For genome sequencing, a 500-mL culture of D. amilsii was grown on acetate and sulfur as described elsewhere (Florentino et al., 2015). Cells were harvested at the early stationary phase, when the sulfide production in the culture reached 10 mM, by centrifuging at 19000 × g for 20 min. Genomic DNA was extracted using the MasterPure^TM Gram Positive DNA Purification Kit (Epicentre, Madison, WI, USA), following the instructions of the manufacturer. The genome was sequenced using the Illumina HiSeq2000 paired-end sequencing platform of GATC Biotech (Konstanz, Germany). Sequence assembly was performed using two independent assemblers: the OLC-assembler Edena (Hernandez et al., 2008) and the de-Bruijn-Graph-assembler Ray (Boisvert et al., 2010). Sets of overlapping sequences were identified from both assembling procedures and further merged into a more contiguous and consistent assembly, using the hybrid sequencing technology assembler Zorro (Argueso et al., 2009). The obtained sequences were further improved by scaffolding with Opera and by gap-closing with GapFiller (Boetzer and Pirovano, 2012). The closed gaps were manually verified.

Automated annotation was performed using the RAST annotation server (Aziz et al., 2008), followed by manual curation. Additional gene prediction analysis and functional annotation were done within the Integrated Microbial Genomes – Expert Review from the DOE – Joint Genome Institute pipeline (Markowitz et al., 2014). The predicted coding sequences (CDSs) were translated into amino acid sequences and used in homology searches in the National Center for Biotechnology Information (NCBI) non-redundant database and the Uniprot, TIGRFam, Pfam, SMART, PRIAM, KEGG, COG, and Interpro databases. These data sources were combined to assign a product description for each predicted protein. Clusters of regularly interspaced repeats (CRISPR) were identified via the web available tools CRISPRFinder (Grissa et al., 2007) and CRISPRTarget (Biswas et al., 2013). The N-terminal twin arginine translocation (Tat) signal peptides and the transmembrane helices were predicted using the online tools from TMHMM server v. 2.03¹ and PROTTER v. 1.0².

The Whole Genome Shotgun project of Desulfurella amilsii has been deposited at DDBJ/ENA/GenBank under the accession MDSU00000000. The version described in this paper is version MDSU01000000. The genome ID in the integrated microbial genomes-expert review (IMG) database is 2693429826.

The genome sequences used for the comparative study (and their accession numbers) were: D. acetivorans strain A63 (CP007051), D. multipotens strain RH-8 (SAMN05660835), H. maritima strain MH2 (CP002606), H. alviniae strain EP5-r (ATUV00000000), H. medeae strain KM1 (JAFP00000000), and H. jasoniae strain Mar08-272r (JQLX00000000).

The average nucleotide identity analysis (ANI) between the genome dataset pairs was performed using the online tool ANI calculator, available at http://enve-omics.ce.gatech.edu/ani/index. The best hits (one-way ANI) and the reciprocal best hits (two-way ANI) were considered, as calculated by Goris et al. (2007). In silico DNA–DNA hybridization (DDH) values were determined using the recommended settings of the Genome-to-Genome Distance Calculator (GGDC) web server version 2.0 (Meier-Kolthoff et al., 2013).

The number of genes shared between Desulfurella and Hippea species was assessed by OrthoMCL tool (Wang et al., 2015) and a Venn diagram was built using the web-based tool InteractiVenn (Heberle et al., 2015). Orthology between two genes was defined as best bidirectional hits, which were required to have at least 30% identity over at least 80% coverage of both sequences (Chen et al., 2006). All analyzed genes and predicted proteins from the Desulfurellaceae members’ genomes were compared using BLAST (Altschul et al., 1990).

The genomes were compared in terms of gene content using the ‘Phylogenetic Profiler for Single Genes’ of JGI-IMG website³ to identify genes in the query genome that have homologs present or absent in other genomes. The ‘Phylogenetic Profiler for Gene Cassettes’ tool of the same website was also used to find part of a gene cassette in a query genome, as well as conserved part of gene cassettes in other genomes. In terms of functional capabilities, comparisons of relative abundance of protein families (COGs, Pfams, TIGRfams) across selected genomes were performed with the ‘Abundance Profile Overview’ and ‘Function Profile’ tools. The potential metabolic capabilities of genomes were compared in the context of KEGG pathways.

The D. amilsii genome consists of 2.010.635 bp with a G + C content of 33.98% mol/mol. The initial sequencing resulted in 2.287.922 paired-end reads with a length of 301 bases, which were assembled into 20 contigs with a 687 fold coverage and a completeness of 99.9%. The largest scaffold consisted of 1,269,579 bp and the second and third largest scaffolds together consisted of 400,000 bp, covering more than 85% of the genome.

From the 2137 genes predicted by automated annotation in the genome, 49 were tRNA and rRNA genes, and 2088 protein coding genes (CDS). Two identical copies of the 16S rRNA gene (100% similarity) were identified. From the 2088 CDS (Supplementary Table S1), 1625 were predicted to have assigned COGs function, whilst 680 could not be assigned to any function in the database, and therefore were annotated as hypothetical proteins or proteins of unknown function. No pseudo genes were detected in the genome of D. amilsii, which is a unique characteristic in the Desulfurellaceae family. Two CRISPR regions were identified in the genome of 684 bp length with 10 spacers, and 291 bp length with 4 spacers, respectively. The spacers’ sequences from the first locus match viral DNA sequences found in several species in a BLAST based search, including Bacillus sp., Ralstonia sp., Shewanella sp., Acinetobacter sp., Propionibacterium sp., Campylobacter sp., Escherichia sp., Staphylococcus sp., Sphingomonas sp., and Moraxella sp. The spacer’s sequences related to the second locus match sequences of viral DNA also detected in Edwardsiella hoshinae. Owenweeksia hongkongensis. Parascaris equorum, and Ovis canadensis species.

The genome encodes a complete tricarboxylic acid (TCA) cycle pathway (Supplementary Table S2). Besides, routes for pyruvate fermentation are encoded, and physiological tests revealed acetate, hydrogen and CO₂ as the end products (Florentino et al., 2016a). D. amilsii is able to grow chemolithotrophically; the CO₂ fixation could be possible via the reductive TCA cycle for which all the genes are encoded (Supplementary Table S3). The genome encodes Ni–Fe, Ni–Fe–Se, and Fe–S hydrogenases, an intracellular formate dehydrogenase (FDH) and a formate-hydrogen lyase. Genes encoding for dinitrogenase iron-molybdenum cofactor, nitrogen fixation protein NifU and glutamine synthetase type I are present in the genome and might be involved in nitrogen fixation by D. amilsii. Sulfur and thiosulfate were reported to serve as electron acceptors for this microorganism (Florentino et al., 2015, 2016a) and genes essential for sulfur and thiosulfate reduction are encoded (Supplementary Table S3). Moreover, the importance of electron transport in this microorganism is highlighted by a high number of electron transport related genes (159). Genes encoding resistance to acidic conditions (Supplementary Table S4), oxygen stress tolerance (Supplementary Table S5), and metals resistance (Supplementary Table S6) are also identified, which is in line with the reported ability of the microorganism to grow at pH as low as 3 (Florentino et al., 2016a) and in the presence of heavy metals in solution (Florentino et al., 2015).

The electron transport chain in sulfur reducers normally links hydrogenases or dehydrogenases to membrane bound or cytoplasmic sulfur/polysulfide reductases (Laska et al., 2003; Fauque and Barton, 2012; Florentino et al., 2016b). However, the electron-transfer pathways in the microorganisms analyzed here are not yet fully understood.

Sulfur metabolism in Desulfurellaceae members is quite diverse, as genes encoding for at least three enzymes involved in sulfur reduction are present in the group. Sulfur, sulfide and polysulfide are present in solution in a pH-dependent equilibrium (HS−+x−18S8↔Sn2−+H+). At higher pH values, polysulfide is present as the dominant form, while at low pH values elemental sulfur prevails (Kleinjan et al., 2005).

Hippea species genomes possess genes encoding for the membrane bound PSR, an integral membrane protein complex responsible for quinone oxidation coupled to polysulfide reduction, and the cytoplasmic sulfide dehydrogenase (SUDH), reported to catalyze the reduction of polysulfide to hydrogen sulfide with NADPH as the electron donor (Macy et al., 1986; Ma et al., 2000). The domains 4Fe-4S, 4Fe-S Mo-bis of the catalytic subunit and Nfr of the membrane-bound subunit with nine transmembrane helices of the PSR are conserved in all the Hippea species. The pH range for growth of Hippea species (Miroshnichenko et al., 1999; Flores et al., 2012) supports the hypothesis of sulfur reduction through polysulfide in these microorganisms.

The alpha and beta subunits of the SUDH encoded in all genomes of the Desulfurellaceae family show domains conserved in all the microorganisms: NAD-binding and iron-sulfur clusters (3Fe-4S and 4Fe-4S) domains in the subunit SudhA and FAD-binding and iron-sulfur cluster 2Fe-2S domains in the subunit SudhB. In D. acetivorans, only SUDH-coding genes are present (Desace_0075-0076), which would suggest that polysulfide is the terminal electron acceptor in its respiration process. D. amilsii is unique as, in addition to SUDH (DESAMIL20_1852-1853), SRE is encoded (DESAMIL20_1357-1361). A SRE was isolated from the acidophile Acidianus ambivalens, and its subunits were partially characterized and compared to their homologous in the PSR isolated from Wolinella succinogenes (Laska et al., 2003). SRE is reported to be involved in direct reduction of elemental sulfur, with the electrons being donated by hydrogenase, quinones and cytochrome c. SRE also uses NADPH as an electron donor, but at low activity (Laska et al., 2003). The SRE encoded in the D. amilsii genome presents, in general, conserved domains for four of its subunits. The membrane anchor subunit (SreC), with nine transmembrane helices, has a PSR domain (Figure 2) similar to the one encoded in A. ambivalens, which was shown by Laska et al. (2003) to be phylogenetically unrelated to the analogous W. succinogenes protein. The catalytic subunit (SreA) contains the conserved molybdopterin domain, predicted to be functional with respect to oxidoreductase activity. The sequence, however, does not present a twin-arginine motif and so, in contrary to the SRE from A. ambivalens, it might be cytoplasm oriented. The subunit SreB also presents the 4Fe-4S domain conserved, which has a high degree of sequence similarity to Mo-FeS enzymes of the DMSO reductase family. The subunit SreD in D. amilsii does not contain the conserved 4Fe-4S domain; but its function in sulfur respiration is not yet clears (Laska et al., 2003). The sreE gene encodes a protein of 209 aa length with similarity to reductase assembly proteins required either for the assembly of the Mo-containing large subunit of DMSO reductase or nitrate reductase (Blasco et al., 1998; Ray et al., 2003).

Since the reduction of elemental sulfur through polysulfide is unlikely at low pH, the SRE encoded in D. amilsii might play a role when this microorganism grows in acidic conditions. Moreover, several thiosulfate sulfurtransferases with rhodanese domains are exclusively encoded in Desulfurella species.

The enzyme SUDH isolated from Pyrococcus furiosus was reported to show SRE activity in vitro. However, the expression of its coding-genes also correlated to the carbon source rather than to elemental sulfur/polysulfide, especially when its intracellular concentration is below 1.25 mM (Ma and Adams, 2001). It is likely that this enzyme acts in vivo as a ferredoxin:NADPH oxidoreductase (NfnAB). In this case, in Hippea species, the sulfur reduction process might be carried out by the PSR, while in Desulfurella species the rhodanese-like thiosulfate sulfurtransferases might play an essential role. In Figure 2, a metabolic reconstruction of the possible sulfur reduction pathways in D. amilsii is depicted.

Desulfurella amilsii is able to use thiosulfate as a terminal electron acceptor in a range of pH from 5 to 7, an ability not reported for any of the other analyzed genomes of the members of Desulfurellaceae. Although D. propionica was also shown in vivo to utilize thiosulfate as an electron acceptor, its genome sequence is not yet available. The known pathway of thiosulfate reduction refers to a two-step process, involving the enzymes thiosulfate reductase and the dissimilatory sulfite reductase (Stoffels et al., 2012). The first is reported to be involved in the conversion of thiosulfate into sulfide and sulfite, which can be toxic for most microorganisms. The dissimilatory reductase converts the generated sulfite into sulfide, eliminating the toxicity of sulfite from the medium. In D. amilsii, it is likely that thiosulfate respiration occurs via this pathway, as the thiosulfate reductase, the dissimilatory sulfite reductase (DsrAB), the DsrC protein and the subunits DsrM and DsrK of the Dsr MKJOP complex are encoded in the genome. The genome of D. acetivorans encodes a thiosulfate reductase and the dissimilatory sulfite reductase, but subunits of the Dsr MKJOP transmembrane complex and the DsrC protein are not encoded. Therefore, the absence of subunits of Dsr MKJOP and DsrC might explain the inability of D. acetivorans to respire thiosulfate. Table 3 summarizes the enzymes involved in sulfur and thiosulfate respiration, with their respective reactions and the orthologs genes.

Desulfurella species grow and produce sulfide and sulfate from sulfur in the absence of an organic electron donor (Florentino et al., 2016a), in a specific redox reaction that undergoes oxidation and reduction, also called disproportionation. Sulfur could be converted into sulfide via a sulfur-reducing enzyme (e.g., SRE/SUDH) and to sulfite by an unidentified enzyme. In general, the sulfite could be oxidized to sulfate by sulfite oxidoreductase (SUOR) or adenosine-5′-phosphosulfate (APS) reductase, with ATP sulfurylase or adenylylsulfate:phosphate adenylyltransferase (APAT) being involved (Finster et al., 1998; Frederiksen and Finster, 2003; Hardisty et al., 2013). Although the enzyme responsible for the conversion of sulfur into sulfite is not known, SUDH/SRE and DSR coding genes were detected in both Desulfurella members’ genomes, suggesting that these bacteria might disproportionate elemental sulfur using this pathway. APS reductase was not detected in any species, which supports the inability of this group to use sulfate as electron acceptor or to disproportionate elemental sulfur via the reverse pathway from sulfite to APS and then to sulfate.

Sulfur metabolism in Desulfurellaceae family members is quite diverse. The presence of unique proteins in D. amilsii might explain its ability to respire elemental sulfur at low pH, where polysulfide is not available. The ability of D. amilsii to respire thiosulfate in a two-step process is also unique among the analyzed members of the family. Besides, disproportionation appears as a feature only shared by members of Desulfurella genus, and so this genus, with a more versatile metabolism, offers more possibilities for biotechnological application based on sulfidogenesis.

Enzymes involved in the central carbon metabolism of Desulfurellaceae members are listed in Supplementary Table S2 and the ones involved in energy metabolism and conservation are listed in Supplementary Table S3. The general metabolic reconstruction of D. amilsii is depicted in Figure 3, in which the differential central carbon metabolism for Desulfurellaceae members can also be seen. Proteins for complete Embden-Meyerhof-Parnas and oxidative TCA cycle pathways are encoded in all the genomes of the Desulfurellaceae members, as well as decarboxylating malate dehydrogenase (ME), which can catalyze the reversible conversion of malate to pyruvate. Although the malate dehydrogenase is present, malate transporters are not encoded in the genome of the analyzed Desulfurella genus members, which might explain their inability to use malate as an electron donor for growth.

Besides the conversion of phosphoenolpyruvate to pyruvate via pyruvate kinase (PYK) and the irreversible carboxylation of pyruvate to form oxaloacetate via pyruvate carboxylase (PYC) common for all Desulfurellaceae members, Desulfurella and H. jasoniae genomes also encode the phosphoenolpyruvate carboxylase (PCK). Pyruvate:ferredoxin oxidoreductase (PFOR) and related 2-oxoacid:ferredoxin oxidoreductases are encoded in all the genomes in the group, where pyruvate oxidation is a main intermediate metabolic reaction. Moreover, all the genomes possess the gene encoding pyruvate:formate lyase (PFL), involved in pyruvate metabolism and leading to the production of acetyl-CoA and formate. D. amilsii and D. acetivorans were shown to ferment pyruvate in laboratorial analyses, but formate could only be used as an electron donor by D. amilsii (Florentino et al., 2016a), despite the subunits FdoG, FdoH and FdoI of a FDH being encoded in D. acetivorans genome.

All members of the Desulfurellaceae family can utilize acetate (Florentino et al., 2016a). The metabolism of acetate starts with its activation to acetyl-CoA, an essential intermediate of various anabolic and catabolic pathways in all forms of life (Ingram-Smith et al., 2006). Acetate activation involves either the enzymes acetyl-CoA synthetase (ACS), acetate kinase (ACK) in combination with phosphate acetyltransferase (PTA), or the enzyme succinyl-CoA: acetate CoA-transferase (SCACT). All Desulfurellaceae species have the enzyme ACS encoded in their genome. In Desulfurella species, however, acetyl-CoA could also be generated from acetate via acetylphosphate involving ACK and PTA. The genome analysis shows both pathways for acetate oxidation are encoded in Desulfurella species. However, experimental studies performed by Schmitz et al. (1990) showed that cell extracts of D. acetivorans had high specific activities of ACK (5 U/mg) and PTA (14 U/mg), but no activity of the alternative ACS nor the SCACT. Although Goevert and Conrad (2010) demonstrated acetate activation via ACK and its metabolization via the TCA cycle in H. maritima, genes encoding ACK are not found in any Hippea members’ genome.

Chemolithotrophic growth of Desulfurellaceae members with H₂ as electron donor and S⁰ as electron acceptor requires at least two enzymes in a short electron transport chain composed by a hydrogenase, an electron carrier, and a sulfur/polysulfide reductase. Only one Ni-Fe type hydrogenase (HybABC), which catalyzes reversible hydrogen production/consumption, is encoded in Desulfurellaceae members together with its maturation protein HypABCDEF (Supplementary Table S3). The subunit HybB is embedded in the membrane and the subunit HybA possess a tat signal, therefore the hydrogenase is membrane-bound facing periplasm. The hydrogen is converted into protons, creating proton motive force and electrons which are transferred via intramembrane electron carriers, such as the encoded menaquinone, to the membrane bound SRE or PSR, or to the cytoplasmic SUDH.

Although physiological tests revealed some differences among the studied species, the comparative genomic analysis on the general metabolism of Desulfurellaceae members does not show great divergence in gene sets involved in chemolithotrophic growth, TCA cycle and pyruvate fermentation. However, the utilization of acetate might have different routes of metabolization by the two analyzed genera.

Acidophiles and acidotolerant microorganisms can have a broad range of adaptation mechanisms to thrive at acidic environments, while ensuring higher cytoplasmic pH values than the surrounding environment (Baker-Austin and Dopson, 2007).

It is predicted that Desulfurella species can synthesize degradative arginine decarboxylase to consume intracellular protons via the amino acid decarboxylation reaction and, consequently, neutralize the medium. Moreover, the analyzed Desulfurella species encode the K⁺-transporting ATPase and a putative regulating histidine kinase, involved in the generation of positive internal membrane potential by influx of potassium ions in order to inhibit the flux of protons in extreme acidophiles (Dopson and Johnson, 2012). ABC phosphate transporters, sodium-coupled antiporters and amino acid antiporters that are pH dependent (Kanjee and Houry, 2013) and related to acid resistance are also encoded in the referred genomes (Supplementary Table S4). The genomic components potentially involved in stress response to acidic environments in Desulfurellaceae members are listed in Supplementary Table S4.

The ability of Desulfurella species to thrive at low pH using acetate as an electron donor requires resistance mechanisms. When the pH of the medium is lower than the pKa value of acetic acid (4.75), the weak organic acid prevails in its protonated form, which crosses the cytoplasmic membrane by diffusion. At neutral cytoplasmic pH, the acid dissociates, leading to the release of protons and respective anions, resulting in the acidification of the cytoplasm (Holyoak et al., 1996). Desulfurella species genomes encode the ATP-binding cassette transporter (AatA) reported to be involved in acetic acid resistance in acetic acid bacteria (Nakano et al., 2006). This putative ABC transporter contains two ABC motifs in tandem on a single polypeptide, which possibly serves as an exporter of acetic acid, maintaining a low level of intracellular acetic acid concentration (Nakano et al., 2006).

The genes encoded in Desulfurellaceae family members possibly involved in resistance to low pH do not vary. However physiological tests showed the ability of Desulfurella species to grow at more acidic environments, with D. amilsii being able to grow at pH as low as 3 (Florentino et al., 2016a) and D. acetivorans at pH 4.3 (Bonch-Osmolovskaya et al., 1990). Different regulation of those genes, or a completely unknown mechanism encoded in those microorganisms, might be key to explain the differences in resistance of high proton concentrations.

Survival of strict anaerobic microorganisms, such as the members of the Desulfurellaceae family, in environments exposed to high redox potential would include antioxidant strategies. Furthermore, the acidotolerant D. amilsii was isolated from acidic sediments from the Tinto River which possess zones with very high redox conditions (up to +400mV) and high concentrations of soluble metals, such as copper, iron, and zinc (Florentino et al., 2015). The excess of metals contributes to redox-active metals toxicity, generating reactive oxygen species (ROS) via the slow Fenton and Haber–Weiss reactions. When the oxidation states of the metal ions switches, reactive species, such as hydrogen peroxide (H₂O₂) and superoxide (•O^2-) are activated to the hydroxyl radical (•OH), resulting in a highly reactive form (Flora et al., 2008). Therefore, the presence of genes encoding oxidative stress related enzymes is of great importance for the survival of this species in its original habitat.

Superoxide reductase desulfoferrodoxin is encoded in all Desulfurellaceae members’ species, as well as rubredoxin, that can transfer electrons and reduce the superoxide dismutase (Supplementary Table S5) (Sheng et al., 2014). Reduction of peroxides is performed by enzymes such as glutathione peroxidase, peroxirredoxin, rubrerythrins, alkylhydroperoxidases and catalases. Rubrerythrin is encoded in all the genomes; in Desulfurella species, H. alviniae and H. jasoniae the rubrerythrin-coding gene is flanked by a peroxiredoxin, while in H. maritima and H. medea it is flanked by a DNA repair mechanism involved in gene spore photoproduct lyase. Peroxiredoxins and thioredoxins-coding genes are present in all Desulfurellaceae genomes studied. Together with rubrerythrin and the ferric uptake regulator (Fur) family, the peroxiredoxins and thioredoxins are well-represented in acidophiles and acidotolerant microorganisms (Cárdenas et al., 2016). The rubrerythrin and the Fur family replace activities of catalase and oxidative stress response regulators in neutrophiles, while peroxiredoxins and thioredoxins remove organic peroxides originated when ROS attack organic molecules (Cárdenas et al., 2012).

Oxidizing agents normally modify the DNA in complex patterns, leading to mutagenic effects. Three different DNA repair pathways are involved in the removal of the oxidized bases in DNA and their mismatches: base excision repair (BER), nucleotide excision repair (NER) and mismatch repair (MMR). The genomes of the Desulfurella species encode DNA repair mechanisms, including the protein RecA, the excinuclease UvrABC and the GroEL protein (Supplementary Table S4). All bacterial genomes analyzed contained genes for the detection and removal of modified purine and pyrimidine bases (BER pathway), including orthologs of the uracyl-DNA glycosylase gene. The UvrABC repair system for NER pathway, which operates on the removal of bulky lesions from the DNA duplex, was present in the genome of all species. Additionally, genes responsible for the SOS response to DNA damage, RecA/RadA were found in all organisms; LexA, however, is only present in D. acetivorans. Genes encoding the Dps protein, endonucleases and the minimal essential complex for mismatched base repair were not detected in any of the analyzed genomes.

Despite the different isolation sources of the Desulfurellaceae members and a lack of physiological data from Hippea species and D. acetivorans, differences in genes encoding resistance to oxidative stress were not detected in the genome, and so regulatory processes might be responsible for them to tackle the harsh conditions.

Several prokaryotes show specific genetic mechanisms of resistance to toxic concentrations of metals in the environment, which include their oxidation or reduction to less toxic valence states, incorporation or precipitation of heavy metals as metal sulfides complexes, and the direct transport of metals out of the membrane (Ji and Silver, 1995). Generally, the mechanisms for uptake of metals can be ATP-independent and driven by chemosmotic gradients across the membrane or is dependent on the energy released from ATP hydrolysis in a substrate-specific manner (Ahemad, 2012).

One of the ATP-based mechanisms proposed for metals resistance in bacteria is the synthesis of polyphosphates via the enzyme polyphosphate kinase, which can interact with metal ions due to its polyanion nature (Pan-Hou et al., 2002). Genes encoding the polyphosphate kinase are present in Desulfurella species and in H. maritima. D. amilsii was shown to be resistant to relatively high concentrations of copper and nickel (Florentino et al., 2015). The resistance to copper can also be related to the presence of genes encoding the copper-exporting P-type ATPase, present in all species.

Desulfurella species and H. maritima genomes encode the Co/Zn/Cd efflux system, components of inorganic ion transport and metabolism. Desulfurella species and H. alviniae encode some cation transporters (Supplementary Table S6), that are unspecific and chemiosmotic gradient driven across their cytoplasmic membrane.

Although genes encoding resistance to heavy metals are in all the analyzed species, the isolation source of D. amilsii is a metal rich environment, and, as many metals are more soluble at acidic pH, this microorganism is more exposed to the high metal concentrations than the other members of Desulfurellaceae family isolated from neutrophilic environments (Bonch-Osmolovskaya et al., 1990; Miroshnichenko et al., 1999; Flores et al., 2012). Besides, as described by Dopson et al. (2014), high concentrations of sulfate are also normally present in acidic environments, which can complex metal cations and lower the concentration of free metals that can enter the microbial cell cytoplasm. Therefore, it is likely that such abiotic factor, in combination with other factors, such as the competition with protons for binding sites, might contribute to the increased tolerance to metals in solution by D. amilsii in comparison to its neutrophilic relatives.