decay nitrification
TRANSCRIPT
-
8/17/2019 Decay Nitrification
1/11
Available at www.sciencedirect.com
jo ur na l home pa ge : ww w. el sevi er. com /l oc at e/ wa tr es
Decay processes of nitrifying bacteria in biological
wastewater treatment systems
Reto Manser, Willi Gujer, Hansruedi Siegrist
Swiss Federal Institute of Aquatic Science and Technology (Eawag) and Swiss Federal Institute of Technology (ETH), CH-8600 Dü bendorf,
Switzerland
a r t i c l e i n f o
Article history:
Received 15 July 2005
Received in revised form
17 April 2006
Accepted 18 April 2006
Available online 6 June 2006
Keywords:
Activated sludge
Decay
Enzyme kinetics
Membrane bioreactor
Modeling
Nitrification
A B S T R A C T
A knowledge of the decay rates of autotrophic bacteria is important for reliably modeling
nitrification in activated sludge plants. The introduction of nitrite to activated sludge
models also requires the separate determination of the kinetics of ammonia- and nitrite-
oxidizing bacteria. Batch experiments were carried out in order to study the effects of
different oxidiation–reduction potential conditions and membrane separation on the
separate decay of these bacteria. It was found that decay is negligible in both cases under
anoxic conditions. No significant differences were detected between the membrane and
conventional activated sludge. The aerobic decay of these two types of bacteria did not
diverge significantly either. However, the measured loss of autotrophic activity was only
partly explained by the endogenous respiration concept as incorporated in activated sludge
model no. 3 (ASM3). In contrast to nitrite-oxidizing bacteria, ammonia-oxidizing bacteria
needed 1–2 h after substrate addition to reach their maximum growth rate measured as a
maximum OUR. This pattern could be successfully modeled using the ASM3 extended by
enzyme kinetics. The significance of these findings on wastewater treatment is discussed
on the basis of the extended ASM3.
& 2006 Elsevier Ltd. All rights reserved.
1. Introduction
Autotrophic decay rates have a significant impact on the
nitrification performance and therefore on the design and
analysis of wastewater treatment plants (WWTP). Safeguard-
ing the plant’s performance against wash-out or overload
depends directly on these kinetic parameters. Furthermore,
the extension of the biological treatment steps from COD
removal alone to nitrification, denitrification and biological
phosphorus removal exposes bacteria to different conditions
of oxidation–reduction potential (ORP). These appear to
influence the decay rates (Lee and Oleszkiewicz, 2003; Siegrist
et al., 1999; Martinage and Paul, 2000). On the other hand,
most activated sludge models (e.g. ASM3) summarize nitrifi-
cation as a single process. As a consequence, nitrite
concentrations cannot be modeled and the kinetics of AOB
and NOB are lumped into a single parameter set. However,
elevated effluent concentrations of nitrite may occur, causing
problems in the receiving water due to its toxicity. System
optimization or operation aspects may also benefit from a
detailed modeling of the nitrite dynamics in activated sludge
systems. An extension of the model to two-step nitrification
is then required, involving the separate determination of the
kinetics of ammonia-oxidizing bacteria (AOB) and nitrite-
oxidizing bacteria (NOB).
Decay is a general term with distinct meanings depending
on the context. From a microbiological point of view, decay
implies maintenance, endogenous respiration, degradation of
enzymes or lysis due to adverse environmental conditions
(Van Loosdrecht and Henze, 1999). In the maintenance
ARTICLE IN PRESS
0043-1354/$ - see front matter &
2006 Elsevier Ltd. All rights reserved.doi:10.1016/j.watres.2006.04.019
Corresponding author. Tel.: +411 823 5054; fax: +41 1 823 5389.E-mail addresses: [email protected] (R. Manser), [email protected] (H. Siegrist).
W A T E R R E S E A R C H 4 0 ( 2 0 0 6 ) 2 4 1 6 – 2 4 2 6
http://localhost/var/www/apps/conversion/tmp/scratch_3/dx.doi.org/10.1016/j.watres.2006.04.019mailto:[email protected]:[email protected]:[email protected]:[email protected]:[email protected]://localhost/var/www/apps/conversion/tmp/scratch_3/dx.doi.org/10.1016/j.watres.2006.04.019
-
8/17/2019 Decay Nitrification
2/11
process, an external substrate is used to keep the current
biological activity going, but the amount of bacteria is not
altered. The endogenous respiration concept involves the
consumption of the cell-internal substrate, which leads to a
loss of activity and slightly reduced biomass. Similarly,
enzyme degradation causes a loss of activity, but this is
rapidly restored if substrate becomes available. In contrast to
the previous processes, lysis leads to death and breaking
apart of the cells and therefore to a loss of bacteria. From a
process engineering point of view, decay describes the loss of
microbial activity in general. In state-of-the-art models (such
as ASM), the activity is directly proportional to the biomass
concentration and the loss of biomass is considered as a
single process. It is important to recall that the primary
objective of activated sludge models is to model nutrient
concentrations and not the number and state of the micro-
organisms. In an engineering context, therefore, decay should
adequately describe the loss of biomass ( ¼ loss of activity)
and was expressed as a single process due to the lack of
experimental data. In wastewater treatment systems, loss of
activity is probably due to a combination of several of the
mechanisms mentioned above. Predation by protozoa may
also play a major role (Van Loosdrecht and Henze, 1999;
Martinage and Paul, 2000), but is hidden in the decay
processes of bacteria in current activated sludge models.
Moussa et al. (2005) presented an extended version of ASM 2d
with two-step nitrification, predation and maintenance: it
was successfully applied to the modeling of a pilot sequen-
cing batch reactor (SBR).
Previous studies merely provide kinetic data on autotrophic
decay rates in activated sludge systems combining nitrifica-
tion as one process (summarized in Martinage and Paul,
2000). Wiesmann (1994) listed the same decay rates for both
AOB and NOB at 20 1C. Due to their different temperature
dependence, NOB has a higher decay rate than AOB at
temperatures below about 20 1C and a lower one above about
20 1C (Hellinga et al., 1998; Wyffels et al., 2004). By contrast,
Morgenroth et al. (2000) found the amount of NOB reduced
more greatly than the AOB after a starvation period over
several days at 23 1C using fluorescent in-situ hybridization
(FISH). It has to be considered that the technique used for the
determination of decay rates has a significant impact on their
values (Martinage and Paul, 2000). Different methods have
been proposed to experimentally study these various me-
chanisms and processes that are lumped under the name of
‘‘decay’’. The WERF report summarizes three different experi-
mental setups like SBR (or fill-and-draw) test, high F/M batch
test and continuous wash-out test (WERF, 2003). On top of
these methods, there is the respirometry-based method
which was used in this study. Activated sludge is placed in
a batch reactor and maximum oxygen utilization rates (OUR)
are regularly determined by adding small amounts of
substrate. Alternatively, substrate utilization rates can be
determined instead of OUR, with the advantage that the
influence of heterotrophic bacteria can be neglected. Under
aerobic conditions, autotrophic growth caused by ammonifi-
cation must be taken into account. Both methods only
provide information about available autotrophic activity; no
discrimination can be made between the reduction in the
amount of bacteria (lysis or predation) and the reduction of
activity (endogenous respiration). Measurement of the de-
crease of organic matter is insufficiently sensitive for
municipal activated sludge, because autotrophic biomass
accounts for only about 2–4% of the organic matter. In
contrast to previous methods, biomolecular techniques (e.g.
FISH) target active single cells. However, uncertainties in the
quantification hamper the identification of decay rates
directly from FISH measurements.
In summary, only little and inconsistent data are available
on the separate decay rates of AOB and NOB. Possible
differences between AOB and NOB may contribute to a better
understanding of nitrite dynamics. Furthermore, many
authors reported diminished decay rates under anoxic
conditions. However, the data from the literature vary
significantly and the exact reason for this decrease is not
yet known. Although the methods for the assessment of
autotrophic decay rates are mainly based on the measure-
ment of the overall activity, the impact of heterotrophic
activity, wastewater characteristics or the treatment process
may explain the different results.
The goal of this study was to determine the decay rates of
both AOB and NOB in municipal wastewater treatment
systems. The influence of the ORP conditions and the
treatment process (conventional and membrane bioreactor,
MBR) was also examined. The technique presented by Copp
and Murphy (1995) for the determination of decay rates using
respirometry was slightly modified. The underlying processes
are discussed and consequences for modeling of activated
sludge systems are presented on the basis of the results.
2. Materials and methods
2.1. Activated sludge samples
Samples were taken from a conventional activated sludge
(CAS) system and a MBR pilot plant (Manser et al., 2005c),
which were operated in parallel to treat domestic wastewater
following a typical diurnal hydraulic variation. The CAS and
the MBR treated wastewater corresponding to 60 (18 m3 d1)
and 2 (0.56m3 d1) population equivalents, respectively. The
oxygen concentration in the aerobic tanks was controlled
between 2.5 and 3gm3. Because the coarse bubble aeration
induced a cross-flow at the membrane surface, the oxygen
concentration was temporarily higher in the MBR. Both plants
were operated with pre-denitrification and the sludge reten-
tion time (SRT) was maintained at 20 days.
2.2. Batch experiments
Activated sludge samples were placed in a batch reactor that
was either continuously aerated (decay under aerobic condi-
tions), only stirred (decay at anoxic conditions) or a combina-
tion of both for a period of 7–10 days (Fig. 1). For the anoxic
experiment, nitrate (NaNO3) was manually added in order to
prevent anaerobic conditions. Autotrophic bacteria are ob-
ligate aerobic and cannot gain ATP under anoxic conditions.
The reactor was therefore aerated once a day for 5min in
order to prevent any effects of a complete lack of ATP. An
experiment with alternating stirred (8h) and aerated (16h)
ARTICLE IN PRESS
W AT E R R E S E A R C H 40 (2006) 2416– 2426 2417
-
8/17/2019 Decay Nitrification
3/11
phases simulating a typical wastewater treatment plant with
33% anoxic volume was conducted in order to investigate a
possible effect of the feast–famine phenomenon on decay
(Lee and Oleszkiewicz, 2003). At intervals of one day, one liter
of activated sludge was withdrawn from the batch reactor andcentrifuged at 3000 rpm for 7 min. The pellet was subse-
quently re-suspended with effluent from the MBR (permeate)
and placed in a secondary batch reactor. The main purpose of
the centrifugation step was to provide low nitrate (ammonia
for anoxic experiment) concentrations for the measurements,
because nitrate concentrations of only 50 g N m3 were found
to lead to a 20% reduction of the nitratation rate for the same
activated sludge (Appendix). After determining the base OUR
(Fig. 1: A), samples were successively spiked with nitrite
(NaNO2, 6–8 g N m3) and ammonia (NH4Cl, 10–18g N m
3),
leading to maximum nitratation (Fig. 1: B) and nitritation
rates (Fig. 1: C). The dissolved oxygen (DO) concentration was
controlled between 3 and 4 g O2 m3. OURs (OURi) werecalculated as the slopes of the measured DO by linear
regression (Fig. 1). The maximum OURs (OURmax) represent
mean values of at least four single OURs (Eq. (1)–(3)). All
experiments were carried out at pH 7.5 and 20 1C. The pH was
controlled using HCl and NaHCO3.
OURHET;m ¼
PnOURHET;i
n , (1)
OURmax;NOB ¼
PnOURNOB;i
n OURHET;m, (2)
OURmax;AOB ¼
P
n
OURAOB;in OURmax;NOB OURHET;m. (3)
2.3. Fluorescence in situ hybridization (FISH)
Samples were taken at maximum OUR of AOB and fixed in 4%
paraformaldehyde as described by Amann et al. (1990).
Ultrasonification (35 kHz, 5 min) was applied to fixed samplesfrom the CAS prior to hybridization in order to break up large
flocs. In situ hybridizations of cells were performed with
fluorescently labeled rRNA-targeted oligonucleotide probes
according to Manz et al. (1992) (Table 1). Parallel hybridization
with the Nso1225 probe targeting most known AOB showed
that the applied probes covered the vast majority of the AOB
(data not shown). Oligonucleotide probes were obtained from
Microsynth (Balgach, Switzerland) and Thermo Hybaid (Inter-
activa Division, Ulm, Germany).
All samples hybridized with oligonucleotide probes were
embedded in Citifluor (Citifluor, Canterbury, United Kingdom)
prior to microscopic observation. Epifluorescence microscopy
was performed on an Olympus BX50 microscope equippedwith HQ-CY3 and HQ-FLUOS filters (both from Analysentech-
nik AG, Tu ¨ bingen, Germany). The nitrifying bacteria were
quantified according to Manser et al. (2005b).
2.4. Modeling
The activated sludge model No. 3 (ASM3, Gujer et al., 1999)
was extended with two-step nitrification to enable separate
modeling of ammonia and nitrite oxidation (Table A1).
Denitrification of nitrite and from nitrate to nitrite was not
included. The loss of activity associated with a loss of bacteria
is modeled as a single process (endogenous respiration) in the
ASM3. The endogenous respiration of heterotrophic bacteria
ARTICLE IN PRESS
0
100
200
300
400
500
600
700
0 60 120 180
time (min)
O
U R ( g O 2 m - 3 d
- 1 )
2
3
4
5
6
7
8
D O
( g O 2 m - 3 )
T = 20±0.2°C
V = 50 l
pH = 7.5±0.1
T = 20±0.1°C
V = 1 l
pH = 7.5±0.1
CentrifugationEffluent MBR
Pellet
DO
NO2 C
BA
NH4
Fig. 1 – Experimental setup for batch experiments. A base oxygen utilization rate (heterotrophic rate), B max. nitratation
rate, C max. nitritation rate.
Table 1 – Oligonucleotide probes and hybridization conditions applied in this study
Probe Target organisms Reference
NEUa
Most halophilic and halotolerant ammonia oxidizers in the beta-subclass of Proteobacteria Wagner et al. (1995)NmII Many members of the Nitrosomonas communis lineage Pommerening-Ro ¨ ser et al. (1996)
Nmo218 Many members of the Nitrosomonas oligotropha lineage Gieseke et al. (2001)
Nso1225 Most known ammonia oxidizers in the beta-subclass except N. mobilis Mobarry et al. (1996)
a Used with an unlabeled competitor as indicated in the reference.
W A T E R R E S E A R C H 4 0 ( 2 0 0 6 ) 2 4 1 6 – 2 4 2 62418
-
8/17/2019 Decay Nitrification
4/11
is a lumped process accounting for the OUR due to growth on
decay products, growth on very slowly degradable COD and
probably also the respiration of protozoa (Van Loosdrecht and
Henze, 1999). In the following, heterotrophic OUR (OURHET,m)
represents the base OUR measured before the addition of
substrate (Fig. 1: B, Eq. (1)), the nitratation rates (OURmax,NOB)
after addition of nitrite (Fig. 1: B, Eq. (2)) and the nitritation
rates (OURmax,AOB) after addition of ammonia and complete
enzyme synthesis (Fig. 1: C, Eq. (3)). During the aerobic
experiments, large amounts of organic nitrogen are released,
probably due to the endogenous respiration of heterotrophic
bacteria, hydrolyzed to ammonium and immediately nitrified
to nitrate. Since this study focuses on nitrifying bacteria and
in order not to extend the model structure of the ASM3, the
heterotrophic endogenous respiration process was adapted
slightly in order to better fit the accumulation of nitrate. A
term considering the observed lag phase of the nitrate
accumulation was therefore introduced for modeling the
aerobic experiments (Table 2) and the nitrogen content of the
bacteria was assumed to be 10% referred to the COD.
All simulations and parameter estimations using a non-
linear least-squares algorithm were performed with the
AQUASIM software package (Reichert, 1994). It was assumed
that all kinetic parameters remain unchanged during the
course of the experiments. A sensitivity analysis showed that
other kinetic parameters, e.g. yield coefficients were not
sensitive on the estimation of the decay rates. Correlations
with other parameters of the extended ASM3 (e.g. f XI or iNXI)
are negligible. The default kinetic parameters provided by
Koch et al. (2000) were therefore used. Applied yield coeffi-
cients were 0.21 and 0.03 g COD g N1 for AOB and NOB, respec-
tively. bHET,aer and XHET,ini were estimated from the nitrate
measurements, whereas the initial autotrophic biomass
concentrations XAOB,ini and XNOB,ini were estimated together
with the decay rates of bAOB and bNOB, respectively.
3. Results
3.1. Decay under aerobic conditions
The results of the aerobic experiment for sludge from the CAS
are shown in Fig. 2. The activity is reduced to about 60% of the
initial value after 7 days for both AOB and NOB. Despite the
fact that nitrate accumulation and the subsequent growth of
autotrophic bacteria on the released nitrogen is well repro-
duced by the adapted ASM3 (Table 2), the sharp loss of
autotrophic activity during the first two days of the experi-
ment does not seem to be consistent with the underlying
model processes. Thus, data points at t ¼ 0 were omitted for
the estimation of the parameters listed in Table 3. Experi-ments with sludge from the CAS and MBR yielded similar
results. The quantification of the major groups of AOB using
FISH confirmed the sharp reduction in activity at the
beginning of the experiment (Fig. 3).
3.2. Decay under anoxic conditions
The results of the anoxic experiment for sludge from the CAS
are shown in Fig. 4. The loss of activity is negligible for both
ARTICLE IN PRESS
Table 2 – Adaptation of ASM3 to reproduce the observeddelay of the ammonia release
Process Process rateequation r
Aerobic endogenous respiration of XH bH;aerSO
KOþSO
tt0 f lag þðtt0Þ
XH
XH ¼ heterotrophic bacteria. f lag ¼ fit parameter. t ¼ simulation
time, t0 ¼ initial time.
0
200
400
600
800
0 2 4 6 8
time (d)
0
50
100
150
200
O U R N O B
( g O 2 m - 3 d
- 1 )
AOB
NOB
heterotrophic
0
2000
4000
6000
0 4 6 8
time (d)
C O D ( g O 2 m - 3 )
0
50
100
150
S N O 3 ( g N
m - 3 )
COD
SNO3
O U R A O B , O U R H E T ( g O 2 m - 3 d
- 1 )
2
Fig. 2 – Results of batch experiment for CAS sludge under aerobic conditions at 20 1C and pH 7.5. The lines represent the best
fit obtained by applying the adapted ASM3. Experiments with MBR sludge yielded similar trends.
Table 3 – Estimated aerobic endogenous respiration rates(with standard errors) at 20 1C using the adapted ASM3
AOB NOB Heterotrophic
bAOB,aerobic (d1) bNOB,aerobic (d
1) bHET,aerobic (d1)
CAS 0.1570.02a 0.1570.01a 0.2870.05a
MBR 0.1470.01 0.1470.01 0.2370.03
a Mean value from two experiments.
W AT E R R E S E A R C H 40 (2006) 2416– 2426 2419
-
8/17/2019 Decay Nitrification
5/11
AOB and NOB over a period of one week. Estimated anoxic
endogenous respiration rates of autotrophic bacteria were
0.02d1 or lower for both CAS and MBR sludge (Table 4).
Heterotrophic endogenous respiration rates were estimated
from the measured nitrate concentrations (denitrification
was only attributed to the anoxic endogenous respiration of
heterotrophic bacteria). It was assumed that nitrite did not
accumulate during denitrification under COD limiting condi-
tions (nitrite concentrations were not measured).
3.3. Decay under alternating anoxic–aerobic conditions
The results of the alternating anoxic–aerobic experiment for
sludge from the CAS are shown in Fig. 5. As in the aerobic
experiment, the ASM3 had to be adapted in order to model
the lag phase observed in the nitrate measurements (Table 2).
The estimated aerobic endogenous respiration rates of AOB
and NOB are shown in Table 5, assuming mean anoxic rates
estimated from the anoxic experiment (0.01 d1).
3.4. Enzyme dynamics
Enzyme processes (activation, synthesis, degradation, inhibi-
tion) are comparatively fast and therefore cannot account for
the loss of autotrophic activity at the beginning of the aerobic
experiments. Enzyme activation is the fastest mechanism for
regulating a process and can be stopped or reactivated within
minutes, depending on the presence of an inhibitor. Our
measurements showed constant activation times of about
10min for nitritation (Fig. 6A). The subsequent enzyme
synthesis took between 1 and 2 h. In contrast, the NOB
reached their maximum OUR immediately. The enzyme
saturation for every measurement was calculated as the ratio
of the OUR after the activation time and the maximum OUR
after complete enzyme synthesis. Cell growth during the
phase of enzyme synthesis was neglected in this calculation.
As shown in Fig. 6B, enzyme saturation was reduced to about
60% of its maximum level after 6 h under aerobic conditions
followed only by a marginal decline. Enzyme degradation was
more enhanced under aerobic than under anoxic conditions
(Fig. 6C). The ASM3 (with already implemented two-step
nitrification) was extended by enzyme kinetics adapted from
Wild et al. (1995) in order to test its sensitivity on the
ammonia and nitrite dynamics in wastewater treatment
systems (Table 6).
In ASM3, the growth rate of XAOB has to be multiplied by the
degree of cell saturation with nitritation enzymes. Esat is
proportional to the actual total amount of enzymes divided by
the actual biomass of XAOB. It is assumed that the anoxic
ARTICLE IN PRESS
0
100
200
300
400
500
0 4 8
time (d)
0
30
60
90
120
150
O U R N O B
( g O 2 m - 3 d -
1 )
0
1000
2000
3000
4000
5000
0 4 6 8
time (d)
C O D ( g O 2 m - 3 )
0
20
40
60
80
100
S N O 3 ( g N
m - 3 )
O U R A O B , O U R H E T ( g O 2 m - 3 d - 1 )
2 62
AOB
NOB
heterotrophic
SNO3
COD
Fig. 4 – Results of batch experiment for CAS sludge under anoxic conditions at 20 1C and pH 7.5. The lines represent the best
fit obtained by applying the ASM3. Experiments with MBR sludge yielded similar trends.
Table 4 – Estimated anoxic endogenous respiration rates(with standard errors) at 20 1C using the ASM3
AOB NOB HeterotrophicbAOB,anoxic (d
1) bNOB,anoxic (d1) bHET,anoxic (d
1)
CAS 0.01570.004 o0.001 0.03370.002
MBR 0.0170.003 0.0270.009 0.06470.002
0
5
10
15
20
0 4 8
time (d)
N.oligotropha
N.communis
N.europaea
Sum AOB
a b u n d a n c
e ( 1 0 3 µ m 3 m m f l o c - 2 )
2 6
Fig. 3 – Quantification of ammonia-oxidizing bacteria (AOB)
in the aerobic experiment using FISH.
W A T E R R E S E A R C H 4 0 ( 2 0 0 6 ) 2 4 1 6 – 2 4 2 62420
-
8/17/2019 Decay Nitrification
6/11
ARTICLE IN PRESS
0
200
400
600
800
0 4 6 8
time (d)
0
50
100
150
200
O U R N O B
( g O 2 m - 3 d
- 1 )
heterotrophic
AOB
NOB
O U R A O B , O
U R H E T ( g O 2 m - 3 d
- 1 )
0
1000
2000
3000
4000
5000
0 4 8
time (d)
C O
D ( g O 2 m - 3 )
0
20
40
60
80
100
S
N O 3 ( g N
m - 3 )
COD
SNO3
2 2 6
Fig. 5 – Results of batch experiment for CAS sludge under alternating anoxic–aerobic conditions at 20 1C and pH 7.5. The lines
represent the best fit obtained by applying the adapted ASM3. AOB and NOB activity during anoxic periods was omitted for
better readability. Experiments with MBR sludge yielded similar trends.
Table 5 – Estimated endogenous respiration rates (with standard errors) from the anoxic–aerobic experiment at 20 1C using
the adapted ASM3
AOB NOB Heterotrophic
bAOB,aerobic (d1) bAOB,anoxic (d
1) bNOB,aerobic (d1) bNOB,anoxic (d
1) bHET,aerobic (d1) bHET,anoxic (d
1)
CAS 0.1570.01 0.01a 0.2270.01 0.01a 0.2770.02 0.0670.004
MBR 0.1370.01 0.01a 0.1870.01 0.01a 0.2370.02 0.1070.01
a Mean value derived from anoxic experiment.
0.0
0.2
0.4
0.6
0.8
1.0
0 4 8
time (d)
E n z y m e s a t u r a t i o n A O B
0.0
0.2
0.4
0.6
0.8
1.0
0 12 18 24
time (h)
E n z y m e s a t u r a t i o n A O B
0
200
400
600
800
1000
0 30 60 90 120 150
time (min)
O U R ( g O 2 m - 3 d
- 1 )
activation
~ 10min
enzyme
synthesiscell
growth
6 2 6
aerobicanoxic-aerobicanoxic
(A) (B) (C)
Fig. 6 – Illustration of enzyme activation and synthesis (AOB) for a single measurement as a possible explanation of the
observed OUR pattern (A). Short-term degradation of enzymes (AOB) under aerobic conditions (B). Long-term degradation of
enzymes (AOB) during decay experiments (C). The enzyme saturation was calculated as a ratio of the OUR after the activation
time and the maximum OUR after complete enzyme synthesis. The lines represent the best fit obtained using the ASM3
extended by enzyme kinetics ( Table 6 ). Data from experiments with conventional activated sludge are shown.
Table 6 – Stoichiometric matrix and process rate equations (adapted from Wild et al., 1995 ).
Process Esat Process rate (r)
Enzyme synthesis of XAOB 1 ksynthSNH
KNH;AOBþSNH
SOKO;AOBþSO
SALKKALK;AOBþSALK
ð1 EsatÞ
Aerobic enzyme decay of XAOB 1 kdecaySO
KO;AOBþSOEsat
Growth of XAOB — mm;AOBSNH
KNH;AOBþSNH
SOKO;AOBþSO
SALKKALK;AOBþSALK
XAOBEsat
Esat ¼ Enzyme saturation (–).
W AT E R R E S E A R C H 40 (2006) 2416– 2426 2421
-
8/17/2019 Decay Nitrification
7/11
decay of nitritation enzymes is negligible. The data presented
in Fig. 6B and several data sets from batch experiments
(sample shown in Fig. 6A) were used to estimate the unknown
parameters ksynth and kdecay. The values obtained at 20 1C are
as follows:
ksynth ¼ 30 4 d1
; kdecay ¼ 3:0 0:3 d1.
The maximum enzyme saturation is less than 1 due to the
continuous decay of the enzymes. With the estimated
parameters, the maximum achievable enzyme saturation is
0.9 at 20 1C. The temperature dependency is assumed to be
equal to the growth of the AOB.
4. Discussion
4.1. Decay rates
The values of the estimated aerobic autotrophic endogenous
respiration rates correspond to the literature data for one-
step nitrification (summarized in Martinage and Paul, 2000).
No differences were found between AOB and NOB. The
aerobic heterotrophic endogenous respiration rates agreed
well with the values used for modeling in previous studies
(Gujer et al., 1999; Koch et al., 2000). No shift was observed
within the AOB population during the experiment. After two
days, a significant amount of AOB had either fallen into a
dormant state (below the detection limit of FISH) or had been
grazed by protozoa.
The values of the estimated anoxic autotrophic endogenous
respiration rates contrast with previous studies (Lee and
Oleszkiewicz, 2003; Siegrist et al., 1999) that stated only a
30–50% reduction of these parameters under anoxic com-
pared to aerobic conditions. In comparison to previous
studies, our experimental setup provided measurements that
always used the same matrix (sludge washed with effluent of
the MBR) and daily aerobic periods of about 10 min. Nitrate
inhibition is a possible reason for the observed difference (see
Appendix). Additionally, starvation and OUR measurements
were carried out in the same reactor in the study of Siegrist et
al. (1999) leading to extended aerobic periods and increasing
decay, which were not considered. Finally, different waste-
water characteristics and community compositions of auto-
trophic bacteria may also play a role here (Martinage and
Paul, 2000).
Bacteria are exposed to alternating ORP conditions in
WWTP with nutrient removal. Since nitrifying bacteria are
obligate aerobes, they are unable to store or utilize their
substrate under anoxic conditions due to the lack of oxygen.
As a result, stress and damage to their metabolisms may
occur under anoxic conditions, leading to increased substrate
requirements during the aerobic period, also known as the
feast–famine phenomenon (Chen et al., 2001). In contrast to
the completely aerobic experiment, the measured decrease of
autotrophic activity could be reasonably modeled using the
adapted ASM3 (Fig. 5). While endogenous respiration rates of
AOB and heterotrophic bacteria from the aerobic experiment
(Table 3) were confirmed, aerobic endogenous respiration
rates of NOB and anoxic endogenous respiration rates
of heterotrophic bacteria are higher. The results suggest
that NOB are more stressed than AOB under alternating
anoxic–aerobic conditions.
Our experiments confirm previous studies (Lee and Olesz-
kiewicz, 2003; Siegrist et al., 1999; Martinage and Paul, 2000)
showing that ORP conditions (aerobic or anoxic) are crucial
for the loss of microbial activity. The extent of the reduction
of microbial activity under anoxic conditions may be influ-
enced by the wastewater characteristics, the microbial
community composition or operational parameters. The floc
structure of the activated sludge does not seem to have an
impact on the decay, since our results exhibit no difference
between a CAS (large flocs) and a MBR (small flocs, Manser et
al., 2005a) operated at the same sludge age. The feast–famine
phenomenon—stress and damage during the fasting period
and therefore enhanced substrate removal rates for repair
processes during the feasting period—resulting in lower
decay rates under alternating anoxic–aerobic conditions as
previously reported (Lee and Oleszkiewicz, 2003) was not
observed in our study. However, the authors neglected
autotrophic growth on released ammonia. Therefore, their
estimated decay rate possibly does not only reflect decay but
also growth of bacteria leading to a lower observed decay rate.
We found similar decay rates for AOB and NOB, which is in
agreement with Wiesmann (1994). Different factors probably
affect the decay of bacteria. From a microbiological point of
view, it is likely that most bacteria do not die—unless they are
exposed to toxic compounds, for instance—but rather be-
come dormant (Kaprelyants and Kell, 1996). However, preda-
tion may play a major role in activated sludge systems (Van
Loosdrecht and Henze, 1999). Studies on modeling predation
in activated sludge systems are a first step towards under-
standing their impact on wastewater treatment (Moussa
et al., 2005). But it remains uncertain as to how protozoa affect
nitrifiers, because the latter prefer to grow in dense aggregates
(Wagner et al., 1995). Furthermore, the transferability of the
decay parameters measured in batch experiments to contin-
uous flow systems has not been addressed so far. Since small
amounts of substrates are always available in activated sludge
plants, the decay pattern in continuous flow systems may be
different. In this regard, in situ measurement of the decay of
radio-labeled nitrifiers in continuous flow systems, for in-
stance, would avoid the change to batch conditions.
4.2. Enzyme dynamics
Enzyme dynamics control the short-term change of biomass
activity. Vanrolleghem et al. (2004) already examined the
transient response of heterotrophic activated sludge activities
to sudden changes in substrate concentration. Although a
transient time of only 5–10 min was measured, the authors
concluded that consideration of the transience phenomenon
is important for correct data interpretation and plays a role in
plants with highly fluctuating loads.
The time needed after activation until the AOB reached
their maximum OUR was 1–2 h, which is in agreement with
the literature data for enzyme synthesis (Aoi et al., 2004;
Sayavedra-Soto et al., 1996). Although the AOB were able to
continuously nitrify small amounts of released ammonia,
enzyme degradation was more enhanced under aerobic
conditions (Fig. 6C). Nonetheless, the continuous release of
ARTICLE IN PRESS
W A T E R R E S E A R C H 4 0 ( 2 0 0 6 ) 2 4 1 6 – 2 4 2 62422
-
8/17/2019 Decay Nitrification
8/11
ammonia due to heterotrophic decay causes the AOB to
maintain a minimal level of enzyme saturation. Our esti-
mated half-life times of the order of hours agree with the
literature data (Sayavedra-Soto et al., 1996; Aoi et al., 2004).
The two new processes allow reasonable reproduction of the
measured values (Fig. 6). Only the long-term degradation
during the aerobic decay experiment is underestimated by
the model (Fig. 6C), but this should not play a role in the
practical operation of WWTP.
4.3. Significance for wastewater treatment
A simulation study was carried out in order to test the
sensitivity of the reduction of anoxic autotrophic decay and
the enzyme kinetics to the nitrification process. Three
different model configurations based on the ASM3 with two-
step nitrification were applied:
Model A: ASM3 default. Anoxic autotrophic
decay ¼ 50% of aerobic decay.Model B: Anoxic decay ¼ 0. No autotrophic decay
under anoxic conditions.
Model C: Including enzyme kinetics. Model B
extended by enzyme kinetics for AOB
(Table 6). Maximum growth rate of AOB
(mm,AOB) was increased by a factor of
1=Esat;max ¼ 0:88 (Fig. 8) in order to exclude
the effect of an overall reduced growth
rate.
A CAS with three completely mixed reactors was assumed.
The hydraulic retention time was chosen to be 12 h. The
temperature was set to 151C. A typical diurnal influent
variation of the ammonia load for municipal wastewater
was used (Fig. 7).
The sensitivity of the model predictions was investigated
on two common plant layouts (Fig. 7): fully aerobic and with a
33% anoxic volume. The DO concentration in the aerobic
reactors was fixed at 2.5 g O2 m3, whereas the aerobic sludge
age was set to 6 d in both layouts.
The results reveal that enzyme kinetics has an impact on
the ammonia concentrations in the effluent for typical
diurnal variation in the influent. Neglecting enzyme dy-
namics leads to underestimating the ammonia concentra-
tions for fully aerobic and partly anoxic plants. Anoxic
conditions diminish the diurnal variation of the enzyme
saturation of AOB (Fig. 8, only aerobic degradation of enzymes
assumed), leading to a slightly lower ammonia peak in the
effluent (Fig. 7). Nonetheless, the enzyme saturation is always
above 75% even under fully aerobic conditions for the chosen
characteristics of the domestic influent. However, the differ-
ences are within the measurement uncertainty of ammonium
and could be compensated by, for example, a 10% increase in
the maximum growth rate of AOB. Pre-denitrification ob-
viously decreases the nitrification performance in Model A
due to the loss of nitrifiers within the anoxic reactor, whereas
Model B (without anoxic autotrophic decay) predicts equal
ARTICLE IN PRESS
0
50
1000
1500
2000
time (d)
0 0.5 1
0.0
0.2
0.4
0.6
0.8
0.0
0.1
0.2
0.3
0 0.2 0.4 0.6 0.8 1
time (d)
0.0
0.2
0.4
0.6
0.8
0.0
0.1
0.2
0.3
0 0.2 0.4 0.6 0.8
time (d)
Mod. A: ASM3 default
Mod. B: anoxic decay = 0
Mod. C: incl. enzyme kinetics
T = 15°C
Influent variation
N H 4 l o a d ( g N
d - 1 )
N O 2 ( g N
m - 3 )
N H 4 ( g
N
m - 3 )
1
Fig. 7 – Simulated concentrations of ammonia and nitrite in the effluent of the third reactors.
0.6
0.7
0.8
0.9
0 0.2 0.4 0.6 0.8
time (d)
e n z y m e s a t u r a t i o n E s a t ( - )
1
fully aerobic
33% anoxic
Fig. 8 – Diurnal variation of the enzyme saturation Esat of
AOB (Model C).
W AT E R R E S E A R C H 40 (2006) 2416– 2426 2423
-
8/17/2019 Decay Nitrification
9/11
-
8/17/2019 Decay Nitrification
10/11
sludge samples were taken from continuous flow systems
and analyzed in batch systems, where other mechanisms
may occur.
2. Anoxic conditions significantly reduce the loss of auto-
trophic activity. The large range of this reduction from 30
to almost 100% found in different studies (Lee and
Oleszkiewicz, 2003; Siegrist et al., 1999; this study) is
partly due to the different experimental setups. It cannot
be excluded that this reduction may be influenced by
wastewater characteristics, the composition of the micro-
bial community and operational parameters. The floc
structure of the activated sludge does not play a role, since
no differences were found between the conventional
activated (large flocs) and membrane activated (small
flocs) sludge. No additional impact of alternating anox-
ic–aerobic conditions was detected on the autotrophic
decay rates due to the feast–famine phenomenon.
3. AOB and NOB exhibited similar endogenous respiration
rates. Since the literature data on the decay rates of two-
step nitrification are scarce and inconsistent, further
research are needed to provide evidence on this issue.
4. AOB needed 1–2 h after substrate addition to reach their
maximum growth rate measured as a maximum OUR.
This pattern could be successfully modeled using the
ASM3 extended by enzyme kinetics. The extension of
activated sludge models by enzyme kinetics for AOB may
lead to a better understanding of ammonia dynamics in
WWTP with highly fluctuating influent loads.
Further research is needed to elucidate the processes involved
in the loss of autotrophic activity in activated sludge systems.
In particular, in situ measurement of the decay of radio-
labeled nitrifiers in continuous flow systems, for example,would avoid the change to batch conditions. The parallel
measurement of protozoa activity (e.g. Moussa et al., 2005)
would provide additional insights into the processes sum-
marized under decay.
Appendix
This appendix gives the results from batch experiments on
the nitrate inhibition of NOB. Fig. A1 shows the measured
decrease of the maximum nitratation rate in relation to the
initial maximum nitratation rate (nitrate concentration
E5 g N m3) as determined by respirometry. The activated
sludge was consecutively spiked with nitrate (NaNO3) and the
influence on the OUR was monitored. The nitrite concentra-
tion was always non-limiting (between 4 and 8 g N m3) and
inhibition due to free nitrous acid should be negligible
(Wiesmann, 1994). OUR were measured between 3 and
4 g O2 m3. All experiments were carried out at pH 7.5 and
16 1C. Three batch experiments were performed within one
month using activated sludge from the conventional pilot
plant (see Section 2.1) (Table A1).
The results show that a nitrate concentration of only
50 g N m3 leads to a 20% reduction and about 120g N m
3 to
as much as a 50% reduction in the nitratation rate. Analysis of
the community composition revealed that the NOB were
dominated by members belonging to the genus Nitrospira,
which seems to be a typical K-strategist (Schramm et al.,
1999). This may explain the inhibition already observed at
moderate nitrate concentrations.
R E F E R E N C E S
Amann, R., Binder, B., Olson, R., Chisholm, S., Devereux, R., Stahl,D.A., 1990. Combination of 16S rRNA-targeted oligonucleotideprobes with flow cytometry for analyzing mixed microbialpopulations. Appl. Environmental Microbiology 56 (6),1919–1925.
Aoi, Y., Masaki, Y., Tsuneda, S., Hirata, A., 2004. Quantitativeanalysis of amoA mRNA expression as a new biomarker of ammonia oxidation activities in a complex microbial com-munity. Lett. Appl. Microbiol. 39 (6), 477–482.
Chen, G.H., Yip, W.K., Mo, H.K., Liu, Y., 2001. Effect of sludgefasting/feasting on growth of activated sludge cultures. WaterRes. 35 (4), 1029–1037.
Copp, J.B., Murphy, K.L., 1995. Estimation of the active
nitrifying biomass in activated-sludge. Water Res. 29 (8),1855–1862.
Gieseke, A., Purkhold, U., Wagner, M., Amann, R., Schramm, A.,2001. Community structure and activity dynamics of nitrifying bacteria in a phosphate-removing biofilm. Appl. Environ.Microbiol. 67 (3), 1351–1362.
Gujer, W., Henze, M., Mino, T., van Loosdrecht, M., 1999. Activatedsludge model No. 3 (Vol. 39, p. 183, 1999). Water Sci. Technol. 39(12) AR1–AR1.
Hellinga, C., Schellen, A., Mulder, J.W., van Loosdrecht, M.C.M.,Heijnen, J.J., 1998. The SHARON process: an innovative methodfor nitrogen removal from ammonium-rich waste water.Water Sci. Technol. 37 (9), 135–142.
Kaprelyants, A.S., Kell, D.B., 1996. Do bacteria need to commu-nicate with each other for growth? Trends Microbiol. 4 (6),
237–242.Koch, G., Kuhni, M., Gujer, W., Siegrist, H., 2000. Calibration and
validation of activated sludge model No. 3 for Swiss municipalwastewater. Water Res. 34 (14), 3580–3590.
Lee, Y., Oleszkiewicz, J.A., 2003. Effects of predation and ORPconditions on the performance of nitrifiers in activated sludgesystems. Water Res. 37 (17), 4202–4210.
Manser, R., Gujer, W., Siegrist, H., 2005c. Membrane bioreactor vs.conventional activated sludge system—population dynamicsof nitrifiers. Water Sci. Technol. 52 (10–11), 417–425.
Manser, R., Gujer, W., Siegrist, H., 2005a. Consequences of masstransfer on the kinetics of nitrifiers. Water Res. 39 (19),4633–4642.
Manser, R., Gujer, W., Siegrist, H., 2005b. A rapid method forquantification of nitrifiers in activated sludge. Water Res. 39(8), 1585–1593.
Manz, W., Amann, R., Ludwig, W., Wagner, M., Schleifer, K.H.,1992. Phylogenetic oligodeoxynucleotide probes for the majorsubclasses of proteobacteria—problems and solutions. Sys-tematic Appl. Microbiol. 15 (4), 593–600.
Martinage, V., Paul, E., 2000. Effect of environmental parameterson autotrophic decay rate (b(A)). Environ. Technol. 21 (1),31–41.
Mobarry, B.K., Wagner, M., Urbain, V., Rittmann, B.E., Stahl, D.A.,1996. Phylogenetic probes for analyzing abundance and spatialorganization of nitrifying bacteria. Appl. Environ. Microbiol. 62(6), 2156–2162.
Morgenroth, E., Obermayer, A., Arnold, E., Bruhl, A., Wagner, M.,Wilderer, P.A., 2000. Effect of long-term idle periods on the
performance of sequencing batch reactors. Water Sci. Technol.41 (1), 105–113.
ARTICLE IN PRESS
W AT E R R E S E A R C H 40 (2006) 2416– 2426 2425
-
8/17/2019 Decay Nitrification
11/11
Moussa, M.S., Hooijmans, C.M., Lubberding, H.J., Gijzen, H.J., VanLoosdrecht, M., 2005. Modeling nitrification, heterotrophicgrowth and predation in activated sludge. Water Res. 39 (20),5080–5098.
Pommerening-Ro ¨ ser, A., Rath, G., Koops, H.P., 1996. Phylogeneticdiversity within the genus Nitrosomonas. Systematic Appl.Microbiol. 19 (3), 344–351.
Reichert, P., 1994. Aquasim—a tool for simulation and data-analysis of aquatic systems. Water Sci. Technol. 30 (2), 21–30.
Sayavedra-Soto, L.A., Hommes, N.G., Russell, S.A., Arp, D.J., 1996.Induction of ammonia monooxygenase and hydroxylamineoxidoreductase mRNAs by ammonium in Nitrosomonas euro-
paea. Mol. Microbiol. 20 (3), 541–548.Schramm, A., de Beer, D., van den Heuvel, J.C., Ottengraf, S.,
Amann, R., 1999. Microscale distribution of populations andactivities of Nitrosospira and Nitrospira spp. along a macroscalegradient in a nitrifying bioreactor: quantification by in situhybridization and the use of microsensors. Appl. Environ.Microbiol. 65 (8), 3690–3696.
Siegrist, H., Brunner, I., Koch, G., Phan, L.C., Le, V.C., 1999.Reduction of biomass decay rate under anoxic and anaerobicconditions. Water Sci. Technol. 39 (1), 129–137.
Van Loosdrecht, M.C.M., Henze, M., 1999. Maintenance, endoge-neous respiration, lysis, decay and predation. Water Sci.Technol. 39 (1), 107–117.
Vanrolleghem, P.A., Sin, G., Gernaey, K.V., 2004. Transientresponse of aerobic and anoxic activated sludge activities tosudden substrate concentration changes. Biotechnol. Bioeng.86 (3), 277–290.
Wagner, M., Rath, G., Amann, R., Koops, H.P., Schleifer, K.H., 1995.In-situ identification of ammonia-oxidizing bacteria. Sys-tematic Appl. Microbiol. 18 (2), 251–264.
WERF 2003. Methods for wastewater characterization in activatedsludge modeling. Foundation, W.E.R. (ed), p. 596.
Wiesmann, U., 1994. Biological nitrogen removal from waste-water. Adv. Biochem. Eng. 51, 113–154.
Wild, D., Vonschulthess, R., Gujer, W., 1995. Structured modeling of denitrification intermediates. Water Sci. Technol. 31 (2),45–54.
Wyffels, S., Van Hulle, S.W.H., Boeckx, P., Volcke, E.I.P., VanCleemput, O., Vanrolleghem, P.A., Verstraete, W., 2004. Mod-eling and simulation of oxygen-limited partial nitritation in amembrane-assisted bioreactor (MBR). Biotechnol. Bioeng. 86(5), 531–542.
ARTICLE IN PRESS
W A T E R R E S E A R C H 4 0 ( 2 0 0 6 ) 2 4 1 6 – 2 4 2 62426