Ecophysiology and Comparative Genomics of Nitrosomonas mobilis Ms1 Isolated from Autotrophic Nitrifying Granules of Wastewater Treatment Bioreactor

Ammonia-oxidizing bacteria (AOB), which oxidize ammonia to nitrite in the first step of nitrification, play an important role in biological wastewater treatment systems. Nitrosomonas mobilis is an important and dominant AOB in various wastewater treatment systems. However, the detailed physiological and genomic properties of N. mobilis have not been thoroughly investigated because of limited success isolating pure cultures. This study investigated the key physiological characteristics of N. mobilis Ms1, which was previously isolated into pure culture from the nitrifying granules of wastewater treatment bioreactor. The pure culture of N. mobilis Ms1 was cultivated in liquid mineral medium with 30 mg-N L^-1 (2.14 mM) of ammonium at room temperature under dark conditions. The optimum growth of N. mobilis Ms1 occurred at 27°C and pH 8, with a maximum growth rate of 0.05–0.07 h^-1, which corresponded to a generation time of 10–14 h. The half saturation constant for ammonium uptake rate and the maximum ammonium uptake rate of N. mobilis Ms1 were 30.70 ± 0.51 μM NH₄⁺ and 0.01 ± 0.002 pmol NH₄⁺ cells^-1 h^-1, respectively. N. mobilis Ms1 had higher ammonia oxidation activity than N. europaea in this study. The oxygen uptake activity kinetics of N. mobilis Ms1 were K_m(O2) = 21.74 ± 4.01 μM O₂ and V _max(O2) = 0.06 ± 0.02 pmol O₂ cells^-1 h^-1. Ms1 grew well at ammonium and NaCl concentrations of up to 100 and 500 mM, respectively. The nitrite tolerance of N. mobilis Ms1 was extremely high (up to 300 mM) compared to AOB previously isolated from activated sludge and wastewater treatment plants. The average nucleotide identity between the genomes of N. mobilis Ms1 and other Nitrosomonas species indicated that N. mobilis Ms1 was distantly related to other Nitrosomonas species. The organization of the genes encoding protein inventory involved in ammonia oxidation and nitrifier denitrification processes were different from other Nitrosomonas species. The current study provides a needed physiological and genomic characterization of N. mobilis-like bacteria and a better understanding of their ecophysiological properties, enabling comparison of these bacteria with other AOB in wastewater treatment systems and natural ecosystems.

Introduction

Nitrification, the oxidation process of ammonia and nitrite followed by denitrification, is an important process in the nitrogen cycle of natural ecosystems and in biological wastewater treatment systems. This process is mainly performed by two groups of nitrifying microbes, ammonia-oxidizing bacteria and archaea (AOB and AOA), which convert ammonia (NH₃) to nitrite (NO₂^-) in two steps, and nitrite-oxidizing bacteria (NOB) that oxidize the nitrite (NO₂^-) to nitrate (NO₃^-). Recently, some species belonging to lineage II of the genus Nitrospira in the NOB group have been reported as complete ammonia oxidizing bacteria (comammox) that perform the complete nitrification of ammonia to nitrate (Daims et al., 2015; van Kessel et al., 2015).

Because of the important role of nitrification in both the natural environment and wastewater treatment systems, researchers have long been trying to understand the ecophysiology of nitrifying microorganisms. Studies on nitrifying microbes in wastewater treatment systems and the natural environment using molecular methods have indicated that Nitrosomonas species are the main AOB populations in wastewater treatment bioreactors (Tsuneda et al., 2003; Chen and Wong, 2004; Mota et al., 2005; Wells et al., 2009), as well as in diverse natural environments including freshwater, coastal and brackish water regions (Stehr et al., 1995; Zhang et al., 2015). Among Nitrosomonas species, Nitrosomonas europaea/Nitrosomonas mobilis cluster 7 was dominant in wastewater treatment bioreactors loaded with high concentrations of ammonia and nitrite, whereas Nitrosomonas oligotropha cluster 6a was dominant in systems with a lower ammonia environment (Suwa et al., 1994, 1997; Bollmann and Laanbroek, 2001; Limpiyakorn et al., 2005, 2007; Tan et al., 2008). Nitrosomonas mobilis-like bacteria were codominant with N. europaea-eutropha- and N. oligotropha-like bacteria in the biofilm’s microbial populations in wastewater treatment bioreactors (Gieseke et al., 2003). In a study of nitrifying granules, N. mobilis-like bacteria were predominant from the nascent stage into maturity where N. europaea- and N. oligotropha-like bacteria were also present (Matsumoto et al., 2010). N. mobilis was also dominant in various wastewater treatment bioreactors (Juretschko et al., 1998; Chen and Wong, 2004; Mota et al., 2005). Because of this environmental distribution, N. mobilis has received a great deal of attention in the field of wastewater treatment.

The first isolation of Nitrosococcus mobilis from brackish water had been reported by Koops et al. (1976). It was later proposed that Nitrosococcus mobilis should be moved into the genus Nitrosomonas (Head et al., 1993). The original isolates (strains Nc2^T, Nc3, Nc8) of N. mobilis were from brackish water, but a few environmental clones and pure strains (Nm 93, Nm104, Nm107) of N. mobilis have also been isolated from activated sludge samples (Koops and Harms, 1985; Juretschko et al., 1998; Purkhold et al., 2000). Studies of pure cultures and environmental clones of N. mobilis have been included in some phylogenetic analyses (Koops and Harms, 1985; Head et al., 1993; Pommerening-Roser et al., 1996; Juretschko et al., 1998; Purkhold et al., 2000; Cantera and Stein, 2007) and investigations of gene expression response to copper and zinc (Radniecki and Ely, 2008, 2011). According to Campbell et al. (2011), Nitrosococcus mobilis was published as Nitrosomonas mobilis with the type strain Nc2. However, to date, no representative strains of N. mobilis suitable for examination of their physiological and genomic characteristics have been reported and detailed information regarding the physiological and genomic characterization of N. mobilis is still lacking because of the limited success in isolating it into pure cultures.

Recently, the pure culture of Nitrosomonas mobilis Ms1 has been successfully isolated from the autotrophic nitrifying granules by selective isolation using a cell-sorting system (Fujitani et al., 2015). These nitrifying granules were produced in the aerobic upflow fluidized bed reactor to treat inorganic wastewater and exhibited an effective ammonia removal rate (Tsuneda et al., 2003). During the granule formation, Nitrosomonas species and Nitrosomonas mobilis act as an important and dominant AOB population (Tsuneda et al., 2003; Matsumoto et al., 2010). To accomplish an ecophysiological study of N. mobilis and related Nitrosomonas species, in this study we investigated key physiological characteristics such as temperature and pH ranges, growth rate, NaCl tolerance, ammonium and oxygen uptakes activity kinetics, ammonium substrate inhibition and nitrite tolerance of N. mobilis Ms1. In addition, genome sequencing and annotation of the genes were conducted. The genes encoding proteins involved in ammonia oxidation and nitrogen oxide metabolism were also identified. This study is the first physiological and genomic characterization of Nitrosomonas mobilis and provides important information regarding N. mobilis-like strains.

Materials and Methods

Cell Cultures, Media, and Cultivation

Nitrosomonas mobilis Ms1 isolated from nitrifying granules (Fujitani et al., 2015) was kept in liquid culture of mineral medium containing 30 mg-N L^-1 of ammonium substrate (NH₄Cl) with the following components per liter of distilled water: NaCl (0.116 g), MgSO₄⋅7H₂O (0.4 g), CaCl₂⋅2H₂O (0.073 g), KCl (0.038 g), KH₂PO₄ (0.034 g), FeCl₂ (0.002 g), EDTA (0.0043 g), MnCl₂⋅4H₂O (0.1 mg), CoCl₂⋅6H₂O (0.024 mg), NiCl₂⋅6H₂O (0.024 mg), CuCl₂⋅2H₂O (0.017 mg), ZnCl₂ (0.068 mg), Na₂WO₄⋅2H₂O (0.033 mg), Na₂MoO₄ (0.024 mg), and H₃BO₃ (0.062 mg). The pH of the culture media was adjusted to 8.0 by NaHCO₃ (0.84 g L^-1), and phenol red (0.4 w/v %) was used as the pH indicator. The cultures were incubated under static and dark conditions at room temperature. For physiological and kinetics studies, mineral media with different ammonium concentrations was used and phenol red was omitted. To determine the effect of NaCl concentration, mineral media without NaCl was used. Nitrosomonas europaea Winogradsky 1892 (NBRC 14298) was purchased from the Biological Resource Center (NBRC), National Institute of Technology and Evaluation (NITE). The HEPES medium 829 as described in the manual NBRC No. 14298 was used as the growth medium in this study. For the activity experiment, media with separately prepared different concentrations of ammonium substrate [(NH₄)₂SO₄] was used. The stock cultures of N. mobilis Ms1 and N. europaea were periodically checked for their culture conditions (pH, ammonium and produced nitrite concentrations), cell growth and morphologies, and transferred into fresh culture media when the nitrite concentrations in media reached approximately 200 mg-N L^-1.

Fluorescence Microscopy

The growth and morphology of the cell cultures during the experiments were observed by fluorescence microscopy. Briefly, 10 μL cell samples were applied to each well of 12-well glass slides and allowed to dry. The samples were then dried and stained with SYTOX Green nucleic acid stain (Life Technologies, Molecular Probes, Eugene, OR, USA) and observed under a fluorescence microscope (Zeiss Axioskop 2plus, lens Zeiss Plan-APOCHROMAT 100×/1.4 oil, Carl Zeiss, Oberkochen, Germany). To count the cell numbers, 1 mL of culture samples were sonicated at intensity of 4 for 1 min (Sonifier II model, Branson, Danbury, CT, USA) and heated at 95°C for 10 min, after which, 1 μL cell samples were applied to each well of the 12-well glass slides. The cell numbers were quantitatively analyzed from each well using a microscopic direct counting method. The mean cell numbers were determined from triplicate wells for each sample.

Measurement of Ammonium and Nitrite Concentrations

The samples for measurement were collected by filtration through a 0.22 μm Micropore filter (Millex, Merck Millipore, Darmstadt, Germany), after which the ammonium and nitrite concentrations of collected samples were measured colorimetrically with a modified indophenol reaction (Kandeler and Gerber, 1988) at an absorbance wavelength of 630 nm and Griess Reagent (Griess-Romijn van Eck, 1966) at an absorbance wavelength of 550 nm, respectively, using a Powerscan HT microplate spectrophotometer (BioTek, Winooski, VT, USA).

Effect of Temperature, pH and NaCl Concentration on the Growth of Ms1

Batch cultures experiments were conducted to investigate the effects of temperature, pH and NaCl concentrations on the growth of N. mobilis Ms1. The culture sample was concentrated by centrifugation at 4,800 × g and 23°C for 30 min. The sample pellet was then mixed with fresh mineral medium containing 30 mg-N L^-1 (2.14 mM) initial ammonium substrate (NH₄Cl) and subjected to weak sonication. To investigate the effect of NaCl concentration, fresh mineral media containing different NaCl concentrations (0, 50, 100, 250, 500, 750, and 1,000 mM) were used. To investigate the effects of pH, the culture media were adjusted to a pH of 4, 5, 6, 7, 8, 9, 11, or 13 by NaOH and HCl, then mixed with the sample pellet and subjected to weak sonication. Next, the cultures were incubated in rotatory shaker incubators at different temperatures (7–47°C, pH 8.0), pHs (pH 4–13, 27°C) and NaCl concentrations (NaCl 0–1,000 mM, 27°C, pH 8.0) for 24 h. Aliquots of samples (1–2 mL) were taken out at the start of the incubation period (0 h), 1 h (for the temperature experiments because the culture samples were assumed to have adapted to each temperature at this point) and the end of the incubation (24 h), then collected by filtration through a 0.22 μm Micropore filter (Millex). The growth of N. mobilis Ms1 was measured based on the nitrite concentrations of the collected samples. All experiments were conducted in triplicate.

Maximum Specific Growth Rate (μ_max)

The growth rate of N. mobilis Ms1 was studied by batch culture of 5 mL aliquots from pure cultures of N. mobilis Ms1 with 100 mg-N L^-1 (7.14 mM) initial ammonium substrate in 100 mL fresh mineral media using 500 mL experimental flasks. The initial pH value of the batch cultures was 8.0 and the initial cell concentrations were approximately 1.64 × 10⁴–3.73 × 10⁵ cells mL^-1. The cultures were incubated at 27°C on a rotatory shaker incubator for 1 week until all ammonium was consumed. During the incubation period, the pH of the culture was kept constant at around 8.0 by adding sterile NaHCO₃. The aliquots of samples (1–2 mL) were taken out daily at the same time from the start until the end of the incubation period and collected by filtering through a 0.22 μm Micropore filter (Millex) to determine the ammonium and nitrite concentrations. The cell numbers were also determined by direct microscopic counting with Sytox green staining. The specific growth rate (μ) and generation time (g) were then calculated using the following equations:

$$\mu =\frac{\text{Ln}({\text{X}}_{\text{2}}{\text{-X}}_{\text{1}})}{({\text{t}}_{\text{2}}{\text{-t}}_{\text{1}})}\left(1\right)$$

$$g\text{=}\frac{\text{Ln}(\text{2})}{\mu }\left(2\right)$$

where X is the number of cells and t is the time (Belser and Schmidt, 1980). All experiments were conducted in duplicate.

Activity Kinetics

The activity kinetics of N. mobilis Ms1 were investigated by measuring the ammonium and oxygen uptake activities. To determine the ammonium uptakes, short-term incubation in a batch culture was conducted. The culture sample of N. mobilis Ms1 was concentrated by centrifugation at 4,800 × g and 23°C for 30 min. The sample pellet was mixed with 100 mL of fresh mineral medium containing 7.0 mg-N L^-1 (500 μM) of ammonium and subjected to weak sonication. The cell concentrations of the experimental cultures were approximately 1.31 × 10⁷–2.82 × 10⁷ cells mL^-1. The ammonium uptake activity kinetics of N. europaea were also studied for comparison with those of N. mobilis Ms1. The culture sample of N. europaea was concentrated as in N. mobilis Ms1 and mixed with 100 mL fresh mineral medium containing 5.0 mg-N L^-1 (357.14 μM). The pH of the media was then adjusted to around 8.0 by NaHCO₃. Next, samples were incubated at 27°C in a rotatory shaker incubator for about 3–6 h until all ammonium was consumed, during which time aliquots of samples (1–2 mL) were taken out every 10 min, filtered through a 0.22 μm Micropore filter (Millex), and measured for ammonium concentration. The cell numbers in the aliquots of the samples collected at 0 h were also counted. The ammonium concentrations obtained over time and the ammonium uptake rates were fitted to the Michaelis–Menten equation, which is as follows:

$$V=\frac{(V_{\text{max}({\text{NH}}_{\text{4}}^{\text{+}})\times }[{\text{NH}}_{\text{4}}^{\text{+}}])}{(K_{\text{m}({\text{NH}}_{\text{4}}^{\text{+}})}\text{+}[{\text{NH}}_{\text{4}}^{\text{+}}])}\left(3\right)$$

where V is the ammonium uptake rate, V _{max ($N{H}_4^{+}$)} is the maximum ammonium uptake rate, K_{m ($N{H}_4^{+}$)} is the half saturation constant for ammonium uptake, and [NH₄⁺] is the ammonium concentration. V _{max ($N{H}_4^{+}$)} was calculated as the ammonium uptake rate per cell concentration. All experiments were conducted in duplicate. The specific affinity for ammonium was calculated using the ratio of kinetics values from ammonium uptake activity (i.e., V _{max ($N{H}_4^{+}$)} × [K_{m ($N{H}_4^{+}$)}]^-1) (Laanbroek and Gerards, 1993).

An O₂ microsensor (OX-MR13831, Unisense, Aarhus, Denmark) was used to measure the oxygen uptake of N. mobilis Ms1. The chamber and sensor were assembled in the water bath, and the temperature of the water bath was set to 30°C, at which time the sensor was calibrated. Next, 2 mL aliquots from N. mobilis Ms1 culture containing with 2.35 × 10⁶–5.20 × 10⁶ cells mL^-1 were added into the chamber with a glass-coated magnet stirrer and the O₂ sensor was immersed in the sample. When the O₂ concentration was stable, measurement of the oxygen levels in the cell culture started. The data (oxygen concentrations over time) obtained by the O₂ sensor were analyzed and smoothed using the SigmaPlot software (SigmaPlot 13.0, Systat software GmbH, Erkrath, Germany). Subsamples from the cell culture were used to count the cell numbers by direct microscopy after Sytox green staining. K_{m (O2)} and V _{max (O2)} were calculated from the measured oxygen uptake rate and the counted cell numbers using the Michaelis–Menten equation:

$$V=\frac{(V_{\text{max}({\text{O}}_{\text{2}})}\times [{\text{O}}_{\text{2}}])}{(K_{\text{m}({\text{O}}_{\text{2}})}\text{+}[{\text{O}}_{\text{2}}])}\left(4\right)$$

where V is the oxygen uptake rate, V _{max (O2)} is the maximum oxygen uptake rate, K_{m (O2)} is the half saturation constant for oxygen uptake rate, and [O₂] is the oxygen concentration. All experiments were conducted in triplicate.

Ammonium and Nitrite Tolerance

To investigate the ammonium and nitrite tolerance of N. mobilis Ms1, batch experiments were conducted using different ammonium and nitrite concentrations. N. mobilis Ms1 was cultivated in 100 mL of fresh mineral media using 500 mL flasks containing different initial ammonium concentrations (10, 50, 100, 200, 300, 400, and 500 mM) and nitrite concentrations (0, 5, 10, 50, 100, 200, 300, 400, and 500 mM) in which an initial ammonium concentration of 5 mM was contained. The pH of all media was adjusted to 8.0 by NaHCO₃. Cultures were incubated at 27°C in a rotatory incubator until all ammonium was consumed. During the experiment, aliquots of samples (1–2 mL) were collected at the start of the incubation period and every other day from 10 to 100 mM ammonium and 0–100 mM nitrite cultures, and every 4th day from 200 to 500 mM ammonium and nitrite cultures by filtering with a 0.22 μm Micropore filter (Millex). The initial ammonium concentrations and produced nitrite concentrations of the collected samples were measured colorimetrically by indophenol and Griess Reagent tests, respectively. During the incubation period, the cell growth was observed by Sytox green fluorescence microscopic examination of the collected samples and the pHs of the media were kept constant at around 8.0 by adding sterile NaHCO₃. All experiments were conducted in duplicate.

Genome Sequencing, Assembly and Gene Annotation

A draft genome sequence of strain Ms1 was performed as follows. Briefly, genomic DNA was extracted from a pure culture of strain Ms1 by using NucleoSpin^® Tissue, a DNA extraction kit (Takara Bio, Otsu, Japan) according to the manufacturer’s instructions, and a Nextera XT paired-end (300–1,000 bp) was prepared from the extracted DNA. The library was then sequenced on an Illumina MiSeq instrument with V2 chemistry (2 × 250 bp reads) at an expected coverage of 120× per genome. Raw sequence reads were merged with SeqPrep with concurrent removal of sequencing adaptors, followed by quality filtering and trimming of the unmerged reads with Nesoni version 0.112. Both merged and processed unmerged reads were combined for assembly using SPAdes version 2.5.0 (Bankevich et al., 2012), followed by manual improvement of the assembly, as described previously (Sekiguchi et al., 2015). The final draft genome assembly of the Ms1 genome consists of 113 contigs. The largest and N50 contig sizes are 251,952 and 65,925 bp, respectively. The total assembly size is 3,083,004 bp. Annotation was performed with MicroScope microbial genome annotation and analysis platform (Vallenet et al., 2013). Coding sequences (CDS) were automatically predicted, annotated and categorized by clusters of orthologous groups (COGs) using MicroScope platform. The contigs of genome sequences of N. mobilis Ms1 have been deposited into European Nucleotide Archive (ENA) database under the accession number FMWO01000001-FMWO01000112 (BioProject number PRJEB15545).

Average Nucleotide Identity Analysis

The average nucleotide identity (ANI) analysis was conducted to determine whether N. mobilis Ms1 represents distant AOB species (Konstantinidis and Tiedje, 2005). The genome sequence of Nitrosomonas mobilis Ms1 was compared with the genome sequences of N. europaea ATCC 19718, N. eutropha C 71, Nitrosomonas sp. AL212, and Nitrosomonas sp. Is79A3. The ANI values between Ms1 and other genomes were calculated using EzGenome provided online by Jongsik Chun, Chunlab, Inc¹.

Results and Discussion

Physiological Characteristics of N. mobilis Ms1

Effect of Temperature, pH and NaCl Concentration

Batch experiments were conducted to investigate the effect of temperature (Figure 1A), pH (Figure 1B) and NaCl concentration (Figure 1C) on the growth of N. mobilis Ms1. The growth and ammonia oxidation activity were confirmed by the nitrite concentrations of the culture samples. N. mobilis Ms1 has a temperature range of 17–37°C, with an optimum temperature of 27°C, which is similar to the optimal ranges of other pure culture AOB strains such as Nitrosomonas europaea ATCC 25978^T (25–29°C), Nitrosomonas eutropha C-91^T (30°C), Nitrosococcus mobilis Nc2^T (25–30°C) in the Nitrosomonas europaea/Nitrosomonas mobilis lineage, as well as Nitrosomonas sp. strain AL212 (25°C) in the Nitrosomonas oligotropha lineage, Nitrosomonas sp. JPCCT2 (28°C) in the Nitrosomonas communis lineage and Nitrosomonas stercoris KYUHI-S^T (25°C) in an unclassified cluster (Table 1) (Koops et al., 1976, 1991; Suwa et al., 1997; Tokuyama et al., 1997; Itoh et al., 2013; Nakagawa and Takahashi, 2015). N. mobilis Ms1 oxidized well at pH 8.0, while other Nitrosomonas species showed their optimal oxidation at pH values ranging from 7.2 to 8.2 (Table 1). Similarly to N. europaea and N. eutropha, N. mobilis Ms1 required no salt and showed NaCl tolerance up to 500 mM (Table 1). Growth temperature and pH ranges, and salt requirement of each strain reflect the diversity and habitat of Nitrosomonas species in both man-made and natural ecosystems (Jones et al., 1988; Koops et al., 1991, 2006; Koops and Pommerening-Roser, 2001; Cortes-Lorenzo et al., 2015).

FIGURE 1

FIGURE 1. Effect of temperature, pH and NaCl concentration on the growth of N. mobilis Ms1. The nitrite concentrations of N. mobilis Ms1 after 24 h of incubation at different temperatures (A), pHs (B), and NaCl concentrations (C). Bars are the standard errors (n = 3).

TABLE 1

TABLE 1. Physiological characteristics of pure cultures of N. mobilis Ms1 and some AOB species.

Growth Rate and Activity Kinetics

The growth rate of N. mobilis Ms1 was studied in batch cultures to calculate the maximum specific growth rate (μ_max) and generation time (g). The initial cell concentrations were 4.07 × 10⁴ ± 9.87 × 10³ cells mL^-1, and the highest number of cells reached 3.53 × 10⁶ ± 4.12 × 10⁵ cells mL^-1 on day 5 of incubation. At this time, almost all ammonium in the cultures was consumed, the produced nitrite concentrations increased and ammonium concentrations decreased (Figure 2). Under the optimum conditions, the maximum specific growth rate (μ_max) of N. mobilis Ms1 cells reached 0.06 ± 0.01 h^-1 and the generation time (g) was 11.87 ± 2.33 h, which is in the range of previous reports for Nitrosomonas species within the N. europaea/N. mobilis lineage, as Nitrosomonas europaea and Nitrosococcus mobilis had generation times of 10–14 and 12–13 h, respectively (Table 1) (Koops et al., 1976; Belser and Schmidt, 1980). Generally, members in the N. europaea/N. mobilis lineage have a shorter generation time than other ammonia oxidizers. For example, members belonging to the N. oligotropha lineage and Nitrosospira lineage had generation times of 28–49 and 18–115 h, respectively, while the newly isolated highly ammonia-tolerant AOB strain, N. stercoris KYUHI-S^T, belonging to an unclassified cluster, had a generation time of 24 h (Suwa et al., 1994; Bollmann and Laanbroek, 2001; Nakagawa and Takahashi, 2015).

FIGURE 2

FIGURE 2. Growth of N. mobilis Ms1 determined by measurement of time courses of ammonium concentrations (triangle), nitrite concentrations (circle) and cell numbers (rectangle) during incubation for 5 days. The maximum growth rate calculated from the increased number of cells was observed on days 3 and 4 (open rectangle).

The activity kinetics of N. mobilis Ms1 were investigated using the ammonium and oxygen uptake rates. To obtain a comparable data set for ammonia oxidation activity of N. mobilis Ms1, the same experiment was also conducted for N. europaea. The K_{m ($N{H}_4^{+}$)} and V _{max ($N{H}_4^{+}$)} values determined from the ammonium uptake rates of N. mobilis Ms1 and N. europaea were 30.70 ± 0.51 μM NH₄⁺ and 0.01 ± 0.002 pmol NH₄⁺ cells^-1 h^-1, and 55.43 ± 4.92 μM NH₄⁺ and 0.0009 ± 0.00003 pmol NH₄⁺ cells^-1 h^-1 (n = 2), respectively (Figure 3). According to the calculated specific affinity from the kinetics values of ammonium uptake activities, N. mobilis Ms1 has higher substrate affinity (0.33 ± 0.06 nL NH₄⁺ cell^-1 h^-1) compared with N. europaea (0.016 ± 0.0008 nL NH₄⁺ cell^-1 h^-1). This result is consistent with a previous study on microbial community structure in nitrifying granules, where the population of N. mobilis was larger compared with N. europaea when the ammonia concentration in the reactor reached almost zero (Matsumoto et al., 2010).

FIGURE 3

FIGURE 3. Representative data describing ammonium uptake activities of N. mobilis Ms1 and N. europaea. The best-fit curve was described according to the Michaelis–Menten equation to obtain K_{m ($N{H}_4^{+}$)} and V _{max ($N{H}_4^{+}$)} values.

Based on our knowledge of N. mobilis Ms1, this strain has a high ammonia oxidation activity, i.e., Ms1 consumes ammonium quickly during both the cultivation period of stock cultures and the batch culture incubation for growth and activity measurements. These cultural and physiological findings were proved by the same experiment for ammonia oxidation activity of N. mobilis Ms1 and N. europaea. The V _{max ($N{H}_4^{+}$)} values of N. mobilis Ms1 (0.01 ± 0.002 pmol NH₄⁺ cells^-1 h^-1) were higher than those of N. europaea (0.0009 ± 0.00003 pmol NH₄⁺ cells^-1 h^-1). These finding are also supported by evidence of cultivation experiments for both strains, in which the ammonium concentration of 5.0 mg-N L^-1 (357.14 μM) was completely consumed by N. mobilis Ms1 within an incubation time of 3 h, but consumed by N. europaea in 8 h, while their cell numbers were nearly same at 2.07 × 10¹⁰–9.55 × 10¹⁰ cells L^-1. However, the activity kinetics of the ammonia oxidizers varied, even among the same species, for example, the activity of N. europaea ranged from 0.001 to 0.023 pmol cells^-1 h^-1 (Belser and Schmidt, 1980; Prosser, 1989).

The kinetics values, K_{m (O2)} and V _{max (O2)}, for the oxygen uptake rate of N. mobilis Ms1 were also determined and the results showed values of 21.74 ± 4.01 μM O₂ and 0.06 ± 0.02 pmol O₂ cells^-1 h^-1 (n = 3), respectively (Figure 4). This K_{m (O2)} value for N. mobilis Ms1 is comparable to those reported in a previous study for oxygen consumption kinetics of N. europaea ATCC 19178^T at a high growth rate and high oxygen concentration [K_{m (O2)} = 3.0–14.9 μM O₂] (Laanbroek and Gerards, 1993). The respiratory cytochrome c oxidases of the nitrifiers are responsible for maintaining their electron chain and adapting to the environment at different oxygen levels (Klotz and Stein, 2011). N. europaea and N. mobilis Ms1 possess the cytochrome aa3 type oxidase, which functions as the low affinity O₂ reductase whereas N. eutropha possesses cytochrome cbb3 type oxidase, which functions as the high affinity O₂ reductase, in addition to cytochrome aa3 and bo3 type oxidases (Stein et al., 2007; Klotz and Stein, 2011). It is likely that N. mobilis Ms1 might not adapt to an environment at different oxygen levels.

FIGURE 4

FIGURE 4. Representative data describing oxygen uptake of N. mobilis Ms1. The best-fit curve was described according to the Michaelis–Menten equation to obtain K_m (O₂) and V_{max (O2)} values.

Ammonium and Nitrite Tolerance

N. mobilis Ms1 exhibits ammonia oxidizing ability at the concentrations of ammonium up to 100 mM (1,400 mg-N L^-1) (Figure 5A). In tests of nitrite tolerance, although inhibition of ammonia oxidation was observed in cultures with concentrations of nitrite of 50 mM and higher (Figure 5B), the initially provided ammonium (5 mM) was finally consumed in cultures with nitrite concentrations of up to 300 mM. Taken together, N. mobilis Ms1 had high ammonium and nitrite tolerance, although the strain was enriched from the nitrifying granules of a low ammonium influent bioreactor and could grow in culture media with only 30 mg-N L^-1 (2.14 mM) of ammonium substrate. These characteristics are consistent with those reported in a previous study by Juretschko et al. (1998), where N. mobilis-like bacteria were dominant in sludge with high ammonium concentrations of up to 5,000 mg-N L^-1 (357.14 mM) in a wastewater treatment plant. Among members of the genus Nitrosomonas, Nitrosomonas nitrosa isolated from a eutrophic environment exhibited the same ammonium tolerance as N. mobilis Ms1, of up to 100 mM (Koops et al., 1991). In contrast, Nitrosomonas sp. strain AL212 belonging to the N. oligotropha lineage isolated from activated sludge exhibited the maximum ammonium tolerance of 10.7 mM (Suwa et al., 1997), which is about 10 times lower than that of N. mobilis Ms1 (100 mM). The results of the pure culture study also support the previous findings for AOB communities in which the N. oligotropha cluster was predominant over the N. europaea-N. mobilis cluster in activated sludge with low ammonium concentrations (Limpiyakorn et al., 2005, 2007). Within Nitrosomonas cluster 7, Nitrosococcus mobilis Nc2, which is phylogenetically similar to N. mobilis Ms1, was tolerant to ammonium concentration at up to 300 mM (Koops et al., 1990), while N. europaea and N. eutropha-like species were tolerant of up to 400 and 600 mM of ammonium, respectively (Koops et al., 1991). Nitrosomonas stercoris KYUHI-S^T isolated from compost (Nakagawa and Takahashi, 2015) exhibited the highest ammonium tolerance (1,000 mM) among Nitrosomonas strains (Table 1). Although the nitrite tolerance of ammonia oxidizers was not surprising because of the accumulation of nitrite during cultivation and enrichment, the 300 mM of nitrite tolerance of N. mobilis Ms1 was extremely high among strains isolated from the activated sludge and wastewater treatment plants. For example, the ammonia monooxygenase (AMO) activity of N. europaea was inhibited by 20 mM of nitrite (Stein and Arp, 1998; Cua and Stein, 2011). However, the high nitrite tolerance of N. mobilis Ms1 is consistent with the results of previous studies that showed enriched cultures of ammonia oxidizers had nitrite tolerance of up to 500 mM, most clones fell into the Nitrosomonas europaea/Nitrosomonas mobilis cluster (Tan et al., 2008), and nitrite effects on ammonia oxidizing activity varied between Nitrosomonas europaea and closely related Nitrosomonas eutropha (Cua and Stein, 2011).

FIGURE 5

FIGURE 5. Ammonium and nitrite tolerance of N. mobilis Ms1. (A) Maximum produced nitrite concentration rate per day of N. mobilis Ms1 incubation with different initial ammonium concentrations (10, 50, 100, 200, 300, 400, and 500 mM). (B) Maximum ammonia oxidation rate per day of N. mobilis Ms1 incubation with different initial nitrite concentrations (0, 5, 10, 50, 100, 200, 300, 400, and 500 mM) under 5 mM initial ammonium concentration. Bars are the standard errors (n = 2).

Genome Overview of N. mobilis Ms1

The genome of N. mobilis Ms1 has a sequence length of 3.09 Mbp and a G+C content of 48.53%. The genome included 3075 protein-coding DNA sequences (CDSs), 41 tRNA genes, and a single copy of the 16S-23S-5S rRNA operon. Based on phylogenetic analyses of N. mobilis Ms1 with other AOB (Fujitani et al., 2015), Ms1 showed the greatest similarity to Nitrosomonas sp. strains Nm107 and Nm104 (99.7–100%) at the 16S rRNA and amoA genes levels and 99.6% similarity to Nitrosococcus mobilis Nc2 at the 16S rRNA gene level, therefore Ms1 was attributed to the N. mobilis lineage. Similarities between N. mobilis Ms1 and other currently available genomes of Nitrosomonas species at 16S rRNA gene level and amoA amino acid level were highest to Nitrosomonas europaea ATCC 19718, 95.8 and 90.9%, respectively, and the similarity at the genomes level (ANI values) was highest to N. eutropha C-91, 71.1% (Table 2), confirming N. mobilis Ms1 was significantly below the species cut-off point for delineation (Konstantinidis et al., 2006). The smaller similarities of whole genomes and 16S rRNA and amoA sequences between N. mobilis Ms1 and other Nitrosomonas species support the physiological uniqueness of N. mobilis Ms1 among other Nitrosomonas species. The general genome features and the inventory of genes involved in the ammonia oxidation and nitrogen oxide metabolism of N. mobilis Ms1 and some currently available genomes of AOB are categorized in Table 2.

TABLE 2

TABLE 2. Genome characteristics of N. mobilis Ms1 and some AOB species.

N. mobilis Ms1 uses ammonia as an energy source in the same manner as other AOB. The genome of N. mobilis Ms1 contains two copies of the gene cluster encoding ammonia monooxygenase (amoCAB), followed by two copies of the amoED operon in which amoD in the first operon was not identified (Figure 6A; Table 2). N. mobilis Ms1 contains the operons encoding hydroxylamine oxidoreductase with associated cytochromes c554 and c_M552 (haoAB-cycAB) in two copies, neither of which includes cycB, whereas other AOB genomes contain two to three copies of the complete haoAB-cycAB operons (Figure 6B; Table 2) (Chain et al., 2003; Stein et al., 2007; Suwa et al., 2011). Unlike other AOB, the two small haoA fragments, which are distantly located from the haoAB-cycA operons and two copies of cycB-fragment cycA operon, but not adjacent to hao, were also identified in the N. mobilis Ms1 genome. The additional amoC singleton gene, which has been found in most other AOB genomes, was not identified in N. mobilis Ms1. As in other AOB, except Nitrosomonas sp. Is79 (Bollmann et al., 2013), the N. mobilis Ms1 genome contains an AOB-specific red-copper protein, nitrosocyanin, which has been proposed to be involved in electron transport, although the detailed vital function of this protein has not been identified (Klotz and Stein, 2011; Stein et al., 2013).

FIGURE 6

FIGURE 6. Organization of the cluster of genes involved in the ammonia oxidation of N. mobilis Ms1. (A) Cluster of genes encoding ammonia monooxygenase; NSMM_350046, the length of 159 bp, is the gene encoding protein with unknown function (B) cluster of genes encoding hydroxylamine oxidoreductase and associated cytochromes. The separate fragments haoA₃, haoA₄, cycA₃, and cycA₄, with the sequence length of 117, 165, 108, and 129 bp, respectively, were shorter than their respective version in the operon, and these were located at the end of the contigs and 3′ ends of the haoA₃ and haoA₄, and 5′ ends of the cycA₃ and cycA₄ were not included in the sequence of the contigs.

Ammonia-oxidizing bacteria are known to produce nitric oxide (NO) and nitrous oxide (N₂O), a greenhouse gas, from the hydroxylamine oxidation (a part of ammonia oxidation), nitrifier denitrification (dissimilatory nitrite reduction) and NO detoxification (nitrosative stress) pathways (Klotz and Stein, 2011). The genes encoding copper-containing nitrite reductase (NirK), membrane-bound cytochrome c nitric oxide reductase cNOR (norCBQD), heme-copper nitric oxide reductase sNOR (norSY-SenC), cytochrome c′ beta (cytS) and cytochrome P460 (cytL), all of which are supposed to be involved in the oxidation of hydroxylamine, the nitrifier partial denitrifying process and NO-detoxification, were identified in the N. mobilis Ms1 genome, whereas one or both types of nitric oxide reductase were not identified in the Nitrosomonas sp. AL212 and Nitrosomonas sp. Is79 genomes (Table 2) (Klotz and Stein, 2011; Suwa et al., 2011; Bollmann et al., 2013). Unlike other AOB, the gene encoding nitric oxide reductase activation protein (norD) did not cluster with norCBQ in the N. mobilis Ms1 genome (Table 2). Overall, the gene contents and the organization of the genes involved in N. mobilis Ms1 were distinct compared to other AOB genomes.

Conclusion

The key physiological and genomic properties of N. mobilis Ms1 were investigated in this study. The temperature and pH ranges and the growth rate of N. mobilis Ms1 were within the ranges of other Nitrosomonas species in the Nitrosomonas europaea/Nitrosomonas mobilis lineage, supporting the previous findings regarding the codominant habitat of N. mobilis-like bacteria with N. europaea–N. eutropha-like bacteria in wastewater treatment systems. In addition, N. mobilis Ms1 can withstand the high ammonia and nitrite concentrations. These physiological findings reveal the habitat and ecophysiology of N. mobilis in the natural ecosystem. Because N. mobilis Ms1 can oxidize at high ammonium and nitrite concentrations, N. mobilis-like strains would be dominant in environments such as wastewater treatment plants where the ammonia and nitrite concentrations are rather high. The genomic information for N. mobilis Ms1 is the first genome sequence of Nitrosomonas mobilis-like bacteria. The genome analysis of N. mobilis Ms1 also indicated that this strain has distinct genome features compared with the other Nitrosomonas species, although other functional genes and unique gene characteristics of Ms1 still needed to be investigated. Overall, the results of the present study provide a better understanding of the ecophysiology of Nitrosomonas mobilis and other nitrifying bacteria, especially among the widely abundant Nitrosomonas species in both natural and wastewater treatment systems.

Author Contributions

SMT, NU, HF, and ST designed the experiments. SMT performed all experiments. SMT, NU, HF, and ST analyzed the data. YS performed and wrote genome sequencing and assembly. SMT performed genome analysis. NU performed ANI analysis. SMT drafted the manuscript. SMT, NU, HF, YS, and ST read and edited the manuscript.

Funding

This research was funded by the Special Research Projects (2014B-323, 2015K-218) program of Waseda University and the Large Research Projects program of the Institute for Fermentation, Osaka.

Conflict of Interest Statement

The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.

Acknowledgments

The authors thank Dr. Akihiko Terada, Tokyo University of Agricultural Technology, for providing equipment and the facility for measurement of oxygen uptake.

Footnotes

1. ^ http://www.ezbiocloud.net/ezgenome/ani

References

Bankevich, A., Nurk, S., Antipov, D., Gurevich, A. A., Dvorkin, M., Kulikov, A. S., et al. (2012). SPAdes: a new genome assembly algorithm and its applications to single-cell sequencing. J. Comput. Biol. 19, 455–477. doi: 10.1089/cmb.2012.0021

PubMed Abstract | CrossRef Full Text | Google Scholar

Belser, L. W., and Schmidt, E. L. (1980). Growth and oxidation kinetics of 3 genera of ammonia oxidizing nitrifiers. FEMS Microbiol. Lett. 7, 213–216. doi: 10.1016/S0378-1097(80)80033-4

CrossRef Full Text | Google Scholar

Bollmann, A., and Laanbroek, H. J. (2001). Continuous culture enrichments of ammonia-oxidizing bacteria at low ammonium concentrations. FEMS Microbiol. Ecol. 37, 211–221. doi: 10.1016/s0168-6496(01)00163-5

CrossRef Full Text | Google Scholar

Bollmann, A., Sedlacek, C. J., Norton, J., Laanbroek, H. J., Suwa, Y., Stein, L. Y., et al. (2013). Complete genome sequence of Nitrosomonas sp. Is79, an ammonia oxidizing bacterium adapted to low ammonium concentrations. Stand. Genomic Sci. 7, 469–482. doi: 10.4056/sigs.3517166

PubMed Abstract | CrossRef Full Text | Google Scholar

Campbell, M. A., Chain, P. S. G., Dang, H., El Sheikh, A. F., Norton, J. M., Ward, N. L., et al. (2011). Nitrosococcus watsonii sp. nov., a new species of marine obligate ammonia-oxidizing bacteria that is not omnipresent in the world’s oceans: calls to validate the names ‘Nitrosococcus halophilus’ and ‘Nitrosomonas mobilis’. FEMS Microbiol. Ecol. 76, 39–48. doi: 10.1111/j.1574-6941.2010.01027.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Cantera, J. J. L., and Stein, L. Y. (2007). Molecular diversity of nitrite reductase genes (nirK) in nitrifying bacteria. Environ. Microbiol. 9, 765–776. doi: 10.1111/j.1462-2920.2006.01198.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Chain, P., Lamerdin, J., Larimer, F., Regala, W., Lao, V., Land, M., et al. (2003). Complete genome sequence of the ammonia-oxidizing bacterium and obligate chemolithoautotroph Nitrosomonas europaea. J. Bacteriol. 185, 2759–2773. doi: 10.1128/JB.185.21.6496.2003

PubMed Abstract | CrossRef Full Text | Google Scholar

Chen, G. H., and Wong, M. T. (2004). Impact of increased chloride concentration on nitrifying-activated sludge cultures. J. Environ. Eng. 130, 116–125. doi: 10.1061/(asce)0733-9372(2004)130:2(116)

CrossRef Full Text | Google Scholar

Cortes-Lorenzo, C., Rodriguez-Diaz, M., Sipkema, D., Juarez-Jimenez, B., Rodelas, B., Smidt, H., et al. (2015). Effect of salinity on nitrification efficiency and structure of ammonia-oxidizing bacterial communities in a submerged fixed bed bioreactor. Chem. Eng. J. 266, 233–240. doi: 10.1016/j.cej.2014.12.083

CrossRef Full Text | Google Scholar

Cua, L. S., and Stein, L. Y. (2011). Effects of nitrite on ammonia-oxidizing activity and gene regulation in three ammonia-oxidizing bacteria. FEMS Microbiol. Lett. 319, 169–175. doi: 10.1111/j.1574-6968.2011.02277.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Daims, H., Lebedeva, E. V., Pjevac, P., Han, P., Herbold, C., Albertsen, M., et al. (2015). Complete nitrification by Nitrospira bacteria. Nature 528, 504–509. doi: 10.1038/nature16461

PubMed Abstract | CrossRef Full Text | Google Scholar

Fujitani, H., Kumagai, A., Ushiki, N., Momiuchi, K., and Tsuneda, S. (2015). Selective isolation of ammonia-oxidizing bacteria from autotrophic nitrifying granules by applying cell-sorting and sub-culturing of microcolonies. Front. Microbiol. 6:1159. doi: 10.3389/fmicb.2015.01159

PubMed Abstract | CrossRef Full Text | Google Scholar

Gieseke, A., Bjerrum, L., Wagner, M., and Amann, R. (2003). Structure and activity of multiple nitrifying bacterial populations co-existing in a biofilm. Environ. Microbiol. 5, 355–369. doi: 10.1046/j.1462-2920.2003.00423.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Griess-Romijn van Eck, E. (1966). Physiological and Chemical Tests for Drinking Water. NEN 1056, IV-2. Rijswijk: Nederlands Normalisatie Instituut.

Head, I. M., Hiorns, W. D., Embley, T. M., McCarthy, A. J., and Saunders, J. R. (1993). The phylogeny of autotrophic ammonia-oxidizing bacteria as determined by analysis of 16s ribosomal RNA gene sequences. J. Gen. Microbiol. 139, 1147–1153. doi: 10.1099/00221287-139-6-1147

PubMed Abstract | CrossRef Full Text | Google Scholar

Itoh, Y., Sakagami, K., Uchino, Y., Boonmak, C., Oriyama, T., Tojo, F., et al. (2013). Isolation and characterization of a thermotolerant ammonia-oxidizing bacterium Nitrosomonas sp JPCCT2 from a thermal power station. Microbes Environ. 28, 432–435. doi: 10.1264/jsme2.ME13058

PubMed Abstract | CrossRef Full Text | Google Scholar

Jones, R. D., Morita, R. Y., Koops, H. P., and Watson, S. W. (1988). A new marine ammonium-oxidizing bacterium, Nitrosomonas cryotolerans sp nov. Can. J. Microbiol. 34, 1122–1128. doi: 10.1139/m88-198

CrossRef Full Text | Google Scholar

Juretschko, S., Timmermann, G., Schmid, M., Schleifer, K. H., Pommerening-Roser, A., Koops, H. P., et al. (1998). Combined molecular and conventional analyses of nitrifying bacterium diversity in activated sludge: Nitrosococcus mobilis and Nitrospira-like bacteria as dominant populations. Appl. Environ. Microbiol. 64, 3042–3051.

PubMed Abstract | Google Scholar

Kandeler, E., and Gerber, H. (1988). Short-term assay of soil urease activity using colorimetric determination of ammonium. Biol. Fertil. Soils 6, 68–72. doi: 10.1007/BF00257924

CrossRef Full Text | Google Scholar

Klotz, M. G., and Stein, L. Y. (2011). “Genomics of ammonia-oxidizing bacteria and insights to their evolution,” in Nitrification, eds B. B. Ward, D. J. Arp, and M. G. Klotz (Washington, DC: ASMPress), 57–94.

Google Scholar

Konstantinidis, K. T., Ramette, A., and Tiedje, J. M. (2006). The bacterial species definition in the genomic era. Phil. Trans. Soc. B 361, 1929–1940. doi: 10.1098/rstb.2006.1920

PubMed Abstract | CrossRef Full Text | Google Scholar

Konstantinidis, K. T., and Tiedje, J. M. (2005). Genomic insights that advance the species definition for prokaryotes. Proc. Natl. Acad. Sci. U.S.A. 102, 2567–2572. doi: 10.1073/pnas.0409727102

PubMed Abstract | CrossRef Full Text | Google Scholar

Koops, H. P., Bottcher, B., Moller, U. C., Pommereningroser, A., and Stehr, G. (1990). Description of a new species of Nitrosococcus. Arch. Microbiol. 154, 244–248. doi: 10.1007/bf00248962

CrossRef Full Text | Google Scholar

Koops, H. P., Bottcher, B., Moller, U. C., Pommereningroser, A., and Stehr, G. (1991). Classification of eight new species of ammonia-oxidizing bacteria: Nitrosomonas communis sp. nov., Nitrosomonas ureae sp. nov., Nitrosomonas aestuarii sp. nov., Nitrosomonas marina sp. nov., Nitrosomonas nitrosa sp. nov., Nitrosomonas eutropha sp. nov., Nitrosomonas oligotropha sp. nov. and Nitrosomonas halophila sp. nov. J. Gen. Microbiol. 137, 1689–1699.

Google Scholar

Koops, H. P., and Harms, H. (1985). Deoxyribonucleic acid homologies among 96 strains of ammonia-oxidizing bacteria. Arch. Microbiol. 141, 214–218. doi: 10.1007/bf00408061

PubMed Abstract | CrossRef Full Text | Google Scholar

Koops, H. P., Harms, H., and Wehrmann, H. (1976). Isolation of a moderate halophilic ammonia-oxidizing bacterium, Nitrosococcus mobilis nov sp. Arch. Microbiol. 107, 277–282. doi: 10.1007/bf00425339

PubMed Abstract | CrossRef Full Text | Google Scholar

Koops, H. P., and Pommerening-Roser, A. (2001). Distribution and ecophysiology of the nitrifying bacteria emphasizing cultured species. FEMS Microbiol. Ecol. 37, 1–9. doi: 10.1111/j.1574-6941.2001.tb00847.x

CrossRef Full Text | Google Scholar

Koops, H. P., Purkhold, U., Pommerening-Roser, A., Timmermann, G., and Wagner, M. (2006). The lithoautotrophic ammonia-oxidizing bacteria,” in Prokaryotes: a Handbook on the Biology of Bacteria, Proteobacteria: Alpha and Beta Subclasses, Vol 5, 3rd Edn, eds M. Dworkin, S. Falkow, E. Rosenberg, K.-H. Schleifer, and E. Stackebrandt (New York, NY: Springer), 778–811. doi: 10.1007/0-387-30745-1_36

CrossRef Full Text | Google Scholar

Laanbroek, H. J., and Gerards, S. (1993). Competition for limiting amounts of oxygen between Nitrosomonas europaea and Nitrobacter winogradskyi grown in mixed continuous cultures. Arch. Microbiol. 159, 453–459. doi: 10.1007/bf00288593

CrossRef Full Text | Google Scholar

Limpiyakorn, T., Kurisu, F., Sakamoto, Y., and Yagi, O. (2007). Effects of ammonium and nitrite on communities and populations of ammonia-oxidizing bacteria in laboratory-scale continuous-flow reactors. FEMS Microbiol. Ecol. 60, 501–512. doi: 10.1111/j.1574-6941.2007.00307.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Limpiyakorn, T., Shinohara, Y., Kurisu, F., and Yagi, O. (2005). Communities of ammonia-oxidizing bacteria in activated sludge of various sewage treatment plants in Tokyo. FEMS Microbiol. Ecol. 54, 205–217. doi: 10.1016/j.femsec.2005.03.017

PubMed Abstract | CrossRef Full Text | Google Scholar

Matsumoto, S., Ishikawa, D., Saeki, G., Aoi, Y., and Tsuneda, S. (2010). Microbial population dynamics and community structure during the formation of nitrifying granules to treat ammonia-rich inorganic wastewater. Microbes Environ. 25, 164–170. doi: 10.1264/jsme2.ME10107

PubMed Abstract | CrossRef Full Text | Google Scholar

Mota, C., Head, M. A., Ridenoure, J. A., Cheng, J. J., and de los Reyes, F. L. (2005). Effects of aeration cycles on nitrifying bacterial populations and nitrogen removal in intermittently aerated reactors. Appl. Environ. Microbiol. 71, 8565–8572. doi: 10.1128/aem.71.12.8565-8572.2005

PubMed Abstract | CrossRef Full Text | Google Scholar

Nakagawa, T., and Takahashi, R. (2015). Nitrosomonas stercoris sp nov., a chemoautotrophic ammonia-oxidizing bacterium tolerant of high ammonium isolated from composted cattle manure. Microbes Environ. 30, 221–227. doi: 10.1264/jsme2.ME15072

PubMed Abstract | CrossRef Full Text | Google Scholar

Pommerening-Roser, A., Rath, G., and Koops, H. P. (1996). Phylogenetic diversity within the genus Nitrosomonas. Syst. Appl. Microbiol. 19, 344–351. doi: 10.1016/S0723-2020(96)80061-0

CrossRef Full Text | Google Scholar

Prosser, J. I. (1989). Autotrophic nitrification in bacteria. Adv. Microb. Physiol. 30, 125–181. doi: 10.1016/S0065-2911(08)60112-5

CrossRef Full Text | Google Scholar

Purkhold, U., Pommerening-Roser, A., Juretschko, S., Schmid, M. C., Koops, H. P., and Wagner, M. (2000). Phylogeny of all recognized species of ammonia oxidizers based on comparative 16S rRNA and amoA sequence analysis: implications for molecular diversity surveys. Appl. Environ. Microbiol. 66, 5368–5382. doi: 10.1128/aem.66.12.5368-5382.2000

PubMed Abstract | CrossRef Full Text | Google Scholar

Radniecki, T. S., and Ely, R. L. (2008). Zinc chloride inhibition of Nitrosococcus mobilis. Biotechnol. Bioeng. 99, 1085–1095. doi: 10.1002/bit.21672

PubMed Abstract | CrossRef Full Text | Google Scholar

Radniecki, T. S., and Ely, R. L. (2011). Transcriptional and physiological responses of Nitrosococcus mobilis to copper exposure. J. Environ. Eng. 137, 307–314. doi: 10.1061/(asce)ee.1943-7870.0000338

CrossRef Full Text | Google Scholar

Sekiguchi, Y., Ohashi, A., Parks, D. H., Yamauchi, T., Tyson, G. W., and Hugenholtz, P. (2015). First genomic insights into members of a candidate bacterial phylum responsible for wastewater bulking. PeerJ 3:e740. doi: 10.7717/peerj.740

PubMed Abstract | CrossRef Full Text | Google Scholar

Stehr, G., Bottcher, B., Dittberner, P., Rath, G., and Koops, H. P. (1995). The ammonia-oxidizing nitrifying population of the river elbe estury. FEMS Microbiol. Ecol. 17, 177–186. doi: 10.1111/j.1574-6941.1995.tb00141.x

CrossRef Full Text | Google Scholar

Stein, L. Y., and Arp, D. J. (1998). Loss of ammonia monooxygenase activity in Nitrosomonas europaea upon exposure to nitrite. Appl. Environ. Microbiol. 64, 4098–4102.

PubMed Abstract | Google Scholar

Stein, L. Y., Arp, D. J., Berube, P. M., Chain, P. S. G., Hauser, L., Jetten, M. S. M., et al. (2007). Whole-genome analysis of the ammonia-oxidizing bacterium, Nitrosomonas eutropha C91: implications for niche adaptation. Environ. Microbiol. 9, 2993–3007. doi: 10.1111/j.1462-2920.2007.01409.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Stein, L. Y., Campbell, M. A., and Klotz, M. G. (2013). Energy-mediated vs. Ammonium-regulated gene expression in the obligate ammonia oxidizing bacterium, Nitrosococcus oceani. Front. Microbiol. 4:277. doi: 10.3389/fmicb.2013.00277

PubMed Abstract | CrossRef Full Text | Google Scholar

Suwa, Y., Imamura, Y., Suzuki, T., Tashiro, T., and Urushigawa, Y. (1994). Ammonia-oxidizing bacteria with different sensitive to (NH4)2SO4 in activated sludges. Water Res. 28, 1523–1532. doi: 10.1016/0043-1354(94)90218-6

CrossRef Full Text | Google Scholar

Suwa, Y., Norton, J. M., Bollmann, A., Klotz, M. G., Stein, L. Y., Laanbroek, H. J., et al. (2011). Genome sequence of Nitrosomonas sp. strain AL212, an ammonia-oxidizing bacterium sensitive to high levels of ammonia. J. Bacteriol. 193, 5047–5048. doi: 10.1128/JB.05521-11

PubMed Abstract | CrossRef Full Text | Google Scholar

Suwa, Y., Sumino, T., and Noto, K. (1997). Phylogenetic relationships of activated sludge isolates of ammonia oxidizers with different sensitivities to ammonium sulfate. J. Gen. Appl. Microbiol. 43, 373–379. doi: 10.2323/jgam.43.373

PubMed Abstract | CrossRef Full Text | Google Scholar

Tan, N. C. G., Kampschreur, M. J., Wanders, W., van der Pol, W. L. J., van de Vossenberg, J., Kleerebezem, R., et al. (2008). Physiological and phylogenetic study of an ammonium-oxidizing culture at high nitrite concentrations. Syst. Appl. Microbiol. 31, 114–125. doi: 10.1016/j.syapm.2008.01.002

PubMed Abstract | CrossRef Full Text | Google Scholar

Tokuyama, T., Yoshida, N., Matsuishi, T., Takahashi, N., Takahashi, R., Kanehira, T., et al. (1997). A new psychrotrophic ammonia-oxidizing bacterium, Nitrosovibrio sp. TYM9. J. Ferment. Bioeng. 83, 377–380. doi: 10.1016/s0922-338x(97)80145-6

CrossRef Full Text | Google Scholar

Tsuneda, S., Nagano, T., Hoshino, T., Ejiri, Y., Noda, N., and Hirata, A. (2003). Characterization of nitrifying granules produced in an aerobic upflow fluidized bed reactor. Water Res. 37, 4965–4973. doi: 10.1016/j.watres.2003.08.017

PubMed Abstract | CrossRef Full Text | Google Scholar

Vallenet, D., Belda, E., Calteau, A., Cruveiller, S., Engelen, S., Lajus, A., et al. (2013). MicroScope-an integrated microbial resource for the curation and comparative analysis of genomic and metabolic data. Nucleic Acids Res. 41, E636–E647. doi: 10.1093/nar/gks1194

PubMed Abstract | CrossRef Full Text | Google Scholar

van Kessel, M. A. H. J., Speth, D. R., Albertsen, M., Nielsen, P. H., Op den Camp, H. J. M., Kartal, B., et al. (2015). Complete nitrification by a single microorganism. Nature 528, 555–559. doi: 10.1038/nature16459

PubMed Abstract | CrossRef Full Text | Google Scholar

Wells, G. F., Park, H.-D., Yeung, C.-H., Eggleston, B., Francis, C. A., and Criddle, C. S. (2009). Ammonia-oxidizing communities in a highly aerated full-scale activated sludge bioreactor: betaproteobacterial dynamics and low relative abundance of Crenarchaea. Environ. Microbiol. 11, 2310–2328. doi: 10.1111/j.1462-2920.2009.01958.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Zhang, Y., Chen, L., Sun, R., Dai, T., Tian, J., and Wen, D. (2015). Ammonia-oxidizing bacteria and archaea in wastewater treatment plant sludge and nearby coastal sediment in an industrial area in China. Appl. Microbiol. Biotechnol. 99, 4495–4507. doi: 10.1007/s00253-014-6352-9

PubMed Abstract | CrossRef Full Text | Google Scholar