the impact of titanium dioxide nanoparticles on biological nitrogen removal from wastewater and...
TRANSCRIPT
ORIGINAL PAPER
The impact of titanium dioxide nanoparticles on biologicalnitrogen removal from wastewater and bacterial communityshifts in activated sludge
Dapeng Li • Fuyi Cui • Zhiwei Zhao •
Dongmei Liu • Yongpeng Xu • Huiting Li •
Xiaonan Yang
Received: 18 December 2012 / Accepted: 3 May 2013
� Springer Science+Business Media Dordrecht 2013
Abstract The potential impact of titanium dioxide
nanoparticles (TiO2 NPs) on nitrogen removal from
wastewater in activated sludge was investigated using a
sequencing batch reactor. The addition of 2–50 mg L-1
of TiO2 NPs did not adversely affect nitrogen removal.
However, when the activated sludge was exposed to
100–200 mg L-1 of TiO2 NPs, the effluent total
nitrogen removal efficiencies were 36.5 % and
20.3 %, respectively, which are markedly lower than
the values observed in the control test (80 %). Further
studies showed that the decrease in biological nitrogen
removal induced by higher concentrations of TiO2 NPs
was due to an inhibitory effect on the de-nitrification
process. Denaturing gradient gel electrophoresis pro-
files showed that 200 mg L-1 of TiO2 NPs significantly
reduced microbial diversity in the activated sludge. The
effect of light on the antibacterial activity of TiO2 NPs
was also investigated, and the results showed that the
levels of TiO2-dependent inhibition of biological nitro-
gen removal were similar under both dark and light
conditions. Additional studies revealed that different
TiO2 concentrations had a significant effect on dehy-
drogenase activity, and this effect was most likely the
result of decreased microbial activity.
Keywords Titanium dioxide nanoparticles �Biological nitrogen removal � Bacterial community
shift � Activated sludge
Introduction
Nanoparticles (NPs) are defined as particles with novel
and distinctive physicochemical properties the size of
which in the range of 1–100 nm in at least one
dimension (Julia et al. 2009; Moore 2006). The
importance of nanotechnology in modern society is
demonstrated by the broad range of scientific and
technological applications that use NPs (Julia et al.
2009; Moore 2006; Nel et al. 2006), including imaging
and medical devices, cosmetics, fabrics, health prod-
ucts, and water remediation technologies (Warren
et al. 1998). Although nanotechnology holds great
potential for valuable environmental uses, the rapid
increase in the number of nanotechnology-enhanced
products raises concerns regarding the potential
adverse effects of these particles on human health
and the environment (Choi and Hu 2008; Giammar
et al. 2007; Kim et al. 2007; Zhang and Karn 2005;
Maynard et al. 2006). Many studies have investigated
the effect of NPs on the environment and attempted to
predict their environmental concentrations (Zheng
et al. 2011; Nowack and Bucheli 2007; Lv et al. 2008),
and the increasing use of nanoparticle-containing
products has resulted in the release of NPs into
wastewater treatment plants (WWTPs) (Blaster et al.
D. Li � F. Cui (&) � Z. Zhao � D. Liu � Y. Xu �H. Li � X. Yang
State Key Laboratory of Urban Water Resource and
Environment, Harbin Institute of Technology,
73 Huanghe Road, Nangang District,
Harbin 150090, China
e-mail: [email protected]
123
Biodegradation
DOI 10.1007/s10532-013-9648-z
2008; Gottschalk et al. 2009). Limbach et al. (2008)
found that large amounts of cerium oxide NPs that
were released into a model WWTP were adsorbed by
activated sludge, and this was the major mechanism
for NP removal in a conventional activated sludge
system (Zheng et al. 2011). Nevertheless, few studies
have been conducted to determine whether the
absorbed NPs induce adverse effects in activated
sludge.
TiO2 is an effective opacifier and is used as a
pigment in paints, paper, inks, and plastics (Adams
et al. 2006). Due to the widespread use of TiO2,
research has been conducted on its potential toxicity
(Adams et al. 2006; Rincon and Pulgarin 2005;
Lonnen et al. 2005). In previous studies, TiO2 particles
that were toxic to bacteria ranged in size from tens of
nanometers to hundreds of micrometers. Recent
studies have confirmed that TiO2 NPs are toxic to
both Gram-negative and Gram-positive bacteria
(Block et al. 1997; Kwark and Kim 2001). Some
studies have found Gram-positive bacteria to be less
sensitive to TiO2 NPs than Gram-negative bacteria,
but other studies have observed the opposite results.
For example, (Rincon and Pulgarin 2005) reported that
Gram-positive Bacillus subtilis was less sensitive to
the effects of TiO2 than a pure culture of Gram-
negative Escherichia coli in a mixed culture experi-
ment. However, Adams et al. (2006) found that the
Gram-positive Bacillus subtilis was more sensitive to
the addition of three types of NPs (TiO2 NPs, SiO2
NPs, and ZnO NPs) than were Gram-negative E. coli.
The toxicity of TiO2 may be related to the mechanisms
by which the particles act on cells, including the
disruption of membranes or the membrane potential,
protein oxidation, genotoxicity, the interruption of
energy transduction, the formation of reactive oxygen
species, and the release of toxic constituents (Klaine
et al. 2008). TiO2 is photosensitive and produces
reactive oxygen species (ROS) in the presence of light
(Adams et al. 2006; Wei et al. 1994). During these
reactions, light of a specific wavelength is usually
provided by sunlight or high-intensity lamps. How-
ever, in one study, inhibitory effects were observed
under dark conditions, suggesting that undetermined
mechanisms may contribute to the observed toxicity.
Nevertheless, the current knowledge of TiO2 NP
toxicity is primarily derived from studies of model
organisms, and these results have largely been
obtained from laboratory studies of cultures treated
with TiO2 NPs. Although such studies are useful for
validating the toxic effect of chemicals, they do not
consider environmental factors. Consequently, the
current understanding of the potential impact of TiO2
NPs on the environment is poor. Specifically, nitrify-
ing bacteria are sensitive to a number of environmental
conditions (i.e., pH, dissolved oxygen concentration,
and temperature) and are therefore susceptible to
inhibition (Zhen et al. 2011). Although silver NPs and
zinc oxide NPs are reportedly toxic to the respiration
processes of nitrifying bacteria (Choi and Hu 2008;
Zheng et al. 2011), little research exists on the
potential effect of TiO2 NPs on biological nitrogen
removal; therefore, this topic should be explored more
fully.
Nitrogen (N) is the key nutrient that causes
eutrophication in waterways. Therefore, nitrogen-
containing materials are compulsorily removed from
wastewater sources in most developed countries. An
important function of activated sludge is biological
nutrient removal (Zheng et al. 2011), which is carried
out via complex microbial populations that perform
nitrification and de-nitrification. Therefore, activated
sludge contains various species of bacteria, and it is
difficult to discern the potential impact of TiO2 NPs on
certain pure species of bacteria. Thus, the diversity of
the microbial populations and a stable bacterial
community structure play important roles in achieving
a high efficiency of biological nitrogen removal.
However, few research studies have been published on
the effect of TiO2 NPs on the bacterial community in
activated sludge. Although phosphorus (P) is also
assumed to be a key nutrient for the eutrophication of
freshwater, much like nitrogen (N), we found that
phosphorus removal was unaffected by the presence of
TiO2 NPs (Zhen et al. 2011). Therefore, we did not
investigate the effect of the presence of TiO2 NPs on
phosphorus removal.
The objectives of this study were to (a) determine
the effects of TiO2 NPs on biological nitrogen removal
from wastewater (b) determine the effect of TiO2 NPs
on the bacterial diversity of activated sludge, and
(c) determine whether natural light stimulates the
toxicity of NPs to the bacteria in activated sludge, thus
affecting biological nitrogen removal. In this study, a
sequencing batch reactor (SBR) known to achieve
nitrogen removal was used to culture the activated
sludge. A scanning electron microscope (SEM) was
used to assess the surface integrity of the activated
Biodegradation
123
sludge, and changes in the bacterial diversity of the
activated sludge were investigated using polymerase
chain reaction-denaturing gradient gel electrophoresis
(PCR-DGGE) analysis.
Materials and methods
Preparation of nanoparticle suspensions
The TiO2 NPs used in this study were purchased from
Sigma-Aldrich (St. Louis, MO, USA). The reported
mean particle size was less than 25 nm, and the purity
was 99.7 %, Different concentrations of TiO2 NPs in
aqueous solutions were prepared as previously
described (Keller et al. 2010). For example, to produce
a 100 mg L-1 NP stock suspension, 100 mg of TiO2
NPs was dispersed into 1 L of Milli-Q water via
sonication for 1 h (25 �C, 250 W, 40 kHz). The actual
size of the particles in suspension in water was
determined to be 16–34 nm using transmission elec-
tron microscopy (TEM) (Fig. 1).
Operation of SBRs
Three SBRs with working volumes of 5 L were seeded
with sludge from the Taiping sewage treatment plant
(Harbin, China) in a biological nutrient removal process
with intermittent (SBR-type) operation. All reactors
were fed with synthetic wastewater that contained the
following (mg L-1): NH4?–N (supplied from NH4Cl),
40; chemical oxygen demand (COD) (supplied from
sodium acetate), 300; KH2PO4, 110; NaHCO3, 500;
MgSO4�7H2O, 50; and CaCl2�2H2O, 10. A microele-
ment solution (1 mL L-1 of the wastewater) contained
(mg L-1): FeCl3�7H2O, 1.5; CuSO4�H2O, 0.03; EDTA,
10; MnCl2�4H2O, 0.12; KI, 0.18; ZnSO4�7H2O, 0.12;
CoCl2�7H2O, 0.15; and H3BO3, 0.15.
The laboratory scale SBR operated at three cycles
per day. Each cycle consisted of five phases, including
fill instant (5 min), aerobic phase (4 h), anoxic phase
(2 h), sludge settling (1 h), and effluent discharge
(5 min) in a temperature-controlled room (25–28 �C).
During the aerobic stage, air was provided intermit-
tently using an air pump controlled by an automatic
on/off switch according to an online DO detector to
maintain a DO level between 0.45 and 0.55 mg L-1.
The pH in the system was recorded but not
controlled, and it fluctuated between 7.4 and 8.2.
The sludge was removed to waste to maintain a solids
retention time (SRT) of approximately 22 days (Zhen
et al. 2011). The effluent concentrations of NH4?–N,
nitrite–nitrogen (NO2-–N), and nitrate–nitrogen
(NO3-–N) in all SBRs were frequently determined
until the nitrogen and phosphorus removals became
relatively stable (at approximately 90 days).
The effect of TiO2 NP accumulation on the
biological nitrogen removal from wastewater was
investigated by continuously dosing SBR 1 and SBR 2
with TiO2 NPs over a seven-day period, and SBR 3
was operated as the control (without the addition of
TiO2 NPs). The daily concentrations of TiO2 NPs in
SBR 1 and SBR2 could gradually decrease as a result
of effluent and sludge discharge; for this reason, TiO2
NPs were supplemented every day (during the first
cycle) to present final concentrations as follows:
0 mg L-1 (day 1), 2 mg L-1 (day 2), 10 mg L-1
(day 3), 25 mg L-1 (day 4), 50 mg L-1 (day 5),
100 mg L-1 (day 6), and 200 mg L-1 (day 7). This
supplementation was performed after determining the
total concentration of TiO2 in each reactor with the
goal of simulating the likely route of exposure in the
Fig. 1 TEM images of TiO2 NPs in suspension in water
Biodegradation
123
environment, because the environmental release of
TiO2 NPs might continuously increase due to their
large-scale production (Kiser et al. 2009).
SBR 1 was covered with aluminum foil to prevent
possible light-induced effects, and each SBR was set
up in triplicate. To examine whether natural light
stimulates the toxicity of TiO2 NPs, which may
subsequently affect biological nitrogen removal,
SBR2 was set up near an east-facing window in the
laboratory in September (N45.761, W126.688).
DNA extraction
The bacterial genomic DNA of the activated sludge
was extracted according to a previous publication
(Wan et al. 2011) using a DNA Isolation Kit (MO Bio
Laboratories, Inc., Carlsbad, CA, USA). The extracted
DNA was dissolved in 60 lL of TE buffer solution.
PCR-DGGE analysis of the bacterial community
in activated sludge
The V3 region of 16S rRNA was amplified by PCR
using the universal bacterial primers (338F, 5-ACT-
CCTACGGGAGGCAGCAG-3 and 534R, 50-ATTA-
CCGCGGCTGCTGG-3 with a GC clamp). The PCR
amplification was conducted in a 50-lL tube contain-
ing 5 lL of 109 PCR buffer (Mg2? Plus), 4 lL of
dNTP mixture (2.5 mM), 1 lL of 338F primer
(20 lM), 1 lL of 534R primer (20 lM), 2.5 ng of
DNA template, and 0.15 U of Taq DNA polymerase
(Takara, Dalian, China). The thermal cycler (model
9700; ABI, Foster, CA, USA) used a cycling program
that began with an initial denaturation of DNA for
10 min at 94 �C, followed by 30 cycles of 1 min at
94 �C, 30 s at 55 �C (decreasing by 0.1 �C per cycle to
52 �C), and 1 min 30 s at 72 �C. The final extension
step was performed for 10 min at 72 �C.
The PCR products were separated using the
DcodeTM universal mutation detection system (Biorad
Laboratories, Hercules, CA, USA). Polyacrylamide
gels with a 40–60 % vertical denaturing gradient
(100 % denaturant corresponds to 7 mol L-1 urea and
40 % deionized formamide) were prepared. A total of
10 lL of each PCR product was loaded, and the gels
were electrophoresed for 7.5 h at 150 V and 60 �C.
The gels were silver stained as described previously
(Bassam et al. 1991), scanned using a transmission
scanner, and examined using PHYLIP 4.0 and SPSS
12.0 software.
The dominant DGGE bands were excised and
dissolved in 20 lL of 19 TE. In total, 2 lL of DNA
solution was used as the PCR amplification template
under the conditions described above, and the same
primers were used. The PCR products were recovered
by agarose gel electrophoresis, ligated into the vector
pMD18 (Takara, Dalian, China), and cloned into
E. coli DH5a. Positive clones were examined for
ampicillin resistance via blue–white spot screening.
The positive clones were sequenced using an ABI3730
instrument, and partial 16S rRNA gene sequences
were analyzed using the BLAST program in GenBank.
The gene sequences of the clones were deposited in
GenBank under the accession numbers FJ440449
through FJ440511.
Scanning electron microscopy (SEM)
The SEM procedure used was as follows: after
exposure to TiO2 NPs, 5 mL of mixture sludge was
centrifuged at 4,000 rpm for 5 min, the supernatant
was discarded, and a pair of tweezers (or a syringe
needle) was used to extract the precipitate (a diameter
of 0.5 mm). The mud was placed in a 5 mL centrifuge
tube, and 2.5 % glutaraldehyde was added for 1.5 h at
4 �C. After rinsing three times with 0.1 M phosphate
buffer (pH 6.8), the mud was dehydrated in a series
of graded ethanol solutions (50, 70, 80, and 90 %,
15 min per step) and then dehydrated in 100 %
ethanol three times for 15 min each time. The ethanol
was then replaced 1:1 100 % ethanol:isoamyl acetate,
followed by pure isoamyl acetate, and the samples
were incubated each time for 15 min. The samples
were then placed in a desiccator and dried for 8 h.
A Giko IB-5 ion sputtering instrument was used to
spray gold at a thickness of 1,500 nm onto the sample
surface. The sample was viewed under a FEI Quanta
200 scanning electron microscope at 20 kV (FEI
Company, USA).
Transmission electron microscopy (TEM)
The TiO2 NP suspension was transferred onto a copper
grid. After the grid was dried in a laminar flow hood, it
was analyzed under a JEOL 2100 field emission gun
transmission electron microscope (Peabody, MA).
Biodegradation
123
Analytical methods
The determinations of NH4?–N, nitrite–nitrogen
(NO2-–N), and nitrate–nitrogen (NO3
-–N) were
conducted in accordance with Nessler’s reagent
spectrophotometry, N-(1-naphthalene)-diaminoethane
spectrophotometry, and ultraviolet spectrophotomet-
ric methods, respectively (APHA 1998). The dis-
solved oxygen (DO) concentration and the pH of the
suspensions were determined online using a WTW
Multi 340i DO meter and a WTW InoLab level 2
instrument, respectively.
Dehydrogenase activity assay
Dehydrogenase activity is often used as the activity
index for activated sludge and is measured by the
reduction of 2,3,5-triphenyltetrazolium chloride
(TTC). Two milliliters of Tris–Hcl buffer solution
(0.2 M, pH 7.3), 5 mL of TTC (5 g L-1), and 2 mL of
glucose solution (0.1 M) were added to 1 mL of
activated sludge. The mixture was shaken at 140 rpm
for 20 min at room temperature and was subsequently
incubated at 37 �C for 12 h. The deoxidization
reaction was stopped by the addition of 100 mL of
concentrated sulfuric acid. The follow-up steps were
performed as previously described (Lv et al. 2008).
Briefly, the absorbance of toluene was measured at
492 nm using a UV spectrometer. The enzyme activity
was expressed as the amount of TTC reduced per mg
of activated sludge per h. The dehydrogenase activity
was calculated using the following equation:
Edehydrogenase ¼ 0:08M= Vs�MLSSð Þ ð1Þ
where Edehydrogenase is the dehydrogenase activity
[lg (g MLSS)-1h-1], M is the TTC quantity calcu-
lated based on the standard line (lg), and Vs is the
volume of the activated sludge sample.
Results and discussion
Effects of TiO2 NPs on biological nitrogen
removal
Figure 2 shows the effluent concentrations of NH4?–N,
NO3-–N, and NO2
-–N in SBR1 over 7 days resulting
from TiO2 NP dosing concentrations of 0, 2, 10, 25, 50,
100, and 200 mg L-1. The effluent concentrations
of NH4?–N at TiO2 NP concentrations ranging from 0
to 200 mg L-1 were relatively stable over 7 days,
suggesting that these TiO2 NP concentrations did not
have a significant influence on NH4?–N removal. The
effluent concentrations of NO3-–N and NO2
-–N at
TiO2 NP concentrations ranging from 2 to 50 mg L-1
were also observed to be stable and similar to those
observed in the absence of TiO2 NPs (day 1). More than
78 % of the total nitrogen (TN) was removed from
SBR1 over the first 4 days. These results indicate that
TiO2 NP concentrations ranging from 2 to 50 mg L-1
had no adverse effects on nitrogen removal. However,
when activated sludge was exposed to 100 and
200 mg L-1 of TiO2 NPs, the respective effluent
NO3-N levels were 8.9 and 8.7 mg L-1, and the
effluent NO2-–N levels were 0.27 and 0.31 mg L-1,
respectively, which were significantly higher than those
observed in the absence of TiO2 NPs (NO3-–N:
4.7 mg L-1 and NO2-–N: 0.01 mg L-1). The corre-
sponding TN removal efficiencies were 36.5 % and
20.3 %, respectively, which were markedly lower than
those observed in the control test (80 %). These results
indicate that nitrogen removal was inhibited by higher
concentrations of TiO2 NPs (C100 mg L-1).
The effect of TiO2 NPs on the transformations of
NH4?–N, NO3
-–N, and NO2-–N was investigated. As
shown in Fig. 3, the variations of NH4?–N were not
significantly different among TiO2 NPs concentrations
ranging from 0 to 200 mg L-1. Additionally, the levels
of NO3-–N and NO2
-–N did not significantly differ in
Fig. 2 Effects of TiO2 NP concentration [0 mg L-1 (day 1),
2 mg L-1 (day 2), 10 mg L-1 (day 3), 25 mg L-1 (day 4),
50 mg L-1 (day 5), 100 mg L-1 (day 6), and 200 mg L-1 (day
7)] on the effluent concentrations of NH4?–N, NO3
-–N, and
NO2-–N. Error bars represent the standard deviations of
triplicate tests
Biodegradation
123
the presence of TiO2 NP concentrations of 0, 2, 10, 25,
and 50 mg L-1 (Fig. 4), indicating that the presence of
2–50 mg L-1 of TiO2 NPs had no acute effect on the
transformations of NO3-–N and NO2
-–N. However,
when the concentrations of TiO2 NPs reached 100 and
200 mg L-1, the NH4?–N removal efficiencies
remained high ([90 %), but the transformations of
NO3-–N and NO2
-–N were significantly inhibited.
Biological nitrogen removal is accomplished
through sequential nitrification, which involves the
oxidation of ammonium to nitrite and the oxidation of
nitrite to nitrate, in addition to de-nitrification pro-
cesses. This study showed that the decrease in
biological nitrogen removal induced by high concen-
trations of TiO2 NPs was not caused by the inhibition
of ammonia oxidation but was instead due to the
inhibition of de-nitrification. Similarly, a recent study
reported that high concentrations of other nanoparti-
cles, such as ZnO NPs (10 and 50 mg L-1), could
inhibit de-nitrification by the release of zinc ions
resulting from ZnO NP dissolution. However, in this
study, no titanium ions were detected in the presence
of 100 and 200 mg L-1 of TiO2 NPs. This result is in
agreement with those of Zhen et al. (2011) and Kiser
et al. (2009), who reported that in wastewater, Ti
occurs solely in the solid phase and not in ionic forms
due to its low solubility. A recent study suggested that
higher concentrations of TiO2 NPs could significantly
decrease TN removal by decreasing the abundance of
ammonia-oxidizing bacteria. However in this study,
we found that the decrease in biological nitrogen
removal induced by high concentrations of TiO2 NPs
was not caused by the inhibition of ammonia oxidation
but rather by the inhibition of de-nitrification. De-
nitrification involves the reduction of nitrate to nitrite,
Fig. 3 Effects of light and TiO2 NP concentration [0 mg L-1
(day 1), 2 mg L-1 (day 2), 10 mg L-1 (day 3), 25 mg L-1 (day
4), 50 mg L-1 (day 5), 100 mg L-1 (day 6), and 200 mg L-1
(day 7)] on the effluent concentrations of NH4?–N, NO3
-–N,
and NO2-–N. Error bars represent the standard deviations of
triplicate tests
Fig. 4 Variations in NH4?–N (a), NO3
-–N (b), and NO2-–N
(c) during one cycle of exposure to various concentrations of
TiO2 NPs. Error bars represent the standard deviations of
triplicate tests
Biodegradation
123
then the reduction of nitrite to nitric oxide (NO) and,
subsequently, to nitrous oxide (N2O) and molecular
nitrogen (N2), which are finally released into the
atmosphere. These transformations are carried out by a
group of bacteria that are capable of using nitrate in
place of oxygen as an electron acceptor for respiration
(Rodrıguez et al. 2011). In previous studies, TiO2 NPs
were revealed to be toxic to both Gram-negative and
Gram-positive bacteria (Adams et al. 2006), which
suggested that higher concentrations of TiO2 NPs in
the activated sludge might also decrease the abun-
dance of denitrifying bacteria. For this reason, the
effects of TiO2 NPs on changes in the bacterial
diversity of activated sludge were investigated.
Effects of light on biological nitrogen removal
We compared the biological nitrogen removal (work-
ing) efficiency between SBR1 and SBR2 (Figs. 2, 4)
and observed that the overall trends of the effluent
concentrations of NH4?–N, NO3
-–N, and NO2-–N
resulting from the addition of TiO2 NPs
(0–200 mg L-1) over a period of 7 days were similar
between the two reactors; this result suggests that the
inhibition of biological nitrogen removal occurred
under both dark and illuminated conditions, and that
illumination did not enhance the inhibition.
Previous studies have shown that the toxicity of TiO2
to bacteria under pure culture conditions was signifi-
cantly greater under light than dark conditions (Adams
et al. 2006), which supports the notion that the
antibacterial activity of TiO2 is related to photo-
catalytic ROS production. However, a significant
decrease in the abundance of ammonia-oxidizing
bacteria (AOB) in activated sludge that was exposed
to 50 mg L-1 of TiO2 under dark conditions still
occurred (Zhen et al. 2011), indicating that an undeter-
mined mechanism may be involved. In this study, the
inhibition of biological nitrogen removal by TiO2 was
similar under both dark and light conditions (Fig. 4),
which suggests that the toxicity of TiO2 to organisms
under pure culture conditions may not reflect natural
systems. The toxicity mechanisms of TiO2 NPs under
dark conditions should be investigated further.
Effects of TiO2 NPs on bacterial diversity
The mechanism of TiO2 NP-mediated de-nitrification
was explored by assessing the microbial community
via PCR-DGGE analysis. As shown in Fig. 5, the
bacterial diversity in activated sludge from SBR1
showed a clear decline over 7 days). This result
indicated that the bacterial abundance in activated
sludge was affected by the presence of TiO2 NPs. This
result was similar to those of previously published
reports showing that TiO2 NPs reduce the diversity of
the microbial community in activated sludge after
70 days of exposure (Zhen et al. 2011). Additionally,
Ge et al. (2011) found that TiO2 NPs were able to alter
the bacterial composition in soil and reduce microbial
populations after 60 days of exposure.
We identified 23 DGGE bands in the activated
sludge sample (Fig. 5), and these bands were excised
and sequenced using BLAST (Table 1). On the first
day, the dominant bacterial communities in the
activated sludge contained typical ammonia-oxidizing
(band 3, related to Nitrosomonas sp.) and denitrifying
bacteria (band 9, related to Pseudomonas sp.), and
these bacteria have been reported to remove nitrogen
from wastewater. However, after 7 days of exposure,
when the concentrations of TiO2 NPs reached
Fig. 5 DGGE profile of
bacterial communities in
SBR1. L1 and L 2 represent
activated sludge in SBR1
with the addition of
0 and 200 mg/L TiO2 NPs.
Detailed information on
bands 1–23 is presented in
Table 1
Biodegradation
123
200 mg L-1, the number of Pseudomonas sp. (band 9
in Fig. 5) declined in the activated sludge; this
microorganism is known to denitrify nitrate. The
above results may explain the inhibitory effect of
TiO2 NPs on the de-nitrification process. Conversely,
ammonia oxidizing bacteria were still observed in the
presence of 200 mg L-1 of TiO2 NPs in the activated
sludge. It is well known that nitrifying bacteria are
sensitive to environmental factors. Nevertheless, the
results of this study indicate that these microorganisms
may be able to tolerate high levels of TiO2 NPs.
Effects of TiO2 NPs on dehydrogenase activity
and the surface integrity of activated sludge
Dehydrogenase activity is a valuable indicator of
microbial viability in various environments, including
Table 1 DGGE bands and
their closely related
sequence
Band Result Accession number Similarity
(%)
L1 Roseomonas sp. AY624051.1 96
L2 Acidobacteria bacterium JF345309.1 99
L3 Uncultured Nitrosomonas sp.
Uncultured ammonia-oxidizing bacterium clone
FM997827.1 DQ154799.1 99
99
L4 Azospirillum sp. FJ386552.1 94
L5 Uncultured Dechloromonas sp. JF808881.1 95
L6 Uncultured Sphingobacterium sp. FN668067.2 99
L7 Uncultured bacterium clone HQ891402.1 99
L8 Uncultured Ruminococcaceae bacterium clone GQ358507.1 94
L9 Pseudomonas sp. HQ438076.1 99
L10 Sphingomonas sp. JF297632.1 96
L11 Uncultured Rheinheimera sp. GQ464399.1 100
L12 Uncultured Arenimonas sp. JN648282.1 94
L13 Uncultured Leptothrix sp. GU572372.1 99
L14 Uncultured Acidobacteria bacterium clone HQ598480.1 100
L15 Uncultured Zoogloea sp. EU639302.1 100
L16 Sphingomonas sp. JF716065.1 99
L17 Prevotella sp. HM245224.1 97
L18 Uncultured Dokdonella sp. JN679193.1 99
L19 Sphingomonas sp. JN848796.1 100
L20 Uncultured Rhodobacteraceae bacterium clone HQ003517.1 100
L21 Uncultured Dechloromonas sp. JN679130.1 97
L22 Acidobacteria bacterium JF345309.1 99
L23 Uncultured Sphingobacterium sp. FN668067.2 100
Fig. 6 Dehydrogenase activities of activated sludge in SBR1
and SBR3. SBR3 was a control reactor to which no TiO2 NPs
were added. Error bars represent the standard deviations of
triplicate tests
Biodegradation
123
activated sludge (Lv et al. 2008). The dehydrogenase
activity of an intracellular enzyme is affected by a
number of antimicrobial and bacteriostatic agents,
such as toluene and chloroform, which exist in various
environments. The effect of TiO2 NPs on dehydroge-
nase activity is presented in Fig. 6, which shows that
dehydrogenase activity was inhibited by all of the
treatments containing TiO2 NPs. Figure 5 shows that
the activity of dehydrogenase decreased with
increased concentrations of TiO2 NPs. Different
concentrations had significant effects on dehydroge-
nase activity, which were likely due to decreased
microbial activity. SEM analysis also revealed the
change of microorganism’s composition structure and
damage on the surface of activated sludge that was
exposed to 100–200 mg L-1 TiO2 NPs (Fig. 7). These
results revealed that high concentrations of TiO2 NPs
may disrupts the balance of microbial populations,
which may be responsible for the antibacterial activity
of TiO2 NPs.
Conclusions
In this study, the potential effects of TiO2 NP
accumulation on biological nitrogen removal from
wastewater and bacterial community shifts in acti-
vated sludge were investigated by continuous dosing
of SBRs with TiO2 NPs. Although TiO2 NP concen-
trations ranging from 2 to 50 mg L-1 had no adverse
effects on nitrogen removal, nitrogen removal was
dramatically inhibited by TiO2 NP concentrations of
100–200 mg L-1, possibly due to the inhibition of de-
nitrification. It was observed that 100–200 mg L-1 of
TiO2 NPs reduced the microbial diversity in activated
sludge, and the abundance of denitrifying bacteria was
significantly decreased, possibly explaining the inhib-
itory effect. Further studies showed that the activity of
dehydrogenase decreased with increased TiO2 NP
concentrations, and high concentrations of TiO2 NPs
damaged the activated sludge surface, thus proving
that high concentrations of TiO2 NPs possess antibac-
terial activity. Moreover, we also examined whether
Fig. 7 SEM images of activated sludge in SBR1. a–c represent
the activated sludge in SBR1 (without the addition of TiO2 NPs,
with the addition of 100 mg L-1 TiO2 NPs, and with the
addition of 200 mg L-1 TiO2 NPs, respectively)
b
Biodegradation
123
natural light stimulates the toxicity of TiO2 NPs,
subsequently affecting biological nitrogen removal.
The results showed that the inhibition of biological
nitrogen removal by TiO2 NPs was similar under both
dark and light conditions, suggesting that the toxicity
mechanisms of TiO2 NPs under dark conditions
require further investigation.
Acknowledgments This work was supported by the National
Natural Science Foundation of China (Grant No. 51078102) and
the Funds for Creative Research Groups of China (Grant No.
51121062).
References
Adams LK, Lyon DY, Alvarez PJJ (2006) Comparative eco-
toxicity of nanoscale TiO2, SiO2, and Zno water suspen-
sions. Water Res 40:3527–3532
APHA (1998) Standard methods for the examination of water
and wastewater, 20th edn. American Public Health Asso-
ciation, Washington DC
Bassam B, Caetano-Anolles G, Gresshoff P (1991) Fast and
sensitive silver staining of DNA in polyacrylamide gels.
Anal Biochem 196:80–83
Blaster SA, Scheringer M, Macleod M, Hungerbuhler K (2008)
Estimation of cumulative aquatic exposure and risk due to
silver: contribution of nano-functionalized plastics and
textiles. Sci Total Environ 390:396–409
Block SS, Seng VP, Goswami DY (1997) Chemically enhanced
sunlight for killing bacteria. J Sol Energy Eng 119:85–91
Choi O, Hu ZQ (2008) Size dependent and reactive oxygen
species related nanosilver toxicity to nitrifying bacteria.
Environ Sci Technol 42:4583–4588
Ge Y, Schimel JP, Holden PA (2011) Evidence for negative
effects of TiO2 and ZnO nanoparticles on soil bacterial
communities. Environ Sci Technol 45:1659–1664
Giammar DE, Maus CI, Xie LY (2007) Effects of particle size
and crystalline phase on lead adsorption to titanium dioxide
nanoparticles. Environ Eng Sci 24:85–95
Gottschalk F, Sonderer T, Schoiz RW, Nowack B (2009)
Modeled environmental concentrations of engineered
nanomaterials (TiO2, ZnO, Ag, CNT, Fullerenes) for dif-
ferent regions. Environ Sci Technol 43:9216–9222
Julia F, Shona RF, Jonna CR, Jamie RL (2009) Silver nano-
particle impact on bacterial growth: effect of pH, concen-
tration, and organic matter. Environ Sci Technol
43:7285–7290
Keller AA, Wang H, Zhou D, Lenihan HS, Cherr G, Cardinale
BJ, Miller R, Ji Z (2010) Stability and aggregation of metal
oxide nanoparticles in natural aqueous matrices. Environ
Sci Technol 44:1962–1967
Kim SC, Harrington MS, Pui DYH (2007) Experimental study
of nanoparticles penetration through commercial filter
media. J Nanopart Res 9:117–125
Kiser MA, Westerhoff P, Benn T, Perez-Rivera J, Hristovskj K
(2009) Titanium nanomaterial removal and release from
wastewater treatment plants. Environ Sci Technol
43:8423–8429
Klaine SJ, Alvarez PJ, Batley GE, Fernandes TF, Handy RD,
Lyon DY, Mahendra S, McLaughlin MJ, Lead JR (2008)
Nanomaterials in the environment: behavior, fate, bio-
availability, and effects. Environ Toxicol Chem
27:1825–1851
Kwark SY, Kim SS (2001) Hybrid organic/inorganic reverse
osmosis (RO) membrane for bactericidal anti-fouling. 1.
Preparation and characterization of TiO2 nanoparticle self-
assembled aromatic polyamide thin film composite (TFC)
membrane. Environ Sci Technol 35:2388–2394
Limbach LK, Bereiter R, Muller E, Krebs R, Galli R, Stark WJ
(2008) Removal of oxide nanoparticles in a model waste-
water treatment plant: influence of agglomeration and
surfactants on clearing efficiency. Environ Sci Technol
42:5828–5833
Lonnen J, Kilvington S, Kehoe SC, Al-Touati F, Mcguigan KG
(2005) Solar and photozoan, fungal and bacterial microbes
in drinking water. Water Res 39:877–883
Lv Z, Yao Y, Min H (2008) Effect of tetrahydrofuran on enzyme
activities in activated sludge. Ecotoxicol Environ Saf
70:259–265
Maynard AD, Aitken RJ, Butz T, Colvin V, Donaldson K,
Oberdoster G, Philbert MA, Ryan J, Seaton A, Stone V,
Tinkle SS, Tran L, Walker NJ, Warheit DB (2006) Safe
handling of nanotechnology. Nature 444:267–269
Moore MN (2006) Do nanoparticles present ecotoxicological
risks for the health of the aquatic environment. Environ Int
32:967–976
Nel A, Xia T, Madler L, Li N (2006) Toxic potential of materials
at the nanolevel. Science 311:622–627
Nowack B, Bucheli TD (2007) Occurrence, behavior and effects
of nanoparticles in the environment. Environ Pollut
150:5–22
Rincon AG, Pulgarin C (2005) Use of coaxial photocatalytic
reactor (CAPHORE) in the TiO2 photo-assisted treatment
of mixed Escherichia coli and Bacillus subtilis and the
bacterial community present in wastewater. Catal Today
101:331–344
Rodrıguez DC, Pino N, Penuela G (2011) Monitoring the
removal of nitrogen by applying a nitrification-de-nitrifi-
cation process in a SBR. Bioresour Technol
102:2316–2321
Wan CL, Du MA, Lee DJ, Yang X, Ma WC, Zheng LN (2011)
Electrokinetic remediation and microbial community shift
of b-cyclodextrin-dissolved petroleum hydrocarbon-con-
taminated soil. Appl Microbiol Biotechnol 89:2019–2025
Warren WS, Ahn S, Mescher M, Ugurbil K, Richter W, Rizi RR,
Hopkins J, Leigh JS (1998) MR imaging contrast
enhancement based on intermolecular zero quantum
coherences. Science 281:247–251
Wei C, Lin WY, Zainal ZZ, Williams NE, Zhu K, Kruzic AP,
Smith RL, Rajeshwar K (1994) Bactericidal activity of
TiO2 photocatalyst in aqueous media: toward a solar-
assisted water disinfection system. Environ Sci Technol
28:934–938
Zhang WX, Karn B (2005) Nanoscale environmental science
and technology: challenges and opportunities. Environ Sci
Technol 39:94A–95A
Biodegradation
123
Zhen X, Chen YG, Wu R (2011) Long term of titanium dioxide
nanoparticles on nitrogen and phosphorus removal from
wastewater and bacterial community shift in activated
sludge. Environ Sci Technol 45:7284–7290
Zheng X, Wu R, Chen YG (2011) Effect of ZnO nanoparticles
on wastewater biological nitrogen and phosphors removal.
Environ Sci Technol 45:2826–2832
Biodegradation
123