Dissimilatory nitrate reduction by Aspergillus terreus isolated from the seasonal oxygen minimum zone in the Arabian Sea
© Stief et al.; licensee BioMed Central Ltd. 2014
Received: 31 January 2014
Accepted: 10 February 2014
Published: 11 February 2014
A wealth of microbial eukaryotes is adapted to life in oxygen-deficient marine environments. Evidence is accumulating that some of these eukaryotes survive anoxia by employing dissimilatory nitrate reduction, a strategy that otherwise is widespread in prokaryotes. Here, we report on the anaerobic nitrate metabolism of the fungus Aspergillus terreus (isolate An-4) that was obtained from sediment in the seasonal oxygen minimum zone in the Arabian Sea, a globally important site of oceanic nitrogen loss and nitrous oxide emission.
Axenic incubations of An-4 in the presence and absence of oxygen and nitrate revealed that this fungal isolate is capable of dissimilatory nitrate reduction to ammonium under anoxic conditions. A 15N-labeling experiment proved that An-4 produced and excreted ammonium through nitrate reduction at a rate of up to 175 nmol 15NH4 + g-1 protein h-1. The products of dissimilatory nitrate reduction were ammonium (83%), nitrous oxide (15.5%), and nitrite (1.5%), while dinitrogen production was not observed. The process led to substantial cellular ATP production and biomass growth and also occurred when ammonium was added to suppress nitrate assimilation, stressing the dissimilatory nature of nitrate reduction. Interestingly, An-4 used intracellular nitrate stores (up to 6–8 μmol NO3 - g-1 protein) for dissimilatory nitrate reduction.
Our findings expand the short list of microbial eukaryotes that store nitrate intracellularly and carry out dissimilatory nitrate reduction when oxygen is absent. In the currently spreading oxygen-deficient zones in the ocean, an as yet unexplored diversity of fungi may recycle nitrate to ammonium and nitrite, the substrates of the major nitrogen loss process anaerobic ammonium oxidation, and the potent greenhouse gas nitrous oxide.
In marine ecosystems, nitrate (NO3 -) serves as both a nitrogen source for assimilation and an electron acceptor for dissimilatory processes when oxygen (O2) is deficient. The latter scenario is ubiquitously encountered in anoxic sediment layers, but also prevails in the water bodies of oxygen minimum zones (OMZs) of the world’s oceans. In denitrification, nitrate is sequentially reduced to dinitrogen, in dissimilatory nitrate reduction to ammonium (DNRA), nitrate is sequentially reduced to ammonium and in anaerobic ammonium oxidation (anammox), ammonium is oxidized by nitrite to form dinitrogen. These different metabolic pathways of dissimilatory or reduction were originally thought to only occur in prokaryotes[2–4]. Meanwhile, denitrification and DNRA have been discovered in a limited set of eukaryotic microorganisms, including marine foraminifers[5, 6] and diatoms[7, 8]. Incomplete denitrification to nitrous oxide (N2O) has also been proven for plant-pathogenic and soil fungi, such as Fusarium oxysporum[9, 10], but so far not for marine isolates. Additionally, a large number of fungal species, mainly belonging to Ascomycota, are capable of “ammonia fermentation”, a form of reduction to ammonium coupled to the fermentation of organic compounds.
Fungi are primarily aerobic heterotrophs, but some species, especially fermentative yeasts, can survive and grow under completely anoxic conditions. Nevertheless, both the abundance and the ecological role of fungi in O2-deficient marine environments are probably underestimated. Recent sequencing approaches revealed a large diversity of marine microbial eukaryotes in environments where O2 occurs in low concentrations or is completely absent. Additionally, it was found that fungal 18S rDNA sequences dominate the eukaryotic microbial communities in anoxic marine habitats (reviewed by). Fungi retrieved from coastal marine sediments are dominated by Ascomycota that may be of terrestrial origin. Amongst others, they are represented by Aspergillus species, including A. terreus. Fungal community structures differ between oxic, seasonally anoxic, and permanently anoxic sites, suggesting adaptation of fungal communities to prevailing O2 conditions.
The Arabian Sea harbors two different O2-deficient conditions, which includes a seasonal OMZ along the continental shelf and an open-ocean, perennial OMZ. The distribution of anaerobic nitrogen cycling in the Arabian Sea is patchy and covers areas with predominant denitrification or anammox activity. The Arabian Sea is also a globally important site of N2O emission[17, 20, 21]. The oversaturation of the water column with this potent greenhouse gas is ascribed to denitrification activity.
Here, the ecophysiology of an A. terreus isolate (An-4) obtained from the seasonal OMZ in the Arabian Sea was studied. An-4 was enriched from coastal sediment sampled during a period of bottom-water anoxia using anoxic,-amended conditions. It was therefore hypothesized that An-4 is capable of dissimilatory NO3 - reduction. The role of O2 and availability in triggering dissimilatory NO3 - reduction was studied in axenic incubations. In a dedicated 15N-labeling experiment, all environmentally relevant products of dissimilatory reduction were determined. Intracellular storage, a common trait of NO3 --respiring eukaryotes, was studied combining freeze-thaw cycles and ultrasonication for lysing-storing cells. Production of cellular energy and biomass enabled by dissimilatory reduction was assessed with ATP and protein measurements, respectively. Using these experimental strategies, we present the first evidence for dissimilatory reduction by an ascomycete fungus that is known from a broad range of habitats, but here was isolated from a marine environment.
Aerobic and anaerobic nitrate and ammonium turnover
Products of anaerobic nitrate turnover
Turnover rates of inorganic nitrogen species by A. terreus isolate An-4 during anaerobic incubation with 15 NO 3 - enrichment (Experiment 2)
NO3 - total
NO2 - total
NH4 + total
Intracellular nitrate storage
The capability of An-4 to store nitrate intracellularly, a common trait of large-celled microorganisms that respire nitrate, was investigated during both aerobic and anaerobic cultivation (Exp. 3). Intracellular NO3 - concentrations (ICNO3) were high when extracellular NO3 - concentrations (ECNO3) were high and vice versa, irrespective of O2 availability (Figure 3A + B). Under oxic conditions, however, ICNO3 and ECNO3 concentrations dropped sharply within the first day of incubation (Figure 3A), whereas under anoxic conditions, steady decreases in ICNO3 and ECNO3 concentrations were noted during 11 days of incubation (Figure 3B).
In the 15N-labeling experiment (Exp. 2), the total amount of N produced in each incubation vial (185.4 ± 29.3 nmol) exceeded the total amount of NO3 - consumed (114.4 ± 27.3 nmol), implying that also 71.0 nmol ICNO3 was consumed during the anoxic incubation. The initial amount of ICNO3 transferred into the incubation vials together with the An-4 mycelia of 77.5 ± 28.9 nmol equaled the calculated amount of ICNO3 needed to close the N budget.
Production of biomass and cellular energy
Correlation between oxygen and nitrate availability and biomass production by A. terreus isolate An-4 (Experiments 1 and 4)
Nitrate in media (μM)
Final biomass in flask (g)
Aerobic + Nitrate
Anaerobic + Nitrate
Aerobic – Nitrate
Aerobic + Nitrate
Anaerobic – Nitrate
Anaerobic + Nitrate
Physiology of isolate An-4
All observations made during incubations of Aspergillus terreus (isolate An-4) in the presence and absence of O2 and NO3 - indicate that this fungus is capable of dissimilatory NO3 - reduction to NH4 +. An-4 produced NH4 + only under anoxic conditions and through NO3 - reduction as proven in the 15N-labeling experiment. The process led to significant cellular ATP production and biomass growth and also occurred when NH4 + was added to suppress NO3 - assimilation, stressing the dissimilatory nature of the observed anaerobic NO3 - reduction activity. For a large number of other fungal species, this type of anaerobic NO3 - metabolism has been termed “ammonia fermentation” in case that the reduction of NO3 - to NH4 + was coupled to the oxidation of organic carbon compounds to acetate and substrate-level phosphorylation[10, 11]. Ammonia fermentation has been found in a wide spectrum of filamentous ascomycetous fungi[11, 22], but so far not in fungi isolated from marine environments. Since the fermentation of organic substrates is not proven for An-4, the anaerobic NO3 - metabolism of this isolate might as well be of respiratory nature and then corresponds to DNRA. This pathway has so far been excluded to occur in fungi because a pentaheme cytochrome c NO2 - reductase typical of DNRA has not been found in fungi with an anaerobic NO3 - metabolism.
Aside from the general accord with fungal ammonia fermentation or DNRA, the anaerobic NO3 - metabolism of An-4 showed several interesting features. Most notably, dissimilatory NO3 - reduction was accompanied by significant N2O production (ca. 15% of NO3 - reduced) and to a lesser extent by NO2 - production (ca. 1.5% of NO3 - reduced). While it was not surprising that traces of NO2 -, an intermediate of dissimilatory NO3 - reduction to NH4 +, were released into the liquid media[8, 11], the production and cellular release of N2O was unexpected. Nitrous oxide is the end product of incomplete denitrification in many plant-pathogenic and soil fungi[9, 25, 26], whereas the marine isolate An-4 obviously produces N2O via dissimilatory NO3 - reduction to NH4 +. Nitrous oxide is not generally known as an intermediate of dissimilatory NO3 - reduction to NH4 +, but may well be a by-product of this reduction pathway as shown for bacteria[27–29].
An-4 is clearly able to store NO3 - intracellularly and use it for dissimilatory NO3 - reduction to NH4 +. Intracellular NO3 - storage is known for a number of prokaryotic and eukaryotic microorganisms capable of dissimilatory NO3 - reduction, but so far has not been reported for fungi, even when capable of denitrification or ammonia fermentation[10, 24]. Large sulfide-oxidizing bacteria[30, 31], foraminifers and gromiids[5, 6, 32, 33], and diatoms[7, 8, 34, 35] store NO3 - in their cells in millimolar concentrations. In our experiments with An-4, the maximum biomass-specific intracellular NO3 - contents were 6–8 μmol g-1 protein. Assuming a cellular protein content of 50% of the dry weight and a cellular water content of 90% of the wet weight, maximum intracellular nitrate concentrations reached ca. 400 μmol L-1. This intracellular NO3 - pool proved to be quantitatively important for dissimilatory NO3 - reduction by An-4, since it contributed up to 38% to the total NO3 - consumption in the 15N-labeling experiment. The initially high rates of NH4 + production may suggest that An-4 is first using up the readily available intracellular NO3 - stores before it switches to using extracellular NO3 - as well, but this scenario needs to be proven in a dedicated 15N-labeling experiment. The general physiology of intracellular NO3 - storage by An-4 is currently unknown. For instance, it is not clear at which growth stage and under which ambient conditions An-4 is taking up NO3 - from the environment because the phase of increasing intracellular NO3 - contents was not captured by our oxic and anoxic incubations. From the observed correlation between ICNO3 and ECNO3 it can be concluded that an unknown enrichment factor cannot be exceeded, meaning that ICNO3 concentrations will increase with ECNO3 concentrations, probably up to an as yet unknown maximum ICNO3 concentration. Benthic microorganisms that store NO3 - often show vertical migration behavior in the sediment that may enable them to take up NO3 - closer to the sediment surface and in the presence of O2[30, 36, 37]. It is conceivable that the hyphae of An-4 grow in direction of NO3 --containing layers closer to the sediment surface to facilitate NO3 - uptake. Finally, it remains to be investigated whether An-4 accumulates NO3 - in acidic vacuoles as recently shown for large sulfur bacteria or in the cytosol of the hyphae.
Ecological implications of anaerobic nitrate turnover by isolate An-4
Aspergillus terreus is a common and globally occurring soil fungus that is also known from substrates as diverse as air, salterns, capybara droppings, lung of pocket mice, corn, cotton plants, milled rice, muesli, and wall paint. The species has been reported from marine and associated habitats, such as mangroves and soft corals, and isolates from these habitats have been widely investigated for the production of bioactive compounds[40–42]. A. terreus has also been isolated from the hypersaline water of the Dead Sea[43, 44]. The species is an important human pathogen causing bronchopulmonary aspergillosis and disseminated infections. Dissimilatory NO3 - reduction by human-associated microorganisms has been demonstrated[46, 47], but it is not known whether fungi are involved. A. terreus is also of considerable biotechnological interest because it produces a wide diversity of secondary metabolites that find pharmaceutical applications, biotechnologically relevant compounds such as itaconic acid and itatartaric acid, as well as mycotoxins that are important for food safety ( and references therein).
The wide habitat spectrum of A. terreus might be significantly expanded by the ability for dissimilatory NO3 - reduction in the absence of O2. This fungus has the potential to survive hypoxic or anoxic conditions that prevail in aquatic sediments mostly just a few millimeters below the surface or even directly at the surface when O2 concentrations are low in the water column[12, 49]. In contrast, NO3 - originating from the water column and/or the nitrification layer at the sediment surface diffuses deeper into the sediment than O2 does. In shallow sediments, NO3 --rich water is introduced into even deeper layers by mixing forces such as bioturbation, bioirrigation, and ripple movement[51, 52]. The sediment habitat in which A. terreus can thrive is further expanded by its NO3 - storage capability. The maximum intracellular NO3 - content of 8 μmol g-1 protein theoretically sustains dissimilatory NO3 - reduction without extracellular NO3 - supply for 2–4.5 days (calculated from rates measured in the 15N-labeling experiment). Survival and growth beyond this time frame will depend on the ability of A. terreus to repeatedly access NO3 - in its natural sediment habitat, which is currently unknown.
The dissimilatory NO3 - reduction activity of An-4 leads to the production and release of NH4 +, N2O, and NO2 -. Thus, unlike the denitrification and anammox activities of other microorganisms, the anaerobic NO3 - metabolism of An-4 cannot directly lead to fixed nitrogen removal. Since the major product of NO3 - reduction is NH4 +, An-4 merely converts one form of fixed nitrogen into another one. It is noteworthy, however, that the production of NH4 + and NO2 - by An-4 might indirectly contribute to fixed nitrogen removal by fueling anammox, the dominant nitrogen loss process in many OMZs. Remarkably, An-4 produces and releases ca. 15% of the total NO3 - reduced as N2O, a potent greenhouse gas[54, 55]. Interestingly, the OMZs of the Arabian Sea have repeatedly been reported to be major sites of N2O production, especially in continental shelf areas and coastal upwelling zones[17, 20, 21, 56].
Before meaningful conclusions on the potential impact of fungi on the marine nitrogen cycle can be drawn, it has to be established how abundant and widespread fungi with an anaerobic NO3 - metabolism are in marine environments. Previous studies reported a high diversity of fungi in O2-deficient marine environments[12, 16], a large proportion of which may have similar physiologies as An-4. Therefore, further concerted efforts should aim at revealing the so far largely ignored influence of fungi on the marine nitrogen cycle and their role in the production of greenhouse gases.
Geographic origin and identity of isolate An-4
The sampling site was located in the coastal, seasonal OMZ off Goa (India), northwest of the river mouths of the Zuari and the Mandovi (15°31′80″N, 73°42′60″E). Sampling was carried out at 14 m water depth in October 2005 and anoxic conditions were recorded in the bottom waters during sampling. Four ascomycete fungi were successfully isolated by the particle-plating technique after enrichment in anoxic, nitrate-amended seawater. One of the ascomycete isolates (An-4) was axenized with antibiotics and is tested here for its capability to reduce nitrate in the absence of oxygen.
Isolate An-4 was identified as Aspergillus terreus (Order Eurotiales, Class Eurotiomycetes) using morphological and DNA sequence data. Macro- and microscopic characters were studied according to. Partial calmodulin (Cmd) and β-tubulin (BenA) gene sequences retrieved from the isolate with previously described methods[57, 58] were used to derive the phylogenetic position of An-4 (Additional file1: Figure S2). The obtained sequences were deposited in the NCBI GenBank sequence database under accession numbers [KJ146014] (Cmd) and [KJ146013] (BenA). The isolate was deposited in the culture collection of the CBS-KNAW Fungal Biodiversity Centre as [CBS 136781] and at the Microbial Type Culture Collection and Gene Bank (MTCC, Chandigarh, India) as [MTCC 11865].
Cultivation for anaerobic nitrate turnover experiments
An-4 was pre-grown on agar plates prepared from YMG broth (i.e., Yeast extract [8 g L-1] + Malt extract [10 g L-1] + Glucose [10 g L-1]) supplemented with penicillin and streptomycin. Every few plate transfers, the antibiotics were omitted to avoid emergence and carry-over of resistant bacteria. Spores of the axenic isolate grown on agar plates were used to inoculate 500-mL Erlenmeyer flasks that contained 250 mL of YMG broth. For aerobic cultivation, the flasks were closed with aseptic cotton plugs. The flasks were placed on a rotary shaker (120 rpm) and incubated at 26°C. Under these conditions, the mycelia of An-4 formed spherical aggregates of 2–5 mm in diameter. The transfers from plate to flask were repeated every 3–4 weeks.
Anaerobic nitrate turnover
The capability of An-4 to reduce nitrate anaerobically was investigated in two experiments: (1) An-4 was cultivated in Erlenmeyer flasks under oxic vs. anoxic conditions in the presence of both NO3 - and NH4 +, and (2) An-4 was pre-cultivated in Erlenmeyer flasks under oxic conditions in the presence of 15NO3 - and then exposed to anoxic conditions in gas-tight incubation vials.
In Experiment 1, the fate of NO3 - and NH4 + added to the liquid media was followed during aerobic and anaerobic cultivation of An-4. Six replicate liquid cultures were prepared as described above, but with the YMG broth adjusted to nominal concentrations of 50 μmol L-1 NO3 - and 50 μmol L-1 NH4 + using aseptic NaNO3 and NH4Cl stock solutions, respectively. Three cultures were incubated aerobically, whereas the other three cultures were incubated anaerobically by flushing the Erlenmeyer flasks with dinitrogen for 30 min and then closing them with butyl rubber stoppers. Subsamples of the liquid media (1.5 mL) were taken after defined time intervals using aseptic techniques. Anaerobic cultures were sampled in an argon-flushed glove box to avoid intrusion of O2 into the Erlenmeyer flasks. Samples were immediately frozen at −20°C for later analysis of NO3 - and NH4 + concentrations.
In Experiment 2, the precursors, intermediates, and end products of dissimilatory nitrate reduction by An-4 were investigated in a 15N-labeling experiment, involving an oxic-anoxic shift imposed on axenic mycelia. For the aerobic pre-cultivation, a liquid culture was prepared as described above, but with the YMG broth adjusted to 120 μmol L-1 15NO3 - (98 atom% 15N; Sigma-Aldrich). For anaerobic incubation, fungal aggregates were transferred to gas-tight glass vials (5.9-mL exetainers; Labco, Wycombe, UK) filled with anoxic NaCl solution (2%) amended with nitrate as electron acceptor and glucose as electron donor. Using aseptic techniques, equally-sized subsamples of fungal aggregates were transferred from the aerobic pre-cultures into 30 replicate exetainers. The wet weight of the aggregates was determined. Then the exetainers were filled with anoxic NaCl solution adjusted to 120 μmol L-1 15NO3 - and 25 μmol L-1 glucose. Care was taken not to entrap any gas bubbles when the exetainers were closed with the septum cap. The exetainers were fixed in a rack that was continuously rotated to keep the aggregates in suspension and were incubated at 26°C in the dark for 24 days.
The anaerobic incubation was terminated in batches of three exetainers after defined time intervals. Subsamples of the liquid media were withdrawn through the septum (and simultaneously replaced with helium) for analyzing the concentrations of extracellular NO3 -, NO2 -, NH4 + total, 15NH4 +, and N2O, while the concentrations of 15N-N2O and 15N-N2 were determined directly in the incubation exetainers. For NO3 -, NO2 -, and NH4 + total analysis, 1.5 mL of the liquid media was immediately frozen at −20°C. For N2O analysis, 1 mL of the liquid media was immediately transferred into an N2-purged 3-mL exetainer and fixed with 100 μL ZnCl2 (50%). For 15NH4 + analysis, 0.5 mL of the liquid media was transferred into a 3-mL exetainer and frozen at −20°C. The liquid media remaining in the incubation exetainers were fixed with 100 μL ZnCl2 (50%) for later 15N-N2O and 15N-N2 analysis. For technical reasons, 15N-N2O could not be quantified for this specific experiment, but only for a slightly modified twin experiment the results of which are presented in the Supporting Information.
Additional exetainers with fungal aggregates were prepared and treated in the same way as the other exetainers for verifying that An-4 remained axenic throughout the anaerobic incubation. At the end of the experiment, these exetainers were opened using aseptic techniques and subsamples of both fungal aggregates (at least two) and liquid medium (100 μL) were plated on YMG agar. After incubation at 26°C for 15 days, the fungal colonies were carefully checked by microscopy for the presence of bacteria and xenic fungi. All microscopic checks were negative. Additionally, DNA was extracted from fungal aggregates and liquid medium with the UltraClean™ Soil DNA Isolation Kit (Mo Bio, Carlsbad, CA) and used as template for PCR targeting the 16S rRNA gene with the universal bacterial primers GM3F/GM4R. All molecular checks were negative, since agarose gel electrophoresis did not reveal any specific amplification product except for in the positive control, a laboratory strain of Agrobacterium sp.
Intracellular nitrate storage
The capability of An-4 to store nitrate intracellularly was investigated during both aerobic and anaerobic cultivation (Experiment 3). Liquid cultures were prepared as described above, but with the YMG broth adjusted to 50 μmol L-1 NO3 -. After defined time intervals, YMG broth and fungal aggregates were subsampled for analysis of NO3 - freely dissolved in the broth (i.e., extracellular nitrate = ECNO3) and NO3 - contained within the fungal hyphae (i.e., intracellular nitrate = ICNO3). Subsamples for ECNO3 analysis (1.5 mL) were cleared from suspended hyphae by mild centrifugation at 1000× g for 10 min and the supernatants (S0) were stored at −20°C for later analysis. Fungal aggregates for ICNO3 analysis were collected in a 2-mL centrifugation tube and the adhering YMG broth was siphoned off using a hypodermic needle. The aggregates were washed with 1 mL nitrate-free NaCl solution (2%) and blotted dry on nitrate-free filter paper. The aggregates were then equally distributed among two 15-mL centrifugation tubes, one for ICNO3 analysis and one for protein analysis.
Aggregates intended for ICNO3 analysis were weighed and thoroughly mixed with 2.5 mL nitrate-free NaCl solution (2%) and centrifuged at 1000× g for 5 min. Half a milliliter of the supernatant (S1) was stored at −20°C for later analysis. To make the fungal hyphae burst and release the ICNO3 into the NaCl solution, the tube was alternately cooled down to −196°C in liquid nitrogen and heated up to +90°C in a water bath for 5 min each. Cell disruption was additionally promoted by a 1-min treatment with an ultrasonic probe (UW70, Bandelin, Germany). The homogenized hyphae were pelleted by centrifugation at 3000× g for 10 min and the supernatant (S2) was stored at −20°C for later analysis.
Aggregates intended for protein analysis were suspended in 4 mL 0.5 M NaOH, sonicated for 1 min, and incubated at +90°C for 15 min for hot alkaline extraction of cellular proteins. The hyphae were pelleted by centrifugation at 3000× g for 5 min and the supernatant was stored at −20°C for later protein analysis according to. Protein extraction was repeated with the pelleted hyphae and the results of the analysis of the two supernatants were combined. A conversion factor (wet weight → protein content) was derived and used for calculating the biomass-specific ICNO3 contents as the difference between NO3 - concentrations in S1 and S2 divided by the protein contents of the hyphae.
Production of biomass and cellular energy
The production of biomass and cellular energy by An-4 was studied during aerobic and anaerobic cultivation in the presence or absence of NO3 - (Experiment 4). For this purpose, the time courses of protein and ATP contents of An-4 mycelia and of NO3 - and NH4 + concentrations in the liquid media were followed. Twelve replicate liquid cultures were prepared as described for Experiment 1, but in six cultures NO3 - addition was omitted. Six cultures (3 cultures each with and without NO3 -) were incubated aerobically, whereas the other six cultures (3 cultures each with and without NO3 -) were incubated anaerobically. Subsamples of the liquid media (1.5 mL) and An-4 mycelia (4–6 aggregates) were taken after defined time intervals using aseptic techniques. Samples were immediately frozen at −20°C for later analysis of NO3 - and NH4 + concentrations and protein and ATP contents. The NO3 --amended cultures received additional NO3 - (to a nominal concentration of 50 μmol L-1) after 1, 3, 7, and 9 days of incubation to avoid premature nitrate depletion.
Nitrate and NO2 - were analyzed with the VCl3 and NaI reduction assay, respectively[61, 62]. In these methods, NO3 - and/or NO2 - are reduced to nitric oxide that is quantified with the chemiluminescence detector of an NOx analyzer (CLD 60, Eco Physics, Munich, Germany). Ammonium was analyzed with the salicylate method. Nitrous oxide was analyzed on a gas chromatograph (GC 7890, Agilent Technologies) equipped with a CP-PoraPLOT Q column and a 63Ni electron capture detector. Isotopically labeled ammonium (15NH4 +) was analyzed with the hypobromite oxidation assay[64, 65] followed by 15N-N2 analysis on a gas chromatography-isotopic ratio mass spectrometer (GC-IRMS; VG Optima, Manchester, UK). Prior to hypobromite addition, care was taken to remove any N2 possibly produced during the anaerobic incubation by flushing with helium for 5 min. Headspace samples for 15N-N2O and 15N-N2 analysis were taken directly from the incubation exetainers and measured on the GC-IRMS.
Biomass-specific contents of adenosine triphosphate (ATP) of An-4 were determined using a modified protocol for ATP quantification in aquatic sediments. Briefly, 1–3 pre-weighed An-4 aggregates were sonicated in 5 mL of ice-cold extractant (48 mmol L-1 EDTA-Na2 in 1 mol L-1 H3PO4) for 1 min and then stored on ice for 30 min. The cell suspension was centrifuged at 3000× g for 10 min and 1 mL of the supernatant was diluted 1:10 with autoclaved deionized water and adjusted to pH 7.8 with NaOH. An ATP assay mix (FLAAM, Sigma-Aldrich) and a luminometer (TD 20e Luminometer, Turner Designs) were used to quantify the extracted ATP with the firefly bioluminescence reaction. The ATP assay mix was diluted 1:25 with a dilution buffer (FLAAB, Sigma-Aldrich). Calibration standards (0–100 μmol L-1) were prepared from ATP disodium salt hydrate (A2383, Sigma-Aldrich) dissolved in 1:10-diluted extractant adjusted to pH 7.8. Biomass-specific ATP contents of An-4 were calculated from the ATP concentrations of the extracts and the protein contents of the An-4 aggregates.
We wish to thank Ingrid Dohrmann (MPI Bremen) for skillful help with laboratory analyses. Eckhard Thines (IBWF Kaiserslautern) is acknowledged for providing laboratory facilities. This study was financially supported by grants from the German Research Foundation awarded to P.S. (STI 202/6), A.K. (KA 3187/2-1), and to T.S. (STO 414/3-2) and by the Max Planck Society, Germany.
- Thamdrup B, Dalsgaard T: Nitrogen cycling in sediments. Microbial ecology of the oceans. Edited by: Kirchman DL. 2008, Hoboken.: John Wiley & Sons, 527-568.View ArticleGoogle Scholar
- Zumft WG: Cell biology and molecular basis of denitrification. Microbiol Mol Biol Rev. 1997, 61: 533-616.PubMed CentralPubMedGoogle Scholar
- Strous M, Fuerst JA, Kramer EHM, Logemann S, Muyzer G, Van de Pas-Schoonen KT, et al: Missing lithotroph identified as new planctomycete. Nature. 1999, 400: 446-449. 10.1038/22749.View ArticlePubMedGoogle Scholar
- Cabello P, Roldan MD, Moreno-Vivian C: Nitrate reduction and the nitrogen cycle in archaea. Microbiology-Sgm. 2004, 150: 3527-3546. 10.1099/mic.0.27303-0.View ArticleGoogle Scholar
- Risgaard-Petersen N, Langezaal AM, Ingvardsen S, Schmid MC, Jetten MSM, Op den Camp HJM, et al: Evidence for complete denitrification in a benthic foraminifer. Nature. 2006, 443: 93-96. 10.1038/nature05070.View ArticlePubMedGoogle Scholar
- Piña-Ochoa E, Høgslund S, Geslin E, Cedhagen T, Revsbech NP, et al: Widespread occurrence of nitrate storage and denitrification among Foraminifera and Gromiida. Proc Natl Acad Sci U S A. 2010, 107: 1148-1153. 10.1073/pnas.0908440107.PubMed CentralView ArticlePubMedGoogle Scholar
- Kamp A, de Beer D, Nitsch JL, Lavik G, Stief P: Diatoms respire nitrate to survive dark and anoxic conditions. Proc Natl Acad Sci U S A. 2011, 108: 5649-5654. 10.1073/pnas.1015744108.PubMed CentralView ArticlePubMedGoogle Scholar
- Kamp A, Stief P, Knappe J, de Beer D: Response of the ubiquitous pelagic diatom Thalassiosira weissflogii to darkness and anoxia. PLoS One. 2013, 8: e82605-10.1371/journal.pone.0082605.PubMed CentralView ArticlePubMedGoogle Scholar
- Shoun H, Tanimoto T: Denitrification by the fungus Fusarium oxysporum and involvement of cytochrome P-450 in the respiratory nitrite reduction. J Biol Chem. 1991, 266: 11078-11082.PubMedGoogle Scholar
- Takaya N: Response to hypoxia, reduction of electron acceptors, and subsequent survival by filamentous fungi. Biosci Biotechnol Biochem. 2009, 73: 1-8. 10.1271/bbb.80487.View ArticlePubMedGoogle Scholar
- Zhou ZM, Takaya N, Nakamura A, Yamaguchi M, Takeo K, Shoun H: Ammonia fermentation, a novel anoxic metabolism of nitrate by fungi. J Biol Chem. 2002, 277: 1892-1896. 10.1074/jbc.M109096200.View ArticlePubMedGoogle Scholar
- Jebaraj CS, Raghukumar C, Behnke A, Stoeck T: Fungal diversity in oxygen-depleted regions of the Arabian Sea revealed by targeted environmental sequencing combined with cultivation. FEMS Microbiol Ecol. 2010, 71: 399-412. 10.1111/j.1574-6941.2009.00804.x.View ArticlePubMedGoogle Scholar
- Stoeck T, Behnke A, Christen R, Amaral-Zettler L, Rodriguez-Mora MJ, Chistoserdov A, et al: Massively parallel tag sequencing reveals the complexity of anaerobic marine protistan communities. BMC Biol. 2009, 7: 1-20. 10.1186/1741-7007-7-1. Article 72View ArticleGoogle Scholar
- Epstein S, Lopez-Garcia P: “Missing” protists: a molecular prospective. Biodiv Conserv. 2008, 17: 261-276. 10.1007/s10531-007-9250-y.View ArticleGoogle Scholar
- Burgaud G, Woehlke S, Rédou V, Orsi W, Beaudoin D, Barbier G, et al: Deciphering the presence and activity of fungal communities in marine sediments using a model estuarine system. Aquat Microb Ecol. 2013, 70: 45-62. 10.3354/ame01638.View ArticleGoogle Scholar
- Mouton M, Postma F, Wilsenach J, Botha A: Diversity and characterization of culturable fungi from marine sediment collected from St. Helena Bay, South Africa. Microb Ecol. 2012, 64: 311-319. 10.1007/s00248-012-0035-9.View ArticlePubMedGoogle Scholar
- Naqvi SWA, Naik H, Pratihary A, D’Souza W, Narvekar PV, Jayakumar DA, et al: Coastal versus open-ocean denitrification in the Arabian Sea. Biogeosciences. 2006, 3: 621-633. 10.5194/bg-3-621-2006.View ArticleGoogle Scholar
- Ward BB, Devol AH, Rich JJ, Chang BX, Bulow SE, Naik H, et al: Denitrification as the dominant nitrogen loss process in the Arabian Sea. Nature. 2009, 461: 78-82. 10.1038/nature08276.View ArticlePubMedGoogle Scholar
- Jensen MM, Lam P, Revsbech NP, Nagel B, Gaye B, Jetten MSM, et al: Intensive nitrogen loss over the Omani Shelf due to anammox coupled with dissimilatory nitrite reduction to ammonium. ISME J. 2011, 5: 1660-1670. 10.1038/ismej.2011.44.PubMed CentralView ArticlePubMedGoogle Scholar
- Naqvi SWA, Jayakumar DA, Narvekar PV, Naik H, Sarma VVSS, D’Souza W, et al: Increased marine production of N2O due to intensifying anoxia on the Indian continental shelf. Nature. 2000, 408: 346-349. 10.1038/35042551.View ArticlePubMedGoogle Scholar
- Bange HW, Andreae MO, Lal S, Law CS, Naqvi SWA, Patra PK, et al: Nitrous oxide emissions from the Arabian Sea: a synthesis. Atmos Chem Phys. 2001, 1: 61-71. 10.5194/acp-1-61-2001.View ArticleGoogle Scholar
- Takasaki K, Shoun H, Yamaguchi M, Takeo K, Nakamura A, Hoshino T, et al: Fungal ammonia fermentation, a novel metabolic mechanism that couples the dissimilatory and assimilatory pathways of both nitrate and ethanol - Role of acetyl CoA synthetase in anaerobic ATP synthesis. J Biol Chem. 2004, 279: 12414-12420.View ArticlePubMedGoogle Scholar
- Kraft B, Strous M, Tegetmeyer HE: Microbial nitrate respiration - Genes, enzymes and environmental distribution. J Biotechnol. 2011, 155: 104-117. 10.1016/j.jbiotec.2010.12.025.View ArticlePubMedGoogle Scholar
- Zhou Z, Takaya N, Shoun H: Multi-energy metabolic mechanisms of the fungus Fusarium oxysporum in low oxygen environments. Biosci Biotechnol Biochem. 2010, 74: 2431-2437. 10.1271/bbb.100482.View ArticlePubMedGoogle Scholar
- Usuda K, Toritsuka N, Matsuo Y, Kim DH, Shoun H: Denitrification by the fungus Cylindrocarpon tonkinense - Anaerobic cell-growth and 2 isozyme forms of cytochrome P-450Nor. Appl Environ Microbiol. 1995, 61: 883-889.PubMed CentralPubMedGoogle Scholar
- Zhou ZM, Takaya N, Sakairi MAC, Shoun H: Oxygen requirement for denitrification by the fungus Fusarium oxysporum. Arch Microbiol. 2001, 175: 19-25. 10.1007/s002030000231.View ArticlePubMedGoogle Scholar
- Costa C, Macedo A, Moura I, Moura JJG, Le Gall J, Berlier Y, et al: Regulation of the hexaheme nitrite/nitric oxide reductase of Desulfovibrio desulfuricans, Wolinella succinogenes and Escherichia coli. FEBS Letts. 1990, 276: 67-70. 10.1016/0014-5793(90)80508-G.View ArticleGoogle Scholar
- Kaspar HF, Tiedje JM: Dissimilatory reduction of nitrate and nitrite in the bovine rumen: Nitrous oxide production and effect of acetylene. Appl Environ Microbiol. 1981, 41: 705-709.PubMed CentralPubMedGoogle Scholar
- Smith MS: Nitrous oxide production by Escherichia coli is correlated with nitrate reductase activity. Appl Environ Microbiol. 1983, 45: 1545-1547.PubMed CentralPubMedGoogle Scholar
- Fossing H, Gallardo VA, Jørgensen BB, Huettel M, Nielsen LP, Schulz H, et al: Concentration and transport of nitrate by the mat-forming sulfur bacterium Thioploca. Nature. 1995, 374: 713-715. 10.1038/374713a0.View ArticleGoogle Scholar
- McHatton SC, Barry JP, Jannasch HW, Nelson DC: High nitrate concentrations in vacuolate, autotrophic marine Beggiatoa spp. Appl Environ Microbiol. 1996, 62: 954-958.PubMed CentralPubMedGoogle Scholar
- Høgslund S, Revsbech NP, Cedhagen T, Nielsen LP, Gallardo VA: Denitrification, nitrate turnover, and aerobic respiration by benthic foraminiferans in the oxygen minimum zone off Chile. J Exp Mar Biol Ecol. 2008, 359: 85-91. 10.1016/j.jembe.2008.02.015.View ArticleGoogle Scholar
- Bernhard JM, Casciotti KL, McIlvin MR, Beaudoin DJ, Visscher PT, Edgcomb VP: Potential importance of physiologically diverse benthic foraminifera in sedimentary nitrate storage and respiration. J Geophys Res-Biogeosci. 2012, 117: 1-14. Article G03002View ArticleGoogle Scholar
- Lomas MW, Glibert PM: Comparisons of nitrate uptake, storage, and reduction in marine diatoms and flagellates. J Phycol. 2000, 36: 903-913. 10.1046/j.1529-8817.2000.99029.x.View ArticleGoogle Scholar
- Needoba JA, Harrison PJ: Influence of low light and a light: dark cycle on NO3 - uptake, intracellular NO3 -, and nitrogen isotope fractionation by marine phytoplankton. J Phycol. 2004, 40: 505-516. 10.1111/j.1529-8817.2004.03171.x.View ArticleGoogle Scholar
- Koho KA, Pina-Ochoa E, Geslin E, Risgaard-Petersen N: Vertical migration, nitrate uptake and denitrification: survival mechanisms of foraminifers (Globobulimina turgida) under low oxygen conditions. FEMS Microbiol Ecol. 2011, 75: 273-283. 10.1111/j.1574-6941.2010.01010.x.View ArticlePubMedGoogle Scholar
- Stief P, Kamp A, de Beer D: Role of diatoms in the spatial-temporal distribution of intracellular nitrate in intertidal sediment. PLoS One. 2013, 8: e73257-10.1371/journal.pone.0073257.PubMed CentralView ArticlePubMedGoogle Scholar
- Beutler M, Milucka J, Hinck S, Schreiber F, Brock J, Mussmann M, et al: Vacuolar respiration of nitrate coupled to energy conservation in filamentous Beggiatoaceae. Environ Microbiol. 2012, 14: 2911-2919. 10.1111/j.1462-2920.2012.02851.x.View ArticlePubMedGoogle Scholar
- Samson RA, Peterson SW, Frisvad JC, Varga J: New species in Aspergillus section Terrei. Stud Mycol. 2011, 69: 39-55. 10.3114/sim.2011.69.04.PubMed CentralView ArticlePubMedGoogle Scholar
- Barakat KM, Gohar YM: Antimicrobial agents produced by marine Aspergillus terreus var. africanus against some virulent fish pathogens. Indian J Microbiol. 2012, 52: 366-372. 10.1007/s12088-012-0255-1.PubMed CentralView ArticlePubMedGoogle Scholar
- He F, Bao J, Zhang XY, Tu ZC, Shi YM, Qi SH: Asperterrestide A, a cytotoxic cyclic tetrapeptide from the marine-derived fungus Aspergillus terreus SCSGAF0162. J Nat Prod. 2013, 76: 1182-1186. 10.1021/np300897v.View ArticlePubMedGoogle Scholar
- Parvatkar RR, D’Souza C, Tripathi A, Naik CG: Aspernolides A and B, butenolides from a marine-derived fungus Aspergillus terreus. Phytochem. 2009, 70: 128-132. 10.1016/j.phytochem.2008.10.017.View ArticleGoogle Scholar
- Grishkan I, Nevo E, Wasser SP: Soil micromycete diversity in the hypersaline Dead Sea coastal area, Israel. Mycol Prog. 2001, 2: 19-28.View ArticleGoogle Scholar
- Oren A, Gunde-Cimerman N: Fungal life in the Dead Sea. Prog Mol Subcell Biol. 2012, 53: 115-132. 10.1007/978-3-642-23342-5_6.View ArticlePubMedGoogle Scholar
- Iwen PC, Rupp ME, Langnas AN, Reed EC, Hinrichs SH: Invasive aspergillosis due to Aspergillus terreus: 12-year experience and review of the literature. Clin Infect Diseases. 1998, 26: 1092-1097. 10.1086/520297.View ArticleGoogle Scholar
- Lundberg JO, Weitzberg E, Cole JA, Benjamin N: Opinion - Nitrate, bacteria and human health. Nature Rev Microbiol. 2004, 2: 593-602. 10.1038/nrmicro929.View ArticleGoogle Scholar
- Schreiber F, Stief P, Gieseke A, Heisterkamp IM, Verstraete W, de Beer D, et al: Denitrification in human dental plaque. BMC Biol. 2010, 8: 1-11. 10.1186/1741-7007-8-1. Article 24View ArticleGoogle Scholar
- Revsbech NP, Jørgensen BB, Blackburn TH: Oxygen in the sea bottom measured with a microelectrode. Science. 1980, 207: 1355-1356. 10.1126/science.207.4437.1355.View ArticleGoogle Scholar
- Stief P, Nazarova L, de Beer D: Chimney construction by Chironomus riparius larvae in response to hypoxia: microbial implications for freshwater sediments. J N Am Benthol Soc. 2005, 24: 858-871. 10.1899/04-137.1.View ArticleGoogle Scholar
- Heisterkamp IM, Kamp A, Schramm AT, de Beer D, Stief P: Indirect control of the intracellular nitrate pool of intertidal sediment by the polychaete Hediste diversicolor. Mar Ecol Prog Ser. 2012, 445: 181-192.View ArticleGoogle Scholar
- Precht E, Franke U, Polerecky L, Huettel M: Oxygen dynamics in permeable sediments with wave-driven pore water exchange. Limnol Oceanogr. 2004, 49: 693-705. 10.4319/lo.2004.49.3.0693.View ArticleGoogle Scholar
- Stief P, de Beer D: Probing the microenvironment of freshwater sediment macrofauna: Implications of deposit-feeding and bioirrigation for nitrogen cycling. Limnol Oceanogr. 2006, 51: 2538-2548. 10.4319/lo.2006.51.6.2538.View ArticleGoogle Scholar
- Wright JJ, Konwar KM, Hallam SJ: Microbial ecology of expanding oxygen minimum zones. Nature Rev Microbiol. 2012, 10: 381-394.Google Scholar
- Dickinson RE, Cicerone RJ: Future global warming from atmospheric trace gases. Nature. 1986, 319: 109-115. 10.1038/319109a0.View ArticleGoogle Scholar
- Ravishankara AR, Daniel JS, Portmann RW: Nitrous oxide (N2O): the dominant ozone-depleting substance emitted in the 21st century. Science. 2009, 326: 123-125. 10.1126/science.1176985.View ArticlePubMedGoogle Scholar
- Naqvi SWA, Bange HW, Farias L, Monteiro PMS, Scranton MI, Zhang J: Marine hypoxia/anoxia as a source of CH4 and N2O. Biogeosciences. 2010, 7: 2159-2190. 10.5194/bg-7-2159-2010.View ArticleGoogle Scholar
- Houbraken J, Frisvad JC, Samson RA: Taxonomy of Penicillium section Citrina. Stud Mycol. 2011, 70: 53-138. 10.3114/sim.2011.70.02.PubMed CentralView ArticlePubMedGoogle Scholar
- Houbraken J, Spierenburg H, Frisvad JC: Rasamsonia, a new genus comprising thermotolerant and thermophilic Talaromyces and Geosmithia species. Antonie Van Leeuwenhoek. 2012, 101: 403-421. 10.1007/s10482-011-9647-1.PubMed CentralView ArticlePubMedGoogle Scholar
- Muyzer G, Teske A, Wirsen CO, Jannasch HW: Phylogenetic relationships of Thiomicrospira species and their identification in deep-sea hydrothermal vent samples by Denaturing Gradient Gel Electrophoresis of 16S rDNA fragments. Arch Microbiol. 1995, 164: 165-172. 10.1007/BF02529967.View ArticlePubMedGoogle Scholar
- Lowry OH, Rosebrough NJ, Farr AL, Randall RJ: Protein measurement with the folin phenol reagent. J Biol Chem. 1951, 193: 265-275.PubMedGoogle Scholar
- Braman RS, Hendrix SA: Nanogram nitrite and nitrate determination in environmental and biological materials by vanadium(III) reduction with chemiluminescence detection. Anal Chem. 1989, 61: 2715-2718. 10.1021/ac00199a007.View ArticlePubMedGoogle Scholar
- Yang F, Troncy E, Francoeur M, Vinet B, Vinay P, Czaika G, Blaise G: Effects of reducing reagents and temperature on conversion of nitrite and nitrate to nitric oxide and detection of NO by chemiluminescence. Clin Chem. 1997, 43: 657-662.PubMedGoogle Scholar
- Bower CE, Holm-Hansen T: A salicylate-hypochlorite method for determining ammonia in seawater. Can J Fish Aquat Sci. 1980, 37: 794-798. 10.1139/f80-106.View ArticleGoogle Scholar
- Warembourg FR: Nitrogen fixation in soil and plant systems. Nitrogen isotope techniques. Edited by: Knowles R, Blackburn TH. 1993, New York: Academic, 157-180.Google Scholar
- Risgaard-Petersen N, Rysgaard S, Revsbech NP: Combined microdiffusion-hypobromite oxidation method for determining 15N isotope in ammonium. Soil Sci Soc Am J. 1995, 59: 1077-1080. 10.2136/sssaj1995.03615995005900040018x.View ArticleGoogle Scholar
- Stief P, de Beer D: Bioturbation effects of Chironomus riparius on the benthic N-cycle as measured using microsensors and microbiological assays. Aquat Microb Ecol. 2002, 27: 175-185.View ArticleGoogle Scholar
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