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. 2022 Mar 22;369(1):fnac029. doi: 10.1093/femsle/fnac029

Cultivation of ammonia-oxidising archaea on solid medium

Timothy Klein 1, Lianna Poghosyan 2, J Elaine Barclay 3, J Colin Murrell 4, Matthew I Hutchings 5, Laura E Lehtovirta-Morley 6,✉
PMCID: PMC9072212  PMID: 35323924

Abstract

Ammonia-oxidising archaea (AOA) are environmentally important microorganisms involved in the biogeochemical cycling of nitrogen. Routine cultivation of AOA is exclusively performed in liquid cultures and reports on their growth on solid medium are scarce. The ability to grow AOA on solid medium would be beneficial for not only the purification of enrichment cultures but also for developing genetic tools. The aim of this study was to develop a reliable method for growing individual colonies from AOA cultures on solid medium. Three phylogenetically distinct AOA strains were tested: ‘Candidatus Nitrosocosmicus franklandus C13’, Nitrososphaera viennensis EN76 and ‘Candidatus Nitrosotalea sinensis Nd2’. Of the gelling agents tested, agar and Bacto-agar severely inhibited growth of all three strains. In contrast, both ‘Ca. N. franklandus C13’ and N. viennensis EN76 tolerated Phytagel™ while the acidophilic ‘Ca. N. sinensis Nd2’ was completely inhibited. Based on these observations, we developed a Liquid-Solid (LS) method that involves immobilising cells in Phytagel™ and overlaying with liquid medium. This approach resulted in the development of visible distinct colonies from ‘Ca. N. franklandus C13’ and N. viennensis EN76 cultures and lays the groundwork for the genetic manipulation of this group of microorganisms.

Keywords: ammonia-oxidising archaea, solid medium, cultivation, colonies, solidifying agent, Phytagel

A novel method for growing ammonia-oxidising archaea as single colonies on solid medium.

Introduction

Ammonia-oxidising archaea (AOA) comprise an important group of microorganisms affiliated with the phylum Thermoproteota, formerly known as Thaumarchaeota (Brochier-Armanet et al.2008, Rinke et al.2021). AOA are involved in the oxidation of ammonia to nitrite, the first and rate-limiting step of nitrification. The role of AOA in nitrification coupled with their ubiquitous distribution in both marine and terrestrial ecosystems, highlights their pivotal role in biogeochemical cycling of nitrogen (de la Torre et al. 2008, Wang et al. 2017, Alves et al. 2018, Beeckman et al. 2018). While nitrification is vital for nitrogen cycling, it is also associated with nitrogen fertilizer loss and leaching of nitrites and nitrates into aquatic systems leading to eutrophication (Raun and Johnson 1999). Thus, there is an urgent need to further explore AOA and the molecular mechanisms underpinning their physiology.

Since the discovery and isolation of the first AOA strain Nitrosopumilus maritimus SCM1 in 2005, our understanding of AOA has steadily expanded through culture-dependent and culture-independent approaches (Könneke et al. 2005). Nonetheless, large gaps in our knowledge of the biochemistry, physiology and niche adaptation of AOA still exist due to limitations to the currently available methods.

Culture-independent methods, which mainly comprise of ‘OMICS’-based approaches, provide valuable insights into the possible functional roles of AOA in the environment. However, the high percentage of archaeal genes of unknown function and the lack of comprehensive nucleic acid and protein databases, limit the ability to decipher molecular pathways in AOA (Marakova et al. 2019). This is exemplified by current efforts to elucidate the archaeal ammonia oxidation pathway which, based on genomic and biochemical studies, differs considerably from that of ammonia-oxidising bacteria (Lehtovirta-Morley 2018).

In many microorganisms, gene function is investigated with knock-out/knock-in genetic experiments. However, this approach is currently not feasible for AOA because a genetic system has not yet been developed. This is a major stumbling block in exploring and validating the hypotheses generated from metagenomics, proteomics and transcriptomics data.

A major limiting factor in the development of a genetic system for AOA is the inability to routinely grow them on solid medium as single colonies (Leigh et al. 2011, Kohler and Metcalf 2012). Single colonies represent a clonal population of cells and facilitate the precise analysis of specific genotypes. Currently, AOA are grown in liquid cultures and reports on their cultivation on solid medium are limited to a single publication by Chu et al. (2015) who demonstrated the growth of Nitrosopumilus sp. AR in low-melting point agarose. However, the growth observed in that study was a continuous mass of cells and no distinct colonies were evident. While the reasons for the limited success in growing AOA on solid medium are unclear, the role of solidifying agents on microbial growth is often overlooked (Janssen et al. 2002, Tamaki et al. 2009).

For instance, Tanaka et al. (2014) demonstrated agar to be inhibitory for microbial growth due to the production of hydrogen peroxide when agar was autoclaved together with phosphates. The inhibition of colony formation of the chemolithoautotroph Thiobacillus ferrooxidans on agar has also previously been reported and is attributed to the release of free sugars (i.e. D-galactose) from agar at low pH (Tuovinen and Kelly 1973). Microbiologists have also experimented with alternative solidifying agents such as gellan gum, resulting in the isolation of novel and previously uncultured microorganisms of the Phylum Verrucomicrobia (Tamaki et al. 2005). It is therefore evident that the choice of solidifying agents is an important consideration for successful cultivation of microbes on solid medium.

The aim of this study was to develop a novel method for the cultivation of AOA on solid medium. We hypothesised that the choice of gelling agent is a key factor to consider when growing AOA on solid medium.

Materials and methods

Archaeal strains and cultivation conditions

The AOA strains used in this study, ‘Ca. Nitrosocosmicus franklandus C13’, Nitrososphaera viennensis EN76 and ‘Ca. Nitrosotalea sinensis Nd2’ were routinely maintained in liquid fresh-water medium (FWM) as previously described (Tourna et al. 2011, Lehtovirta-Morley et al. 2014, Lehtovirta-Morley et al. 2016). The pH indicator, phenol red, was added to the medium of both neutrophilic AOA strains at a final concentration of 1.4 μM. All cultures were incubated at 37°C in the dark under static conditions. Cultures were regularly monitored for the presence of heterotrophic bacteria by plating on LB and R2A agar plates.

Nitrite measurements

Growth of AOA cultures was monitored by measuring nitrite accumulation. Nitrite concentration in the culture medium was measured using the Greiss colorimetric assay with sulphanilamide and N-(1-naphthyl) ethylenediamide in a 96-well plate format as previously described (Lehtovirta-Morley et al. 2016). Absorbance was measured at 540 nm using a VersaMax™ plate reader (Molecular Devices).

Assessing the effect of solidifying agents on the growth of AOA

The inoculum was prepared by harvesting 500 ml of a mid-late exponential liquid culture onto a 0.2 µM membrane filter (PES, Millipore). Cells were washed on the membrane with 50–100 ml of sterile FWM basal salts. The membrane filter was subsequently transferred into 10 ml of FWM basal salts and briefly vortexed. This cell suspension was serially diluted (1:10) as required.

To assess the effects of 1.5% (w/v) Agar (Formedium, UK), 1.5% (w/v) Bacto-Agar (BD Difco™), 1.4% (w/v) Noble-Agar (BD Difco™), 1.4% (w/v) Agarose (Melford, UK) and 1.7% (w/v) Phytagel™ (Sigma-Aldrich®) on the growth of AOA, a biphasic mixture of the gel and liquid medium was prepared. Briefly, to each 30 ml plastic screw-cap vial (Greiner Bio-One), 10 ml of the molten gelling agent (containing all medium supplements) was added and allowed to solidify. The solid layer was subsequently overlayed with an equal volume of liquid medium and inoculated with 80–100 µl of a diluted cell suspension (10−1, ∼106 cells mL −1) as described above. All experiments were performed in triplicate and control experiments were performed in the absence of a gelling agent. Vials were incubated in the dark at 37°C under static conditions.

Cultivation of AOA on solid media

‘Ca. N. franklandus C13’ and N. viennensis EN76 were grown on solid medium using the Liquid - Solid method (LS-method). The LS-method consists of a solid-phase (Phytagel™) in which the cells are embedded and a liquid-phase in which the gel-embedded cells are submerged. The LS-method involves four main steps (i) cell harvesting (ii) gel preparation (iii) inoculation and (iv) maintenance. Experiments were performed in triplicate in acid-washed 100 ml Duran glass bottles. The method was repeated five times and has been validated independently in our laboratory.

Cells were harvested aseptically from a mid-late exponential culture onto a 0.2 µm pore size membrane filter (PES, Millipore) using a vacuum filtration manifold. Cells were resuspended in a sterile solution of FWM basal salts. A four-fold (1:10) serial dilution series of this cell suspension was performed.

Phytagel™ (0.6% (w/v)) was dissolved in FWM basal salts (containing phosphates) and sterilized by autoclaving at 121°C for 15 min (15 psi). All heat-labile medium supplements including streptomycin (50 µg mL−1) were added once the molten gel had cooled to approximately 42°C. Ammonia concentration was 5 mM and 3 mM for 'Ca. N. franklandus C13' and N. viennensisEN76, respectively. A 20–25 ml aliquot of the molten Phytagel™ was transferred to each 100 ml Duran bottle and allowed to set.

The second Phytagel™ layer was prepared as above but inoculated with 50–80 µl of the diluted cell suspension (i.e. 10−1 (∼107cells mL−1) or 10−4 (∼104 cells mL −1)) prior to solidifying. The Phytagel™: cell mixture was gently swirled to ensure even distribution of the cells. Once the inoculated Phytagel™ layer had solidified, it was overlayed with 20 - 25 ml of FWM medium containing streptomycin (50 µg mL−1). Note: A single Phytagel™ layer may also be used. The bottles were incubated in the dark at 37°C under static conditions.

Nitrite accumulation in the top liquid layer was measured to monitor growth of the cells in the gel. The bottles were also monitored for a change in colour of the pH indicator (phenol red) from pink to yellow indicating acidification of the medium. Once nitrite accumulation had ceased, the liquid layer was regularly replaced with the same volume of fresh medium.

Nucleic acid extraction

Cellular biomass growing within the Phytagel™ was harvested aseptically using a sterile glass Pasteur pipette. Samples from three replicates were pooled (approximately 100 µl) and resuspended in 100 µl of FWM basal salts. DNA was extracted using a phenol:chloroform:isoamyl alcohol (25:24:1) protocol as described previously (Tourna et al. 2010). The DNA pellet was resuspended in 50 µl of TE buffer containing 100 mM Tris-HCl (pH 8) and 0.1 mM EDTA and stored at  -20°C.

Polymerase Chain Reaction (PCR)

PCR products for the archaeal and AOA-specific 16S rRNA gene were generated using the primer sets A109F/1492R and 771F/957R, respectively (Table S2). The ‘Ca. N. franklandus C13’ specific urease gene (ureC subunit) was amplified using the primer set ureC1F/ureC1R (Table S2). PCR targeting the bacterial 16S rRNA gene was performed with primer set 27F/1492R (Table S2). PCR reactions were performed in 50 µl volumes containing: 1X Q5 polymerase reaction buffer, 0.2 mM dNTP mixture, 0.4 µM of each primer, 0.02 U/µl units of Q5 high-fidelity DNA polymerase (New England BioLabs, UK). All primers and PCR thermocycling parameters are listed in Table S2. All PCR generated sequences were analysed using BioEdit sequence alignment editor v.7.2.5 (Hall 1999) and the NCBI BLAST tool (Altschul et al. 1990).

Fluorescence in-situ hybridisation (FISH) and transmission electron microscopy (TEM)

FISH analysis was performed according to the method previously described by Daims et al. (2005). A detailed technical description of sample preparation and visualisation for both FISH (Table S1) and TEM analysis may be found in the Supplementary section.

Results

Effects of different solidifying agents on AOA growth

Three AOA strains were grown in the presence of different solidifying agents to determine their effect on growth. In the presence of Phytagel™, ‘Ca. N. franklandus C13’ grew at comparable rates to the control cultures with growth rates of 0.47 d−1 and 0.40 d−1, respectively (Fig. 1A). In comparison, agarose resulted in a mild decrease in the growth rate of ‘Ca. N. franklandus C13’ cultures (0.22 d− 1). These observations were in sharp contrast to agar, Bacto-agar and Noble-agar that all severely inhibited nitrite accumulation in ‘Ca. N. franklandus C13’ cultures (Fig. 1B and C).

Figure 1.

Figure 1.

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Effects of different solidifying agents on the growth of ‘Ca. N. franklandus C13’: (A) Phytagel™ and agarose (B) agar and Bacto-agar (C) Noble-agar and (D) Phytagel™ and Bacto-agar (50:50) mixture. The control cultures were grown in the absence of a solidifying agent. Nitrite concentrations plotted represent the average of three replicate cultures. Error bars are standard errors of the means and may be smaller than the size of the symbol.

To further validate the toxic effects of Bacto-agar, a blended mixture (50:50) of Phytagel™: Bacto-agar was prepared. In this gel mixture, the growth rates of the ‘Ca. N. franklandus C13’ cultures declined to 0.34 d−1 compared to 0.45 d-1 in pure Phytagel™. This strongly suggested the presence of a toxic component in the Bacto-agar that negatively affects growth.

The effects of Phytagel™ and Bacto-agar on growth were further tested on N. viennensis EN76 and the acidophilic ‘Ca. N. sinensis Nd2’ (Table 1, Fig. S1). The growth rates of N. viennensis EN76 in Phytagel™ (0.56 d−1) and the control (0.54 d−1) were comparable to the pattern observed in ‘Ca. N. franklandus C13’. In contrast, the acidophilic ‘Ca. N. sinensis’ Nd2 was virtually unable to grow in the presence of both solidifying agents. These data are summarised in Table 1.

Table 1.

The effects of different gelling agents on the growth of AOA cultures.

Strain Agar Bacto-Agar Agarose Phytagel™ Noble-Agar
‘Ca. N. franklandus C13’ - - + ++ -
N. viennensis EN76 NT - - ++ NT
‘Ca. N. sinensis Nd2’ NT - NT - NT
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NT: Not tested

(−): Poor/no growth

(+): Moderate growth

(++): No effect on growth

Cultivation of AOA on solid medium

Phytagel™ was selected as a suitable solidifying agent for both ‘Ca. N. franklandus C13’ and N. viennensis EN76 cultures as it did not negatively affect their growth. We proceeded to develop the LS-method to produce single colonies from both strains. The LS-method involved inoculating AOA cells into molten Phytagel™ and allowing this mixture to solidify. The solidified cell:Phytagel™ layer was subsequently overlayed with liquid medium. Cultures were monitored by measuring nitrite accumulation in the top liquid layer (Fig. S2).

‘Ca. N. franklandus C13’ and N. viennensis EN76 cells growing within the gel accumulated nitrite (Fig. S2). This agreed with the pre-screening experiments and confirmed that the cells within the Phytagel™ were indeed actively growing. In addition, a change in colour of the liquid medium from pink to yellow, indicated acidification, consistent with ammonia oxidation.

Colony development

Colonies developed from ‘Ca. N. franklandus C13’ and N. viennensis EN76 cultures once the liquid-phase had been replaced approximately twice (Fig. 2 and S3). The high-density inoculum resulted in a lawn of colonies that took approximately 4–5 weeks to appear. In comparison, colonies from the low-density inoculum took a longer time to appear at about 7–8 weeks. The colonies from both strains were white/off-white in appearance and gradually became more distinct with regular replacement of the medium.

Figure 2.

Figure 2.

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‘Ca. N.  franklandus C13’ colonies developing in Phytagel™. Colonies are grown and maintained in 100 ml Duran glass bottles, and measure <1 mm in diameter.

Plating efficiency

The plating efficiency for ‘Ca. N. franklandus C13’ was determined as a measure of the number of colonies observed to the number of cells plated (number of colonies counted/number of cells plated). The number of colonies ranged between 100 and 154. Based on the number of cells inoculated, a plating efficiency of >85% was determined, indicating that majority of the cells formed colonies. This supports the gel-toxicity tests which showed that Phytagel™ did not impact growth of ‘Ca. N. franklandus C13’.

Sequence analysis of colonies

PCR amplification of the 16S rRNA gene from the ‘Ca. N. franklandus C13’ colonies, using both archaeal and AOA-specific primers, generated bands of the expected size i.e. ∼1,383 bp and ∼200 bp respectively (Fig. S4). A BLASTn analysis of these amplicons revealed a 100% and 99.5% nucleotide identity respectively (query cover:100%) to the 16S rRNA gene sequence in the published genome of ‘Ca. N. franklandus C13’ with the accession number LR216287.1. The query sequences used ranged between 1247 bp (archaeal) and 190 bp (AOA-specific) in length. In addition, we amplified the urease alpha subunit gene (ureC) specific to ‘Ca. N. franklandus C13’. A BLASTx analysis using a 119 bp sequence, revealed a 100% amino acid identity to the urease alpha subunit (UreC) from ‘Ca. N. franklandus C13’ with the accession number WP_145988037.1.

Fluorescence microscopy

Fluorescent in situ hybridisation (FISH) using archaeal probes was used to confirm the identity the colony-forming cells within the Phytagel™ (Fig. 3). The counterstain DAPI (blue), indiscriminately labels all cells within the sample and revealed irregular cocci, a characteristic cell morphology of ‘Ca. N. franklandus C13’. A signal from the archaeal probes (violet) confirmed the presence of archaeal cells and overlapped with the DAPI signal. The lack of signal from the bacterial probes (green) suggests the absence of bacterial cells demonstrating a homogenous population of archaeal cells within the Phytagel™.

Figure 3.

Figure 3.

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Fluorescent micrographs of cells growing with the PhytagelTM. Cells growing within PhytagelTM (left column) and cells from a pure liquid culture of ‘Ca. N. franklandus C13’ as a control (right column). Cells from a pure culture of Nitrosomonas europaea ATCC 19178 were used as a control (not shown). Cells are stained with FISH probes for archaea (ARCH-915, violet), bacteria (EUB338 mix, green) and DAPI (blue). Images were viewed at 1000 X magnification.

Transmission electron microscopy (TEM)

Colonies growing within the Phytagel™ were sampled and visualised with high-resolution TEM. The cell morphology and internal structures were compared to cells from a pure liquid batch culture of ‘Ca. N. franklandus C13’ as a control (Fig. 4). At low magnification (2000 X), a homogenous population of irregular cocci was observed which is typical of this AOA strain. At higher magnification (28,000 X), we were able to distinctly visualise the unusual vesicle-like structures characteristic of ‘Ca. N. franklandus C13’, the function and identity of which is currently unknown. Nonetheless, these data indicate that the cells growing within Phytagel™ share both internal and external structural similarity to the reference sample.

Figure 4.

Figure 4.

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Transmission electron microscopy of cells growing within PhytagelTM (left column) and cells from a pure liquid batch grown culture of ‘Ca. N. franklandus C13’ (right column).

Subculturing from AOA colonies

A small sample of the gel-embedded cells were scraped and transferred to fresh liquid medium and nitrite accumulation measured (Fig. 5). Nitrite accumulation in all three replicates indicated the presence of viable and actively growing ammonia-oxidising cells. Further analysis of the resulting biomass using archaeal FISH probes also demonstrated the presence of a homogeneous population of AOA cells. A signal from the bacterial probes was not detected.

Figure 5.

Figure 5.

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Fluorescent micrographs of cells grown from a colony of ‘Ca. N.  franklandus C13’. Cells were stained with FISH probes for archaea (Arch-915, violet), bacteria (EUB338 mix, green) and DAPI (blue). Images were viewed at 1000 X magnification. The graph shows nitrite accumulation from the subcultured colonies. Nitrite concentrations were measured in triplicate and error bars are standard errors of the means and may be smaller than the size of the symbol.

Discussion

Our findings highlight and emphasize the importance of selecting a suitable solidifying agent for the cultivation of AOA on solid medium. Although all AOA strains tested were inhibited by agar-based gels, the response to agarose and Phytagel™ varied between strains. Inhibition of microbial growth by solidifying agents such as agar has been well documented and is attributed to various factors including the production of hydrogen peroxide and the release of free sugars. This may be important as some AOA strains lack catalases, which normally detoxify hydrogen peroxide (Qin et al. 2014, Kim et al. 2016). Sand and Bennett (1966) also discuss numerous case studies on the variable effect that agar has on microbial growth based on the source of the agar as well as the brand. Other possible contributors to growth inhibition by agar is the presence of sulfated polysaccharides which exhibit a range of bioactive properties (Farias et al. 2000, Ngo and Kim 2013). Evidently, there is a large number of possible reasons for the inhibition of the AOA strains by agar-based gels that warrant further investigation, but are beyond the scope of the present study.

Phytagel™ is the trade name for gellan gum, an exopolysaccharide produced by Sphingomonas elodea (Vartak et al. 1995). Gellan gum is a tetrasaccharide composed of repeating units of D-glucose (2), L-rhamnose (1) and D-glucuronic acid (1) (Kang et al. 1982, Das et al. 2015). Both ‘Ca. N. franklandus C13’ and N. viennensis EN76 tolerated Phytagel™ well, whilst ‘Ca. N. sinensis Nd2’ did not. Reasons for inhibition of the acidophilic AOA strain are unclear but may be linked to the low pH and requires further testing. It is interesting to note that gellan gum was previously used to successfully isolate an ammonia-oxidising bacterium (AOB) from soil (Takahashi et al. 1992). Phytagel™ is an excellent alternative to agar as it exhibits desirable physical properties such as high optical clarity and gel strength (Jaeger et al. 2015). We emphasise that the growth of the AOA strains in this study on Phytagel™ was dependent on the batch and brand used (data not shown). The inability to reproduce previously published data upon changing to a new batch of Phytagel™ has also been reported. Differences in hardness between Phytagel™ batches, which may influence the reproducibility were observed (Jacques et al. 2020). Nonetheless, our data highlight the need to pre-screen solidifying agents prior to cultivation of AOA on solid medium.

The accumulation of toxic levels of nitrite, coupled with the slow growth rates, likely contributes to the difficulty in cultivating AOA on solid medium. To overcome this issue, we have developed the Liquid-Solid approach (LS). The principle behind the LS-method, which consists of a biphasic growth matrix, is that the nitrite excreted by the AOA cells within the gels diffuses into the overlaying liquid phase which is subsequently aspirated off and replaced with fresh medium. This overcomes or at the very least minimises the toxic accumulation of nitrite, thus facilitating the continuous growth of the cells.

In this study, we have demonstrated that the LS-approach facilitates the development of visible distinct single colonies from AOA cultures. Furthermore, a high plating efficiency (>85%) has been determined for ‘Ca. N. franklandus C13’ which is highly desirable in the context of developing a genetic system. It is also possible to pick the single colonies produced from the low-density inoculum using a thin sterile glass Pasteur pipette. However, due to the three-dimensional growth of the colonies within the gel, picking single colonies is challenging as the pipette may easily contact nearby colonies.

To validate that the colonies indeed originate from AOA cells, we employed both molecular and microscopy-based methods. Cells growing within the gel were labelled with FISH probes targeting archaeal and bacterial 16S rRNA. A signal was detected for the archaeal-specific probes but not for the bacterial probes indicating the presence of only archaeal cells. The cells exhibited a cellular morphology (irregular cocci) identical to the cells from a pure culture of ‘Ca. N. franklandus C13’. However, the use of the Cy3-labeled Arch-915 probe resulted in a weak fluorescent signal from the ‘Ca. N. franklandus C13’ cells as observed in Fig. 3. This may result from low rRNA content and poor cell permeability (Wagner et al. 2003). Therefore, FISH was coupled with high-resolution TEM, PCR and sequence analysis which all indicate that the cells are ‘Ca. N. franklandus C13’. A very faint band was amplified with the bacterial primers which is most likely transient DNA as no signal was detected from the bacterial FISH probes and no bacterial cells could be discerned from the high-resolution electron micrographs. In addition, no bacterial cells were detected by FISH from the colonies that were subcultured.

The LS-method has potential future applications for pure culture isolation of AOA which is currently restricted to time-consuming enrichment procedures. For example, if a dilute sample of a highly enriched AOA culture is grown using the LS-method and visible colonies are produced, then it may be possible to pick a desired colony expediting the purification process. This approach may also be useful for the purification of bacteria capable of the complete oxidation of ammonia to nitrate via nitrite also known as comammox. Currently a single pure culture of a comammox exists, which hinders their thorough physiological characterisation (Daims et al. 2015, Sakoula et al. 2020). The ability to produce single colonies from AOA is a major advance in facilitating the development of a genetic system for these archaea.

A main caveat with the LS-method is that it is seemingly not applicable to acidophilic AOA. Further work is necessary to better understand the inhibition of Phytagel™ and agar-based gels on ‘Ca. N. sinensis Nd2’. Also, it is difficult to determine colony counts due to their three-dimensional arrangement. We also observed the presence of free-floating cells in the liquid phase presumably due to the detachment from the gel-matrix. Lastly, although visible colonies from the high-density inoculum took on average 5–6 weeks, colonies from the low-density inoculum took a longer time (about two months) to reach a size that can easily be picked.

Conclusion

In conclusion, we have demonstrated that selection of a suitable solidifying agent is crucial for the successful cultivation of AOA on solid medium. Furthermore, we describe here a novel method for the cultivation of ‘Ca. N. franklandus C13’ and N. viennensis EN76 on solid medium that results in visible and distinct colonies. The relative simplicity and no requirement for specialised equipment makes the LS-method accessible to any microbiology laboratory working with this group of microbes.

Supplementary Material

fnac029_Supplemental_File
Click here for additional data file. (6.8MB, docx)

ACKNOWLEDGEMENTS

We thank Prof. Christa Schleper (University of Vienna) for providing the N. viennensis EN76 culture. We thank Kim Findlay (John Innes Centre) for the advice on electron microscopy.

Contributor Information

Timothy Klein, School of Biological Sciences, University of East Anglia, Norwich Research Park, Norwich, NR4 7TJ, UK.

Lianna Poghosyan, School of Biological Sciences, University of East Anglia, Norwich Research Park, Norwich, NR4 7TJ, UK.

J Elaine Barclay, Bioimaging Facility, John Innes Centre, Norwich Research Park, Norwich, NR4 7UH, UK.

J Colin Murrell, School of Environmental Sciences, University of East Anglia, Norwich Research Park, Norwich, NR4 7TJ, UK.

Matthew I Hutchings, Department of Molecular Microbiology, John Innes Centre, Norwich Research Park, Norwich, NR4 7UH, UK.

Laura E Lehtovirta-Morley, School of Biological Sciences, University of East Anglia, Norwich Research Park, Norwich, NR4 7TJ, UK.

Funding

This work was supported by the Natural Environment Research Council and ARIES DTP [Grant number NE/S007334/1]; Royal Society Dorothy Hodgkin Research Fellowship [Grant number DH150187 to LLM] and the European Research Council starting grant [Grant number UNITY 852993 to LLM]. This work was also supported by the Biotechnology and Biological Sciences Research Council via Institute Strategic Programme to the John Innes Centre [Grant number BBS/E/J/000PR9790].xs

Conflict of interest statement. Authors declare no conflict of interest.

References

  1. Altschul SF, Gish W, Miller Wet al. Basic local alignment search tool. J Mol Biol. 1990;215:403–10. [DOI] [PubMed] [Google Scholar]
  2. Alves RJE, Minh BQ, Urich Tet al. Unifying the global phylogeny and environmental distribution of ammonia-oxidising archaea based on amoA genes. Nat Commun. 2018;9:1517. [DOI] [PMC free article] [PubMed] [Google Scholar]
  3. Beeckman F, Motte H, Beeckman T. Nitrification in agricultural soils: impact, actors and mitigation. Curr Opin Biotechnol. 2018;50:166–73. [DOI] [PubMed] [Google Scholar]
  4. Brochier-Armanet C, Boussau B, Gribaldo Set al. Mesophilic Crenarchaeota: proposal for a third archaeal phylum, the Thaumarchaeota. Nat Rev Microbiol. 2008;6:245–52. [DOI] [PubMed] [Google Scholar]
  5. Chu YJ, Lee JY, Shin SRet al. A Method for Cell Culture and Maintenance of Ammonia-Oxidizing Archaea in Agar Stab. Indian J Microbiol. 2015;55:460–3. [DOI] [PMC free article] [PubMed] [Google Scholar]
  6. Daims H, Lebedeva EV, Pjevac Pet al. Complete nitrification by Nitrospira bacteria. Nature. 2015. DOI: 10.1038/nature16461. [DOI] [PMC free article] [PubMed] [Google Scholar]
  7. Daims H, Stoecker K, Wagner M.. Fluorescence in situ hybridization for the detection of prokaryotes. In: Osbourne AM, Smith CJ (eds). Molecular Microbial Ecology. New York: Taylor & Francis, 2005, 213–39. [Google Scholar]
  8. Das N, Tripathi N, Basu Set al. Progress in the development of gelling agents for improved culturability of microorganisms. Front Microbiol. 2015;6:698. [DOI] [PMC free article] [PubMed] [Google Scholar]
  9. De La Torre JR, Walker CB, Ingalls AEet al. Cultivation of a thermophilic ammonia oxidizing archaeon synthesizing crenarchaeol. Environ Microbiol. 2008;10:810–8. [DOI] [PubMed] [Google Scholar]
  10. Farias WRL, Valentei AP, Pereira MSet al. Structure and Anticoagulant Activity of Sulfated Galactans. J Biol Chem. 2000;275:29299–307. [DOI] [PubMed] [Google Scholar]
  11. Hall TA. BioEdit: a User-Friendly Biological Sequence Alignment Editor and Analysis Program for Windows 95/98/NT. Nucl Acids Symp Ser. 1999;41:95–8. [Google Scholar]
  12. Jacques CN, Hulbert AK, Westenskow Set al. Production location of the gelling agent Phytagel has a significant impact on Arabidopsis thaliana seedling phenotypic analysis. PLoS One. 2020;15:e0228515. [DOI] [PMC free article] [PubMed] [Google Scholar]
  13. Jaeger PA, McElfresh C, Wong LRet al. Beyond Agar: gel Substrates with Improved Optical Clarity and Drug Efficiency and Reduced Autofluorescence for Microbial Growth Experiments. Appl Environ Microbiol. 81, 2015. DOI: 10.1128/AEM.01327-15. [DOI] [PMC free article] [PubMed] [Google Scholar]
  14. Janssen PH, Yates PS, Grinton BEet al. Improved culturability of soil bacteria and isolation in pure culture of novel members of the divisions Acidobacteria, Actinobacteria, Proteobacteria, and Verrucomicrobia. Appl Environ Microbiol. 2002;68:2391–6. [DOI] [PMC free article] [PubMed] [Google Scholar]
  15. Kang KS, Veeder GT, Mirrasoul PJet al. Agar-Like Polysaccharide Produced by a Pseudomonas Species: production and Basic Properties. Appl Environ Microbiol. 1982;43:1086–91. [DOI] [PMC free article] [PubMed] [Google Scholar]
  16. Kim JG, Park SJ, Damsté JSSet al. Hydrogen peroxide detoxification is a key mechanism for growth of ammonia-oxidizing archaea. Proc Natl Acad Sci. 2016;113:7888–93. [DOI] [PMC free article] [PubMed] [Google Scholar]
  17. Kohler PRA, Metcalf WW. Genetic manipulation of Methanosarcina spp. Front Microbiol. 2012;3:259. [DOI] [PMC free article] [PubMed] [Google Scholar]
  18. Könneke M, Bernhard AE, de la Torre JRet al. Isolation of an autotrophic ammonia-oxidizing marine archaeon. Nature. 2005;437:543–6. [DOI] [PubMed] [Google Scholar]
  19. Lehtovirta-Morley LE, Ge C, Ross Jet al. Characterisation of terrestrial acidophilic archaeal ammonia oxidisers and their inhibition and stimulation by organic compounds. FEMS Microbiol Ecol. 2014;89:542–52. [DOI] [PMC free article] [PubMed] [Google Scholar]
  20. Lehtovirta-Morley LE, Ross J, Hink Let al. Isolation of ‘Candidatus Nitrosocosmicus franklandus’, a novel ureolytic soil archaeal ammonia oxidiser with tolerance to high ammonia concentration. FEMS Microbiol Ecol. 2016;92:fiw057. [DOI] [PMC free article] [PubMed] [Google Scholar]
  21. Lehtovirta-Morley LE. Ammonia oxidation: ecology, physiology, biochemistry and why they must all come together. FEMS Microbiol Lett. 2018;365. DOI: 10.1093/femsle/fny058. [DOI] [PubMed] [Google Scholar]
  22. Leigh JA, Albers SV, Atomi Het al. Model organisms for genetics in the domain Archaea: methanogens, halophiles, Thermococcales and Sulfolobales. FEMS Microbiol Rev. 2011;35:577–608. [DOI] [PubMed] [Google Scholar]
  23. Makarova KS, Wolf YI, Koonin EV. Towards functional characterization of archaeal genomic dark matter. Biochem Soc Trans. 2019;47:389–98. [DOI] [PMC free article] [PubMed] [Google Scholar]
  24. Ngo DH, Kim SK. Sulfated polysaccharides as bioactive agents from marine algae. Int J Biol Macromol. 2013;62:70–5. [DOI] [PubMed] [Google Scholar]
  25. Qin W, Amin SA, Martens-Habbena Wet al. Marine AOA show mixotrophy and ecotypic variation. Proc Natl Acad Sci. 2014;111:12504–9. [DOI] [PMC free article] [PubMed] [Google Scholar]
  26. Raun WR, Johnson GV. Improving Nitrogen Use Efficiency for Cereal Production. Agron J. 1999;91:357–63. [Google Scholar]
  27. Rinke C, Chuvochina M, Mussig AJet al. A standardized archaeal taxonomy for the Genome Taxonomy Database. Nat Microbiol. 2021;6:946–59. [DOI] [PubMed] [Google Scholar]
  28. Sakoula D, Koch H, Frank Jet al. Enrichment and physiological characterization of a novel comammox Nitrospira indicates ammonium inhibition of complete nitrification. ISME J. 2020;15:1010–24. [DOI] [PMC free article] [PubMed] [Google Scholar]
  29. Sands JG, Bennett EO. Effect of Different Commercial Agar Preparations on the Inhibitory Activities of Phenols. Appl Microbiol. 1966;14. DOI: 10.1128/am.14.2.196-202.1966. [DOI] [PMC free article] [PubMed] [Google Scholar]
  30. Takahashi R, Kondo N, Usui Ket al. Pure Isolation of a New Chemoautotrophic Ammonia-Oxidizing Bacterium on Gellan Gum Plate. J Ferment Bioeng. 1992;74. DOI: 10.1016/0922-338X(92)90268-Y. [Google Scholar]
  31. Tamaki H, Hanada S, Sekiguchi Yet al. Effect of gelling agent on colony formation in solid cultivation of microbial community in lake sediment. Environ Microbiol. 2009;11:1827–34. [DOI] [PubMed] [Google Scholar]
  32. Tamaki H, Sekiguchi Y, Hanada Set al. Comparative Analysis of Bacterial Diversity in Freshwater Sediment of a Shallow Eutrophic Lake by Molecular and Improved Cultivation-Based Techniques. Appl Environ Microbiol. 2005;71:2162–9. [DOI] [PMC free article] [PubMed] [Google Scholar]
  33. Tanaka T, Kawasaki K, Daimon Set al. A hidden pitfall in the preparation of agar media undermines microorganism cultivability. Appl Environ Microbiol. 2014;80:7659–66. [DOI] [PMC free article] [PubMed] [Google Scholar]
  34. Tourna M, Freitag TE, Prosser JI. Stable Isotope Probing Analysis of Interactions between Ammonia Oxidizers. Appl Environ Microbiol. 2010;76:2468–77. [DOI] [PMC free article] [PubMed] [Google Scholar]
  35. Tourna M, Stieglmeier M, Spang Aet al. Nitrososphaera viennensis, an ammonia oxidizing archaeon from soil. Proc Natl Acad Sci. 2011;108:8420–5. [DOI] [PMC free article] [PubMed] [Google Scholar]
  36. Tuovinen OH, Kelly DP. Studies on the Growth of Thiobacillus ferrooxidans. Archiv für Mikrobiologie. 1973;88:285–98. [PubMed] [Google Scholar]
  37. Vartak NB, Lin CC, Cleary JMet al. Glucose metabolism in ‘Sphingomonas elodea’: pathway engineering via construction of a glucose-6-phosphate dehydrogenase insertion mutant. Microbiology. 1995;141:2339–50. [DOI] [PubMed] [Google Scholar]
  38. Wagner M, Horn M, Daims H. Fluorescence in situ hybridisation for the identification and characterisation of prokaryotes. Curr Opin Microbiol. 2003;6:302–9. [DOI] [PubMed] [Google Scholar]
  39. Wang J, Kan J, Zhang Xet al. Archaea Dominate the Ammonia-Oxidizing Community in Deep-Sea Sediments of the Eastern Indian Ocean—from the Equator to the Bay of Bengal. Front Microbiol. 2017;8:415. [DOI] [PMC free article] [PubMed] [Google Scholar]

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