection of CEGs, respectively, for all genomes except Physcia. For comparison we assessed the two publicly available and well-assembled genomes of Aspergillus fumigatus AF293 [62] and Neurospora crassa or74a [63] with this method and determined scores of 96% complete and 97-98% partial CEGs detection. Data on the assemblies is shown in Table 2, and statistics on the raw data is presented in Table 3.

Table 1 Statistics on the completeness of lichen genome assemblies as determined by CEGMA
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Table 2 Statistics on the genome assemblies for five cultured lichens and metagenome assemblies for three lichen thalli
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Table 3 Statistics on the raw data for eight lichen genomes
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These data were of interest as of the eight lichens sequenced, four were actually metagenome projects. Lichens can be seen as micro-communities, hosting not just the mycobiont (fungal) and photobiont (algal or cyanobacterial symbionts), but a rich internal microbiota composed of bacteria and endolichenic fungi [64, 65]. As lichenizing fungi have only infrequently been successfully cultured compared to other fungi (although see [66, 67]), and because it can take up to three years to produce enough tissue to extract sufficient DNA for a genome sequence, sequencing a metagenome from thalli taken directly from nature would greatly reduce the time required for a genome project, were the final product of useful quality. The lichens used for metagenomes here included two cyanolichens symbiotic with cyanobacteria, and two lichens symbiotic with green algae, one of which has a very tight association with the algal symbiont, and one of which produces large fungal fruiting stalks (podetia) essentially devoid of the algal symbiont. The data show that where the symbiont is a cyanobacterium (prokaryote), or where the fungal portion of the thallus can be easily removed from the algal portion, the assembly suffers only a little compared to the assembly of a genome from a fungal culture. However, when the fungal and algal portions of the lichen cannot be easily dissected, as with Physcia cf. stellaris, the assembly is more problematic. It is therefore deemed not strictly necessary, but preferable, to sequence these fungi from culture where feasible.

In further test queries, 20 putative single-copy nuclear genes, which are conserved throughout the fungi were chosen as references. These genes are of approximately comparable size to the AMTP genes. If part or all of each of the 20 test sequences could be recovered from a genome, then it was considered likely that homology searches for genes of interest, i.e. AMTPs and particularly the MEP α gene(s), would identify at least a portion of the gene(s) if such were present in the genome. All 20 of the test genes were recovered from each of the eight genomes (Table 4). In addition, unexpected duplicate copies of some of the genes, including Fal1 and Mcm7, were discovered. It was therefore concluded that the genomes were complete enough to recover genes of interest, and further to lend confidence to calls of absence were the genes not recovered. It was deemed important to be able to comment on absence since initial attempts to amplify by PCR the MEP α gene from several of the lineages included here consistently failed. Using the four Cladonia grayi MEP genes as queries, the MEP genes from all eight genomes were identified (Table 4) as described below.

Table 4 Presence/absence of ammonium transporter/ammonia permease genes and 20 conserved test genes
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Plant-like MEP α AMTPs are missing from the genomes of lichens growing in high-nitrogen habitats

Previously, the MEP α genes had been amplified from the Lecanorales but not from any other order sampled within the subclass Lecanoromycetidae (Figure 1). The genomes of lichens in two additional orders within the Lecanoromycetidae, the Caliciales (sensu[59]) and the Peltigerales, were sequenced here. One more order, the Teloschistales, is now represented by a genome of the lichenizing fungus Xanthoria parietina[68]. These orders are particularly interesting in terms of nitrogen tolerance and acquisition. Lichens in the Teloschistales and Caliciales tend to grow in nitrogen-rich environments, such as rocks or tree limbs on which birds perch. Because nitrogen is not limiting in these environments, it was hypothesized that the previous failure to amplify by degenerate PCR any MEP α genes in the lichens in these orders was evidence that the plant-like AMTPs genes had been lost. As predicted, no plant-like AMTP was found in Physcia cf. stellaris (Table 4). The same was true for Xanthoria parietina. The loss of plant-like AMTPs in the lichens in these orders might suggest why many of these lichens are constrained to living in high-nitrogen environments; alternatively, the expansion of lichens in the Teloschistales and Caliciales into high-nitrogen niches may have removed the selective pressure to retain the MEP α genes.

Figure 1
figure1

Simplified phylogenetic tree showing the placement of the eight lichenizing fungi used for genome sequencing. Lichenizing fungi used for genome sequencing are underlined. Species with plant-like transporters in the MEP α clade are shown in bold. Simplified from [56, 69].

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Plant-like MEP α AMTPs are missing from the genomes of lichens that are symbiotic with nitrogen-fixing cyanobacteria

Another order of lichens within the Lecanoromycetidae for which no plant-like AMTPs were amplified by degenerate PCR is the Peltigerales. This order is primarily composed of lichens in which the photobiont is a nitrogen-fixing cyanobacterium (Nostoc). Also in this order are lichens with both a green alga and a cyanobacterium as photobionts, but these lichens have secondarily regained the green algal photobiont [58]. Data from two unpublished genome projects on various species of Peltigera showed that each species of Peltigera had high- affinity fungal AMTPs and one low-affinity fungal AMTP, but no plant-like AMTPs (Ólafur S. Andrésson, personal communication and unpublished data; Bernard Goffinet, unpublished data). The fact that one lichen genus that is symbiotic with a nitrogen fixer seemed to have lost the plant-like AMTPs led to the hypothesis that cyanolichens in general have lost the MEP α AMTPs. To test this hypothesis, the lichen Leptogium austroamericanum in a separate suborder of the Peltigerales was chosen for genome sequencing. No MEP α AMTPs were found (Table 4). Thus, because lichens in both suborders of the Peltigerales lack the plant-like AMTPs, we suggest that all the lichens in the Peltigerales lack the plant-like AMTPs. Previous studies have reconstructed the ancestral state of the Peltigerales as a bi-membered association with a cyanobacterium [58]. It is possible that, having acquired a nitrogen fixer as a symbiont, the need for the nitrogen presumably provided by the horizontally transferred AMTPs was alleviated, allowing this gene to be lost during the early evolution of the Peltigerales. This suggests that the MEP α AMTPs will not be found in any of the green-algal associated members of the order either, as the symbiosis with a green alga is secondarily acquired. This may also suggest a reason why even most green algal members of the order continue to retain cyanobacteria in cephalodia—to supplement the nitrogen budget. Likewise, it is unusual for a fungus to have just two AMTP genes, particularly a filamentous ascomycete. Perhaps the presence of a nitrogen-fixing symbiont provides sufficient nitrogen so that there is no pressure to duplicate the AMTPs. In addition to the Peltigerales, cyanolichens are also found in the Lichinomycetes, a small class of lichenizing fungi evolutionarily distant from the bulk of lichens found in the Lecanoromycetes (Figure 1). Lichen-forming fungi in the Lichinales are mostly symbiotic with cyanobacteria other than Nostoc, such as Anacystis[70]. It was hypothesized that, like the lichens in the Peltigerales, lichens in the Lichinomycetes would also have lost the MEP α AMTPs upon acquisition of a cyanobacterium as a photobiont. No MEP α AMTPs were found in this genome. It seems likely that the other members of this class which are also symbiotic with cyanobacteria may also have lost the MEP α AMTP.

Plant-like AMTPs are found in the Ostropomycetidae but not the Acarosporomycetidae, and are distributed patchily in the Chaetothyriomycetidae

If loss of MEP α AMTPs is strictly associated with the photobiont of a lichen, then it would be expected that lichens with green algal photobionts should retain the MEP α gene(s). However, the failure to identify MEP α genes in other subclasses within the Lecanoromycetes by degenerate PCR argued against this hypothesis. To determine whether MEP α genes were present in other subclasses within the Lecanoromycetes, namely the Ostropomycetidae and the Acarosporomycetidae (Figure 1), the genomes of Dibaeis baeomyces (Ostropomycetidae), Graphis scripta (Ostropomycetidae) and Acarospora strigata (Acarosporomycetidae) were sequenced. MEP α genes were identified in Graphis scripta and Dibaeis baeomyces, both members of the Ostropomycetidae (Table 4, Figure 1). This finding represents an extension of the known distribution of MEP α genes. Further, Dibaeis and Graphis are in different orders within this subclass, suggesting that the MEP α gene may be widespread in the subclass (Figure 1). No plant-like AMTPs were found in the genome of Acarospora strigata, which is found in the earliest diverged subclass within the Lecanoromycetidae. Previously, one lichen in the subclass Chaetothyriomycetidae (Pyrenula cruenta) was shown to have a MEP α gene. Genome sequencing of Endocarpon pallidulum, a second lichen in the subclass Chaetothyriomycetidae but in a different order, revealed that no MEP α AMTP was present in the genome. This was surprising as Trypethelium virens and Laurera megasperma in the Dothidiomycetes, even more distantly related class, were shown to have the MEP α genes [10].

The MEP α gene replaces the high-affinity MEP γ gene in Graphis scripta

Low-affinity fungal AMTPs falling into the MEP γ clade were found in all genomes, as expected given the presence of these genes in the genomes of all Dikarya fungi sequenced to date (Table 4). Likewise, high-affinity fungal AMTPs in the MEP γ clade have been found in all fungi to date [10]. However, high-affinity fungal AMTPs were recovered in only seven of the eight lichen genomes sequenced here. Graphis scripta appeared to be lacking a high-affinity MEP γ gene, which is unprecedented among the Dikarya fungi. The similarity of MEP genes is high throughout the transmembrane domains, such that any MEP gene used as a query will find all other MEP genes in the genome. Furthermore, the Graphis scripta genome was produced from the cultured fungus, and the genome is very high coverage (173×). Of the eight new genomes presented here, this is the genome that received the highest CEGMA score for complete genes, a score nearly identical to the CEGMA score obtained by the Neurospora crassa genome (Table 1). Therefore, it is unlikely that no portion of the high-affinity MEP γ gene would have been sequenced if it were in the genome. Thus, it seems likely that this fungus actually lacks the high-affinity MEP γ gene.

Other lichens like Arthonia rubrocincta or Leptogium austroamericanum that have only two AMTPs have the fungal high-affinity MEP γ gene and the fungal low-affinity MEP γ gene (Table 4). Dibaeis baeomyces, which like Graphis scripta is in the Ostropomycetidae, has two copies of a MEP α gene as well as one fungal high-affinity AMTP and one fungal low-affinity AMTP, suggesting that perhaps the ancestor to the Ostropomycetidae or even the Lecanoromycetes had all four AMTPs. It would appear that in Graphis scripta the MEP α gene has replaced the high-affinity fungal AMTP from the MEP γ clade. Graphis scripta has a very thin crustose thallus, quite unlike the large thalli produced by many lichens in the Lecanorales. It is perhaps no surprise that less nitrogen is needed to support this comparatively reduced thallus. That the MEP α gene is retained in preference to the high-affinity fungal AMTP suggests that it was perhaps more efficient than the high-affinity fungal AMTP.

The MEP genes are functional AMTPs

The fungal high-affinity AMTP (mep2), fungal low-affinity AMTP (mep3), and two plant-like AMTPs (mep1a and mep1b) were introduced individually into a strain of Saccharomyces cerevisiae in which all three native AMTPs had been deleted. All four C. grayi genes complemented the mutant, although growth was not robust. Therefore, each of the genes was deemed to be a functional AMTP (Figure 2). Of the four genes, the low-affinity AMTP (mep3) appeared generated the most robust growth under the conditions tested, albeit marginally so. This observation is consistent with the predicted function of this gene as a low-affinity (high-capacity) AMTP. Importantly, the mep1a and mep1b are the first genes from the fungal subclade of the MEP α clade for which a function has been demonstrated.

Figure 2
figure2

Heterologous expression of Cladonia grayi AMTP genes in a strain of Saccharomyces cerevisiae lacking AMTPs. Left: Ten-fold serial dilutions (107 to 103 cells/ml) of a S. cerevisiae (Sc) AMTP triple knockout complemented with AMTPs from the lichenizing fungus Cladonia grayi (Cg). Left, limiting ammonium (5 mM); right, control plate with excess ammonium (20 mM). Top to bottom, 1–6, transformants of MLY131 (a/α) carrying a centromeric plasmid (p416-GPD) containing the following genes expressed the constitutive GPD promoter: 1. CgMep1a, 2. CgMep1b, 3. CgMep3, 4. CgMep2, 5. Plasmid only (negative control) 6. Saccharomyces cerevisiae Mep2 (positive control).

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Discussion

Nitrogen is an important currency in the cell, arguably second in importance only to carbon. A recent work on fungal genomes has validated 323 horizontal gene transfer events into fungi [71] of which the two top categories are genes involved in the acquisition and metabolism of carbon and nitrogen. If all the categories involving nitrogen are grouped, horizontal gene transfers of genes involved in nitrogen acquisition and metabolism are in fact the most populous category. Evidently fungi have been capturing new technology for nitrogen acquisition since the very beginning.

AMTPs in particular show an intriguing pattern of expansion in the fungi. The microsporidia, considered to be the earliest diverging fungi [69], lack AMTPs. Interestingly, the microsporidia are intracellular pathogens. Intracellular pathogens tend to experience genome contraction as they outsource more and more of their life functions to their hosts. If other early fungi also lack AMTP genes, it would lend support to the hypothesis that fungi first lost the eukaryotic AMTPs and then obtained by horizontal gene transfer a prokaryotic AMTP. In fact, the seemingly high levels of horizontal gene transfer seen in the fungi could be explained similarly, as fungi slowly rebuilding their genomic toolkits after a period of gene loss as intracellular pathogens during their early evolution.

After a period of time with no AMTPs, fungi acquired by horizontal gene transfer a bacterial AMTP. Sampling of the Neocallimastigomycota and the Monoblephardiomycetes (chytrids sensu lato) is poor, so it isn’t yet possible to pinpoint the entry of AMTPs into the fungi, but AMTPs had entered the fungi at least by the time of the divergence of the chytrid Batrachochytrium. Then, as the Dikarya diverged there was a duplication event followed by a subfunctionalization into high-affinity (low-capacity) and low-affinity (high-capacity) AMTPs. In mycorrhizal basidiomycetes (but not rusts or smuts), a gene family expansion followed. In ascomycetes, there may also have been a slow gene family expansion perhaps starting as early as the divergence of the Taphrinomycotina. Layered on top of this slow gene family expansion was a second horizontal transfer of the MEP α AMTP from hyperacidophilic chemoautolithotrophic prokaryotes into the leotiomyceta [10].

MEP α has been subsequently lost in almost all non-lichenized lineages [10] and, as shown here, in certain lichenized lineages. What the lichenized lineages that have lost the plant-like MEP α have in common with each other is not entirely clear. At the outset of this work, it was hypothesized that nitrogen availability was the major factor governing the retention or loss of the MEP α genes. It was expected that lichens with a rich enough internal or external source of nitrogen would have lost the MEP α genes, while other lichens would retain it. While this appears to hold true within the Lecanoromycetes with the current sampling, this hypothesis cannot explain the apparent loss of the genes in Endocarpon pallidulum (Chaetothyriomycetidae) or Arthonia rubrocincta (Arthoniomycetes). Since retention of the AMTPs is not solely dependent on low nitrogen availability, evidently some other factors govern the loss of AMTPs.

Because the MEP α genes are missing from some lichens, these genes may not be intimately involved in the lichen symbiosis, assuming that there is some ancestral core “symbiosis program” shared by ascomycete lichens, nor are the MEP α genes absolutely mandatory to supplying nitrogen to the lichenizing fungus. It is possible however, that the MEP α genes are involved specifically in balancing the nitrogen budget between the fungal and green algal symbionts. If lichenization is considered a controlled parasitism of the photobiont by lichenizing fungi, it follows that the fungus would also control the nitrogen budget of the alga, perhaps by outcompeting the photobiont for ammonium but then exporting, for example, amino acids or some other form of nitrogen on which the alga is dependent. If so, this would predict that large lichens that live on nitrogen-poor substrates, such as Umbilicaria (Lecanoromycetes, uncertain placement) or Dermatocarpon (Chaetothyriomycetidae) should have retained the MEP α AMTPs, while explaining why smaller lichens on nitrogen-poor substrate like the aforementioned Arthonia and Endocarpon have lost them. Of course, the alga might also scavenge its own ammonium, and may in fact be fed by the fungus releasing ammonium through ammonium exporters (e.g. those encoded by the ATO genes in yeast).

Perhaps the MEP α genes have been retained for a reason other than nitrogen acquisition. Aside from transporting ammonium/ammonia, AMTP proteins (specifically, only high-affinity fungal AMTPs) have also been shown to be involved in pseudohyphal filamentation in Saccharomyces cerevisiae and in Cryptococcus neoformans, where they serve as sensors of nitrogen starvation [72, 73]. High-affinity AMTPs from the basidiomycetes Ustilago maydis and Hebeloma cylindrosporum can complement this function in strains of Saccharomyces cerevisiae with the high-affinity AMTP Mep2 deleted [31, 74]. Presumably, the high-affinity fungal AMTP from C. grayi should also complement this function, while the low-affinity fungal AMTP should not, in keeping with the functional data from other fungi. It is not yet known whether the MEP α AMTPs are involved in sensing nitrogen, nor is it known whether they can stimulate pseudohyphal filamentation, since they are high-affinity AMTPs, or in a perhaps more likely scenario, will fail to do so due to amino acid sequence differences in regions shown to be critical for pseudohyphal filamentation [72].

In order to determine the function of the new clade of AMTPs, transcriptional profiling of the fungus C. grayi grown on nitrogen-rich or nitrogen-poor media would be helpful. Identifying genes co-regulated with the MEP α AMTPs could reveal whether MEP α AMTPs are involved in mating, morphological change, growth, nutrient scavenging, or other pathways. Understanding this could shed light on why these genes have been retained in some lichenizing fungi but not others, and why these genes were horizontally transferred in the first place.

Conclusions

Over evolutionary time, lichenizing fungi have retained the MEP α AMTPs except if an environmental or symbiotic source of nitrogen is available. Additional conditions precipitating the loss of the MEP α AMTPs exist and remain unelucidated.

Methods

Media and culture conditions

For yeast strains, standard yeast media were used including: Synthetic Limiting Ammonium and Dextrose (SLAD) composed of 0.17% yeast nitrogen base (without amino acids and ammonium sulfate), 2% glucose and 2% agar [72, 75] with modifications including 2 mM, 5 mM, 7 mM, 10 mM and 20 mM ammonium sulfate; and Synthetic Complete medium (SC) lacking uracil, which contains 6.7 g/l yeast nitrogen base without amino acids, supplemented with all amino acids except uracil, 2% glucose and 2% agar. Yeast strains were grown at 30°C or at room temperature. Cladonia grayi was maintained at room temperature in liquid shaking cultures of MEYE medium consisting of 20 g/l malt extract and 2 g/l yeast extract [1].

Construction of plasmids

RNA was extracted from Cladonia grayi cultures growing in liquid medium. Tissue from liquid cultures was harvested, rinsed in distilled water, lyophilized, then ground to a fine powder under liquid nitrogen in a pre-chilled mortar and pestle. The ground tissue was resuspended in TRIzol Reagent (Invitrogen, Carlsbad, CA) and RNA extraction proceeded according to the manufacturer’s instructions.

The first strand of the cDNA was generated using the following reverse transcription reaction mix: 1.0 μl 10× PCR buffer, 2.0 μl 25 mM MgCl2 (both supplied with AmpliTaq DNA Polymerase, Applied Biosystems), 2.0 μl dNTPs (10 mM each), 0.5 μl RNAse inhibitor (20 μg/μl, Applied Biosystems) 0.5 μl MulV reverse transcriptase (Applied Biosystems), 1.75 μl of distilled water, and 1.25 μl reverse primer. The thermocycling conditions for this first strand synthesis reaction were: 42°C for 35 minutes, then 99°C for 5 minutes. Primers are listed in Additional files 1 and 2. PCR to regenerate the second strand of the cDNA was performed using the entire volume of first strand reaction plus 31.25 μl distilled water, 4 μl 20x PCR buffer, 3 μl 25 mM MgCl2, 1.25 μl of a forward primer, 0.25 μl of AmpliTaq polymerase (Applied Biosystems) and 0.25 μl of an antibody to Taq polymerase (Clontech). The thermocycling program consisted of 24 cycles of 94°C for 30 seconds, 55°C for 30 seconds with a 0.4 degree decrease in temperature for each cycle, and 72° for 1 minute, followed by 12 cycles of 94°C for 30 seconds, 45°C for 30 seconds, and 72°C for 2 minutes with a 3 second increase per cycle, followed by a final extension at 72°C for 10 minutes. cDNA of each AMTP from Cladonia grayi was cloned into the TOPO TA vector as described above. Plasmid DNA was restricted to release the full-length AMTP cDNA which was then subcloned into the pRS306-GAL1-TADH vector (unpublished, a gift from Mark Chee) carrying a uracil selectable marker, an inducible Gal promoter and a Cyc terminator or the p416-GPD vector [76] carrying a uracil selectable marker and a constitutive GPD promoter and Cyc terminator, for transformation into Saccharomyces cerevisiae. The DNA sequence of the constructed plasmids was confirmed by PCR and sequencing as described below.

Construction of yeast strains

Yeast strains are listed in Additional file 3. Yeast transformations were performed using the TRAFO lithium acetate method [77] or by the gapped plasmid method [78]. Following the TRAFO method, a yeast culture in log phase was centrifuged for 5 minutes at 6000 RPM, and the pellet washed with distilled water, and resuspended in an equal volume of distilled water, pelleted again, then resuspended in 1 ml of 100 mM lithium acetate. This solution was pelleted at maximum speed (>14,000 RPM) in a microcentrifuge and the pellet resuspended in approximately 400 μl of 100 mM lithium acetate. A transformation mix of 50 μl yeast cells, 240 μl PEG, 36 μl 1 M lithium acetate, 50 μl salmon sperm DNA and 34 μl of diluted plasmid (approximately 100 ng plasmid) was incubated at 30°C for 30 minutes and heat shocked at 42°C for 30 minutes. The mix was then centrifuged and the pellet resuspended in 300 μl water. 100 μl of the cell suspension was plated onto selective medium and transformants confirmed by colony PCR as described below. For gapped plasmid construction, cDNA of AMTPs from C. grayi which had been cloned into the TopoTA vector (Invitrogen, Carlsbad, CA) was amplified with primers composed of 40 base pairs of homology on either side of the multiple cloning site of the centromeric plasmid p416GPD [76] carry the uracil selectable marker and joined to the first or last 20 base pairs of the gene [78]. The PCR product was cleaned in a Microcon column (Millipore, Bilerica, MA) and approximately 1 μg of amplicon was transformed into yeast along with 0.1 μg of restricted plasmid DNA. Yeast recombine the two fragments into a functional plasmid. Transformants were screened by PCR and the inserts sequenced as described below.

DNA amplification and Sanger Sequencing

For PCR performed directly on colonies of yeast or E. coli, the PCR reaction mix consisted of 17.3 μl distilled water, 2.5 μl of 10x PCR buffer, 2.5 μl dNTPs, 1.25 μl each of a forward primer and a reverse primer, and 0.3 μl Taq polymerase (Denville). Colonies were touched lightly with the tip of a pipette which was then dipped briefly into the PCR tube and removed. PCR was performed on a MJ Research PTC200 thermocycler or an Applied Biosystems (Foster City, CA) Veriti thermocycler using a cycling program consisting of 10 minutes at 94°C to lyse the cells and release the DNA, followed by 25 cycles of 30 seconds at 94°C, 30 seconds at 55°C and 2 minutes at 72°C, followed a final elongation step at 72°C for 7 minutes. PCR products were visualized on a TAE 1% agarose gel stained with SYBR Safe (Invitrogen, Carlsbad, CA). If necessary, faint products or products with multiple bands were cloned with the TOPO TA cloning kit (Invitrogen, Carlsbad, CA) following the manufacturer’s instructions. For each cloning reaction, at least 8 clones were screened by colony PCR using T7 and M13R primers and a PCR program consisting of a 10-minute initial denaturation step, followed by 25 cycles of 30 seconds at 94°C, 30 seconds at 52°C and 60 seconds at 72°C followed by a final elongation step of 7 minutes. PCR products were cleaned with a Montage PCR filter column (Millipore, Bilerica, MA) or with an Exo-SAP clean-up using 1 μl SAP dilution buffer, 0.5 μl Exonuclease 1, 0.5 μl Shrimp Alkaline Phosphatase, added to 10 μl PCR reaction and incubating on one of the aforementioned thermocyclers for 30 minutes at 37°C, then 15 minutes at 80°C. Cleaned PCR products were sequenced in 10 μl reactions using: 1 μl primer, 3 μl purified PCR product, 0.5 μl Big Dye (Big Dye Terminator Cycle sequencing kit, ABI PRISM version 3.1; PE Applied Biosystems, Foster City, CA), 1.5 μl Big Dye buffer, and 4 μl double-distilled water. Automated reaction clean-up and visualization was performed at the Duke IGSP Genome Sequencing & Analysis Core Facility using Big Dye chemistry with an ABI 3730xl automated sequencer (PE Applied Biosystems, Foster City, CA). Sequencher version 4.8 (Gene Codes Corporation, Ann Arbor, MI) was used to edit sequences and assemble contigs.

Genomic DNA isolation

DNA from cultures of the lichenizing fungi Acarospora strigata (Acarosporomycetidae, Lecanoromycetes), Arthonia rubrocincta (Arthoniomycetidae), Endocarpon pallidulum (Eurotiomycetes) Graphis scripta (Ostropomycetidae, Lecanoromycetes) and from lichen thalli of Dibaeis baeomyces (Ostropomycetidae, Lecanoromycetes), Leptogium austroamericanum, Physcia cf. stellaris (both Lecanoromycetidae, Lecanoromycetes), and Peltula cylindrica (Lichinomycetes) was prepared following the DTAB/CTAB method outlined in [79]. Briefly, tissue was ground to a fine powder under liquid nitrogen using a pre-chilled mortar and pestle. Twenty volumes of a DTAB solution (with 1% DNAse-free RNAse) was added to the powder and incubated for ~3 minutes at 65°C. Polysaccharides and other contaminants were precipitated by adding 1/3 volume 5M NaCl and centrifuging at 6000 RPM for 5 minutes. The supernatant was removed and extracted once with one volume of phenol, after which the supernatant was removed and then extracted with one volume of chloroform. The supernatant was removed, and DNA precipitated with one volume of isopropanol and left to incubate at room temperature for 5 minutes, then centrifuged at 6000 RPM for 5 minutes to pellet the DNA. The pellet was resuspended in DTAB + RNAse, with heating and gentle agitation. Remaining polysaccharides were precipitated by adding 1/3 volume of 5M NaCl and centrifuging at 6000 RPM for 5 minutes. The supernatant was removed and undissolved material was pelleted by centrifugation at 6000 RPM. DNA was precipitated by adding 2 volumes of 100% ethanol, incubating at room temperature for five minutes, and centrifuging at maximum speed (14,000 RPM) for five minutes. The pellet was washed once with 70% ethanol, and allowed to dry. When dry, the pellet was resuspended in 100 μl TE and quantified by Qubit. DNA was then further purified using the PowerClean kit (Mo Bio) following the manufacturer’s instructions. DNA was again quantified after purification by Qubit.

Illumina sequencing and genome assembly

One to six μg of purified DNA were submitted to the sequencing facility at Duke University for 75-base pair paired-end barcoded Illumina sequencing using the HiSeq technology. Four lichen cultures were multiplexed onto a lane, and DNA from two lichen thalli (yielding both fungal and algal DNA) were multiplexed onto a lane. A total of three lanes were used to sequence the eight fungal genomes (~80 million to 600 million reads). Preliminary draft assemblies were generated with Velvet [80] (Table 1). Data is housed in the Sequence Read Archive (SRA) accessible through the National Center for Biotechnology Information (NCBI) website.

Phylogenetic analysis

AMTP sequences generated for this study (Additional file 4) were included in a modified alignment from [10] and phylogenetic analysis was performed as in [10]. Genes in the MEP clade of AMTPs were retained in the analysis (Additional file 5), while all others were discarded. All excluded regions were reexamined, and additional sites that became alignable were included in the analysis, including 90 base pairs of transmembrane region one, which in the previous analysis had been entirely excluded. The first well-supported clade outside of the MEP group in the MEP grade was used as an outgroup. In one analysis, the three AMTPs from the green alga Asterochloris sp., which fall into the AMT clade of AMTPs, were also included and used as an outgroup. Manual alignments were performed using MacClade 4.08 [81]. Ambiguously aligned regions and introns were delimited manually and excluded from phylogenetic analyses. Models of molecular evolution which had been selected using the Akaike Information Criterion (AIC) implemented in jModeltest [82] or MrModeltest 2.3 [83] were implemented on this dataset. Phylogenetic relationships and confidence values were inferred using a maximum likelihood approach at the nucleotide level. Maximum likelihood analysis at the nucleotide level used GTR GAMMAI (with a gamma parameter and a proportion of invariable sites, = GTR + Γ + I). The program RAxML-VI-HPC [84] was used for the maximum likelihood search for the most likely tree. The same program using the same settings was used for the bootstrap (BS) analysis with 1000 BS replicates run in batches of 100 replicates and pooled. Bootstrap values were calculated and visualized using the majority rule consensus tree command in PAUP 4.0d701 [85] (Additional file 6).

Abbreviations

AMTPs:

Ammonium transporters/Ammonia permeases

MEP:

Methylammonium permease.

References

  1. 1.

    Ahmadjian V: Artificial Reestablishment of the Lichen Cladonia cristatella. Science. 1966, 151 (3707): 199-201. 10.1126/science.151.3707.199.

    Article  CAS  PubMed  Google Scholar 

  2. 2.

    Ahmadjian V, Heikkilä H: The culture and synthesis of Endocarpon pusillum and Staurothele clopima. Lichenologist. 1970, 4: 259-267. 10.1017/S0024282970000336.

    Article  Google Scholar 

  3. 3.

    Ahmadjian V: The lichen symbiosis. 1993, New York: John Wiley

    Google Scholar 

  4. 4.

    Trembley ML, Ringli C, Honegger R: Morphological and molecular analysis of early stages in the resynthesis of the lichen Baeomyces rufus. Mycol Res. 2002, 106 (7): 768-776. 10.1017/S0953756202006081.

    Article  CAS  Google Scholar 

  5. 5.

    Armaleo D, Joneson S, McDonald T, Wray G, Dietrich F, Miadlikowska J, Lutzoni F: Decoding symbiosis: sequencing the two genomes of the lichen Cladonia grayi [abstract]. 2008, The sixth International Association for Lichenology Symposium and Annual Meeting of the American Bryological and Lichenological Society

    Google Scholar 

  6. 6.

    Armaleo D, Mueller O, Lutzoni F, Martin F, Blanc G, Merchant S, Collart F: Decoding symbiosis: the two genomes of the lichen Cladonai grayi [abstract]. Book of abstracts. 2012, The 7th Symposium of the International Association for Lichenology, 21-

    Google Scholar 

  7. 7.

    Gogarten JP, Doolittle WF, Lawrence JG: Prokaryotic evolution in light of gene transfer. Mol Biol Evol. 2002, 19 (12): 2226-2238. 10.1093/oxfordjournals.molbev.a004046.

    Article  CAS  PubMed  Google Scholar 

  8. 8.

    Marcet-Houben M, Gabaldon T: Acquisition of prokaryotic genes by fungal genomes. Trends Genet. 2010, 26 (1): 5-8. 10.1016/j.tig.2009.11.007.

    Article  CAS  PubMed  Google Scholar 

  9. 9.

    Slot JC, Hibbett DS: Horizontal transfer of a nitrate assimilation gene cluster and ecological transitions in fungi: a phylogenetic study. PLoS One. 2007, 2 (10): e1097-10.1371/journal.pone.0001097.

    PubMed Central  Article  PubMed  Google Scholar 

  10. 10.

    McDonald TR, Dietrich FS, Lutzoni F: Multiple horizontal gene transfers of ammonium transporters/ammonia permeases from prokaryotes to eukaryotes: toward a new functional and evolutionary classification. Mol Biol Evol. 2012, 29 (1): 51-60. 10.1093/molbev/msr123.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  11. 11.

    Marini AM, Vissers S, Urrestarazu A, Andre B: Cloning and expression of the MEP1 gene encoding an ammonium transporter in Saccharomyces cerevisiae. EMBO J. 1994, 13 (15): 3456-3463.

    PubMed Central  CAS  PubMed  Google Scholar 

  12. 12.

    Ninnemann O, Jauniaux JC, Frommer WB: Identification of a high affinity NH4+ transporter from plants. EMBO J. 1994, 13 (15): 3464-3471.

    PubMed Central  CAS  PubMed  Google Scholar 

  13. 13.

    Blakey D, Leech A, Thomas GH, Coutts G, Findlay K, Merrick M: Purification of the Escherichia coli ammonium transporter AmtB reveals a trimeric stoichiometry. Biochem J. 2002, 364 (Pt 2): 527-535.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  14. 14.

    Simon-Rosin U, Wood C, Udvardi MK: Molecular and cellular characterisation of LjAMT2;1, an ammonium transporter from the model legume Lotus japonicus. Plant Mol Biol. 2003, 51 (1): 99-108. 10.1023/A:1020710222298.

    Article  CAS  PubMed  Google Scholar 

  15. 15.

    Sohlenkamp C, Shelden M, Howitt S, Udvardi M: Characterization of Arabidopsis AtAMT2, a novel ammonium transporter in plants. FEBS Lett. 2000, 467 (2–3): 273-278.

    Article  CAS  PubMed  Google Scholar 

  16. 16.

    Winkler FK: Amt/MEP/Rh proteins conduct ammonia. Pflugers Arch. 2006, 451 (6): 701-707. 10.1007/s00424-005-1511-6.

    Article  CAS  PubMed  Google Scholar 

  17. 17.

    Zheng L, Kostrewa D, Berneche S, Winkler FK, Li XD: The mechanism of ammonia transport based on the crystal structure of AmtB of Escherichia coli. Proc Natl Acad Sci U S A. 2004, 101 (49): 17090-17095. 10.1073/pnas.0406475101.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  18. 18.

    Yang H, Xu Y, Zhu W, Chen K, Jiang H: Detailed mechanism for AmtB conducting NH4+/NH3: molecular dynamics simulations. Biophys J. 2007, 92 (3): 877-885. 10.1529/biophysj.106.090191.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  19. 19.

    Javelle A, Lupo D, Zheng L, Li XD, Winkler FK, Merrick M: An unusual twin-his arrangement in the pore of ammonia channels is essential for substrate conductance. J Biol Chem. 2006, 281 (51): 39492-39498. 10.1074/jbc.M608325200.

    Article  CAS  PubMed  Google Scholar 

  20. 20.

    Khademi S, O'Connell J, Remis J, Robles-Colmenares Y, Miercke LJ, Stroud RM: Mechanism of ammonia transport by Amt/MEP/Rh: structure of AmtB at 1.35 A. Science. 2004, 305 (5690): 1587-1594. 10.1126/science.1101952.

    Article  CAS  PubMed  Google Scholar 

  21. 21.

    Lamoureux G, Javelle A, Baday S, Wang S, Berneche S: Transport mechanisms in the ammonium transporter family. Transfus Clin Biol. 2010, 17 (3): 168-175. 10.1016/j.tracli.2010.06.004.

    Article  CAS  PubMed  Google Scholar 

  22. 22.

    Lamoureux G, Klein ML, Berneche S: A stable water chain in the hydrophobic pore of the AmtB ammonium transporter. Biophys J. 2007, 92 (9): L82-L84. 10.1529/biophysj.106.102756.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  23. 23.

    Marini AM, Urrestarazu A, Beauwens R, Andre B: The Rh (rhesus) blood group polypeptides are related to NH4+ transporters. Trends Biochem Sci. 1997, 22 (12): 460-461. 10.1016/S0968-0004(97)01132-8.

    Article  CAS  PubMed  Google Scholar 

  24. 24.

    Kustu S, Inwood W: Biological gas channels for NH3 and CO2: evidence that Rh (Rhesus) proteins are CO2 channels. Transfus Clin Biol. 2006, 13 (1–2): 103-110.

    Article  CAS  PubMed  Google Scholar 

  25. 25.

    Li X, Jayachandran S, Nguyen HH, Chan MK: Structure of the Nitrosomonas europaea Rh protein. Proc Natl Acad Sci U S A. 2007, 104 (49): 19279-19284. 10.1073/pnas.0709710104.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  26. 26.

    Gruswitz F, Chaudhary S, Ho JD, Schlessinger A, Pezeshki B, Ho CM, Sali A, Westhoff CM, Stroud RM: Function of human Rh based on structure of RhCG at 2.1 A. Proc Natl Acad Sci U S A. 2010, 107 (21): 9638-9643. 10.1073/pnas.1003587107.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  27. 27.

    Monahan BJ, Askin MC, Hynes MJ, Davis MA: Differential expression of Aspergillus nidulans ammonium permease genes is regulated by GATA transcription factor AreA. Eukaryot Cell. 2006, 5 (2): 226-237. 10.1128/EC.5.2.226-237.2006.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  28. 28.

    Monahan BJ, Fraser JA, Hynes MJ, Davis MA: Isolation and characterization of two ammonium permease genes, meaA and mepA, from Aspergillus nidulans. Eukaryot Cell. 2002, 1 (1): 85-94. 10.1128/EC.1.1.85-94.2002.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  29. 29.

    Monahan BJ, Unkles SE, Tsing IT, Kinghorn JR, Hynes MJ, Davis MA: Mutation and functional analysis of the Aspergillus nidulans ammonium permease MeaA and evidence for interaction with itself and MepA. Fungal Genet Biol. 2002, 36 (1): 35-46. 10.1016/S1087-1845(02)00004-X.

    Article  CAS  PubMed  Google Scholar 

  30. 30.

    Marini AM, Soussi-Boudekou S, Vissers S, Andre B: A family of ammonium transporters in Saccharomyces cerevisiae. Mol Cell Biol. 1997, 17 (8): 4282-4293.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  31. 31.

    Javelle A, Andre B, Marini AM, Chalot M: High-affinity ammonium transporters and nitrogen sensing in mycorrhizas. Trends Microbiol. 2003, 11 (2): 53-55. 10.1016/S0966-842X(02)00012-4.

    Article  CAS  PubMed  Google Scholar 

  32. 32.

    Lopez-Pedrosa A, Gonzalez-Guerrero M, Valderas A, Azcon-Aguilar C, Ferrol N: GintAMT1 encodes a functional high-affinity ammonium transporter that is expressed in the extraradical mycelium of Glomus intraradices. Fungal Genet Biol. 2006, 43 (2): 102-110. 10.1016/j.fgb.2005.10.005.

    Article  CAS  PubMed  Google Scholar 

  33. 33.

    Marini AM, Andre B: In vivo N-glycosylation of the Mep2 high-affinity ammonium transporter of Saccharomyces cerevisiae reveals an extracytosolic N-terminus. Mol Microbiol. 2000, 38 (3): 552-564. 10.1046/j.1365-2958.2000.02151.x.

    Article  CAS  PubMed  Google Scholar 

  34. 34.

    Montanini B, Moretto N, Soragni E, Percudani R, Ottonello S: A high-affinity ammonium transporter from the mycorrhizal ascomycete Tuber borchii. Fungal Genet Biol. 2002, 36 (1): 22-34. 10.1016/S1087-1845(02)00001-4.

    Article  CAS  PubMed  Google Scholar 

  35. 35.

    Sohlenkamp C, Wood CC, Roeb GW, Udvardi MK: Characterization of Arabidopsis AtAMT2, a high-affinity ammonium transporter of the plasma membrane. Plant Physiol. 2002, 130 (4): 1788-1796. 10.1104/pp.008599.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  36. 36.

    Schoch CL, Sung GH, Lopez-Giraldez F, Townsend JP, Miadlikowska J, Hofstetter V, Robbertse B, Matheny PB, Kauff F, Wang Z, et al: The Ascomycota tree of life: a phylum-wide phylogeny clarifies the origin and evolution of fundamental reproductive and ecological traits. Systematic biology. 2009, 58 (2): 224-239. 10.1093/sysbio/syp020.

    Article  CAS  PubMed  Google Scholar 

  37. 37.

    Spatafora JW, Sung GH, Johnson D, Hesse C, O'Rourke B, Serdani M, Spotts R, Lutzoni F, Hofstetter V, Miadlikowska J, et al: A five-gene phylogeny of Pezizomycotina. Mycologia. 2006, 98 (6): 1018-1028. 10.3852/mycologia.98.6.1018.

    Article  CAS  PubMed  Google Scholar 

  38. 38.

    Couturier J, Montanini B, Martin F, Brun A, Blaudez D, Chalot M: The expanded family of ammonium transporters in the perennial poplar plant. New Phytol. 2007, 174 (1): 137-150. 10.1111/j.1469-8137.2007.01992.x.

    Article  CAS  PubMed  Google Scholar 

  39. 39.

    Ludewig U, von Wiren N, Frommer WB: Uniport of NH4+ by the root hair plasma membrane ammonium transporter LeAMT1;1. J Biol Chem. 2002, 277 (16): 13548-13555. 10.1074/jbc.M200739200.

    Article  CAS  PubMed  Google Scholar 

  40. 40.

    Mayer M, Dynowski M, Ludewig U: Ammonium ion transport by the AMT/Rh homologue LeAMT1;1. Biochem J. 2006, 396 (3): 431-437. 10.1042/BJ20060051.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  41. 41.

    Mayer M, Ludewig U: Role of AMT1;1 in NH4+ acquisition in Arabidopsis thaliana. Plant Biol (Stuttg). 2006, 8 (4): 522-528. 10.1055/s-2006-923877.

    Article  CAS  Google Scholar 

  42. 42.

    Andrade SL, Dickmanns A, Ficner R, Einsle O: Crystal structure of the archaeal ammonium transporter Amt-1 from Archaeoglobus fulgidus. Proc Natl Acad Sci U S A. 2005, 102 (42): 14994-14999. 10.1073/pnas.0506254102.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  43. 43.

    Itoh T, Suzuki K, Sanchez PC, Nakase T: Caldivirga maquilingensis gen. nov., sp. nov., a new genus of rod-shaped crenarchaeote isolated from a hot spring in the Philippines. Int J Syst Bacteriol. 1999, 49 (Pt 3): 1157-1163.

    Article  CAS  PubMed  Google Scholar 

  44. 44.

    Brock TD, Brock KM, Belly RT, Weiss RL: Sulfolobus: a new genus of sulfur-oxidizing bacteria living at low pH and high temperature. Arch Mikrobiol. 1972, 84 (1): 54-68. 10.1007/BF00408082.

    Article  CAS  PubMed  Google Scholar 

  45. 45.

    She Q, Singh RK, Confalonieri F, Zivanovic Y, Allard G, Awayez MJ, Chan-Weiher CC, Clausen IG, Curtis BA, De Moors A, et al: The complete genome of the crenarchaeon Sulfolobus solfataricus P2. Proc Natl Acad Sci U S A. 2001, 98 (14): 7835-7840. 10.1073/pnas.141222098.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  46. 46.

    Suzuki T, Iwasaki T, Uzawa T, Hara K, Nemoto N, Kon T, Ueki T, Yamagishi A, Oshima T: Sulfolobus tokodaii sp. nov. (f. Sulfolobus sp. strain 7), a new member of the genus Sulfolobus isolated from Beppu Hot Springs, Japan. Extremophiles. 2002, 6 (1): 39-44. 10.1007/s007920100221.

    Article  PubMed  Google Scholar 

  47. 47.

    Futterer O, Angelov A, Liesegang H, Gottschalk G, Schleper C, Schepers B, Dock C, Antranikian G, Liebl W: Genome sequence of Picrophilus torridus and its implications for life around pH 0. Proc Natl Acad Sci U S A. 2004, 101 (24): 9091-9096. 10.1073/pnas.0401356101.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  48. 48.

    Schleper C, Puehler G, Holz I, Gambacorta A, Janekovic D, Santarius U, Klenk HP, Zillig W: Picrophilus gen. nov., fam. nov.: a novel aerobic, heterotrophic, thermoacidophilic genus and family comprising archaea capable of growth around pH 0. J Bacteriol. 1995, 177 (24): 7050-7059.

    PubMed Central  CAS  PubMed  Google Scholar 

  49. 49.

    Dopson M, Baker-Austin C, Hind A, Bowman JP, Bond PL: Characterization of Ferroplasma isolates and Ferroplasma acidarmanus sp. nov., extreme acidophiles from acid mine drainage and industrial bioleaching environments. Appl Environ Microbiol. 2004, 70 (4): 2079-2088. 10.1128/AEM.70.4.2079-2088.2004.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  50. 50.

    Goltsman DS, Denef VJ, Singer SW, VerBerkmoes NC, Lefsrud M, Mueller RS, Dick GJ, Sun CL, Wheeler KE, Zemla A, et al: Community genomic and proteomic analyses of chemoautotrophic iron-oxidizing "Leptospirillum rubarum" (Group II) and "Leptospirillum ferrodiazotrophum" (Group III) bacteria in acid mine drainage biofilms. Appl Environ Microbiol. 2009, 75 (13): 4599-4615. 10.1128/AEM.02943-08.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  51. 51.

    Kelly DP, Wood AP: Reclassification of some species of Thiobacillus to the newly designated genera Acidithiobacillus gen. nov., Halothiobacillus gen. nov. and Thermithiobacillus gen. nov. Int J Syst Evol Microbiol. 2000, 50 (Pt 2): 511-516.

    Article  PubMed  Google Scholar 

  52. 52.

    Valdes J, Ossandon F, Quatrini R, Dopson M, Holmes DS: Draft genome sequence of the extremely acidophilic biomining bacterium Acidithiobacillus thiooxidans ATCC 19377 provides insights into the evolution of the Acidithiobacillus genus. J Bacteriol. 2011, 193 (24): 7003-7004. 10.1128/JB.06281-11.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  53. 53.

    Valdes J, Pedroso I, Quatrini R, Dodson RJ, Tettelin H, Blake R, Eisen JA, Holmes DS: Acidithiobacillus ferrooxidans metabolism: from genome sequence to industrial applications. BMC Genomics. 2008, 9: 597-10.1186/1471-2164-9-597.

    PubMed Central  Article  PubMed  Google Scholar 

  54. 54.

    Valdes J, Quatrini R, Hallberg K, Dopson M, Valenzuela PD, Holmes DS: Draft genome sequence of the extremely acidophilic bacterium Acidithiobacillus caldus ATCC 51756 reveals metabolic versatility in the genus Acidithiobacillus. J Bacteriol. 2009, 191 (18): 5877-5878. 10.1128/JB.00843-09.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  55. 55.

    Clum A, Nolan M, Lang E, et al: Glavina Del Rio T, Tice H, Copeland A, Cheng JF, Lucas S, Chen F, Bruce D, et al: Complete genome sequence of Acidimicrobium ferrooxidans type strain (ICP). Stand Genomic Sci. 2009, 1 (1): 38-45. 10.4056/sigs.1463.

    PubMed Central  Article  PubMed  Google Scholar 

  56. 56.

    Hibbett DS, Binder M, Bischoff JF, Blackwell M, Cannon PF, Eriksson OE, Huhndorf S, James T, Kirk PM, Lucking R, et al: A higher-level phylogenetic classification of the Fungi. Mycol Res. 2007, 111 (Pt 5): 509-547.

    Article  PubMed  Google Scholar 

  57. 57.

    Lutzoni F, Kauff F, Cox CJ, McLaughlin D, Celio G, Dentinger B, Padamsee M, Hibbett D, James TY, Baloch E, et al: Assembling the fungal tree of life: progress, classification, and evolution of subcellular traits. Am J Bot. 2004, 91 (10): 1446-1480. 10.3732/ajb.91.10.1446.

    Article  PubMed  Google Scholar 

  58. 58.

    Miadlikowska J, Lutzoni F: Phylogenetic classification of peltigeralean fungi (Peltigerales, Ascomycota) based on ribosomal RNA small and large subunits. Am J Bot. 2004, 91 (3): 449-464. 10.3732/ajb.91.3.449.

    Article  CAS  PubMed  Google Scholar 

  59. 59.

    Gaya E, Högnabba F, Holguin A, Molnar K, Fernández-Brime S, Stenroos S, Arup U, Søchting U, Van den Boom P, Lücking R, Sipman HJM, Lutzoni F: Implementing a cumulative super-matrix approach for a comprehensive phylogenetic study of the Teloschistales (Pezizomycotina, Ascomycota. Mol Phylogenet Evol. 2012, 63: 374-387. 10.1016/j.ympev.2012.01.012.

    Article  PubMed  Google Scholar 

  60. 60.

    Parra G, Bradnam K, Ning Z, Keane T, Korf I: Assessing the gene space in draft genomes. Nucleic Acids Res. 2009, 37 (1): 289-297. 10.1093/nar/gkn916.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  61. 61.

    Parra G, Bradnam K, Korf I: CEGMA: a pipeline to accurately annotate core genes in eukaryotic genomes. Bioinformatics. 2007, 23 (9): 1061-1067. 10.1093/bioinformatics/btm071.

    Article  CAS  PubMed  Google Scholar 

  62. 62.

    Aspergillus Genome Database. http://www.aspergillusgenome.org/,

  63. 63.

    Neurospora crassa Database. http://www.broadinstitute.org/annotation/genome/neurospora/MultiHome.html,

  64. 64.

    Arnold AE, Miadlikowska J, Higgins KL, Sarvate SD, Gugger P, Way A, Hofstetter V, Kauff F, Lutzoni F: A phylogenetic estimation of trophic transition networks for ascomycetous fungi: are lichens cradles of symbiotrophic fungal diversification?. Syst Biol. 2009, 58 (3): 283-297. 10.1093/sysbio/syp001.

    Article  PubMed  Google Scholar 

  65. 65.

    Hodkinson BP, Gottel NR, Schadt CW, Lutzoni F: Photoautotrophic symbiont and geography are major factors affecting highly structured and diverse bacterial communities in the lichen microbiome. Environmental microbiology. 2012, 14 (1): 147-161. 10.1111/j.1462-2920.2011.02560.x.

    Article  CAS  PubMed  Google Scholar 

  66. 66.

    Crittenden PD, David JC, Hawksworth DL, Campbell FS: Attempted isolation and success in the culturing of a broad spectrum of lichen-forming and lichenicolous fungi. New Phytol. 1995, 130: 267-297. 10.1111/j.1469-8137.1995.tb03048.x.

    Article  Google Scholar 

  67. 67.

    Sangvichien E, Hawksworth DL, Whalley AJ: Ascospore discharge, germination and culture of fungal partners of tropical lichens, including the use of a novel culture technique. IMA Fungus. 2011, 2: 143-153. 10.5598/imafungus.2011.02.02.05.

    PubMed Central  Article  PubMed  Google Scholar 

  68. 68.

    Xanthoria parietina. http://genome.jgi-psf.org/Xanpa1/Xanpa1.home.html,

  69. 69.

    James TY, Kauff F, Schoch CL, Matheny PB, Hofstetter V, Cox CJ, Celio G, Gueidan C, Fraker E, Miadlikowska J, et al: Reconstructing the early evolution of Fungi using a six-gene phylogeny. Nature. 2006, 443 (7113): 818-822. 10.1038/nature05110.

    Article  CAS  PubMed  Google Scholar 

  70. 70.

    Brodo IM: The Lichen Genus Coccotrema in North America. The Bryologist. 1973, 76 (2): 260-270. 10.2307/3241328.

    Article  Google Scholar 

  71. 71.

    Richards TA, Soanes DM, Foster PG, Leonard G, Thornton CR, Talbot NJ: Phylogenomic analysis demonstrates a pattern of rare and ancient horizontal gene transfer between plants and fungi. Plant Cell. 2009, 21 (7): 1897-1911. 10.1105/tpc.109.065805.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  72. 72.

    Lorenz MC, Heitman J: The MEP2 ammonium permease regulates pseudohyphal differentiation in Saccharomyces cerevisiae. EMBO J. 1998, 17 (5): 1236-1247. 10.1093/emboj/17.5.1236.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  73. 73.

    Rutherford JC, Lin X, Nielsen K, Heitman J: Amt2 permease is required to induce ammonium-responsive invasive growth and mating in Cryptococcus neoformans. Eukaryot Cell. 2008, 7 (2): 237-246. 10.1128/EC.00079-07.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  74. 74.

    Smith DG, Garcia-Pedrajas MD, Gold SE, Perlin MH: Isolation and characterization from pathogenic fungi of genes encoding ammonium permeases and their roles in dimorphism. Mol Microbiol. 2003, 50 (1): 259-275. 10.1046/j.1365-2958.2003.03680.x.

    Article  CAS  PubMed  Google Scholar 

  75. 75.

    Gimeno CJ, Ljungdahl PO, Styles CA, Fink GR: Unipolar cell divisions in the yeast S. cerevisiae lead to filamentous growth: regulation by starvation and RAS. Cell. 1992, 68 (6): 1077-1090. 10.1016/0092-8674(92)90079-R.

    Article  CAS  PubMed  Google Scholar 

  76. 76.

    Mumberg D, Muller R, Funk M: Yeast vectors for the controlled expression of heterologous proteins in different genetic backgrounds. Gene. 1995, 156 (1): 119-122. 10.1016/0378-1119(95)00037-7.

    Article  CAS  PubMed  Google Scholar 

  77. 77.

    Gietz RD, Schiestl RH: Quick and easy yeast transformation using the LiAc/SS carrier DNA/PEG method. Nature Protocols. 2007, 2 (1): 35-37. 10.1038/nprot.2007.14.

    Article  CAS  PubMed  Google Scholar 

  78. 78.

    Raymond CK, Pownder TA, Sexson SL: General method for plasmid construction using homologous recombination. Biotechniques. 1999, 26 (1): 134-138. 140–141

    CAS  PubMed  Google Scholar 

  79. 79.

    Armaleo D, May S: Sizing the fungal and algal genomes of the lichen Cladonia grayi through quantitative PCR. Symbiosis. 2009, 49: 43-51. 10.1007/s13199-009-0012-3.

    Article  Google Scholar 

  80. 80.

    Zerbino DR, Birney E: Velvet: algorithms for de novo short read assembly using de Bruijn graphs. Genome Res. 2008, 18 (5): 821-829. 10.1101/gr.074492.107.

    PubMed Central  Article  CAS  PubMed  Google Scholar 

  81. 81.

    Maddison DR, Maddison WP: MacClade 4: Analysis of phylogeny and character evolution. 4.08ath edition. 2005, Sunderland, MA: Sinauer Associates

    Google Scholar 

  82. 82.

    Posada D: jModeltest: phylogenetic model averaging. Mol Biol Evol. 2008, 25: 1253-1256. 10.1093/molbev/msn083.

    Article  CAS  PubMed  Google Scholar 

  83. 83.

    Nylander JAA: Mr. ModelTest v2. 2004, Evolutionary Biology Centre, Upsalla University, Program distributed by the author

    Google Scholar 

  84. 84.

    Stamatakis A, Ludwig T, Meier H: RAxML-III: a fast program for maximum likelihood-based inference of large phylogenetic trees. Bioinformatics. 2005, 21 (4): 456-463. 10.1093/bioinformatics/bti191.

    Article  CAS  PubMed  Google Scholar 

  85. 85.

    Swofford DL: PAUP*. Phylogenetic analysis using parsimony (*and other methods). 4.0 b 10th edition. 2002, Sunderland, MA: Sinauer Associates

    Google Scholar 

  86. 86.

    Grenson M, Mousset M, Wiame JM, Bechet J: Multiplicity of the amino acid permeases in Saccharomyces cerevisiae I. Evidence for a specific arginine-transporting system. Biochim Biophys Acta. 1966, 127 (2): 325-338. 10.1016/0304-4165(66)90387-4.

    Article  CAS  PubMed  Google Scholar 

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Acknowledgements

The authors would like to thank Duke Institute for Genome Sciences and Policy (IGSP), especially Huntington Willard and Gregory Wray, for funding support for the Cladonia grayi and Asterochloris sp. genome projects and Daniele Armaleo for his contribution to the original discovery of MEP α in Cladonia grayi. This project was also funded in part by a subcontract (112442) to Daniele Armaleo, Fred Dietrich and François Lutzoni as part of the Pacific Northwest National Laboratory (PNNL) foundational scientific focus area (FSFA) under DOE-BER’s genomic sciences program in collaboration with Scott Baker and Jon Magnuson. This work would not have been possible without the Duke Shared Cluster Resource (DSCR) and outstanding services provided by John Pormann and Tom Milledge. We would like to thank Geir Hestmark for specimens of Umbilicaria, Suzanne Joneson for sharing the culture of Endocarpon pallidulum, Brendan Hodkinson for sharing transcriptome data from Peltigera phyllidiosa, Bernard Goffinet for sharing genomic data from Peltigera dolichorrhiza, Mark Chee for the pGal and p416 plasmids, and Joseph Heitman for the MLY131 strains of Saccharomyces cerevisiae. TM would like to thank Jolanta Miadlikowska for assistance with graphics software, and the Duke University sequencing facility, particularly Fangfei Ye, for sample preparation and sequencing and acknowledge a FESIN/Nordforsk travel grant, and travel grants from the Duke University Graduate School, an Anne T. and Robert M. Bass Fellowship for Undergraduate Instruction from Duke University Graduate School, and a James B Duke Fellowship from the Duke University Graduate School.

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  1. Tami R McDonald

    Present address: Department of Microbiology, University of Minnesota, Minneapolis, MN, 55455, USA

Affiliations

  1. Department of Biology, Duke University, Durham, NC, 27708, USA

    Tami R McDonald & François Lutzoni

  2. Department of Molecular Genetics and Microbiology, Duke University, Durham, NC, 27710, USA

    Olaf Mueller & Fred S Dietrich

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  2. Olaf Mueller
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Correspondence to Tami R McDonald.

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The authors declare that they have no competing interests.

Authors’ contributions

TM carried out the molecular genetic studies, the phylogenetic analyses, sequenced the genomes, performed bioinformatics analyses, and drafted the manuscript. OM performed genome assemblies and downstream bioinformatics analyses. FD assisted in strain construction and bioinformatics. FL critically reviewed the manuscript and was the main advisor of TM for her Ph.D. from which this article is derived. All authors read and approved the final manuscript.

Electronic supplementary material

Additional file 1: PCR and sequencing primers (5’ to 3’).(PDF 32 KB)

Additional file 2: Gapped plasmid construction plasmids.(PDF 25 KB)

Additional file 3: Strains of Saccharomyces cerevisiae carrying AMTP genes from Cladonia grayi[86].(DOCX 7 MB)

Additional file 4: Accession numbers for AMTP genes from lichen genomes.(DOCX 16 KB)

Additional file 5: Accession numbers and genome coordinates of ammonium transporter/ammonia permease genes included in the phylogenetic tree.(PDF 183 KB)

Additional file 6: Phylogenetic placement of ammonium transporters/ammonia permeases from eight lichen genomes. Maximum likelihood analysis of 300 ammonium transporter/ammonia permease genes details the phylogenetic placement of ammonium transporter/ammonia permease genes in the well-supported predominantly prokaryotic clade (MEP) in which eukaryotic lineages demonstrate horizontal gene transfer. (PDF 2 MB)

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McDonald, T.R., Mueller, O., Dietrich, F.S. et al. High-throughput genome sequencing of lichenizing fungi to assess gene loss in the ammonium transporter/ammonia permease gene family. BMC Genomics 14, 225 (2013). https://doi.org/10.1186/1471-2164-14-225

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Keywords

  • Ammonium transporter
  • Ammonia permease
  • Phylogeny
  • Lichen symbiosis
  • Fungi
  • Genome
  • Illumina
  • Horizontal gene transfer

BMC Genomics

ISSN: 1471-2164

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