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Manuscript for review
Nitrification in fixed-bed reactors treating salinewastewater
Journal: Applied Microbiology and Biotechnology
Manuscript ID: AMB-09-18698.R1
Manuscript Category: Original Paper
Date Submitted by theAuthor:
07-Oct-2009
Complete List of Authors: Sudarno, Utomo; Universität Karlsruhe, Institut fürIngenieurbiologie und Biotechnologie des AbwassersBathe, Stephan; Universität Karlsruhe, Institut fürIngenieurbiologoe und Biotechnologie des Abwassers; UniversitätKarlsruhe, Institut für Ingenieurbiologie und Biotechnologie desAbwassersWinter, Josef; Universität Karlsruhe, Institut für Ingineurbiologieund Biotechnologie des AbwassersGallert, Claudia; Universität Karlsruhe, Institut für Ingenieurbiologieund Biotechnologie des Abwassers
Keyword:Halophilic nitrification; saline wastewater; Nitrosomonas;Nitrosospira; fixed-bed reactors, saline wastewater;, Nitrosomonas;, Nitrosospira; , Fixed-bed reactors
Applied Microbiology and Biotechnology
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Nitrification in fixed-bed reactors treating saline wastewater
Sudarno, S. Bathe, J. Winter, C. Gallert *
Institute of Biology for Engineers and Biotechnology of Wastewater
University of Karlsruhe
76128 Karlsruhe
Am Fasanengarten
Corresponding author*:
PD. Dr. Claudia Gallert
Phone: +49-721-6082297
Fax: +49-721-6087704
Sudarno
Department of Environmental Engineering
University of Diponegoro UNDIP
Semarang, Indonesia
Present address: Institute of Biology for Engineers and Biotechnology of Wastewater
University of Karlsruhe
76128 Karlsruhe
Prof. Dr. Josef Winter
Institute of Biology for Engineers and Biotechnology of Wastewater
University of Karlsruhe
76128 Karlsruhe
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Abstract
Halophilic nitrifyers belonging to the genus Nitrosomonas and Nitrospira were
enriched from sea water and marine sediment samples of the North Sea. The
maximal ammonia oxidation rate (AOR) in batch enrichments with sea water was
15.1 mg N L-1 d-1. An intermediate nitrite accumulation was observed.
Two fixed-bed reactors for continuous nitrification with either polyethylene/clay sinter
lamellas (FBR A) or porous ceramic rings (FBR B) were run at two different ammonia
concentrations, three different ALRs, ± pH adjustment and at an increased upflow
velocity. A better overall nitrification without nitrite accumulation was observed in FBR
B. However, FBR A revealed a higher AOR and nitrite oxidation rate of 6 and 7 mg N
L-1 h-1, compared to FBR B with 5 and 5.9 mg N L -1 h-1, respectively. AORs in the
FBRs were at least 10 times higher than in suspended enrichment cultures.
Whereas a shift within the ammonia oxidizing population in the genus Nitrosomonas
at the subspecies level occurred in FBR B with synthetic sea water at an increasing
ammonia loading rate (ALR) and a decreasing pH, the nitrite oxidizing Nitrospira
population apparently did not change.
Key words
Halophilic nitrification; saline wastewater; Nitrosomonas ; Nitrosospira ; fixed-bed
reactors
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Introduction
Most biological wastewater treatment processes are running with polluted water
sources that contain either no or only little salt, whereas in coastal regions sea water
dominated domestic wastewater may be generated (Wu et al. 2008). In addition
several sources of industrial wastewater may contain 3 % sodium chloride or an even
higher salt content. Thus, carbon removal, nitrification and denitrification in biological
wastewater treatment processes should function over a wide range of salt
concentrations to meet wastewater discharge criteria. Halo-tolerant or halophilic
bacteria must be present to cope with the salt content of a certain wastewater.
Saline wastewater containing high amounts of nitrogen and carbonaceous
compounds for instance is generated during aqua culturing of marine fish or shrimps
or by the fish canning industry. Nitrogen removal in real or artificial wastewater in the
presence of 0 – 6 % NaCl in lab- or full-scale SBR systems has been investigated
(Campos et al. 2002, Fontenot et al. 2007, Huilinir et al. 2008). With increasing salt
concentrations up to 6 % removal efficiencies decreased drastically in the lab-scale
SBRs inoculated with salt-adapted, but non-halophilic microorganism (Intrasungkha
et al. 1999, Uygur and Kargi 2004), whereas the highest nitrifying activity of a
halophilic bacterial population was obtained for an in-situ NaCl concentration of 28 g/l
(Fontenot et al. 2007).
Removal of carbonaceous and nitrogenous pollutants before discharging the
wastewater into a water body is essential to avoid oxygen depletion and
eutrophication. Conventional nitrogen removal processes for protein or ammonia
containing wastewater are designed for aerobic carbon removal and nitrification,
followed by anoxic denitrification with addition of an external carbon source, e.g. in
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The implementation of biological nitrification in a technical process can be
attempted with suspended or immobilized bacteria in different types of bioreactors.
The activated sludge system for wastewater treatment works with sludge floc
enrichment. The effect of high inorganic salt concentrations on settling of sludge flocs
is mainly related to disintegration of flocculated sludge. The smaller flocs tend to float
as a result of a larger surface and the buoyancy force increases with increasing salt
contents due to a higher water density (Wu et al. 2008). Attached growth of bacteria
in biofilm systems offers several advantages as compared to suspended growth,
such as a long sludge retention time, prevention of wash-out of biomass from the
reactor and better process stability in terms of withstanding shock loadings or short-
term inhibitory effects (Fitch et al. 1998; Nogueira et al. 1998). For biofilm systems,
the selected support material as a “substratum” for attached growth has a great
influence on process stability and therefore a huge variety of different materials were
tested. Biofilm systems for wastewater treatment are well established but the
treatment of saline wastewater in biofilm reactors has not been studied extensively.
Nitrification of saline wastewater in biofilm reactors using PVC plastic tubes
(Gharasallah et al. 2002), wrinkled PVC plates (Rosa et al. 1998) or PVC discs
(Windey et al. 2005) was reported.
The aim of this study was i) to determine the original nitrifying activity in brine and
seawater samples to obtain a suitable inoculum for nitrification of an ammonia-
containing wastewater with 3% NaCl content, ii) to establish continuously operated
fixed-bed reactors (FBRs) for stable ammonia and nitrite removal rates with the most
suitable enrichment and iii) to characterize the nitrifying population in these
enrichments.
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Materials and methods
Water and sediment sampling from different sites
Water and sediment samples A–D were collected from different costal locations at
the North Sea in January 2008 (Table 1). The water samples (10 L) and the sediment
samples (5 L) were filled into sterilized canisters and stored at 4 oC in a cool box
during transportation to the laboratory.
Batch assays for determination of the nitrifying activity
Water or sediment samples (250 mL each) from the different collection places at the
North Sea were filled into glass reactors of 500 mL total volume. A magnetic stirrer
was used to mix the samples in the reactors. The reactors were aerated with 2 L min -
1 air blown in via a syringe needle just above the stirrer. After addition of 50 mg N L -1
(190 mg L-1 NH4Cl) incubation at room temperature (20-23oC) was started. At
different time intervals, liquid samples were taken for analysis of dissolved oxygen
(DO), pH, ammonia, nitrite and nitrate. For pH correction, e.g. at day 42 and 52 (Fig.
1A,1C,1D), 1-3 mL 0.25 M KOH was added to the reactors until a pH > 8.0 was
reached. The DO in all samples was kept above 5 mg L-1.
Fixed bed reactors
Two cylindrical FBRs with 9 cm internal diameter and 45 cm height were used
(scheme see Fig. 1). The feed was pumped into the reactor at the bottom with a
Gilson Minipuls 3 pump (Abimed, Dreieich) and effluent was flowing out at the top of
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the reactor through an overflow pipe, maintaining a working volume of 2.1 L.
Polyethylene/clay sinter lamellas (PELIA, Herding, Amberg, Germany) with a specific
surface area of 440 m2 m-3, a fixed bed area of 0.46 m2 and a porosity of 59% were
used as support material in FBR A and porous ceramic rings (Poro Ring, Tropical)
with a specific surface area of 934 m2 m-3, a fixed bed area of 0.60 m2 and a porosity
of 38% in FBR B. Both FBRs were filled with sea water from Hafen Büsum (Table 1)
that contained 100 mg N L-1 (380 mg L-1 NH4Cl). During the first 40 days the FBRs
were operated batchwise until all ammonia and nitrite was oxidized to nitrate.
Afterwards, the FBR´s were operated continuously. The ammonia loading rate (ALR)
was increased by reducing the hydraulic retention time (HRT) or by increasing the
ammonia concentration. The reactors were aerated from the bottom with an air
diffuser at a flow rate of 2.5 L h-1, which was adjusted by a micro valve and controlled
by a TG 05 gas meter (Ritter, Bochum-Langendreer, Germany). This maintained an
oxygen concentration of ≥ 5 mg L-1 and a homogeneous distribution of the feeding.
To further improve liquid mixing, an external recirculation loop was installed from the
overflow to the inlet pipe for both FBRs. The reactor effluent was re-circulated at a
flow rate of 8 L h-1 into the inlet pipe of the reactor with a tube pump (model 604 U,
Watson-Marlow, Fallmouth, Cornwall, England). The pH was kept at 7.6 by a pH
titrator (Dulcometer D1C, Prominent, Heidelberg, Germany) and a dosing pump
(Prominent Gamma 74) with 0.25 M KOH solution. The reactors were run at room
temperature.
Synthetic seawater
The reactors were fed with a synthetic sea water containing in g L-1
: NaCl (28.13),
KCl (0.77), CaCl2.2H2O (1.6), MgCl2
.6H2O (4.8), NaHCO3 (0.11), MgSO4 .7H2O (3.5)
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and 0.3 mL L-1 nutrient solution of the following composition (g L-1): FeCl3 .6H2O (1.5),
H3BO3 (0.15), CuSO4 (0.03), KI (0.18), MnCl2 4.H2O (0.12), Na2MoO4
.2H2O (0.06),
ZnSO4.7H2O (0.12), CoCl2
.6H2O (0.15) and EDTA (10).
Sample preparation for analyses and physicochemical analyses
All samples were centrifuged at 10000 rpm for 5 min in a laboratory centrifuge (model
Z 233 M-2, Hermle, Gosheim, Germany). The clear supernatant was further
analyzed. Ammonia and nitrite were measured colorimetrically according to DEV
(1983), procedures E5 (DIN 38406) and D28 (DIN 38405), respectively. Nitrate was
analyzed spectrophotometrically at 320 nm according to Standard Methods (APHA
1998). The DO, pH, temperature and electrical conductivity (salinity) were measured
with respective standard probes attached to a multi meter (Inolab multi level 1, WTW
Weilheim, Germany). The alkalinity of the samples was calculated after titration to a
pH value of pH 4.5 with 0.02 M HCl and expressed as CaCO3 (mg L-1).
Nitritation and nitratation rates in the FBRs
To determine the ammonia oxidation rate (AOR, nitritation rate) and the nitrite
oxidation rate (NOR, nitratation rate), the continuously operated FBRs were run in
batch-mode for one day during a time period where the ammonia and nitrite removal
rates were high and no accumulation of ammonia or nitrite was observed. The
respective nitrogen sources, NH4Cl (60 mg N L-1) for nitritation or KNO2 (30 mg N L
-1)
for nitratation, were then added. Decreasing ammonia and nitrite concentrations were
monitored in the reactors. After complete removal of ammonia and nitrite, continuous
operation of the FBRs was re-established.
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Molecular biological analyses.
Five pieces of ceramic carrier material from FBR B were removed from the reactor
per sampling for analyses of the biofilm composition. They were placed in a 50 ml
Falcon tube, and 30 ml 0.85% KCl solution was added. The tube was vigorously
vortexed for 5 min to release the biofilm from the carrier material and the resulting
suspension was transferred into new tubes. Bacteria were sedimented by
centrifugation and the pellet was washed by re-suspension in 0.85% KCl and
repeated centrifugation. DNA from the pelleted bacteria was then extracted using an
SDS/CTAB detergent lysis protocol followed by phenol-chloroform extraction
(Ausubel et al. 1999).
PCR was conducted in a Biometra TGradient thermal cycler. Sequences of the
primers used in this study are listed in Table 2.
The following individual primer combinations were used in separate reactions to
target different organism groups: 8fm/1492r for Bacteria , βAMOf/NSO1225 for β-
subclass ammonia-oxidizing bacteria, 8fm/Ntspa662 for Nitrospira spp., 8fm/NIT3 for
Nitrobacter spp., and Arch-amoAF/Arch-amoAR for ammonia-oxidizing archaea. All
reactions were carried out in 25 µl volumes containing 0.5 units of polymerase
(Fermentas TrueStart Taq DNA polymerase) in 1x reaction buffer, 2.5 mM MgCl2, 0.2
mM of each dNTP, 0.2 µM of each primer, and approx. 10-50 ng of template DNA.
Thermal cycling was conducted with an initial denaturation of 5 min at 95 °C followed
by 35 cycles of 95 °C for 30 s, 54 °C for 1 min, and 72 °C for 2 min. The programme
was concluded by a final extension for 5 min at 72 °C.
The products of positive 16S rRNA gene targeted PCR reactions (Bacteria, AOB,
Nitrospira) were then used as templates in a second round of PCR (nested PCR) with
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primers 341f-GC/518r to generate amplicons suitable for analysis by DGGE. One µl
of the first-round product was used in 25 µl reactions under the same concentrations
as listed above. The PCR program consisted of an initial denaturation at 95 °C for 5
min. followed by 20 cycles of 95 °C for 30 s, 58 °C for 30 s, and 72 °C for 1 min and
was concluded by a 20 min extension period at 72 °C.
DGGE was carried out in a CBS DGGE-2401 apparatus. Between 10 and 20 µl of
PCR product were separated in 10% poly acryl amide gels with a denaturant gradient
from 50 to 75% for 16.5 h at 60 V and a temperature of 60 °C. Gels were silver-
stained to visualize the DNA.
Products from AOB- and Nitrospira -specific first round PCR reactions were
additionally cloned using the GeneJet PCR cloning kit (Fermentas). The inserts of
individual clones were obtained by colony-PCR using primers pJET1f/pJET1r flanking
the MCS of the cloning vector pJET1. Reactions were carried out using a PCR
program consisting of 95 °C for 5 min. followed by 35 cycles of 95 °C for 30 s, 58 °C
for 30 s, and 72 °C for 2 min. Amplicons were screened by RFLP using RsaI, and the
PCR products of selected clones were then re-amplified using primers 341f-GC/518r
followed by DGGE analysis in order to identify clones co-migrating with dominant
bands in community profiles. The identified colony-PCR products were then custom-
sequenced (Seqlab Laboratories, Göttingen, Germany) using primer 341f.
Sequences were analysed using BLAST at NCBI and sequence alignments followed
by construction of phylogenetic trees were conducted using MEGA4 (Tamura et al.
2007). The evolutionary history was inferred using the Neighbor-Joining method. The
percentage of replicate trees in which the associated taxa clustered together in the
bootstrap test (1000 replicates) is shown next to the branches (Figures 6, 7 later on).
The evolutionary distances were computed using the Jukes-Cantor method and are
shown in the units of the number of base substitutions per site. All positions
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B also revealed the highest salinity and alkalinity, presumably caused by its mud
content. The influence of pollution by domestic waste water on the ammonia or
nitrate content can clearly be seen by comparing samples C and D from St. Peter-
Ording (Table 1). Wastewater discharge at the coast into brine water (sample C) led
to elevated ammonia and nitrate contents. At the point where the brine water flows
into the open sea (sample D) ammonia and nitrate concentrations were much lower
due to dilution with sea water.
To test the nitrifying capability of sea water or sea water/mud mixtures, samples A-
D (Table 1) were supplemented with 50 mg N L-1 ammonia. Portions of 250 ml were
filled into batch reactors for nitrification by the autochthonic bacteria. Ammonia
depletion, nitrite formation and utilization as well as nitrate formation were analysed.
After a lag-phase of approximately 10 d, ammonia oxidation began in all samples and
led to the formation of abundantly nitrite (samples A, B, D) or nitrate (sample C).
Ammonia conversion to nitrite or nitrate was incomplete in samples A, C and D
apparently due to the low alkalinity and a pH drop below or far below 7 (Fig. 2).
Ammonia was, however, completely converted to nitrite and then to nitrate in sea
water/mud-sample B, which had a high alkalinity and a stable pH with a minimal
value of 7.5 (Fig. 2B). When a second portion of ammonia was fed to this reactor at
day 42, ammonia was oxidized rapidly to nitrite. The nitrite was further oxidized to
nitrate within less than 10 d, indicating the successful enrichment of halophilic or at
least halotolerant nitrifyers. In the reactor with brine water sample C very little
ammonia was oxidized at the beginning due to the rapid drop of the pH (sample C
had the lowest alkalinity of all samples), but nitritation and nitratation proceeded
shortly after titrating the pH to 8.7 (Fig. 2C, day 42). The strict dependence of
ammonia oxidation on an alkaline pH can be seen in the three reactors where sea
water samples with a low alkalinity were incubated for the establishment of halophilic
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nitrification (Fig. 2A,C,D). In these reactors the pH dropped rapidly when ammonia
oxidation started and nitrite was produced. When the pH was raised to around 8.5 by
addition of KOH at day 42 and 52, ammonia oxidation was completed and nitrite
conversion to nitrate started (Fig. 2A,C) or was finished (Fig. 2D).
The initial AOR of the enrichment culture obtained with sea water from Hafen
Büsum (sample source A) after the lag-phase and after pH correction was around
11.5 mg N L-1 d-1, that of enrichments from brine and sea water of St. Peter-Ording
(sample sources C and D) 7.3 and 6.6 mg N L-1 d-1, respectively. In the sea
water/mud-mixture (sample source B), the AOR during the first feeding cycle was
only 4.9 mg N L-1 d-1. It increased three-fold to 15.1 mg N L-1 d-1 during the second
feeding cycle after day 42 (Fig. 2B).
Start-up of fixed-bed reactors with polyethylene/clay sinter lamellas (FBR A) and
porous ceramic rings (FBR B) for continuous nitrification
Sea water sample A from Hafen Büsum was used as an inoculation of FBR A and
FBR B. Sample A was preferred over sample B because it did not contain mud and
its AOR of 11.5 mg N d-1 was only slightly lower than that of sample B. Both FBRs
were filled with 2 L sea water sample A (Table 1). After addition of 104 mg N L-1
ammonia FBR A and FBR B were operated under batch conditions for 3 weeks to
acclimatize the nitrifying microorganisms.
After acclimatization a synthetic sea water medium was supplemented with NH4Cl
as indicated in Table 3 and both FBRs were run for more than 300 d. Four phases
were distinguished, concerning the HRT, ALR and installation of an external water
recirculation to improve the mixing intensity for better conversion rates (Table 3).
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In the initial phase a (day 0 - 56, Fig. 3a) in FBR A ammonia was oxidized
completely and more nitrite than nitrate was formed. Due to malfunction of the pH
titrator at day 12, causing an increase of the pH to 9.1, 60 mg N L-1 ammonia were
remaining in the reactor effluent. Restoration of the full AOR was obtained after
exchange of the pH probe within the next 10 d. From day 45 onward all ammonia
was oxidized to the expected stoichiometric amount of nitrate without intermediary
nitrite accumulation (Fig. 3a). An optimum pH of 8.0 – 8.3 was reported for Nitrospira
spec. (Blackburne et al. 2007).
In phase b (day 56 – 156, Fig. 3b) the HRT was reduced from 1.25 to 1 d and the
ALR was increased from 83 to 104 mg N L-1 d-1. Under steady state conditions
ammonia was still oxidized completely. Due to a failure of the pH probe at day 66 and
88 the pH fell below 6.5. Ammonia accumulation started immediately, but after
replacement of the pH probe degradation of ammonia resumed. From day 112 - 132
and 140 – 150 the aeration rate in FBR A increased drastically due to a leak of the
internal aeration system. The higher air flow rates caused higher shear forces and
this led to biofilm detachment from the carrier material and sedimentation/wash-out.
Ammonia was no longer completely oxidized and little nitrite accumulated at the
beginning of the disturbance (Fig. 3b, day 112).
In phase c (day 156 – 216, Fig. 3c) the ALR was further increased to 130 mg N L -1
d-1 by increasing the ammonia concentration in the medium. Ammonia was not
oxidized completely and some nitrite accumulated (Fig. 3c). Due to problems with the
stability of pH probes in the saline environment the titration system was switched off
and the medium was buffered by addition of NaHCO3 from day 186 - 194. Ammonia
oxidation to nitrate improved significantly, but precipitates in the sodium bicarbonate
buffered medium led to clogging of the inlet-tubes and thus to a disturbance of high
rate reactor operation. After re-installation of the pH titration system and the omission
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of sodium bicarbonate from day 194 onwards ammonia oxidation improved, leading
to around 20 mg N L-1 nitrite and up to 100 mg N L-1 nitrate, respectively (Fig. 3c).
In phase d of FBR A (conditions see Table 3), an effluent recirculation of 8 L h-1
(1.25 m h-1 upstream velocity) was installed. Immediately after starting recirculation of
the reactor content, ammonia was completely oxidized without intermediate formation
of nitrite (Fig. 3d, day 219 - 250). From day 250 to the end of reactor operation 20–40
mg N L-1 ammonia remained in the effluent, but no nitrite accumulated. The
decreasing AOR from day 250 onwards may have been due to a slow biofilm
detachment from the support material by effluent recirculation. The detached
biomass visibly settled in the conical bottom of the reactor.
Contrary to FBR A, the biofilm on the porous ceramic rings of FBR B oxidized all
ammonia to nitrate in phase a from the start of continuous operation (Fig. 4a). A
failure of the pH probe due to only short-term stability in saline medium caused a pH
decrease at day 8, 15 and 46, which led to short term incomplete oxidation of
ammonia until recalibration, but no significant amounts of nitrite accumulated. (Fig.
4a). An increase of the ALR to 104 mg N L -1 d-1 in phase b of FBR B led to an
increase of the ammonia and a decrease of the nitrate concentration from day 60–70
in the reactor effluent but no nitrite accumulated. All ammonia was oxidized to nitrate
from day 90 onwards (Fig. 4b). A further increase of the ALR to 130 mg N L -1 d-1 in
phase c did not affect the nitrifying performance of the reactor initially (Fig. 4c).
However, after day 180 ammonia was no longer oxidized completely, nitrite
accumulated and nitrate decreased. Replacing the titration unit by a bicarbonate
buffered medium (day 187-194) could not stop the decrease of the nitrate formation
(Fig. 4c, day 186–194). When the bicarbonate was omitted and the pH-titrator re-
installed, ammonia oxidation and nitrate formation was shortly improved but
accumulating nitrite led to a reversal of the improvement (Fig. 4c). To overcome this
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decreasing efficiency, an external recirculation was installed in phase d after day 216
to improve mixing. This led to a short recovery of ammonia and nitrite oxidation (Fig.
4d, day 219-240), but similar as in FBR A, the increased shear forces during
recirculation apparently led to a slow biofilm detachment, visible by the sludge, that
accumulated at the bottom of the reactor. The AOR decreased dramatically and at
first around 60, later on 80 mg N L-1 ammonia remained in the reactor effluent (Fig.
4d, day 248 and following).
Ammonia and nitrite oxidation rates in FBR A and FBR B
For determining the AORs and NORs in FBR A and FBR B, substrate supply was
stopped one day before rate analyses to obtain depletion of ammonia and nitrite. At
the respective days (Table 4) either NH4Cl or KNO2 was added to the reactor to
reach a final concentration of 60 or 30 mg N L-1, respectively. AORs and NORs were
determined from the slope of consumption curves and a surface area related
nitritation and nitratation rate for FBR A and FBR B was calculated (Table 4). The
NOR was always higher than the AOR, except for day 64 in FBR A and day 215 and
217 in FBR B, where nitrite accumulated due to an unknown disturbance (Fig. 4c,
4d). The surface area related AORs and NORs in FBR B with ceramic rings were
always lower than those in FBR A with polyethylene/clay sinter lamellas. The NOR,
especially in FBR B, was relatively stable, whereas the AOR showed a higher
fluctuation with time. After starting the external recirculation (phase d, Table 3), the
AOR in FBR A increased more than two-fold and the NOR more than 1.5-fold,
whereas the AOR and NOR in FBR B were not improved (Table 4. Day 217). There
was no positive short-term effect in FBR B as in FBR A, where the AOR at first
increased and then slowly decreased to the initial rates before recirculation, but the
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capacity for nitrite oxidation remained high. The NOR was not increased by a better
homogenization through recirculation in FBR B (Table 4).
Microbial population
Group-specific PCR analyses yielded
products with primer pairs specific for Bacteria , Nitrosomonas spp., and Nitrospira
spp. (Fig. 4). No products were obtained with primers specific for Nitrobacter spp.
and the archaeal amoA gene (not shown). Thus, the nitrifying population in the
reactors seemed to be dominated by Nitrosomonas spp. and Nitrospira spp..
The composition and dynamics of the nitrifyer populations was investigated using
PCR-DGGE followed by sequence analysis of cloned DGGE-bands. DGGE analyses
of samples from operational phases b and c (Fig. 5, Table 3: days 127, 160 and 210)
of FBR B showed in all cases relatively few bands for the bacterial profiles, indicating
that bacterial communities were represented by only a few phylo types. The most
dominant band was the same for all three sampling dates and migrated at the same
position as the single, dominant band (E) of Nitrospira -specific analyses (Fig. 5). The
ocurrence of only one band in the case of the Nitrospira -specific analyses indicated
that only one dominant organism was responsible for nitrite oxidation in the reactors,
which apparently did not change over time for different ALRs and pH-values. In
contrast, the AOB-specific profiles contained three bands each (A-C) for the first two
sampling dates, representing an ALR of 104 and 130 mg N L -1 d-1 at a pH of 7.5.
Band B disappeared and was replaced by a new band (D) in the third sample,
representing an ALR of 130 mg N L-1 d-1 in a bicarbonate buffered medium. Whereas
AOB-specific PCR products were not dominant or could not be seen in the DGGE
profiles for Bacteria of the first two samples, they were clearly recognizable in the
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third sample, indicating that AOB as well as Nitrospira spp. represented a significant
or even dominant part of the total bacterial population under these conditions (Fig. 5).
Elucidation of the sequences corresponding to dominant DGGE bands was done
by cloning of Bacteria -, AOB- and Nitrospira -specific PCR products and screening of
individual clones by RFLP and DGGE. Clones co-migrating with dominant DGGE
bands were sequenced. Figures 6 and 7 show the phylogenetic relatedness of the
obtained sequences to known sequences of AOB and Nitrospira spp., respectively.
The four detected AOB sequences (Fig. 5) were all related to salt-tolerant or salt-
requiring Nitrosomonas spp.: The DGGE-band A and B sequences were closely
related to Nitrosomonas aestuarii, which has been described as a common species in
marine and estuarine water with an obligate requirement for salt and an optimal
growth around 300 mM NaCl (1.7%) (Koops et al. 1991). The sequence related to
DGGE band D was more distantly related to N. aestuarii , but still clustered within the
N. aestuarii / N. marina clade of salt-requiring Nitrosomonas spp. The DGGE-band C
related sequence clustered within the Nitrosomonas Nm143 lineage, which contains
sequences found in coastal water and sediments with salinities above 1% (Purkhold
et al. 2003). The sequences of clones co-migrating with the Nitrospira -specific DGGE
band E were all closely related to the species N. marina , which was the first
obligately salt-requiring, marine nitrite oxidizer in this genus (Watson et al. 1986).
Discussion
Saline wastewater with a high load of nitrogen compounds is released by many
industries, such as sea food processing companies, tanneries, gelatin producers or
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even metal refining companies. An often reported but not always successful
approach for biological nitrification of saline wastewater is the stepwise adaption of
sweat water bacteria to halophilic conditions (e.g. Moussa et al. 2006). Adaption of a
sweat water nitrifying population to salt water conditions of up to 40 g/l NaCl seems
not to be possible (Moussa et al. 2006), whereas an enrichment of halophilic nitrifyers
from halophilic environmental sources would be a more promising approach, since
most halophilic nitrifyers are apparently ubiquitous in seawater environment (Francis
et al. 2005). Enrichment of halophilic nitrifying consortia from sea water or mud
samples of the coastal region of the North Sea in Germany with a salinity of about
3% NaCl (conductivity > 30 mS cm-1, Table 1) seemed thus to be most suitable to
establish halophilic nitrification in the laboratory. The applicability of marine
sediments as inocula for nitrification under saline conditions was also reported by
Antileo et al. (2002), who found ammonia oxidation after a lag-phase of 15 d. In our
first enrichments from different marine sources, AORs ranged between 4.9 and 15.1
mg N L-1d-1, which was in accordance with the work of Rejish Kumar et al. (2009),
who measured AORs of 4.6 and 12.2 mg N L-1d-1.
Villaverde et al. (1997) described a linear correlation between alkalinity (e.g. mg L -1
CaCO3) and pH with a stoichiometric coefficient of 7.1 mg CaCO3 consumed per mg
NH4+-N oxidized. If the alkalinity was not sufficient, the pH decreased during
oxidation of 50 mg N L-1 ammonia as it was observed in our samples A and C and to
a minor extent in sample D to values below pH 5 (Fig. 2). Sample B, a sea water/mud
mixture had the highest alkalinity and the pH was stable above 7.5 during the whole
experiment, including a second feeding with 50 mg N L -1 ammonia (Fig. 2b). Under
batch conditions, in samples A–D, a short lag-phase of approximately 10 d was
observed before ammonia oxidation started. An intermediate nitrite accumulation was
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observed in all samples (Fig. 2a-2d, 3a, 3c) independently of the pH. Whether nitrous
oxide was also formed in trace amounts under halophilic nitrification conditions, as
reported by Tsuneda et al. (2005) was not analysed.
In FBRs the support material seems to play a major role during the early stages of
a biofilm formed by fast-growing heterotrophic bacteria and during a much longer
time for biofilms with slow-growing autotrophic bacteria. Surface characteristics of the
support material are important, e.g. the roughness of surfaces and other surfaces
properties significantly influence bacterial colonization (Gjaltema et al. 1997, Verran
et al. 1991;). Crevices and pores act as niches for attachment of bacteria and protect
the biofilm from shear forces (Fox et al. 1990). In both of our FBRs, biomass
detachment was observed at increased shear forces after installation of liquid
recirculation. Concomitant with this phenomenon, AORs decreased notably, while the
NORs were apparently not influenced (Fig. 3d and 4d). The decrease was more
pronounced in FBR B with porous ceramic rings as a carrier material than in FBR A
with polyethylene-clay sinter lamellas. Turbulence in this reactor was visibly higher
than in FBR A due to more rugged surfaces through which the water must find it way
to the top. This might indicate, that the ammonia oxidizing nitrifyers were mainly
located in the outer layers of the biofilm on the support material and therefore may
have been sheared off to a higher extent by increased shear forces during liquid
recirculation. This would be in accordance with the report of Okabe et al. (1999), who
found a layering of AOB at the surface and of nitrite oxidizing bacteria in deeper
zones in nitrifying biofilms fed with domestic wastewater. A short-term effect
immediately after installation of the liquid recirculation was the increase of the AOR
and NOR in FBR A (Table 4, day 217) indicating that the better mixing, created by
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aeration and an increased up flow velocity (1.25 m h-1), apparently improved mass
transfer of oxygen and ammonia from the bulk liquid into the biofilm. Zhu and Chen
(2001) also observed an influence of turbulence on the AOR. The performance of
their nitrifying biofilters could be significantly improved by increasing the Reynolds
number in their biofilm reactor. In FBR B the aeration system was apparently
sufficient for an optimal supply of the nitrifyers in the biofilm with oxygen and
ammonia since the AOR and the NOR did not increase after starting the liquid
recirculation (Table 4, after day 215).
In FBR B, ceramic rings with a specific surface area of 934 m2 m-3 were used as
support material for biofilm formation, which was a twice as high specific surface area
than with polyethylene/clay sinter lamellas of FBR A. FBR B had a better nitrification
performance from the beginning of the continuous operation. Ammonia oxidation was
almost complete except when titration failed. Nitrite accumulation was only seen
during stage 3 (Table 3) after re-installation of the pH titrator (Fig. 4c). This was in
accordance with Krüner and Rosenthal (1983) who reported that the AOR was
proportional to the surface of the support material that was used for biofiltration. It
might be generalized, that the surface area of the support material significantly
influences the conversion rates when only a faint biofilm, as in the case of autotrophic
nitrifyers was formed, whereas the inner surfaces play only a minor role if a thick
biofilm was obtained as for carbon-rich industrial wastewater. Inner surfaces are then
blocked and diffusion of substrates into pores is highly limited.
The maximum AORs and NORs before installation of the liquid recirculation were 6
and 7 mg N L-1 h-1, respectively in FBR A, and 5 and 5.9 mg N L -1 h-1 in FBR B. To
correlate the specific surface area of the support material with the maximum N-
removal rate, area related AORs and NORs were calculated. For FBR A a maximum
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surface area related AOR and NOR of 312 and 386 mg N m -2 d-1 and for FBR B of
199 and 236 mg N L-1 d-1, respectively, was determined (Table 4). Maximal and area
related AORs and NORs were better in FBR A than in FBR B, but the overall
performance (residual ammonia in reactor effluent, intermediate nitrite accumulation)
was better in FBR B. This may be due to a surface oriented and a more dense biofilm
in FBR A with higher rates but less efficient conversion. Nijhof and Bovendeur (1990)
determined an area related AOR under saline conditions at 24 oC of 280 mg N m-2 d-
1, whereas a much better AOR under fresh water conditions of 690 mg N m -2 d-1 was
obtained .
In continuously run FBRs for halophilic nitrification, that were inoculated with sea
water, organisms that were targeted specifically by a universal primer for Bacteria
were rather rare. DGGE revealed that the one dominant band, present at all sampling
times, represented Nitrospira spp.. The bands for AOB in the first two samples were
the same and were almost invisible with the primer for Bacteria. The nitrifyer
populations in FBR B were composed of salt-requiring ammonia- and nitrite-oxidizing
bacteria. The AOB population remained the same between the first two sampling
dates, consisting of three organisms related to Nitrosomonas aestuarii and
Nitrosomonas sp. Nm143. Between the second and the third sampling date, the
organism corresponding to DGGE band B became less dominant and was replaced
by the organism corresponding to DGGE band D. The nitrite oxidizer population
consisted of organisms closely related to Nitrospira marina , which yielded a single
strong DGGE band present in all three samples.
Acknowledgment
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This work was supported by a grant from the German Academic Exchange Service
DAAD to Mr. Sudarno.
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Rosa MF, Furtado AAL, Albuquerque RT, Leite SGF, Medronho RA (1998) Biofilm
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Schenk H, Hegemann W (1995) Nitrification inhibition by high salinity concentrations
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wastewater in a sequencing batch reactor. Enzyme Microb Tech 34:313-318
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adhesion of Candida albicans to acrylic. Biofouling 3:183-192
Villaverde S, Garcia-Encina.A, Polanco (1997) Influence of pH over nitrifying biofilm
activity in submerged biofilters. Water Res 31:1180-1186
Wagner M, Rath G, Koops HP, Flood J, Amann R (1996). In situ analysis of nitrifying
bacteria in sewage treatment plants. WatSciTechn 34: 237-244
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Legends of Figures
Figure 1: Arrangement of the fixed-bed reactors used for nitrification experiments
Figure 2: Initiation of nitrification of ammonia (50 mg N L -1) by autochthonic nitrifyers
from different sea water and mud samples
Sample sources: A: Hafen Büsum (sea water), B: Town Norden (sea water), C: Town
St. Peter-Ording (brine water), D: Town St. Peter-Ording (sea water). At day 42 and
52 the pH was raised with KOH. In assay B ammonia was added a second time at
day 42. Symbols: ---- Ammonia, ---- Nitrite, ---- Nitrate, pH. The incubation
temperature was 20-23 oC.
Figure 3: Ammonia, nitrite and nitrate concentrations during continuous operation of
FBR A (support material: polyethylene/clay sinter lamellas) for conditions of Table 3.
Fig. 3a: day 0–55, phase a; Fig. 3b: day 55–155, phase b; Fig. 3c: day 155–215,
phase c; Fig. 3d: day 215–305, phase d. Symbols: ---- Ammonia, ---- Nitrite and --
-- Nitrate. The incubation temperature was 20-23 oC at an air flow rate of 2.5 L h -1.
Figure 4: Ammonia, nitrite and nitrate concentrations during continuous operation of
FBR B (support material: porous ceramic rings) for conditions of Table 3.
Fig. 4a: day 0–55, phase a; Fig. 4b: day 55–155, phase b; Fig. 4c: day 155–215,
phase c; Fig. 4d: day 215–305, phase d. Symbols: ---- Ammonia, ---- Nitrite and --
-- Nitrate. The incubation temperature was 20-23o
C at an air flow rate of 2.5 L h-1
.
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Figure 5: DGGE analysis of samples from FBR B.
The image shows DGGE profiles specific for Bacteria , ammonia-oxidizing bacteria,
and Nitrospira spp.. Samples were taken at day 127, 160 and 210 from FBR B.
Figure 6: Evolutionary relationships of ammonia-oxidizing bacteria.
Figure 7: Evolutionary relationship of Nitrospira spp.
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Table 1: Characterization of the used seawater/mud samples
___________________________________________________________________
Sample Conductivity Alkalinity NH4+-N NO2
--N NO3- -N
(mS cm-1) (mg L-1) (mg L-1) (mg L-1) (mg L-1)as CaCO3
___________________________________________________________________A Sea water from 31.9 120 0 0.11 2.3Hafen Büsum
B Sea water-mud 37.5 400 0.2 0.32 10.3mixture from townNorden
C Brine water from 1.34 53 0.9 0.37 5.1
town St. Peter-Ording
D Sea water from 32.1 130 0.6 0.68 1.7town St. Peter-Ording ___________________________________________________________________
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Table 2. PCR primers used in this study.The indicated primers for Nitrospira and Nitrobacter spp. were used as reverseprimers in combination with 8fm as forward primer.
Primer
name
Sequence (5’-3’) Reference
8fm AGA GTT TGA TC(AC) TGGCTC AG
Lane 1991
1492r G(CT)T ACC TTG TTA CGA CTT Lane 1991βAMOf TGG GGR ATA ACG CAY CGA
AAGMcCaig et al. 1994
NSO1225 CGC CAT TGT ATT ACG TGTGA
Mobarry et al. 1996
Ntspa662 GGA ATT CCG CGC TCC TCT Daims et al. 2001NIT3 CCT GTG CTC CAT GCT CCG Wagner et al. 1996Arch-amoAF
(GC)TA ATG GTC TGG CTTAGA CG
Francis et al. 2005
Arch-amoAR
GCG GCC ATC CAT CTG TATGT
Francis et al. 2005
341f-GC CGC CCG CCG CGC GCG GCGGGC GGG GCG GGG GCACGG GGG GCC TAC GGG AGGCAG CAG
Muyzer et al. 1993
518r ATT ACC GCG GCT GCT GG Muyzer et al. 1993pJET1f GCC TGA ACA CCA TAT CCA
TCCPromega
pJET1r GCA GCT GAG AAT ATT GTAGGA GAT
Promega
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Table 3: Operational phases a-d of FBR A and FBR B.
___________________________________________________________________
Phase a b c d
___________________________________________________________________
Days 0-55 55-155 155-186 187-194 195-215 215-305
HRT (d) 1.25 1 1 1 1 1
pH adjustment with KOH KOH KOH NaHCO3 KOH KOH
NH4+-Nin (mg L
-1) 104 104 130 130 130 130
ALR mg NH4+-N L-1 d-1 83 104 130 130 130 130
External recirculation - - - - - 8 L h-1
___________________________________________________________________
HRT = Hydraulic Retention Time, ALR = Ammonia Loading Rate.
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Table 4: Surface area specific ammonia and nitrite oxidation rates in FBR A and FBR
B.
________________________________________________________________
Days AOR Days NOR
(mg N m-2 d-1) (mg N m-2 d-1)
FBR A FBR B FBR A FBR B
__________________________________________________________________
48 274 230
64 306 156 65 230 226
84 176 51 85 386 236
113 145 156
173 312 199
215 207 197 216 363 182
217 502 197 218 547 181
257 295 112 258 484 210
284 272 149
295 218 82 296 525 214
___________________________________________________________________
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127 160 210127 160 210 127 160 210
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Nitrosospira spp.
AM295526
AM295525
AB212171
AM295527
AB239753
FN394308 DGGE band C
EF092247
AY123794 N. sp. Nm143
Nitrosomonas Nm143 lineage
AF272423 Nitrosomonas cryotolerans
AF272420 N. aestuarii
FN394309 DGGE band B
FN394310 DGGE band A
AF272424 N. sp. Nm51
AF272418 N. marina
M96400 N. sp. C-56
AJ621032 N. sp. Is343
AF386752 N. sp. R7c131
AF386751 N. sp. R7c155
EF092216
FN394311 DGGE band D
Nitrosomonas marina / aestuarii
Nitrosomonas ureae / oligotropha
Nitrosomonas nitrosa / communis
Nitrosococcus mobilis
Nitrosomonas halophila
Nitrosomonas eutropha / europaea
Outgroups
99
92
75
88
67
95
53
100
68
97
92
97
97
89
86
92
89
64
65
81
91
95
53
97
0.01
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Lineage I
Lineage II
AY555798 AY555810
AY532586
EF018873
EU084879 Candidatus N. bockiana
EF626882
EU097147
Lineage III
AB015550
EU491612
EU491406
EF999362
AJ863251
EF157239
FN394314 DGGE band E-1
FN394312 DGGE band E-2
DQ058673
X82559 N. marina
FN394313 DGGE band E-3
AM295541
Lineage IV
Outgroups
100
100
99
97
66
68
100
50
40
30
99
64
100 75
93
99
10028
96
67
67
94
56
66
0.02
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