Skip to main content

Advertisement

Archaea dominate the microbial community in an ecosystem with low-to-moderate temperature and extreme acidity

Article metrics

Abstract

Background

The current view suggests that in low-temperature acidic environments, archaea are significantly less abundant than bacteria. Thus, this study of the microbiome of Parys Mountain (Anglesey, UK) sheds light on the generality of this current assumption. Parys Mountain is a historically important copper mine and its acid mine drainage (AMD) water streams are characterised by constant moderate temperatures (8–18 °C), extremely low pH (1.7) and high concentrations of soluble iron and other metal cations.

Results

Metagenomic and SSU rRNA amplicon sequencing of DNA from Parys Mountain revealed a significant proportion of archaea affiliated with Euryarchaeota, which accounted for ca. 67% of the community. Within this phylum, potentially new clades of Thermoplasmata were overrepresented (58%), with the most predominant group being “E-plasma”, alongside low-abundant Cuniculiplasmataceae, ‘Ca. Micrarchaeota’ and ‘Terrestrial Miscellaneous Euryarchaeal Group’ (TMEG) archaea, which were phylogenetically close to Methanomassilicoccales and clustered with counterparts from acidic/moderately acidic settings. In the sediment, archaea and Thermoplasmata contributed the highest numbers in V3-V4 amplicon reads, in contrast with the water body community, where Proteobacteria, Nitrospirae, Acidobacteria and Actinobacteria outnumbered archaea. Cultivation efforts revealed the abundance of archaeal sequences closely related to Cuniculiplasma divulgatum in an enrichment culture established from the filterable fraction of the water sample. Enrichment cultures with unfiltered samples showed the presence of Ferrimicrobium acidiphilum, C. divulgatum, ‘Ca. Mancarchaeum acidiphilum Mia14’, ‘Ca. Micrarchaeota’-related and diverse minor (< 2%) bacterial metagenomic reads.

Conclusion

Contrary to expectation, our study showed a high abundance of archaea in this extremely acidic mine-impacted environment. Further, archaeal populations were dominated by one particular group, suggesting that they are functionally important. The prevalence of archaea over bacteria in these microbiomes and their spatial distribution patterns represents a novel and important advance in our understanding of acidophile ecology. We also demonstrated a procedure for the specific enrichment of cell wall-deficient members of the archaeal component of this community, although the large fraction of archaeal taxa remained unculturable. Lastly, we identified a separate clustering of globally occurring acidophilic members of TMEG that collectively belong to a distinct order within Thermoplasmata with yet unclear functional roles in the ecosystem.

Background

Prokaryotic organisms which optimally grow at pH 3 and below are termed acidophiles. Acidophilia is a trait widely distributed among numerous prokaryotic phyla. Historically, a few bacterial species, such as Acidithiobacillus spp. and Leptospirillum spp. were believed to be the most ubiquitous and abundant acidophiles. However, current knowledge suggests that acidophilic bacterial diversity stretches over numerous representatives of Proteobacteria, Nitrospirae, Firmicutes, Actinobacteria, Acidobacteria, Aquificae and Verrucomicrobia [1, 2]. Furthermore, the signatures of Chloroflexi and various uncultured candidate taxa have been documented in acidic environments [3]. In these environments, culture-independent molecular techniques suggested the affiliation of the archaeal acidophilic component to the phyla Euryarchaeota, Crenarchaeota, Thaumarchaeota, ‘Candidatus Parvarchaeota’ and “Ca. Micrarchaeota” [1], whereas the few well-studied archaeal acidophilic isolates exclusively belonged to the order Thermoplasmatales of Euryarchaeota and to the phylum Crenarchaeota [2, 4, 5]. More recent metagenomic surveys of acidic sites have, however, revealed that a large proportion of organisms therein are affiliated with yet uncultured and unstudied taxa within Thermoplasmata [1, 6, 7]. Groups of uncultured archaea affiliated with the order Thermoplasmatales [8] have been predicted in acid mine drainage (AMD), one of which, ‘G-plasma’, has successfully been isolated, characterised and described as Cuniculiplasma divulgatum [9, 10]. A handful of members from the families Ferroplasmaceae and Cuniculiplasmataceae are currently the only isolated and characterised mesophilic extremely acidophilic species of archaea. The major physico-chemical drivers regulating the relative abundances of the bacterial and archaeal components in the acidophilic microbiome, however, remain unclear. Temperature, pH, redox potential and dissolved oxygen are considered the main factors influencing the composition of any acidic microbial community [11]. Temperature is often assumed to be the most important factor regulating the relative abundance of archaeal vs bacterial components with a general assumption that bacteria are more prevalent at lower temperatures [12]. In contrast, the prevailing pH is considered to be of secondary importance [12]. It has been shown that at pH < 2, the relative abundance of archaea in AMD systems increases with up to 25% of all prokaryotes belonging to this Domain [2]. It was also reported that at pH values below 1.9, the relative abundance of Thermoplasmatales archaea increased at the expense of populations of proteobacteria [13]. Moreover, biofilm samples in sites with pH values of about 1 and temperatures around 38 °C taken from underground site on Richmond Mine (CA, USA) demonstrated an extremely high proportion of archaeal reads (69–98% of the total) [14]. Representatives of Euryarchaeota and ‘Ca. Parvarchaeota’ were reported as major components in certain acidic environments, characterised by pH 1.9 and 43.3 °C and by pH 2.7 and 21.4 °C, respectively [15]. Furthermore, the data of [16, 17] pointed at the prevalence of archaeal reads in low pH ecosystems in warm subtropical climate with an annual mean temperature of 18 °C. However, the Archaea inhabiting ecosystems with rather moderate or constantly low temperatures are frequently considered to constitute only a minor proportion of the entire microbial community or to be completely absent [3, 11, 18]. Parys Mountain (Parys Mt), located on the Island of Anglesey (North Wales, UK), is an example of such a cool environment, and the microbiome of its acidic stream was chosen for the present study.

Parys Mt is historically one of the most important copper mines in Europe and is a site of intense geological interest: there is evidence for ancient black smokers, which existed 480–360 M years BP at the site of Parys Mt [19]. During a volcanic eruption at the end of Silurian, sulfidic minerals composed mostly of copper, but also iron, lead and zinc formed large ore deposits [20]. These ores were mined for copper from the early Bronze Age until 1900 when all commercial mining ceased. Currently, the site is characterised by open casts with an underground system of AMD streams and man-made channels. Significant research has previously been conducted to investigate microorganisms and their communities associated with this site, which has resulted in a number of new bacterial species being isolated and described and a few PCR-based studies using terminal restriction fragment length polymorphism (T-RFLP) fingerprinting and 16S rRNA gene amplicon libraries [18, 21, 22]. Only a minor proportion of archaeal signatures affiliated with Euryarchaeota were detected in low pH subterranean water and in acidic streamer of Dyffryn Adda on Parys Mt, characterised by 8–9 °C in subsurface environments and air temperatures fluctuating on average between 8 and 18 °C across seasons [18, 21].

The primary goal of the present study was the analysis of prokaryotic community composition in an acidic stream, a shallow mine water flow, which originates from an open pit pond passing through the sulfidic deposits/gravel of Parys Mt. This system is different to the filamentous growth/acid streamer ecosystem within the channel Dyffryn Adda studied previously [18] but represents a free running acidic mine water flow without a characteristic red colour but with some algal growth on the surface (Additional file 1: Figure S1). Another goal of this study was attempted to cultivate archaea using sample pre-treatment and amendment with complex organic substrates to establish the taxonomic affiliation of culturable archaea.

Results and discussion

Chemical composition of sediment and water samples

Chemical analysis was performed on two types of samples, the sediment and the overlying water (Table 1, Additional file 1: Table S1). Overall, both contained high contents of iron and sulphur, respectively ca. 66.7 and 217 g/kg in sediment and 1.93 and 80.8 g/L in water sample. Al, K, Pb and Ti in the sediment and Zn, Cu, Pb and Ca for water fraction were also present in high concentrations. Total C and N values in the sediments were detected at 2.8% and 0.3% (w/w), respectively. In situ measurements for pH indicated 1.74 for both sample types. Upon arrival to laboratory, the values of pH showed a slight increase to 2.84 for the sediment and 1.90 for the aqueous fraction. The redox measured in the laboratory was found to be + 272 mV in the sediment and + 577 mV in the water sample. Electrical conductivity was found to be very high in the water sample (10.3 mS/cm). Total chemical data are shown for the particulate fraction in Table 1 and for the water fraction in Additional file 1: Table S1.

Table 1 Chemical data obtained in the samples of sediment and water of the acidic stream of Parys Mt. Values represent means ± SEM

Microbial community composition in sediment and water samples

Analysis of V3-V4 rRNA region profiling data revealed 123 significantly presented ASVs, corresponding to 12 different phyla (Fig. 1). Analysis of microbial diversity in the samples showed that while the water communities were similar between replicates, the sediment was much more heterogeneous: both alpha-diversity measures in the two sediment samples were significantly different from each other (Additional file 1: Figure S2). This is a similar finding to samples taken from the Los Rueldos mine [7], and represents the physical non-uniformity of the sediment.

Fig. 1
figure1

Abundance of SSU rRNA barcoded amplicon reads in water and sediment samples of acidic stream. Figure was performed under R programing environment using basic R packages

Sediment-associated archaea

In both analysed sediment samples, euryarchaeal class Thermoplasmata was the most abundant group constituting 31.7–65.5% of all amplicon reads. Within class Thermoplasmata, the Thermoplasmatales representatives were present in the highest abundance, with a dominance of ‘E-plasma’ reads (up to 43.5%, MH574490). The second abundant archaeon (ASV MH574492) (5.9–17.2% of total reads) was similar to the uncultured Thermoplasmatales archaeon ‘B_DKE’, previously reported in stable acidophilic enrichment of samples from a pyrite mine in the Harz Mountains, Germany [23]. The uncultured member of Thermoplasmatales (ASV MH574497), which is common in extreme acidophilic sites, was also represented constituting between 3.4 and 12.0% of total reads. The members of the latter group were detected in the abandoned mercury mine in Los Rueldos [7], those are almost equally related to Thermoplasmatales archaeon ‘A-plasma’ (94% 16S rRNA gene sequence identity) and Cuniculiplasma divulgatum (93% identity). Another novel Thermoplasmatales archaeon was detected in minor quantities (< 1.7% reads) and was represented by ASV MH57451 and is phylogenetically positioned between ‘A-plasma’ and ‘E-plasma’ (both 94% identity). Archaeal Cuniculiplasma-related taxa with cultivated representatives, earlier been isolated from this same mine site [10] were found only in minor quantities (0.2–0.5%). Small numbers of reads were also apparent for TMEG (0.2–4.5%) and for ‘Ca. Micrarchaeota’ (0.3–0.4%), which resembles the earlier reports on the low TMEG numbers in Los Rueldos acidic ecosystem [1].

Planktonic archaea

In surface water samples, archaea constituted a much lower proportion in comparison to sediment (8.1–11.7% of the total reads). ‘E-plasma’ and ‘B_DKE’ were also detected in moderate numbers (6.4–9.4% and 0.8–1.6%, respectively). Cuniculiplasma and TMEG-related reads were only present in very small quantities (0.7–0.3% and 0.2–0.08%, correspondingly) as was ‘Ca. Micrarchaeota’ (1.7–1.4%). In relation to this, an increase of the content of ‘Ca. Micrarchaeota’ organisms in water was seen, albeit their overall total representation was below 2%. The member of ‘Ca. Micrarchaeota’, namely ‘Ca. Mancarchaeum acidiphilum’ originated from this environment was reported recently to be co-cultured in vitro with Cuniculiplasma divulgatum [24].

Sediment-associated bacteria

Barcoded V3-V4 amplicon sequencing analysis revealed that sediment-associated groups encountered for 14.9–29.9% reads derived from Actinobacteria and 12.3–21.8% from Proteobacteria, the largest proportion of which was attributed to yet uncultured organisms. Other groups were found in lower quantities. Actinobacteria can constitute a large proportion of organisms in nutrient-limited environments [25]. Thus, actinobacterial species Ferrimicrobium acidiphilum was isolated from the mine site in North Wales and was described as a mesophilic heterotrophic iron oxidiser/reducer and as the predominant bacteria in Parys Mt AMD systems [18, 26]. The phylum Proteobacteria is known to include the most common acidophilic bacteria [1] accounted for 12.3–21.8% reads affiliated with γ-Proteobacteria Subgroup 1 (2.4–4.6%) and Metallibacterium spp. (family Xanthomonodaceae) (1.1–9.4%) detected alongside unclassified proteobacterial sequences, followed by Acidithiobacillales ‘cluster RCP 1-48’ (5.7–6.3%). Metallibacterium schleffleri, the cultured representative of metallibacteria, was described as acid-tolerant and organotrophic bacterium, sequences of related organisms were found to be broadly represented in mine-impacted environments being found in both biofilms and sediments [27]. Acidithiobacillales ‘cluster RCP 1-48’ was previously found to be associated with anaerobic sediments of Rio Tinto and mercury mine streamers [7, 28]. Furthermore, the reads from candidate phylum AD3 (3.6–6.2%) and Nitrospiraceae (1.6–5.8%) were also identified. Additionally, a few cyanobacterial signatures were also determined in the sediments.

Planktonic bacteria

The principal bacterial members inhabiting the water fraction were Leptospirillum spp. (Nitrospirae) (22.9–30.6% of total reads), that are renowned iron oxidising colonisers of acidic environments and are considered as the one of the most low pH-resistant bacterial species [1]. These were followed by Ferrimicrobium spp. (Actinobacteria) (11–12.2%) and other Acidimicrobiia from the same phylum. These patterns have previously been detected and reflect the predominance of Leptospirillum in mine waters and of Actinobacteria in filamentous growth matrix [18]. Similarly, the elevated presence of Thermoplasmata has been observed in sediment columns of Rio Tinto with Leptospirillum prevailing in the planktonic biomass [29].

Other important groups were Proteobacteria (19.6–22.3%) with detectable number of reads related to γ-proteobacterial genus Metallibacterium (5.9–6%), Acidithiobacillus (family Acidithiobacillaceae) (3.4–4.6%) and α-proteobacterial Acidiphilium (family Acetobacteraceae) (3.6–3.9%). Above taxa contain a number of well-studied organisms. Thus, chemolitotrophic, mesophilic, moderately thermophilic and low temperature-adapted Acidithiobacillus spp. were the first isolated acidophiles and possibly the best-studied species from acidic environments [1]; heterotrophic iron-reducing Acidiphilium are also known to be widely represented in low pH settings [1]; significant quantities of Acidobacteria (13.2–17.3%) were also revealed, mainly affiliated to a Subdivision 1 cluster. It was reported that the highest relative abundance of subdivision 1 cluster of Acidobacteria was present in ecosystems with moderately acidic pH (about 4), with the only acidobacterial species known to inhabit AMD environments being the mesophilic and obligately heterotrophic Acidobacterium capsulatum [1, 30]. Other bacterial taxa were present in only minor quantities (< 2% of the total). Interestingly, Actinobacteria, whose cultured representatives were shown to be heterotrophic, were among the most abundant bacterial counterparts in both fractions. Other groups of bacteria Acidithiobacillales, Xanthomonodales (Proteobacteria) and Chloroflexi were present in larger proportions in sediment as compared to acidic water fractions (Fig. 1).

Metagenomic sequencing of AMD microbiome

Metagenomic analysis of water interface and sediment samples revealed that the microbial community consisted of Archaea (67%) and Bacteria (33%) (Fig. 2, Additional file 1: Figure S3). Among the archaea, Euryarchaeota accounted for 64%, ‘Ca. Micrarchaeota’ for 3% and ‘Ca. Parvarchaeota’ for 0.2%, both belonging to the candidate superphylum ‘DPANN’ (‘Diaphetotrites-Parvarchaeota-Aenigmarchaeota-Nanohaloarchaeota-Nanoarchaeota’), with the rest of the archaea contributing 0.5% of total prokaryotic reads. Thermoplasmata (64% from all prokaryotes) were the most abundant within euryarchaea, the majority of the former was represented by Thermoplasmatales (62%), specifically by unclassified Thermoplasmatales (58% of total sequencing reads) and Cuniculiplasmataceae (4%). Unclassified Thermoplasmatales were affiliated mainly with ‘E-plasma’ clonal variant. A better understanding the physiology and in situ function of this group could be achieved after its successful cultivation. Phylogenetic positioning of archaeal sequences deduced by V3-V4 amplicon sequencing and metagenome shotgun sequencing is presented in Fig. 3. The indigenous Thermoplasmatales archaea showed high SSU rRNA gene sequence identities with counterparts from other acidic environments: Iron Mountain [8], Tongling AMD samples (see Accession Numbers in Fig. 3), floating macroscopic filaments from Rio Tinto [28, 31], Pb/Zn mine tailing [32] and Frasassi cave system/acidic snottite biofilm [33]. All these Thermoplasmatales-related sequences belong to organisms still evading isolation. Since the archaea of the order Thermoplasmatales are known scavengers of proteinaceous substrates from microbial biomass [5], we hypothesise that the metabolic functioning Parys Mt archaea may be considered as heterotrophic to a large extent. The substantial archaeal proportions in samples with low total C and N values (Table 1) and lesser numbers of prokaryotic primary producers (Leptospirillum sp. or Acidithiobacillus spp.) may be associated with green algae populating the surface (Chlamydomonas spp.). Accordingly, Chlamydomonas is a renowned inhabitant of AMD systems [34] and is capable of exudation of low molecular weight organic compounds [35] that can further be utilised by other members of the microbial consortia. Altogether, these archaea, due to their elevated numbers, can be considered as significant contributors to the community functioning and to elemental cycling (carbon and probably iron) in this low-temperature ecosystem. Another factor favouring the elevated numbers of Thermoplasmatales is the high acidity of this environment. Preliminary analysis of the Parys Mt. microbial community showed that a large number (almost 57%) of total Illumina reads, resulting from shotgun sequencing of Parys Mt metagenome, were related to Thermoplasmatales archaea [24].

Fig. 2
figure2

Taxonomic classification of microbial community from metagenomic DNA sequencing data. Taxonomic classification was obtained using 1GraftM, classifying short reads belonging to marker genes from metagenomic datasets. Graphical representation was performed under R programing environment using basic R packages. https://github.com/geronimp/graftM (This program does not have a publication yet, but they suggest to cite their github page)

Fig. 3
figure3

16S rRNA gene sequence-based phylogenetic reconstruction of Thermoplasmatales clones from Parys Mt samples obtained in the course of this work. V3-V4 hypervariable region amplicon sequences and sequences extracted from metagenome contigs are highlighted by green. Number of amplified sequence variants, corresponding to each branch indicated in brackets. Reference sequences (brown) were taken from the Silva SSU 132 Ref NR 99 database (see the methods section). ‘Plus’ sign denotes presence of corresponding sequences in 16S V3-V4 amplicon, environmental and enrichment metagenomes

Bacteria (33% of the total prokaryotic reads) showed affiliation to Proteobacteria (11%), with γ-Proteobacteria (8%) and α-Proteobacteria (2%) being the major classes. The closest γ-proteobacterial reads were similar to Xanthomonodaceae, with a significant number of Lysobacter spp. (2% of all prokaryotic and 7% of all bacterial reads). These microorganisms inhabit neutral soil and freshwater environments and are known to be a rich source of antibiotics [36]. α-Proteobacterial sequences (2% from total reads) were affiliated with Rhodospirillales with other groups present in minor numbers. Representatives of Rhodospirillales (Acidiphilium spp., Acidicaldus organivorans, Acidocella spp. and Acidisphaera spp.) are known acidophilic heterotrophic bacteria able to use exudates and lysates from primary producers and were detected previously at Parys Mt site Dyffryn Adda streamers [18]. Other bacterial phyla were identified as Actinobacteria (6%), Nitrospirae (4%), Bacteroidetes (3%), Acidobacteria (2%), Firmicutes (2%) and others, present in minor proportions. Acidithiobacillales were represented in lesser quantities (0.3%). Unassigned bacterial sequences comprised 13% of total bacterial reads. The Shannon and Simpson diversity indices were calculated as 1.97 and 0.64, respectively (Additional file 1: Figure S3).

Earlier studies of Parys Mt sites using PCR-based methods revealed the dominance of bacteria with only a minor presence of archaea [22]. In addition, analysis of the Parys Mt Dyffryn Adda AMD community proposed that Acidithiobacillus ferrivorans (order Acidithiobacillales), ‘Ferrovum myxofaciens’ (Proteobacteria) and Acidithrix ferrooxidans (Actinobacteria) were the dominant bacteria in this environment [18]. The ratios of bacteria to archaea have not been assessed in the study; however, archaeal sequences were distantly related to cultured members of Euryarchaeota and were much less diverse than bacteria. In addition, the authors concluded that the presence of archaea in other North Wales acidic mine sites is low [18]. In that context, our results found archaea to be in the clear majority. We suggest that this disparity between different studies may be connected with general limitation of PCR-based methods used and the different physico-chemical conditions in both sites, including higher pH values in Dyffryn Adda streamers (2.5 vs 1.8), notable increase in Eh (+ 669 vs + 577 and + 272) and significantly low concentrations of metals [18].

TMEG and Methanomassilicoccales-related archaea

Additionally, 2% of the sequences were identified as TMEG-related (Thermoplasmata). The phylogenetic position of TMEG-related sequences suggested this group had Methanomassiliicoccus luminyensis strain B10 as the nearest cultured representative with the 16S rRNA gene sequence identity of 83% (Fig. 4, Additional file 2: Table S2). The phylogenetic tree (Fig. 4) clearly shows clustering of Parys Mt TMEG-related reads with other clones identified in acidic and moderately acidic environments discriminative to sequences from other places.

Fig. 4
figure4

16S rRNA gene sequence-based phylogenetic relationships of microorganisms from the Terrestrial Miscellaneous Euryarchaeotal Group (TMEG). The tree was constructed using a total of 82 16S rRNA sequences that were assigned and documented in the literature to TMEG, including the clone described in this research (referred as PM clone) and two sequences from Methanosarcina sp. and Methanomassiliicoccus luminyensis, respectively. Environmental pH is shown by coloured dots from acidic (purple) to neutral-low basic (green). Sequences from environments with unknown pH are shown in black. Two distinct clusters of sequences can be identified, corresponding to sequences from acidic (red cluster) and non-acidic environments (green cluster). The list of analysed sequences is presented in the Additional file 2: Table S2 ‘TMEG Data’

These archaea are considered to be minor constituents of the communities, but were shown to be more associated with sediment rather than with the water fraction in this particular environment. Recent metagenomic studies indicated that this group might be linked to anoxic sulfate- and methane-containing settings. For instance, it was revealed that the highest number of clones associated with TMEG was detected in sediments with low amounts of SO42− (2 mM) and moderate concentrations of CH4 (3.5 mM) [37]. Another study [38] reported on the presence of TMEG in methane hydrate-bearing sediments of freshwater Baikal Lake comprising ca. 15% of the total microbial community in an upper level and at about 10% in sediments. Interestingly, the athalassohaline inland aquatic system, Salar de Huasco, located in the Chilean Altiplano and characterised by low temperatures showed a predominance of this group in a water sample with the highest sulfate concentration (40 mM) [39]. Thus, the physiology and functions of TMEG group still remain completely unexplored either in aquatic environments or sediments [40]. It was predicted that they have a potential to undertake fatty acid oxidation and anaerobic respiration via reduction of sulphite and/or sulfonate (bin Bg1) [41]. In relation to TMEG, an important point was recently made about a strong phylogenetic separation of gut-associated and free-living clades of Methanomassilicoccales-related archaea [42]. Furthermore, it was noted that the latter ‘environmental clade’ of Methanomassilicoccales was previously assigned to TMEG [43]. We detected the presence of 16S rRNA gene sequences with the identity of about 81–83% to those of M. luminyensis in sediments of the stream of Parys Mt in barcoded 16S rRNA gene amplicon sequences (V3-V4 region) and by shotgun metagenomic sequencing. Almost identical to Parys Mt sediment, TMEG-derived SSU rRNA gene sequences were earlier detected in La Zarza, Perrunal acid mine effluent (Iberian Pyritic Belt, Spain, HM745465 [44], Rio-Tinto, DQ303248 [31], terrestrial acidic spring AB600345 [45] and many other acidic or slightly acidic environments [7, 46, 47]). In some cases, the affiliation of these sequences to the order Thermoplasmatales has been erroneously considered. Our analysis pointed at a compact co-clustering of TMEG-related sequences from a wide range of acidic and moderately acidic ecosystems that were very distinct from the cluster of their counterparts from neutral environments. These acidophilic/acidotolerant TMEG archaea form a group on the level of a new order within Thermoplasmata, and are only distantly related to M. luminyensis. T-RFLP and clone library analyses conducted earlier identified similar organisms in other Parys Mt settings: in impounded water (corresponding microorganisms were referred as a ‘methanogens’) [21] and in filamentous growth streamers in the Dyffryn Adda mine adit [18]. The presence of a group of rRNA gene sequences with about 80% identity to M. luminyensis was also mentioned in a study of arsenic-rich creek sediments of Carnoulès Mine, France [48], in Los Rueldos acidic streamers ( [7] and elsewhere).

Enrichment cultures

An attempt to enrich and isolate archaea from this environment was undertaken. For this, we applied various treatments of samples, followed by enrichment and consequent shotgun sequencing of these variants (see ‘Methods’ section). After 25 days of cultivation of enriched samples (NN 4 and 5), certain diversification between variants was observed (Fig. 5). The EP culture containing sediment matrix was dominated by Ferrimicrobium acidiphilum, showing 99% 16S rRNA nucleotide identity with Fm. acidiphilum strain T23T previously isolated from the Cae Coch sulphur mine [26]. Archaea were represented by Cuniculiplasma divulgatum and ‘Ca. Mancarchaeum acidiphilum Mia14’, corresponding to 14.4% and 2.3% of classified metagenomic reads, respectively.

Fig. 5
figure5

Abundance of archaea and bacteria according to the results of metagenomic sequencing of DNA isolated from enrichment cultures with differential pre-processing methods (samples EP, ES and EF). Proportion of classified (pink) vs. unclassified (light green) reads is shown by small pie-charts on top right corner of each bar

The ES culture was established using the supernatant of the above centrifugate as an inoculum to reduce the numbers of large algal cells and solid particulate matter. Upon incubation, Fm. acidiphilum was the predominant organism with a lower abundance of Cuniculiplasmataceae than in EP culture. Nevertheless, ES culture was significantly more diverse than EP. Small numbers or ‘Ca. Micrarchaeota’-related reads, with 16S rRNA gene sequence almost identical to that of ‘A_DKE’ organism from the enrichment culture of ‘Drei Kronen und Ehrt’ pyrite mine microbial consortium [23] and ‘Ca. Mancarchaeum acidiphilum’ Mia14, corresponding to 0.4% and 0.9% of classified metagenomic reads, respectively, were detected. Minor bacterial taxa were represented by uncultivated species of Leptospirillum (0.6%) and Aciditerrimonas (1.3%). Closest 16S rRNA gene sequences for the latter were reported in clones from acid mine effluent of La Zarza, Perrunal mine located in the Iberian Pyritic Belt [44].

Finally, an enrichment culture (EF) was set up using the filtrate which had passed through a 0.45 μm pore membrane. This was used as an inoculum but required a longer cultivation time (45 days). It showed a predominance of C. divulgatum with only a minor fraction of bacteria (0.7%) of Leptospirillum and Ferrimicrobium spp. In contrast to the other enrichment cultures, no ‘Ca. Micrarchaeota’ signatures were detected in the EF culture. However, one needs to consider that similar culturing conditions have been previously optimised for Cuniculiplasma divulgatum [9] and may be less favourable to other Parys Mt archaea.

Conclusions

Our metagenomic and metabarcoding amplicon sequencing analyses have unambiguously pointed at the predominance of archaea in the low-to-moderate temperature environment of Parys Mt, in contrast to earlier considerations of the prevalence of bacteria in such environments. One particular group of uncultured Thermoplasmatales, dubbed ‘E-plasma’ was present in a clear majority. The overwhelming archaeal numbers in this natural acidic microbiome implies their pivotal functional and ecological role in the community. Our sample pre-treatment and cultivation attempts were successful in obtaining enrichment cultures with very high proportion of Cuniculiplasma spp., which, however were represented in natural samples as a minor component. An important finding is related to the TMEG archaeal group previously overlooked in acidophilic communities. Our analysis showed their presence in the microbial community of Parys Mt and suggested that at a global scale, there is a strong phylogenetic clustering of TMEG sequences from the low pH settings that form a separate clade at the level of the Order within Thermoplasmata. Considering the majority of microbiome constituents were represented by yet uncultured organisms, this environment is a good resource for isolation of apparent new archaeal taxa within the order Thermoplasmatales and class Thermoplasmata. Its exploration may also further expand the list of highly ranked taxa previously unknown to accommodate acidophilic members.

Methods

Sample collection and DNA extraction

Samples were collected from the surface layer (1–3 cm depth) of the water-saturated sediments of an acidic stream located in Parys Mt (North Wales, UK, 53° 23′ 13.6′′ 4° 20′ 58.6′′ W) in October, 2014. These samples were used for (1) bulk native DNA extraction for the metagenomic sequencing and SSU rRNA gene (full-length) PCR amplification (sample designated as ‘PM Mona’), and (2) for setting up enrichment cultures and consequent DNA extraction from these enrichments. Additional sampling was conducted at the same site in October 2016 (water and sediment as separate fractions taken from closely located spots) for barcoded amplicon sequencing. Water samples were filtered through Millipore Sterivex GV 0.2 μm syringe filters to recover the microbial biomass.

For enrichment cultures, the modified Medium DSMZ 88 (https://www.dsmz.de/microorganisms/medium/pdf/DSMZ_Medium88.pdf) was used [9]. The media was supplemented with Bacto™ beef extract, tryptone and casamino acids (BD Biosciences, Wokingham, UK), with each compound at a final concentration of 1 g l−1. For enrichment cultures, samples taken in October 2014 underwent three different treatments. Brief (5 s) vortexing and centrifugation at a low speed (10 min at 250 RCF) with subsequent (i) use of the pellet as the inoculum (‘enrichment from pellet’, EP), and (ii) collecting and using the supernatant produced above as the inoculum (‘enrichment from supernatant’, ES). Finally, (iii) the supernatant fraction (ES), which passed through the Millipore Sterivex GV 0.45 μm syringe membrane, was used as the inoculum for another enrichment culture (‘enrichment from filtrate’, EF).

The DNA from all samples was extracted using a MoBio PowerSoil® DNA Isolation Kit (Qiagen, Germany).

Chemical analysis

The sediment samples were sieved to pass 2 mm and the stones (> 2 mm) retained, weighed and their volume calculated using a density value of 2.65 g cm−3. The water content of the sediment was determined by oven drying (105 °C, 24 h). Water- and air-filled porosity were calculated according to [49]. Total C and N were analysed with a Truspec® CN analyser (Leco Corp., St Joseph, MI). Metals in the samples were analysed using a S2 PicoFox TXRF Spectrometer (Bruker AXS Inc., Madison, WI). Electrical conductivity and pH were measured with standard electrodes. Soil redox potential was determined using a SenTix® probe (WTW Wissenschaftlich-Technische Werkstätten GmbH, Weilheim, Germany). The water samples were evaporated to dryness and the particulate fraction recovered and analysed as described above.

Shotgun sequencing and analysis of Parys Mt metagenome

Shotgun metagenomic libraries were prepared from (i) environmental DNA extracted from samples taken in October 2014 (see Sample collection and DNA extraction), and (ii) genomic DNA extracted from enrichment cultures EF, ES and EP. DNA was fragmented using a Bioruptor sonicator (Diagenode, Belgium) to achieve an average fragment length of 500–700 bp. Further steps of library preparation were accomplished using NebNext® Ultra™ DNA Library prep kit for Illumina® according to the manufacturer’s instructions. Sequencing was performed on Illumina MiSeq™ platform using 500-cycles reagent kit. Then, 18.27, 1.88, 4.18 and 8.38 millions of read pairs were obtained for samples PM Mona, EP, ES and EF, respectively.

Quality trimming and filtering of reads was performed with CLC Genomics Workbench 9.5 (Qiagen, Germany) while overlapping reads were merged with the SeqPrep tool (https://github.com/jstjohn/SeqPrep/). Metagenomic assembly was performed using SPAdes (v. 3.10) without a read error correction step [50]. The resulting contigs were used only for the extraction of sequences of phylogenetic markers.

Community composition analysis of environmental metagenome (sample PM.Mona) was performed using raw sequencing reads, graftM package ver 0.11.1 [51] provided rpsB reference database, extended with sequences of Cuniculiplasma divulgatum PM4 (GCA_900090055.1), Thermoplasmatales archaea ‘A-plasma’ (GCA_000447225.1), ‘E-plasma’ (GCA_000496135.1), ‘I-plasma’ (GCA_001856825.1), ‘Candidatus Methanoplasma termitum’ (GCA_000800805.1), ‘Ca. Micrarchaeum’ sp. AZ1 (GCA_001896515.1), ‘Ca. Mancarchaeum acidiphilum’ (GCA_002214165.1), ‘Ca. Parvarchaeum acidiphilum’ ARMAN-4 (GCA_002412065.1), ‘Ca. Parvarchaeum acidophilus’ ARMAN-5 (GCA_002412085.1) as well as rpsB sequences from metagenomic bins related to TMEG-group and ‘Ca. Micrarchaeota’. Due to the distinct phylogenetic position of members of Parys Mt extremely acidophilic microbial community, and therefore the high possibility of wrong taxonomic affiliation, the reference database was extended by rpsB sequences, identified in our shotgun metagenomic assembly. All resulting sequencing were aligned and used to build an HMM model for the search step of graftM.

Sequences obtained from less diverse communities of enrichment cultures were analysed by CLARK k-mer-based sequence classification system [52]. In the first step, 16S and 23S were extracted using barrnap tool (https://github.com/tseemann/barrnap). All sequences were then aligned using blastn algorithm against refseq genomes, wgs and HTGS NCBI databases. The nearest genomic contigs were used as references for the creation of CLARK database. In the second step, preliminary metagenomic contigs, assembled with SPAdes, were classified with CLARK against NCBI-derived reference database (kmer = 32 was used for better reliability). After that step, CLARK reference database was complemented by reliably classified contigs. Finally, resulting database was used for the final classification of shotgun metagenomic reads (kmer = 22 was used for better reliability).

16S rRNA V3-V4 amplicon sequencing

Metabarcoding libraries of 16S rRNA amplicons corresponding to V3-V4 variable region were prepared by single PCR with double-indexed fusion primers as described by [53]. 16S rRNA annealing part of forward primers corresponded to Pro341F (CCTACGGGNBGCASCAG) primer described in [54]; reverse primers corresponded to modified R806 prokaryotic primer (GGACTACHVGGGTWTCTAAT) [55]. PCR amplification of 16S rRNA genes was performed by qPCRmix-HS™ SYBR mastermix (Evrogen, Russia) using the following conditions: 30 cycles of denaturation at 95 °C for 15 s; primer annealing at 58 °C, 15 s; DNA synthesis at 72 °C, 25 s, followed by final incubation for 5 min at 72 °C. Purification of PCR products was done using the Cleanup Mini kit (Evrogen, Russia). The quality of the final libraries was assessed using the electrophoresis in agarose gel.

Libraries were sequenced with MiSeq™ Personal Sequencing System technology of Illumina Inc. (San Diego, CA, USA) using paired-end 250-bp reads. Demultiplexing was performed as described previously [53]. After demultiplexing, all reads were subjected to stringent quality filtering, and parts of reads, corresponding to 16S rRNA primers were removed using CLC Genomics Workbench 10.0 (Qiagen, Germany). At the end, 18–22 thousand of reads were used for each analysed sample.

The resulting demultiplexed paired sequenced files for each sample were used as an input for the DADA2 high-resolution 16S amplicon analysis package [56] according to the standard pipeline published on DADA2 web page (https://benjjneb.github.io/dada2/index.html). As a result, 384 individual amplified sequenced variants (ASVs) were produced, while only 123 ASVs were represented by 10 or more reads in all samples analysed. Taxonomic classification of resulting ASVs was performed by Bayesian classification algorithm [57] built in DADA2 package against the Silva132 database [58]. Visualisation of data and calculation of alpha diversity metrics was performed using the R phyloseq package [59].

16S rRNA phylogenetic analysis

SSU rRNA gene sequence phylogenetic analysis for TMEG group was performed as described previously [9]. Briefly, a set of 16S rRNA nucleotide sequences assigned in the literature as related to TMEG-group were selected and aligned using Muscle algorithm [60]. Phylogenetic analysis was performed in MEGA6 Program [61] using the Maximum Likelihood method with 1000 repetitions bootstraps [62]. The general time-reversible model (GTR, G + I, four categories) [63] was used for inferring the evolutionary distances. The trees are drawn to scale, with branch lengths measured in the number of substitutions per site with corrections, associated with the model. All positions with less than 80% site coverage were eliminated. There were a total of 82 nucleotide sequences and 747 positions, involved in the calculations. The tree was displayed in packages ape [64] and phangorn [65] in the R programing environment.

Phylogenetic analysis for SSU rRNA genes sequences from barcode libraries and that extracted from the metagenomic sequences were performed using ARB-parsimony tool [66]. Briefly, all 16S rRNA gene sequences of V3-V4 fragments as well as that extracted from all four metagenomes (PM.Mona, EP, ES and EF) were added to the Silva SSU 132 Ref NR 99 arb file (including an alignment and a tree, https://www.arb-silva.de/download/arb-files/) where they have been co-aligned and placed on the Silva SSU 132 Ref NR 99 tree using the ARB-parsimony tool [66].

References

  1. 1.

    Mendez-Garcia C, Pelaez AI, Mesa V, Sanchez J, Golyshina OV, Ferrer M. Microbial diversity and metabolic networks in acid mine drainage habitats. Front Microbiol. 2015;6:475.

  2. 2.

    Chen LX, Huang LN, Méndez-García C, Kuang JL, Hua ZS, Liu J, Shu WS. Microbial communities, processes and functions in acid mine drainage ecosystems. Curr Opin Biotechnol. 2016;38:150–8.

  3. 3.

    García-Moyano A, Austnes AE, Lanzén A, González-Toril E, Aguilera Á, Øvreås L. Novel and unexpected microbial diversity in acid mine drainage in Svalbard (78°N), revealed by culture-independent approaches. Microorganisms. 2015;3(4):667–94.

  4. 4.

    Golyshina OV, Pivovarova TA, Karavaiko GI, Kondratéva TF, Moore ER, Abraham WR, et al. Ferroplasma acidiphilum gen. nov., sp. nov., an acidophilic, autotrophic, ferrous-iron-oxidizing, cell-wall-lacking, mesophilic member of the Ferroplasmaceae fam. nov., comprising a distinct lineage of the archaea. Int J Syst Evol Microbiol. 2000;50(3):997–1006.

  5. 5.

    Golyshina OV. Environmental, biogeographic, and biochemical patterns of archaea of the family Ferroplasmaceae. Appl Environ Microbiol. 2011;77:5071–8.

  6. 6.

    Yelton AP, Comolli LR, Justice NB, Castelle C, Denef VJ, Thomas BC, Banfield JF. Comparative genomics in acid mine drainage biofilm communities reveals metabolic and structural differentiation of co-occurring archaea. BMC Genomics. 2013;14:485.

  7. 7.

    Méndez-García C, Mesa V, Sprenger RR, Richter M, Diez MS, Solano J, et al. Microbial stratification in low pH oxic and suboxic macroscopic growths along an acid mine drainage. ISME J. 2014;6:1259–74.

  8. 8.

    Baker BJ, Banfield JF. Microbial communities in acid mine drainage. FEMS Microbiol Ecol. 2003;44:139–52.

  9. 9.

    Golyshina OV, Lünsdorf H, Kublanov IV, Goldenstein NI, Hinrichs KU, Golyshin PN. The novel extremely acidophilic, cell-wall-deficient archaeon Cuniculiplasma divulgatum gen. nov., sp. nov. represents a new family, Cuniculiplasmataceae fam. nov., of the order Thermoplasmatales. Int J Syst Evol Microbiol. 2016;66(1):332–40.

  10. 10.

    Golyshina OV, Kublanov IV, Tran H, Korzhenkov AA, Lünsdorf H, Nechitaylo TY, et al. Biology of archaea from a novel family Cuniculiplasmataceae (Thermoplasmata) ubiquitous in hyperacidic environments. Sci Rep. 2016;6:39034.

  11. 11.

    Hallberg KB, Coupland K, Kimura S, Johnson DB. Macroscopic streamer growths in acidic, metal-rich mine waters in north wales consist of novel and remarkably simple bacterial communities. Appl Environ Microbiol. 2006;72(3):2022–30.

  12. 12.

    Quatrini R, Johnson DB. Microbiomes in extremely acidic environments: functionalities and interactions that allow survival and growth of prokaryotes at low pH. Curr Opin Microbiol. 2018;43:139–47.

  13. 13.

    Kuang J, Huang LN, Chen LX, Hua ZS, Li SJ, Hu M, et al. Contemporary environmental variation determines microbial diversity patterns in acid mine drainage. ISME J. 2013;7:1038–50.

  14. 14.

    Justice NB, Pan C, Mueller R, Spaulding SE, Shah V, Sun CL, et al. Heterotrophic archaea contribute to carbon cycling in low-pH, suboxic biofilm communities. Appl Environ Microbiol. 2012;78:8321–30.

  15. 15.

    Chen LX, Hu X, Huang LN, Hua ZS, Kuang JL, Li SJ, Shu WS. Comparative metagenomic and metatranscriptomic analyses of microbial communities in acid mine drainage. ISME J. 2015;9:1579–92.

  16. 16.

    Chen LX, Li JT, Chen YT, Huang LN, Hua ZS, Hu M, Shu WS. Shifts in microbial community composition and function in the acidification of a lead/zinc mine tailings. Environ Microbiol. 2013;15:2431–44.

  17. 17.

    Huang LN, Zhou WH, Hallberg KB, Wan CY, Li J, Shu WS. Spatial and temporal analysis of the microbial community in the tailings of a Pb-Zn mine generating acidic drainage. Appl Environ Microbiol. 2011;77:5540–4.

  18. 18.

    Kay CM, Rowe OF, Roccheti L, Coupland K, Hallberg K, Johnson DB. Evolution of microbial “streamer” growths in an acidic, metal-contaminated stream draining an abandoned underground copper mine. Life. 2013;3(1):189–210.

  19. 19.

    Pointon CR, Ixer RA. Parys Mountain mineral deposit, Anglesey, Wales: geology and ore mineralogy. Trans. Inst. Mining Metallurgy (section B: Appl Earth Sci). 1980;89:B143–55.

  20. 20.

    North FJ. Mining for metals in Wales. Cardiff: National Museum of Wales; 1962.

  21. 21.

    Coupland K, Johnson DB. Geochemistry and microbiology of an impounded subterranean acidic water body at Mynydd Parys, Anglesey, Wales. Geobiology. 2004;2:77–86.

  22. 22.

    Johnson DB. Geomicrobiology of extremely acidic subsurface environments. FEMS Microbiol Ecol. 2012;81(1):2–12.

  23. 23.

    Krause S, Bremges A, Munch PC, McHardy AC, Gescher J. Characterisation of a stable laboratory co-culture of acidophilic nanoorganisms. Sci Rep. 2017;7(1):3289.

  24. 24.

    Golyshina OV, Toshchakov SV, Makarova KS, Gavrilov SN, Korzhenkov AA, La Cono V, et al. “ARMAN” archaea depend on association with euryarchaeal host in culture and in situ. Nat Commun. 2017;8:60.

  25. 25.

    Hoskisson PA, Fernández-Martínez LT. Regulation of specialised metabolites in Actinobacteria—expanding the paradigms. Environ Microbiol Rep. 2018;10(3):231–8.

  26. 26.

    Johnson DB, Bacelar-Nicolau P, Okibe N, Thomas A, Hallberg KB. Ferrimicrobium acidiphilum gen. nov., sp. nov. and Ferrithrix thermotolerans gen. Nov., sp. nov.: heterotrophic, iron-oxidizing, extremely acidophilic actinobacteria. Int J Syst Evol Microbiol. 2009;59:1082–8.

  27. 27.

    Bartsch S, Gensch A, Stephan S, Doetsch A, Gescher J. Metallibacterium scheffleri: genomic data reveal a versatile metabolism. FEMS Microbiol Ecol. 2017;93(3):fix011.

  28. 28.

    Sánchez-Andrea I, Rodríguez N, Amils R, Sanz JL. Microbial diversity in anaerobic sediments at Rio Tinto, a naturally acidic environment with a high heavy metal content. Appl Environ Microbiol. 2011;77:6085–93.

  29. 29.

    García-Moyano A, González-Toril E, Aguilera A, Amils R. Comparative microbial ecology study of the sediments and the water column of the Río Tinto, an extreme acidic environment. FEMS Microbiol Ecol. 2012;81(2):303–14.

  30. 30.

    Belova SE, Ravin NV, Pankratov TA, Rakitin AL, Ivanova AA, Beletsky AV, Mardanov AV, Sinninghe Damsté JS, Dedysh SN. Hydrolytic capabilities as a key to environmental success: chitinolytic and cellulolytic Acidobacteria from acidic sub-arctic soils and boreal peatlands. Front Microbiol. 2018;9:2775.

  31. 31.

    García-Moyano A, González-Toril E, Aguilera A, Amils R. Prokaryotic community composition and ecology of floating macroscopic filaments from an extreme acidic environment, Río Tinto (SW, Spain). Syst Appl Microbiol. 2007;8:601–14.

  32. 32.

    Tan GL, Shu WS, Hallberg KB, Li F, Lan CY, Zhou WH, et al. Culturable and molecular phylogenetic diversity of microorganisms in an open-dumped, extremely acidic Pb/Zn mine tailings. Extremophiles. 2008;12:657–64. Available from: http://www.ncbi.nlm.nih.gov/pubmed/18512002.

  33. 33.

    Jones DS, Albrecht HL, Dawson KS, Schaperdoth I, Freeman KH, Pi Y, et al. Community genomic analysis of an extremely acidophilic sulfur-oxidizing biofilm. ISME J. 2012;6:158–70.

  34. 34.

    Gyure RA, Konopka A, Brooks A, Doemel W. Algal and bacterial activities in acidic (pH 3) strip mine lakes. Appl Environ Microbiol. 1987;53(9):2069–76.

  35. 35.

    Tittel J, Bissinger V, Gaedke U, Kamjunke N. Inorganic carbon limitation and mixotrophic growth in Chlamydomonas from an acidic mining lake. Protist. 2005;156(1):63–75.

  36. 36.

    Panthee S, Hamamoto H, Paudel A, Sekimizu K. Lysobacter species: a potential source of novel antibiotics. Arch Microbiol. 2016;198(9):839–45.

  37. 37.

    Li Q, Wang F, Chen Z, Yin X, Xiao X. Stratified active archaeal communities in the sediments of Jiulong River estuary, China. Front Microbiol. 2012;3:311.

  38. 38.

    Kadnikov VV, Mardanov AV, Beletsky AV, Shubenkova OV, Pogodaeva TV, Zemskaya TI, et al. Microbial community structure in methane hydrate-bearing sediments of freshwater Lake Baikal. FEMS Microbiol Ecol. 2012;79:348–58.

  39. 39.

    Dorador C, Vila I, Remoncellez F, Imhoff JF, Witzel K-P. Unique clusters of Archaea in Salar de Huasco, an athalassohaline evaporitic basin of the Chilean Altiplano. FEMS Microbiol Ecol. 2010;73:291–302.

  40. 40.

    Fillol M, Auguet J-C, Casamayor EO, Borrego CM. Insights in the ecology and evolutionary history of the miscellaneous Crenarchaeotic group lineage. ISME J. 2015;10:665–77.

  41. 41.

    Lin X, Handley KM, Gilbert JA, Kostka JE. Metabolic potential of fatty acid oxidation and anaerobic respiration by abundant members of Thaumarchaeota and Thermoplasmata in deep anoxic peat. ISMEJ. 2015;29:2740–4.

  42. 42.

    Söllinger A, Schwab C, Weinmaier T, Loy A, Tveit AT, Schleper C, Urich T. Phylogenetic and genomic analysis of Methanomassiliicoccales in wetlands and animal intestinal tracts reveals clade-specific habitat preferences. FEMS Microbiol Ecol. 2016;92(1):fiv149.

  43. 43.

    Becker KW, Elling FJ, Yoshinaga MY, Söllinger A, Urich T, Hinrichs K-U. Unusual butane- and pentanetriol-based tetraether lipids in Methanomassiliicoccus luminyensis, a representative of the seventh order of methanogens. Appl Environ Microbiol. 2016;82:4505–16.

  44. 44.

    González-Toril E, Aguilera A, Souza-Egipsy V, López Pamo E, Sánchez España J, Amils R. Geomicrobiology of La Zarza-Perrunal acid mine effluent (Iberian Pyritic Belt, Spain). Appl Environ Microbiol. 2011;77(8):2685–94.

  45. 45.

    Kato S, Itoh T, Yamagishi A. Archaeal diversity in a terrestrial acidic spring field revealed by a novel PCR primer targeting archaeal 16S rRNA genes. FEMS Microbiol Lett. 2011;319(1):34–43.

  46. 46.

    Urbieta MS, González-Toril E, Bazán ÁA, Giaveno MA, Donati E. Comparison of the microbial communities of hot springs waters and the microbial biofilms in the acidic geothermal area of Copahue (Neuquén, Argentina). Extremophiles. 2015;19:437–50.

  47. 47.

    Qiu GZ, Wan MX, Qian L, Huang ZY, Liu K, Liu XD, Shi WY, Yang Y. Archaeal diversity in acid mine drainage from Dabaoshan mine, China. J Basic Microbiol. 2008;48(5):401–9.

  48. 48.

    Volant A, Desoeuvre A, Casiot C, Lauga B, Delpoux S, Morin G, et al. Archaeal diversity: temporal variation in the arsenic-rich creek sediments of Carnoulès mine, France. Extremophiles. 2012;16:645–57.

  49. 49.

    Soil Science RDL. Methods and Applications. Harlow: Prentice Hall; 1994.

  50. 50.

    Bankevich A, Nurk S, Antipov D, Gurevich AA, Dvorkin M, Kulikov AS, et al. SPAdes: a new genome assembly algorithm and its applications to single-cell sequencing. J Comput Biol. 2012;19(5):455–77.

  51. 51.

    Boyd JA, Woodcroft BJ, Tyson GW. GraftM: a tool for scalable, phylogenetically informed classification of genes within metagenomes. Nucleic Acids Res. 2018;46(10):e59.

  52. 52.

    Ounit R, Wanamaker S, Close TJ, Lonardi S. CLARK: fast and accurate classification of metagenomic and genomic sequences using discriminative k-mers. BMC Genomics. 2015;16:236.

  53. 53.

    Fadrosh DW, Ma B, Gajer P, Sengamalay N, Ott S, Brotman RM, Ravel J. An improved dual-indexing approach for multiplexed 16S rRNA gene sequencing on the Illumina MiSeq platform. Microbiome. 2014;2(1):6.

  54. 54.

    Takahashi S, Tomita J, Nishioka K, Hisada T, Nishijima M. Development of a prokaryotic universal primer for simultaneous analysis of Bacteria and and archaea using next-generation sequencing. PLoS One. 2014;9(8):e105592.

  55. 55.

    Kublanov IV, Perevalova AA, Slobodkina GB, Lebedinsky AV, Bidzhieva SK, Kolganova TV, et al. Biodiversity of thermophilic prokaryotes with hydrolytic activities in hot springs of Uzon caldera, Kamchatka (Russia). Appl Environ Microbiol. 2009;75(1):286–91.

  56. 56.

    Callahan BJ, McMurdie PJ, Rosen MJ, Han AW, Johnson AJ, Holmes SP. DADA2 high-resolution sample inference from Illumina amplicon data. Nat Methods. 2016;13(7):581–3.

  57. 57.

    Wang Q, Garrity GM, Tiedje JM, Cole JR. Naive Bayesian classifier for rapid assignment of rRNA sequences into the new bacterial taxonomy. Appl Environ Microbiol. 2007;73(16):5261–7.

  58. 58.

    Quast C, Pruesse E, Yilmaz P, Gerken J, Schweer T, Yarza P, et al. The SILVA ribosomal RNA gene database project: improved data processing and web-based tools. Nucleic Acids Res. 2013;41:D590–6.

  59. 59.

    McMurdie PJ, Holmes S. Phyloseq: an R package for reproducible interactive analysis and graphics of microbiome census data. PLoS One. 2013;8(4):e61217.

  60. 60.

    Edgar RC. MUSCLE: multiple sequence alignment with high accuracy and high throughput. Nucleic Acids Res. 2004;32:1792–7.

  61. 61.

    Tamura K, Stecher G, Peterson D, Filipski A, Kumar S. MEGA6: molecular evolutionary genetics analysis version 6.0. Mol Biol Evol. 2013;30:2725–9.

  62. 62.

    Felsenstein J. Confidence limits on phylogenies: an approach using the bootstrap. Evolution. 1985;39:783–91.

  63. 63.

    Nei M, Kumar S. Molecular evolution and Phylogenetics. New York: Oxford University Press; 2000.

  64. 64.

    Paradis E, Claude J, Strimmer KA. APE: analyses of phylogenetics and evolution in R language. Bioinformatics. 2004;20:289–90.

  65. 65.

    Schliep KP. Phangorn: phylogenetic analysis in R. Bioinformatics. 2011;27(4):592–3.

  66. 66.

    Westram R, Bader K, Prüsse E, Kumar Y, Meier H, Glöckner FO, et al. ARB: A Software Environment for Sequence Data. Handb Mol Microb Ecol I. Hoboken: Wiley; 2011. p. 399–406.

Download references

Acknowledgements

The work of OVG, PNG and SVT was supported by the Royal Society UK-Russia Exchange Grant #IE 160224 (RFBR 16-54-10072 КО project). OVG and PNG acknowledge ERA Net IB2 Project MetaCat through UK Biotechnology and Biological Sciences Research Council (BBSRC) Grant BB/M029085/1 and the support of the Centre of Environmental Biotechnology Project funded by the European Regional Development Fund (ERDF) through the Welsh Government. RB and PNG acknowledge the support of the Supercomputing Wales project, which is part-funded by the European Regional Development Fund (ERDF) via the Welsh Government. The work of AAK and IVK was supported by the Russian Science Foundation grant # 18-44-04024. MF acknowledges grants PCIN-2014-107 (within ERA NET IB2 grant ERA-IB-14-030—MetaCat), PCIN-2017-078 (within the Marine Biotechnology ERA-NET (ERA-MBT) funded under the European Commission’s Seventh Framework Programme, 2013-2017, Grant agreement 604814), BIO2014-54494-R and BIO2017-85522-R from the Spanish Ministry of Economy and Competitiveness.

Availability of data and materials

Shotgun metagenomic reads were submitted to NCBI SRA archive under run accession number SRR7268657. Reads resulted from sequencing of genomic material of enrichment cultures were submitted to SRA archive under accession numbers SRR7303206-SRR7303208. The 50 most abundant ASVs from 16S metabarcoding experiments were submitted to GenBank under accession numbers MH574490-MH574538.

Author information

OVG, SVT and PNG conceived the research. OVG, PNG and HG did the wet laboratory work (sample pretreatment, DNA isolation and enrichment cultures). DLJ did the chemical analysis of water and sediments. AAK, SVT, IVK and AVT did the shotgun sequencing of metagenomes and 16S rRNA V3-V4 amplicon. RB, AAK, SVT and IVK collected the data and did phylogenetic analysis. OVG drafted the manuscript. SVT, AAK, RB, IVK, MF, DLJ and PNG contributed to the manuscript writing. All authors read and approved the final manuscript.

Correspondence to Stepan V. Toshchakov or Olga V. Golyshina.

Ethics declarations

Ethics approval and consent to participate

Not applicable.

Competing interests

The authors declare that they have no competing interests.

Publisher’s Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Additional files

Additional file 1:

Figure S1. Photos of sampling sites (A) and (B) and scheme of water flow in copper-containing sulfidic deposits (C). Figure S2. Shannon index for the sediment and water microbial communities. Figure S3. Rarefaction plot and species richness calculated in GraftM from the taxonomic annotation of the Parys Mountain metagenome sequencing data. Table S1. Soil pore water chemistry for the sediment and for the overlying surface water for the acidic stream of Parys Mt. (DOCX 860 kb)

Additional file 2:

Metadata on TMEG-related sequences, used for diversity analysis of TMEG-related environmental clones. (XLS 40 kb)

Rights and permissions

Open Access This article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Keywords

  • Cuniculiplasma
  • Cuniculiplasmataceae
  • Thermoplasmatales
  • Acidophilic archaea
  • Terrestrial miscellaneous Euryarchaeotal group (TMEG)
  • Acid mine drainage (AMD) systems
  • Mine-impacted environments