Shotgun metagenomic analysis of metabolic diversity and microbial community structure in experimental vernal pools subjected to nitrate pulse
© Carrino-Kyker et al.; licensee BioMed Central Ltd. 2013
Received: 11 February 2013
Accepted: 1 April 2013
Published: 10 April 2013
Human activities have greatly increased nitrogen (N) levels in natural habitats through atmospheric N deposition and nutrient leaching, which can have large effects on N cycling and other ecosystem processes. Because of the significant role microorganisms play in N cycling, high inputs of nitrogenous compounds, such as nitrate (NO3-), into natural ecosystems could have cascading effects on microbial community structure and the metabolic processes that microbes perform. To investigate the multiple effects of NO3- pollution on microbial communities, we created two shotgun metagenomes from vernal pool microcosms that were either enriched with a solution of 10 mg NO3--N (+NO3-) or received distilled water as a control (−N).
After only 20 hours of exposure to NO3-, the initial microbial community had shifted toward one containing a higher proportional abundance of stress tolerance and fermentation environmental gene tags (EGTs). Surprisingly, we found no changes to N metabolism EGTs, even though large shifts in denitrification rates were seen between the +NO3- and –N microcosms. Thus, in the absence of NO3- addition, it is plausible that the microbes used other respiratory pathways for energy. Respiratory pathways involving iron may have been particularly important in our –N microcosms, since iron acquisition EGTs were proportionally higher in the –N metagenome. Additionally, we noted a proportional increase in Acidobacteria and Alphaproteobacteria EGTs in response to NO3- addition. These community shifts in were not evident with TRFLP, suggesting that metagenomic analyses may detect fine-scale changes not possible with community profiling techniques.
Our results suggest that the vernal pool microbial communities profiled here may rely on their metabolic plasticity for growth and survival when certain resources are limiting. The creation of these metagenomes also highlights how little is known about the effects of NO3- pollution on microbial communities, and the relationship between community stability and function in response to disturbance.
KeywordsNitrate Metagenome 454 Sequencing Environmental gene tag Microcosm
Human activities, particularly agricultural practices and fossil fuel emissions, have greatly increased inputs of nitrogen (N) to terrestrial and aquatic habitats . In agricultural regions, N is leached from soil in the form of nitrate (NO3-), which is often found in high concentrations in groundwater and groundwater-fed surface waters [2, 3]. Moreover, high NO3- in surface runoff is often observed when fertilizer is used [4, 5]. These sources of NO3- pollution pose a particular threat to aquatic habitats where groundwater and surface runoff are a significant or primary source of input. Vernal pools are temporary aquatic habitats that are common to temperate regions and filled by surface runoff following snowmelt, spring rain, and rising water table . As such, N enrichment from NO3- leaching can alleviate N limitation and have a significant influence on N cycling. Because vernal pools are shallow depressions that often experience low dissolved oxygen concentrations [7–9], increased NO3- availability can favor anaerobic N cycling processes, such as denitrification and anaerobic ammonium oxidation, while suppressing anoxic pathways adapted to low NO3- conditions, such as dissimilatory nitrate reduction to ammonium.
N cycling is almost exclusively mediated by microorganisms; therefore high NO3- inputs can influence N cycling and also have cascading structural effects on the microbial communities involved. By studying genes for the enzymes responsible for the conversion of N between oxidized and reduced forms, there have been large advances in our knowledge of microbial functional groups involved in N cycling [10, 11]. However, the N cycle is a complex network of pathways that can share some enzymes and can also be simultaneously influenced by the input of one nitrogenous compound, such as NO3- . Therefore, studies which profile only one or a subset of N cycling enzymes may provide a limited view of how NO3- pollution impacts microbial processes. In addition, most previous studies on the effects of NO3- on microbial functional genes have limited their assessment to N cycling genes (e.g., [13, 14]), even though elevated NO3- is known to affect other microbial processes, such as those involved in C cycling (e.g., [15, 16]). One method that could help overcome these limitations is a shotgun metagenomic approach, where multiple functional genes can be examined.
In this study, we utilized a shotgun metagenomic approach to examine the multiple effects of NO3- addition on vernal pool microbial communities in a microcosm experiment . Two metagenomes were created, one for replicate microcosms that received NO3- (labeled +NO3-) and one for replicate microcosms where NO3- was not added (labeled –N). Our previous study using these microcosms found that the addition of NO3- increased denitrification, while denitrification was not detected in the absence of NO3- . This functional change was not accompanied by any change in the denitrifier community structure, which was profiled with the nosZ gene using terminal restriction fragment length polymorphism (TRFLP) . It is unclear, however, if this lack of response by the denitrifying community was physiological in nature or related to our functional gene choice. For the shotgun metagenomic method utilized here, the microbial genomes were randomly amplified, thus allowing for the potential inclusion of multiple N cycling genes, as well as genes involved in other microbial processes. In addition to denitrifier community structure, our previous analyses used TRFLP to profile the structure of general bacteria and fungi, which also did not respond to NO3- addition . Because shotgun metagenomes also provide taxonomic information for microbial communities, we hypothesized that inclusion of more than one functional gene and obtaining taxonomic composition using a shotgun metagenomic approach would reveal community structural responses to NO3- pulses not observed with the profiling technique, TRFLP.
Environmental gene tag (EGT) matches to lower levels in the SEED database that were significantly different with Fisher exact tests
Proportional representation (%)
Fatty acids, lipids, and isoprenoids
Glycerolipid and Glycerophospholipid Metabolism in Bacteria
Fatty acids, lipids, and isoprenoids
Iron acquisition and metabolism
Iron acquisition in Vibrio
Alkyl hydroperoxide reductase subunit C-like protein
RNA processing and modification
NAD-dependent glyceraldehyde-3-phosphate dehydrogenase
Acetyl-CoA fermentation to Butyrate
Protein processing and modification
G3E family of P-loop GTPases (metallocenter biosynthesis)
Urease beta subunit
Nitrogen metabolism gene matches and the number of sequences from the +NO 3 - metagenome that matched with the genes, as determined with a BLASTN comparison
N Metabolism gene
# Database sequences
Average alignment length
+NO3- seq. 1
+NO3- seq. 2
Metagenomic analysis revealed treatment differences both for functional and taxanomic EGTs between our +NO3- and –N metagenomes. These differences were apparent even though the metagenome sequencing conducted here returned a lower number of sequences than are typically reported for shotgun metagenome studies [20–22]. However, a shotgun metagenomic sequencing effort conducted by Fierer et al. , where comparable sequence numbers to ours are reported, was able to elucidate increases in functional genes with increased N fertilization, suggesting that our sequence numbers are adequate for determining relative metabolic and taxonomic changes.
A somewhat surprising result was no proportional abundance change in any of the N metabolism EGTs between our treatments with the BLASTX comparison to the SEED database. Particularly surprising was no change in the denitrification EGTs (determined with the BLASTX) between treatments and no detection of denitrification genes with the BLASTN, other than two sequence matches to nitrate reductase in the +NO3- treatment. The two sequence matches with the BLASTN in the +NO3- metagenome were to the nitrate reductase genes napA and napB. Because the periplasmic nitrate reductases, which are the products of napA and napB, are used in both denitrification and DNRA , no conclusions can be drawn on which of these microbial groups grew to a level where they could be detected in the +NO3- microcosms. This lack of EGT response was despite the fact that we observed denitrification rate responses to our treatments , where the microcosms receiving NO3- displayed a denitrification rate near or higher than the upper range of what has been measured in flooded soils in the field . This result is consistent with a number of other studies that have found no link between function (including measurements of denitrification rate and denitrifying enzyme activity) and denitrifier gene copy number using QPCR [13, 25–27]. We previously suggested that, in the absence of NO3- addition, denitrifiers in our microcosms used other electron acceptors for respiration when NO3- was not available , since denitrifiers are known to use other respiratory pathways [see review 10]. There were proportionally higher EGTs in the iron acquisition and metabolism category in the –N metagenome, and the specific EGT match was to a TonB-dependent receptor (Table 1). TonB-dependent receptors are a category of energy-coupling proteins, which are known to be involved in iron uptake by members of the genus Pseudomonas[28, 29], and there is some evidence that one specific TonB-dependent receptor is involved in dissimilatory iron reduction by Shewanella oneidensis. This suggests that the microbial community in the –N microcosms contained a greater number of organisms capable of acquiring iron and, perhaps, utilizing it for energy, which may have been a potential survival strategy in the absence of the NO3- addition. To our knowledge, evidence to support this hypothesis is sparse (but see Hauck et al. , who found that denitrifiers can also perform anaerobic ferrous iron oxidation). It is accepted, however, that denitrifying organisms primarily perform aerobic respiration and then switch to denitrification under anoxic conditions where NO3- supply is sufficient . There is a category available through MG-RAST for respiration genes. There were close to 400 EGT matches from the two metagenomes to this category for genes involved in both aerobic and anaerobic respiratory pathways. However, there were no proportional changes in respiration EGT abundance between the +NO3- and the –N conditions (data not shown), likely because the microcosms were made anoxic prior to the metagenome creation, which could negate any advantage to aerobic organisms in either treatment. Though we did not observe proportional changes for EGTs involved in a known alternative respiratory pathway for denitrifiers, the observed proportional increase in iron acquisition and metabolism EGTs in the –N metagenome suggests that iron might be biogeochemically important under anoxic N-limited conditions.
Another possible reason for lack of denitrifier EGT treatment response is that denitrifiers may have been in low abundance compared to other microbial groups, making changes to their population undetectable relative to the background population numbers. For example, the denitrification gene nosZ is known to be in low abundance compared to 16S genes , and there are estimates that only 0.1 – 5% of culturable soil bacterial species can carry out denitrification . This conclusion is supported by our BLASTN results, which found only two sequences from either metagenome that matched with a N metabolism gene. With the BLASTX comparison to the SEED database, however, over 1% of our sequences from each metagenome matched with nitrogen metabolism subsystems. The fact that we found no differences in nitrogen metabolism EGT relative abundance after NO3- addition suggests that microbial populations involved in N cycling did not shift in the 20 hours following exposure to a NO3- pulse. This lack of treatment response could be due to insufficient time between treatment initiation and sampling (i.e. populations were slow to respond to the treatment). However, we did see other EGT changes, suggesting that some microbial populations grew and experienced a detectable community shift in response to acute changes in NO3- concentration. The initial microbial community response to NO3- in our metagenomes was toward organisms that contained stress response, carbohydrate, and fatty acids, lipids, and isoprenoid EGT matches (Figure 1). The stress response EGT that was higher in the +NO3- metagenome was for an alkyl hydroperoxide reductase subunit C-like protein. The gene for alkyl hydroperoxide reducates, subunit C is upregulated by NO3- exposure after only 30 minutes in Desulfovibrio vulgaris, suggesting that such increases in this and other oxidative stress genes may be a general stress response by the bacteria . Within the carbohydrates category, one EGT match that was higher in the +NO3- metagenome was for fermentation. Recently, there has been evidence for fermentation that is coupled to NO3- reduction in both bacteria and fungi [36, 37]. Fermentation in the +NO3- microcosms may have been particularly prominent for the fungi, because a switch to NO3- -coupled fermentation as the primary source of energy for soil fungi under anoxic conditions has been suggested .
The sequencing effort described here also showed changes to the proportional representation of taxonomic EGTs. There were highly significant increases in the relative abundance of Alphaproteobacteria and Acidobacteria EGTs in the +NO3- metagenome. Similarly, using freshwater microcosms, Barlett and Leff  found an increase in Alphaproteobacteria abundance when NO3- was present as a N source and suggested a competitive advantage to this group of organisms under these conditions. Under anoxic conditions, such as our microcosms, higher physiological activity and substrate uptake have been reported in several Alphaproteobacteria species when NO3- or NO2- were present as an electron acceptor . Therefore, in our microcosms, there could have been a competitive advantage to the Alphaproteobacteria due to greater growth compared to other facultative organisms in an anoxic environment with abundant NO3-. To our knowledge, there have been no other studies that found such an increase in Acidobacteria with NO3- addition. However, a sequencing effort in cultured strains of Acidobacteria recently found that these organisms possess NO3- and NO2- reducing genes . Alphaproteobacteria, and likely Acidobacteria, are adapted to low nutrient conditions. While this seems counterintuitive to our microcosm study, vernal pools in nature are known to be oligotrophic . The Alphaproteobacteria and Acidobacteria in vernal pools, then, may be adapted to survival in the disturbed, low nutrient conditions of these habitats and once NO3- becomes readily available they have a competitive advantage due to their growth capabilities in the presence of NO3-.
These taxonomic changes were not found in a previous examination of general bacteria or general fungi in these microcosms with TRFLP . The metagenomic analysis reported here provides a greater resolution than TRFLP, which is a coarse community profiling tool. Therefore, there may have been fine-scale changes in bacterial community structure that were not detected with TRFLP. Another reason for this discrepancy is that our previous TRFLP analyses used the gene regions of bacterial 16S and fungal ITS for profiling  and, in the current study, a nonredundant protein database was used for taxonomic comparisons. Therefore, the conclusions drawn here regarding taxonomic changes may be limited to the taxonomic groups that changed functionally. The fact that whole genome amplification (WGA) was used prior to 454 sequencing could also be contributing to the differences seen between the metagenomes that were not noted with TRFLP. This is because amplification techniques with the Phi29 DNA polymerase, which was used in the current study, have been shown to exclude the amplification of certain DNA sequences, particularly those in low abundance or those that are GC rich, and can skew the representation of certain OTUs compared to sequencing efforts of non-amplified DNA of the same sample [42–44]. Additionally, our study design cannot exclude the possibility that the communities changed between the treatments over the 30 day incubation period prior to our sample collection. Thus, differences seen between the metagenomes may not be only because of the NO3- addition, but could also be due to an incubation period that changed the communities in the separate microcosms. There were six replicate microcosms to help control for variability between each jar, and our previous TRFLP profiling of the bacterial and fungal communities and the nosZ gene showed no differences in community structure between the +NO3- and –N microcosms . Therefore, we expect community changes in response to the 30 day incubation to be minimal compared to the NO3- addition. Nevertheless, the observed proportional increase in Alphaproteobacteria and Acidobacteria in response to NO3- addition in the metagenomes requires more in depth study on the ecology of these groups and how they tolerate NO3- pollution.
These results suggest that NO3- additions to vernal pool habitats may be accompanied by relatively rapid microbial community changes at both the functional and taxonomic level. The initial community shift after only 20 hours of NO3- exposure was toward a more stress tolerant community capable of performing fermentation and away from a community more dependant on respiratory pathways involving iron, as evidenced by higher iron acquisition EGTs in the –N microcosms. Surprisingly, we found no changes to N metabolism EGTs with the BLASTX in response to our treatments and only a two sequence increase in detection of nitrate reductase genes, despite a vast increase in denitrification rate with NO3- addition. Thus, in the absence of an NO3- addition, it is plausible that denitrifying microbes used other respiratory pathways for energy and, although NO3- addition altered their metabolic response, it did not alter or affect community structure or size. Because microbial communities are diverse, they are thought to be functionally redundant [45–47]. Our results suggest that the vernal pool microbial communities profiled here may rely on this metabolic plasticity for growth and survival when certain resources are limiting.
The construction of these metagenomes also highlights how little is known about the effects of NO3- pollution on microbial communities, and the relationship between community stability and function in response to disturbance. Future research could begin to unravel the importance of stress tolerance and fermentation for microbial survival following short-term exposure to NO3-. In addition, future studies on the presence of Acidobacteria, a group that is understudied as a whole, in high NO3- conditions can also help to understand the distribution of this taxonomic group.
Vernal pool microcosms were replicated in 500 mL glass jars by adding 50 g of soil collected from four vernal pools located in a temperate deciduous forest of Northeast Ohio, USA. The soil was air dried and sieved to remove extraneous matter and mixed with 50 g of autoclaved coarse sand to prevent excessive compaction of the soil media prior to addition to the microcosms. Each microcosm received 800 mg of dried leaf discs on the surface of the soil media and 150 mL of sterile water. Throughout the experiment, the microcosms were held in an incubator with a 12/12 hour day night cycle, with temperatures between 15–17°C to mimic spring forest conditions. The microcosms were subjected to an initial pH manipulation (5, 6, 7, or 8) on day zero and N addition on day 30 (D30). This experimental design was used to simulate persistent pH changes previously observed in vernal pools across an urbanization gradient  and NO3- pulses that are often associated with polluted runoff , which can be a significant source of input into vernal pools. While the complete experiment contained 72 microcosms and full details of the experimental set up are described elsewhere , a subset of 12 microcosms were used for the metagenomic analysis reported here and were those that were manipulated to a pH of 6.0 ± 0.3 at the beginning of the experiment and received either an addition of 10 mg NO3--N or an equal volume of distilled water as a control on D30. There were six replicate microcosms for each treatment (NO3- addition and control). The NO3- addition and distilled water treatments were used because denitrification rate differed in these microcosms (an average of 3.84 ± 0.44 mg N (kg soil)-1 day-1 when NO3- was added and not detected in the microcosms receiving distilled water) . Two replicate soil samples were collected and pooled from each microcosm on D30 approximately 20 hours after the NO3- addition and frozen at −70°C until used for DNA extraction. Soil samples were further pooled by combining 125 mg of soil from two replicate microcosms in the same treatment and then subjecting this pooled soil sample to DNA extraction as described elsewhere . Therefore, there were three replicate DNA samples for each treatment that were used to create two metagenomes: one for the nitrate treatment (labeled +NO3-) and one for the distilled water treatment (labeled --N).
Similar to other shotgun metagenomic studies [20, 49–51], DNA was amplified with the illustra Genomiphi V2 amplification kit (GE Healthcare Life Sciences, Inc., Piscataway, NJ) following the manufacturer’s protocol. Two replicate Genomiphi reactions were prepared for each microcosm DNA sample, making six reactions total for each treatment (three replicate microcosm DNA samples × two replicate Genomiphi reactions). The Genomiphi reactions randomly amplified regions of genomic DNA using primers of random sequences and resulted in 8 μg of amplified DNA from the +NO3- sample and the 10 μg of amplified DNA from the –N sample. Because of the use of random primers, these amplified DNA samples potentially included segments of DNA from all microbial species present in the samples and from regions throughout the microbial genomes. The amplified DNA from Genomiphi reactions was precipitated with sodium acetate and purified with 80% cold ethanol before being sent to Inqaba Biotec (Pretoria, South Africa) for 454 pyrosequencing on a GS-FLX platform.
Because the metagenomes constructed from our microcosms contained DNA reads from multiple species, they were analyzed unassembled using the MG-RAST server  and are publicly available with the MG-RAST ID numbers 4445106.3 (+NO3-) and 4445130.3 (−N). Metagenomes are also available through the NCBI site [GenBank: SRP005560]. A BLASTX comparison to a non-redundant protein database was used to match the EGTs in the metagenomes to SEED subsystems . The SEED protein-coding database has been used successfully for comparing shotgun metagenomes to taxonomic [20, 21, 51] and metabolic sequences [20, 21, 49–51] in environmental samples. Only matches that had an e-value of 10-5 or lower and had sequence similarity of 50 base pairs or greater were included in our MG-RAST analysis.
Metagenomes were also analyzed with a local BLASTN to a database of N metabolism genes that we constructed with searches at the NCBI site. The database included the known genes for the enzymes involved in denitrification, DNRA, and Annamox (using [12, 52] as guides for the genes to include), as these processes are nitrate reduction pathways. The highly profiled functional genes for nitrification (amoA, amoB, and amoC) and nitrogen fixation (nifD, nifH, and nifK) were also included. The database contained a total of 111,502 sequences and a complete list of the genes included in the database can be found in Additional file 2: Table S5. The searches for the genes to include in the database at the NCBI site were to the “Nucleotide” collection of the International Nucleotide Sequence Database Collaboration (DDBJ/EMBL/GenBank) with limits, which excluded sequence tagged sites (STSs), third party annotation (TPA) sequences, high throughput genomic (HTG) sequences, patents, and whole genome shotgun (WGS) sequences. Additional limits were that the search field was gene name and the molecule was genomic DNA/RNA., We also excluded hits that included “complete genome” in any field. (The search field was as follows: “xxxX [Gene Name] AND biol_genomic [PROP] NOT “complete genome” [All Fields]”, where “xxxX” corresponds to the gene that was being searched for, such as “nosZ”.) The local BLASTN was conducted at Case Western Reserve University’s Genome and Transcriptome Analysis Core facility. A number of sequences in our database were complete chromosome sequences that included genes other than the N metabolism genes we were interested in. If sequences from the metagenomes matched with these database entries, they were only retained if the gene region of the BLASTN match was to a N metabolism gene of interest (e.g., if the match between the metagenome sequence and the database entry was to the gene region coding for a N metabolism gene of interest, such as the napA gene, it was kept, but if the match was to a non-N metabolism gene, such as the trpS gene, it was removed.) The BLASTN comparison included an e-value cutoff of 10-5 or lower and sequence similarity cutoff of 50 base pairs or greater.
The Statistical Analysis of Metagenomic Profiles (STAMP) program was used to compare the +NO3- and –N metagenomes by identifying the proportional representation of different metabolic or phylogenetic groups and determining if they were statistically different between the two metagenomes with two-sided Fisher exact tests . The MG-RAST functional matches at all levels and taxonomic matches at the class level and higher were compared with Fisher exact tests. Storey’s false discovery rate (FDR) method was applied to the Fisher exact tests as a multiple comparison test correction, resulting in q-values, which are the FDR equivalent of p-values. Confidence intervals were determined with the Newcome-Wilson method at α = 0.05. Statistically significant features that had less than five sequences or low effect sizes (<0.5 difference between proportions or <1.0 ratio of proportions) were removed from the analysis. In addition, a two sided chi-square test, with Yates’ correction for continuity, was conducted, also using STAMP, on the level two subsystems. This test was done specifically to investigate if any level two EGTs in the N metabolism category were statistically different with a less conservative test . Confidence intervals were calculated and effect size filters were used as with the Fisher exact tests. The multiple comparison test correction used was the Benjamini-Hochberg FDR. Only biologically meaningful categories were included in the results reported here (i.e., the miscellaneous category for subsystems was removed and, for the phylogenetic EGT matches, unclassified taxonomic groups were removed).
We thank Dr. Wendy M. Mahaney, Dr. Juan Carlos López-Gutiérrez, and Charlotte R. Hewins for help with collecting samples. Thank you also to Dr. Xiaodong Bai for his assistance with database creation and for running the local BLASTN for us and to Dr. Laurel A. Kluber for advice on data analysis. This work was funded by the Holden Arboretum Trust and the Corning Institute for Education and Research.
- Vitousek PM, Aber JD, Howarth RW, Likens GE, Matson PA, Schindler DW, Schlesinger WH, Tilman DG: Human alteration of the global nitrogen cycle: sources and consequences. Ecol Appl. 1997, 7: 737-750.
- Power JF, Schepers JS: Nitrate contamination of groundwater in north america. Agric Ecosyst Environ. 1989, 26: 165-187. 10.1016/0167-8809(89)90012-1.View Article
- Almasri MN, Kaluarachchi JJ: Assessment and management of long-term nitrate pollution of ground water in agriculture-dominated watersheds. J Hydrol. 2004, 295: 225-245. 10.1016/j.jhydrol.2004.03.013.View Article
- Owens LB, Edwards WM, Van Keuren RW: Peak nitrate-nitrogen values in surface runoff from fertilized pastures. J Environ Qual. 1984, 13: 310-312.View Article
- King KW, Torbert HA: Nitrate and ammonium losses from surface-applied organic and inorganic fertilizers. J Agric Sci. 2007, 145: 385-393. 10.1017/S0021859607006946.View Article
- Colburn EA: Vernal Pools: Natural History and Conservation. 2004, Blacksburg, VA: The McDonald & Woodward Publishing Company
- Carrino-Kyker SR, Swanson AK: Seasonal physicochemical characteristics of thirty northern Ohio temporary pools along gradients of GIS-delineated human land-use. Wetlands. 2007, 27: 749-760. 10.1672/0277-5212(2007)27[749:SPCOTN]2.0.CO;2.View Article
- Carrino-Kyker SR, Swanson AK: Temporal and spatial patterns of eukaryotic and bacterial communities found in vernal pools. Appl Environ Microbiol. 2008, 74: 2554-2557. 10.1128/AEM.01482-07.PubMedPubMed CentralView Article
- Carrino-Kyker SR, Swanson AK, Burke DJ: Changes in eukaryotic microbial communities of vernal pools along an urban–rural land use gradient. Aquat Microb Ecol. 2011, 62: 13-24. 10.3354/ame01432.View Article
- Philippot L, Hallin S: Molecular analyses of soil denitrifying bacteria. Molecular Techniques for Soil, Rhizosphere and Plant Microorganisms. Edited by: Cooper JE, Rao JR. 2006, Cambridge, MA: CAB International Publishing, 146-165.View Article
- Bothe H, Jost G, Schloter M, Ward BB, Witzel K-P: Molecular analysis of ammonia oxidation and denitrification in natural environments. FEMS Microbiol Rev. 2000, 24: 673-690. 10.1111/j.1574-6976.2000.tb00566.x.PubMedView Article
- 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.PubMedView Article
- Kandeler E, Brune T, Enowashu E, Dörr N, Guggenberger G, Lamersdorf N, Philippot L: Response of total and nitrate-dissimilating bacteria to reduced N deposition in a spruce forest soil profile. FEMS Microbiol Ecol. 2009, 67: 444-454. 10.1111/j.1574-6941.2008.00632.x.PubMedView Article
- Deiglmayr K, Philippot L, Kandeler E: Functional stability of the nitrate-reducing community in grassland soils towards high nitrate supply. Soil Biol Biochem. 2006, 38: 2980-2984. 10.1016/j.soilbio.2006.04.034.View Article
- DeForest JL, Zak DR, Pregitzer KS, Burton AJ: Atmospheric Nitrate Deposition, Microbial Community Composition, and Enzyme Activitiy in Northern Hardwood Forests. Soil Sci Soc Am J. 2004, 68: 132-138.View Article
- Smemo KA, Zak DR, Pregitzer KS: Chronic NO3- deposition reduces the retention of fresh leaf litter-derived DOC in northern hardwood forests. Soil Biol Biochem. 2006, 38: 1340-1347. 10.1016/j.soilbio.2005.09.029.View Article
- Carrino-Kyker SR, Smemo KA, Burke DJ: The effects of pH change and NO3- pulse on microbial community structure and function: a vernal pool microcosm study. FEMS Microbiol Ecol. 2012, 81: 660-672. 10.1111/j.1574-6941.2012.01397.x.PubMedView Article
- Meyer F, Paarmann D, D’Souza M, Olson R, Glass EM, Kubal M, Paczian T, Rodriguez A, Stevens R, Wilke A: The metagenomics RAST server - a public resource for the automatic phylogenetic and functional analysis of metagenomes. BMC Bioinforma. 2008, 9: 386-10.1186/1471-2105-9-386.View Article
- Overbeek R, Begley T, Butler RM, Choudhuri JV, Chuang HY, Cohoon M, de Crécy-Lagard V, Diaz N, Disz T, Edwards R: The subsystems approach to genome annotation and its use in the project to annotate 1000 genomes. Nucleic Acids Res. 2005, 33: 5691-5702. 10.1093/nar/gki866.PubMedPubMed CentralView Article
- Pfister CA, Meyer F, Antonopoulos DA: Metagenomic profiling of a microbial assemblage associated with the california mussel: a node in networks of carbon and nitrogen cycling. PLoS One. 2010, 5: e10518-10.1371/journal.pone.0010518.PubMedPubMed CentralView Article
- Varin T, Lovejoy C, Jungblut AD, Vincent WF, Corbeil J: Metagenomic analysis of stress genes in microbial Mat communities from antarctica and the high arctic. Appl Environ Microbiol. 2012, 78: 549-559. 10.1128/AEM.06354-11.PubMedPubMed CentralView Article
- Gomez-Alvarez V, Revetta RP, Santo Domingo JW: Metagenomic analyses of drinking water receiving different disinfection treatments. Appl Environ Microbiol. 2012, 78: 6095-6102. 10.1128/AEM.01018-12.PubMedPubMed CentralView Article
- Fierer N, Lauber CL, Ramirez KS, Zaneveld J, Bradford MA, Knight R: Comparative metagenomic, phylogenetic and physiological analyses of soil microbial communities across nitrogen gradients. ISME J. 2012, 6: 1007-1017. 10.1038/ismej.2011.159.PubMedPubMed CentralView Article
- Groffman PM, Teidje JM: Denitrification hysteresis during wetting and drying cycles in soil. Soil Sci Soc Am J. 1988, 52: 1626-1629. 10.2136/sssaj1988.03615995005200060022x.View Article
- Kandeler E, Brune T, Enowashu E, Dörr N, Guggenberger G, Norbert L, Philippot L: Response of total and nitrate-dissimilating bacteria to reduced N deposition in a spruce forest soil profile. FEMS Microbiol Ecol. 2006, 67: 444-454.View Article
- Ma WK, Bedard-Haughn A, Siciliano SD, Farrell RE: Relationship between nitrifier and denitrifier community composition and abundance in predicting nitrous oxide emissions from ephemeral wetland soils. Soil Biol Biochem. 2008, 40: 1114-1123. 10.1016/j.soilbio.2007.12.004.View Article
- Dandie CE, Wertz S, Leclair C, Goyer C, Burton DL, Patten CL, Zebarth BJ, Trevors JT: Abundance, diversity and functional gene expression of denitrifier communities in adjacent riparian and agricultural zones. FEMS Microbiol Ecol. 2011, 77: 69-82. 10.1111/j.1574-6941.2011.01084.x.PubMedView Article
- Cornelis P, Badillis J: A survey of TonB-dependent receptors in fluorescent pseudomonads. Environ Microbiol Rep. 2009, 1: 256-262. 10.1111/j.1758-2229.2009.00041.x.PubMedView Article
- Folschweiller N, Schalk IJ, Celia H, Kieffer B, Abdallah MA, Pattus F: The pyoverdin receptor FpvA, a TonB-dependent receptor involved in iron update by Pseudomonas aeruginosa (review). Mol Membr Biol. 2000, 17: 123-133. 10.1080/09687680050197356.PubMedView Article
- Qian Y, Shi L, Tien M: SO2907, a putative TonB-dependent receptor, is involved in dissimilatory iron reduction by Shewanella oneidensis straing MR-1. J Biol Chem. 2011, 286: 33973-33980. 10.1074/jbc.M111.262113.PubMedPubMed CentralView Article
- Hauck S, Benz M, Brune A, Schink B: Ferrous iron oxidation by denitrifying bacteria in profundal sediments of a deep lake (Lake Constance). FEMS Microbiol Ecol. 2001, 37: 127-134. 10.1111/j.1574-6941.2001.tb00860.x.View Article
- Philippot L, Hallin S, Schloter M: Ecology of denitrifying prokaryotes in agricultural soil. Adv Agron. 2007, 96: 249-305.View Article
- Henry S, Bru D, Stres B, Hallet S, Philippot L: Quantitative detection of the nosZ gene, encoding nitrous oxide reductase, and comparison of the abundances of 16S rRNA, narG, nirK, and nosZ genes in soils. Appl Environ Microbiol. 2006, 72: 5181-5189. 10.1128/AEM.00231-06.PubMedPubMed CentralView Article
- Tiedje JM: Ecology of denitrification and dissimilatory nitrate reduction to ammonium. Biology of Anaerobic Microorganisms. Edited by: Zehnder AJB. 1988, New York, NY: John Wiley & Sons, Inc, 179-244.
- He Q, He Z, Joyner DC, Joachimiak M, Price MN, Yang ZK, Yen H-CB, Hemme CL, Chen W, Fields MW: Impact of elevated nitrate on sulfate-reducing bacteria: a comparative study of Desulfovibrio vulgaris. ISME J. 2010, 4: 1386-1397. 10.1038/ismej.2010.59.PubMedView Article
- Zhou Z, 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.PubMedView Article
- Seifritz C, Daniel SL, Göbner A, Drake HL: Nitrate as a preferred electron sink for the acetogen Clostridium thermoaceticum. J Bacteriol. 1993, 175: 8008-8013.PubMedPubMed Central
- Bartlett AF, Leff MA: The effects of N:P ration and nitrogen form on four major freshwater bacterial taxa in biofilms. Can J Microbiol. 2010, 56: 32-43. 10.1139/W09-099.View Article
- Kragelund C, Kong Y, van der Waarde J, Thelen D, Eikelboom D, Tandoi V, Thomsen VR, Nielsen PH: Ecophysiology of different filamentous Alphaproteobacteria in industrial wastewater treatment plant. Microbiol. 2006, 152: 3003-3012. 10.1099/mic.0.29249-0.View Article
- Ward NL, Challacombe JF, Janssen PH, Henrissat B, Coutinho PM, Wu M, Xie G, Haft DH, Sait M, Badger J: Three genomes from the phylum Acidobacteria provide insight into the lifestyles of these microorganisms in soils. Appl Environ Microbiol. 2009, 75: 2046-2056. 10.1128/AEM.02294-08.PubMedPubMed CentralView Article
- Pinhassi J, Berman T: Differential growth response of colony forming α- and γ-Proteobacteria in dilution culture and nutrient addition experiments from lake Kinneret (Israel), the eastern Mediterranean Sea, and the Gulf of Eilat. Appl Environ Microbiol. 2003, 69: 199-211. 10.1128/AEM.69.1.199-211.2003.PubMedPubMed CentralView Article
- Bodelier PLE, Kamst M, Meima-Franke M, Stralis-Pavese N, Bodrossy L: Whole-community genome amplification (WCGA) leads to compositional bias in methane-oxidizing communities as assessed by pmoA-based microarray analyses and QPCR. Environ Microbiol Rep. 2009, 1: 434-441. 10.1111/j.1758-2229.2009.00066.x.PubMedView Article
- Yilmaz S, Allgaier M, Hugenholtz P: Multiple displacement amplification compromises quantitative analysis of metagenomes. Nat Methods. 2010, 7: 943-944. 10.1038/nmeth1210-943.PubMedView Article
- Kim K-H, Bae J-W: Amplification methods bias metagenomic libraries of uncultured single-stranded and double-stranded DNA viruses. Appl Environ Microbiol. 2011, 77: 7663-7668. 10.1128/AEM.00289-11.PubMedPubMed CentralView Article
- McGrady-Steed J, Harris PM, Morin PJ: Biodiversity regulates ecosystem predictability. Nature. 1997, 390: 162-165. 10.1038/36561.View Article
- Wertz S, Degrange V, Prosser JI, Poly F, Commeaux C, Guillaumaud N, Le Roux X: Decline of soil microbial diversity does not influence the resistance and resilience of key soil microbial functional groups following a model disturbance. Environ Microbiol. 2007, 9: 2211-2219. 10.1111/j.1462-2920.2007.01335.x.PubMedView Article
- Naeem S, Li S: Biodiversity enhances ecosystem reliability. Nature. 1997, 390: 507-509. 10.1038/37348.View Article
- Moldan B, Cerny J: Biogeochemistry of Small Catchments. 1994, West Sussex, England: John Wiley & Sons Ltd
- Dinsdale E, Pantos O, Smriga S, Edwards RA, Angly F, Wegley L, Hatay M, Hall D, Brown E, Haynes M: Microbial ecology of four coral atolls in the Northern Line Islands. PLoS One. 2008, 3: e1584-10.1371/journal.pone.0001584.PubMedPubMed CentralView Article
- Edwards RA, Rodriguez-Brito B, Wegley L, Haynes M, Breitbart M, Peterson DM, Saar MO, Alexander S, Alexander EC, Rohwer F: Using pyrosequencing to shed light on deep mine microbial ecology. BMC Genomics. 2006, 7: 57-10.1186/1471-2164-7-57.PubMedPubMed CentralView Article
- Vega Thurber R, Willner-Hall D, Rodriguez-Mueller B, Desnues C, Edwards RA, Angly F, Dinsdale E, Kelly L, Rohwer F: Metagenomic analysis of stressed coral holobionts. Environ Microbiol. 2009, 11: 2148-2163. 10.1111/j.1462-2920.2009.01935.x.PubMedView Article
- Philippot L, Hallin S: Finding the missing link between diversity and activity using denitrifying bacteria as a model functional community. Curr Opin Microbiol. 2005, 8: 234-239. 10.1016/j.mib.2005.04.003.PubMedView Article
- Parks DH, Beiko RG: Identifying biologically relevant differences between metagenomic communities. Bioinformatics. 2010, 26: 715-721. 10.1093/bioinformatics/btq041.PubMedView Article
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