microbial communities and biodegradation in lab-scale btex-contaminated groundwater remediation...
TRANSCRIPT
ORIGINAL PAPER
Microbial communities and biodegradation in lab-scaleBTEX-contaminated groundwater remediation usingan oxygen-releasing reactive barrier
Chi-Wen Lin Æ Li-Hsuan Chen Æ Yet-Pole I ÆChi-Yung Lai
Received: 5 April 2009 / Accepted: 24 May 2009 / Published online: 10 June 2009
� Springer-Verlag 2009
Abstract To remediate benzene, toluene, ethylbenzene
and xylene (BTEX) -contaminated groundwater, a bio-
treatment process including biostimulation and bioaug-
mentation was simulated using oxygen-releasing reactive
barriers (ORRB) and water with added BTEX in a lab-scale
system. The results showed that the capability for BTEX
removal decreases in the order of benzene, toluene,
p-xylene, ethylbenzene for both added-nitrogen and no-
added-nitrogen under BTEX concentrations at 30 mg l-1.
The removal efficiencies in ORRB systems were higher in
the nitrogen-added condition for biostimulation compared
with the no-nitrogen-added condition; moreover, an
increased pattern for removal was observed during the
bioaugmentation process. The oxygen content was found to
be inversely proportional to the distance from the ORRB,
as evidenced by observing that the average bacteria den-
sities were two orders higher when located at 15 cm
compared with 30 cm from the ORRB. The microbial
community structure was similar in both cases of added-
nitrogen and the no-added-nitrogen conditions.
Keywords Biostimulation � Bioaugmentation �Microbial community structure �Oxygen-releasing reactive barrier (ORRB)
Introduction
BTEX (benzene, toluene, ethylbenzene and xylene) has
been widely used in the petrochemical industry, printing
and laminating facilities, foundries, electronics, and paint
manufacturing plants. BTEX is frequently found at haz-
ardous waste sites [1]. Tank leaks or ruptured pipelines
cause BTEX-polluted soil and groundwater. In recent
years, several studies on BTEX treatment have been
implemented to remediate BTEX-contaminated sites
[2, 3]. In situ bioremediation has been applied because of
its capabilities for providing bacteria with environmen-
tally appropriate substances such as oxygen and nitrogen
[4, 5]. A permeable reactive barrier (PRB) is technolog-
ically suitable for contaminated groundwater treatment.
When a PRB is used, contaminated groundwater flows
through a vertically reactive material in which contami-
nants are physically, chemically or biologically degraded
[6]. For groundwater in situ remediation, it should
be more suitable when the technology is applied for
increasing aerobic metabolism than for anaerobic. There-
fore, using an oxygen-releasing reactive barrier (ORRB)
both renders the environmental condition aerobic and
overcomes the reduction state caused by an anaerobic
condition, thereby obtaining higher degradation effi-
ciency. Oxygen-releasing compounds (ORC), a mixture
of CaO2 or MgO2, cement, sand and other materials of
certain proportions have all been researched and applied
to contaminated groundwater studies and remediation
projects [7–9]. The use of such substances (i.e., ORC) is
C.-W. Lin (&) � Y.-P. I
Department of Safety, Health and Environmental Engineering,
National Yunlin University of Science and Technology, 123
University Road, Sect. 3, Douliou, Yunlin 64002, Taiwan, ROC
e-mail: [email protected]
L.-H. Chen
Department of Environmental Engineering, Da-Yeh University,
Dacun, Changhua, Taiwan, ROC
C.-Y. Lai
Department of Biology, National Changhua University
of Education, Changhua, Taiwan, ROC
123
Bioprocess Biosyst Eng (2010) 33:383–391
DOI 10.1007/s00449-009-0336-7
extendible for 6 months or even 1 year, having shown
more economic benefits than pump and treat or air
stripping (50–70% cheaper) [10].
Studies of biostimulation (added nutrients, electron
donor or acceptor) and bioaugmentation (added degrad-
ing strains) applications have also been reported. For
example, nitrogen, phosphorus and oil-degrading bacteria
have been added to petroleum-hydrocarbons contami-
nated soil. The results showed that the addition of such
bacteria enhances the removal of hydrocarbons; more-
over, adding nitrogen and phosphorus stimulates the
microbial growth [5, 11, 12]. Hristova et al. [4] and
Salanitro et al. [13] used bioventing along with the
addition of MTBE-degrading bacteria to demonstrate that
higher efficiency can be achieved by combing the two
methods than by using a single one. Oxygen-releasing
compounds have been used to provide oxygen to stim-
ulate the microbial growth, for which NaNO3 and
(NH4)2SO4 can be used as nutrients. When there is a
lack of oxygen, NO3-and SO4
2- can also function as
electronic receptors [14, 15].
The factors influencing the effectiveness of bioremedi-
ation are closely related to microbial distribution and
growth conditions [16]. Consequently, it is important to
investigate the relationships between the factors including
types of contaminants and environmental conditions, and
microbial communities. Microbial data collected by using
molecular biotechnology techniques are more useful than
traditional ones. SSCP (single-strand-conformation poly-
morphism), a low-cost and highly sensitive method [17,
18], has been used in recent years to detect microbial
diversity [19–21].
ORCs have also been used for recovery at sites con-
taminated by some organic pollutants. For example, an
ORC method was applied to 50 monitoring wells to treat
MTBE pollution in a fuel tank leakage of contaminated
water [22]. In a lab-scale system, a string of double-wall
bioreactor systems was tested to deal with tetrachloro-
ethylene pollutants [7]. In another study, bioaugmenta-
tion and oxygen used were focused on accelerating the
biodegradation process [8]. Microorganisms play an
important role in the degradation of pollutants; however,
microorganisms easily change with the environmental
factors. Therefore, this study employed a polymerase
chain reaction and single-strand conformation polymor-
phism (PCR-SSCP) technique to analyze changes in
microbial population dynamics and to overcome the
limits of traditional quantitative plating methods in
which microorganism analyses cannot fully reveal the
species and the resulting microbial community
composition in the environment. The study also ana-
lyzed the effectiveness of ORC, biostimulation and
bioaugmentation.
Materials and methods
Microorganisms
Mixed cultures were obtained from two sources, one from
a gasoline-contaminated groundwater site, and the other
from industrial wastewater treatment sludge in Mailiao
Industrial Park, Taiwan. A mixture of the two sources was
further defined as ‘in situ microorganisms’. BTEX-
degrading strains were isolated from laboratories in which
the incubation occurred. GenBank BLAST analysis of 16S
rDNA genes (http://www.ncbi.nlm.nih.gov), based on the
sequence of a *1,400-bp fragment has previously revealed
that the accession numbers, percentage of similarities and
E values for the matching score (indicated in parentheses)
are Pseudomonas sp. (DQ211692, 100%, 0.0), Pseudomo-
nas sp. (AF065166, 99%, 0.0), Pseudomonas putida
(AY686638, 100%, 0.0), and Pseudomonas sp. (DQ124297,
99%, 0.0), respectively.
Degradation of BTEX in an ORRB system
An oxygen-releasing reactive barrier (ORRB) system was
divided into three parts: oxygen-releasing reaction wall, a
water supply and collection systems, and a temperature
control system, as shown in Fig. 1. Table 1 lists the system
specifications. The inlet concentrations of benzene, tolu-
ene, ethylbenzene, p-xylene were maintained at 25–36, 26–
36, 26–39, and 27–38 mg l-1, respectively. The inflow rate
was set at 3.45 ml min-1 with 50 cm of flow velocity per
day. The ORRB reactor was maintained at a temperature of
23–25 �C by using temperature-controlled circulating
water outside the reactor. The ORRB reactor was filled
with approximately 25-kg Ottawa quartz sands (E-315,
GEOTEST, USA). The reactive barrier in ORRB reactor
(Fig. 1) was filled with 800 g of ORC [23] consisting of
cement, sand, 40% CaO2, KH2PO4, K2HPO4, NaNO3, and
H2O. The reactor was completely closed; thus, loss of
BTEX in the analytical process was restricted.
Two systems (A and B) were tested in this study. System
A was supported by a nitrogen nutrient and filled with an
ORC consisting of 40% CaO2 and 11% NaNO3. System B
was filled with an ORC composed of only 40% CaO2.. Both
systems were run with the same phases, the first phase being
biostimulated by the added ORC and the implantation of
3,000 ml in situ microorganisms (4.62 9 108 CFU ml-1).
The second phase was a continuation of the first with bio-
augmentation (added of BTEX-degrading strains at sites #1,
#2, and #3; 200 ml per well; 8.49 9 109 CFU ml-1). After
a 15- to 20-day start-up period, the system remained nor-
mally stable with a difference in removal efficiency of less
than 5% (the first phase), which continued in the second
phase.
384 Bioprocess Biosyst Eng (2010) 33:383–391
123
Pollutants and water analysis
A purge water procedure was performed for effectively
eliminating the production of purge water when obtaining a
groundwater sample from a monitoring well. According to
the procedure, the equivalent volumes of water of 2–3
times the wells’ volume were first removed and discarded
at sites #4-a, #4-b, and #4-c using needles and a peristaltic
pump. Subsequently, 10-ml water samples were collected
from the wells, to await water quality analysis for dissolved
oxygen (DO), oxidation reduction potential (ORP), chem-
ical oxygen demand (COD), pH and SSCP. Moreover, 3 ml
of samples were taken by the needles, after which 1 ml of a
subsample was sealed in a 3-ml glass bottle to await further
analysis.
Key physical and chemical properties of BTEX include
Henry’s law coefficient, vapor pressure, and water solu-
bility. The change of pollutant concentrations in the gas
and liquid phases in each bottle can be related using
Henry’s law. Because Henry’s law coefficients of benzene,
toluene, ethylbenzene and xylene are 0.22, 0.27, 0.32 and
0.20 at 25 �C, respectively, show BTEX compounds are
volatile organic compounds, mass transfer rates between
the gas and aqueous phases of BTEX are rapid, and gas
concentrations approach equilibrium with the liquid phase.
Therefore, use of gas-phase measurements for biodegra-
dation experiments satisfactorily captures the pollutant
concentrations in the liquid. Gaseous samples of BTEX
obtained from the headspace of each 3-ml glass bottle were
then injected onto GC-FID (gas chromatograph, model
GC-14B, Shimadzu, Japan) by 250-ll gastight syringes
equipped with Teflon Mininert valve fittings. Concentra-
tions of BTEX were quantified against primary standard
curves.
Similarly, water samples from sites #1 to #4 were col-
lected and analyzed for COD, DO, ORP, pH, NO3--N and
colony-forming units (CFU). Each volume of 15-ml sample
taken by the needles was used for water quality analysis,
and an additional 1.5 ml water sample was collected by a
microcentrifuge tube and preserved at -20 �C for DNA
extraction.
DNA extraction, PCR and SSCP gel electrophoresis
DNA was extracted by using an improvement on a bead-
beating method developed by Stach et al. [19]. A ground-
water sample (200 ll) was mixed with 0.8 g of 0.106-mm
glass beads (Biospec Products, 11079101), 600 ll of
phenol/chloroform/isoamyl alcohol (25:24:1), and 200 ll
of an air-excluding disrupting buffer (50 mM NaCl,
50 mM Tri–HCl, pH 8 and 5% SDS) in a 1.5-ml screw-cap
microcentrifuge tube. The microbial communities were
analyzed by using the PCR-SSCP method described by Lee
et al. [17] and Schwieger and Tebbe [18]. Region V3 of the
16S rDNA, corresponding to nucleotide positions 334–514
of the E. coli gene, was amplified with the primers EUB1
(50-CAGACTCCTACGGGAGG CAGCAG-30) and UNV2
(50-GTATTACCGCGGC TGCTGGCAC-30). A Hoefer
SE600 vertical gel electrophoresis apparatus was used for
Fig. 1 Schematic diagram of an
oxygen-releasing reactive
barrier system
Table 1 Summary of oxygen-releasing reactive barrier system
specifications
Items Specification
Material Crystalloid PVC
Total volume 15.9 L (530 9 150 9 200 mm)
Filler Quartz sand
Oxygen filler Oxygen-releasing compounds
(ORC)
Inside-pore volume 5.1 L
Porosity 0.338
Water-surface slope 0.0099 m m-1
Hydraulic conductivity 2.9 9 10-2 cm s-1
Circulating water volume
(outside)
6.3 L
Temperature control (outside) 20–25 �C
Bioprocess Biosyst Eng (2010) 33:383–391 385
123
SSCP analysis in 10% polyacrylamide gel for 6 h at a
constant voltage of 300 V. The gel temperature was
maintained at 4 �C by using a circulating water bath.
Details of this procedure can be found in the protocol
described by Lin et al. [16].
Statistical comparison of SSCP pattern
The relative positions of the DNA bands in the SSCP gels
were analyzed by using LabWork software. Similarities
between microbial groups were calculated as Dice indices
according to procedures appearing in previous reports [16,
24]. Dendrograms were calculated by using a clustering
algorithm of a UPGMA using cluster analysis of similarity
indices, constructed by NTSYSpc Version 2.1e software
(Exeter Software, USA).
Results and discussion
Preliminary tests for ORC, DO and nitrogen effects
Figure 2 shows the results of background tests with DO
distribution sampled from monitoring wells in an ORRB
system during a 6-day operation. Na2SO3 was added to the
inflow water at 80 mg l-1 to ensure a low DO of inflow
(0–0.5 mg l-1). The average DO concentration at site #1
(-10 cm) was as much as 4 mg l-1, a result caused by the
higher diffusion rate of oxygen released from the ORC than
by the flow rate of the groundwater, which further provided
an elevated DO near the upstream region at site #1. The
average DO was detected in a range of 7.51–8.27 mg l-1 in
the downstream region at sites #2 (10 cm), #3 (15 cm) and
#4 (30 cm), showing that oxygen escaping into the atmo-
sphere was negligible. A column containing ORC was
tested, and thereby indicating that oxygen was stably
released, having persisted at least 35 days (data not
shown). A large quantity of DO of 8 mg l-1, approxi-
mately, was found around this column, thus indicating that
the ORCs create an aerobic circumstance by releasing
oxygen, and DO functions as an electron acceptor in the
aerobic metabolism of bacteria in an ORRB system for
BTEX biodegradation, the results being consistent with
other studies [25, 26].
Figure 2 also depicts the NO3--N concentration distri-
butions for the ORRB system during the 6-day operation.
At site #1, the average concentration of NO3--N was below
1 mg l-1, while the values downstream ranged between
100 and 200 mg l-1. The low concentration of NO3--N
detected at site #1 revealed that the diffusion rate was not
as high as that of the oxygen, the release rate of which was
higher than the flow rate. The detected NO3--N concen-
tration downstream was approximately 1% of the designed
concentration in the ORC, thereby indicating that the
nitrogen source was successfully released.
BTEX removal efficiency
This study was implemented to test the efficiency of an
ORRB system and the biodegradation of pollutants. A
comparison of systems A and B indicated higher removal
efficiency in the first phase, wherein nitrate was added
because this nutrient enhances BTEX-degrading bacteria
activities under both aerobic and anaerobic conditions, as
illustrated in Fig. 3. Nitrogen is one of the most essential
elements for living, and nitrate is an electron acceptor.
These findings are consistent with other published reports
[2, 27]. In the first-phase experiment (biostimulation) for
system A, DO functioned as an electron acceptor; whereas,
NO3--N can be assumed to promote the capacity of the
biodegradation [2]. Therefore, the removal efficiency for
benzene, toluene, ethylbenzene and p-xylene in system A
was greater than in system B by 14.3, 22.6, 24.9, and
27.3%, respectively. In the second phase (bioaugmenta-
tion), the overall removal efficiency of system A was still
slightly higher than that of system B. In contrast, a note-
worthy improvement in removal efficiency by 16, 14, 20,
and 28% for BTEX, respectively, was observed for system
B as a result of the addition of BTEX-degrading bacteria.
These observations are in agreement with other recent
reports [28, 29]. The improvement in removal efficiency in
system A just increased by 15, 11, 5, and 1% for BTEX,
respectively. The limited enhancement in system A was
believed to be due to the fact that nitrogen addition had
only a small effect in phase 2.
Water sample analysis
In this study, ORP, COD, BTEX, DO, pH and biomass
were used as biological indicators for the bioremediation
process. The ORP values at the monitoring wells for sys-
tems A and B ranged between 100 and 200 mV, thereby
indicating that both systems were aerobic throughout. High
pH values (8–10) were observed during the first 6 days of
Fig. 2 Oxygen distribution and NO3--N concentration in an ORRB
system (background tests) at four sites
386 Bioprocess Biosyst Eng (2010) 33:383–391
123
testing; whereas, neutral values (6.8–7.5) were consistently
detected thereafter. Figure 4 plots the COD variation in the
systems (A and B), showing different values between the
inflow and site #4 (30 cm downstream). The COD values
were unstable during the first 10 days, but subsequently
decreased from 143 to 38 (system A) and 48 mg l-1
(system B); therefore, the removal efficiencies increased
73.4% for system A and 66.1% for system B. In the
second-phase experiment, the removal efficiency increased
during the first several days but remained in the range from
75 to 85% for system A and 65 to 75% for system B.
(A)
(B)
p
Fig. 3 Average removal efficiencies in systems A (with added
nitrogen) and B (without nitrogen). ‘biostimulation’ applied in the
first phase (average removal efficiencies during days 10–20), and both
‘biostimulation and bioaugmentation’ applied in the second phase
(average removal efficiencies during days 25–45)
-1
(A)
(B)
-1
Fig. 4 Variation in COD and removal efficiency in systems A (with
added nitrogen) and B (without nitrogen)
-1-1
(A)
(B)
Fig. 5 Variation in DO in systems A (with added nitrogen) and B(without nitrogen)
-1
(A)
(B)
-1
Fig. 6 Variation in cell density in systems A (with added nitrogen)
and B (without nitrogen)
Bioprocess Biosyst Eng (2010) 33:383–391 387
123
Similarities were observed when comparing the COD
values and the BTEX concentrations. This finding indicates
that BTEX can be effectively decomposed into CO2 and
water or other substances (biomass and other organic
compounds); moreover, the changes in COD concentration
were obvious evidences for BTEX degradation.
Figure 5 shows that the amount of DO was quite high at
the beginning of the first phase, an observation interpreted
as being due to a rapid reaction of ORC with water, thereby
generating a great quantity of oxygen, which still had not
been depleted by bacterial utilization at this time. After the
first 10 days of operation, the DO was significantly reduced
(a)
(b)
Fig. 7 Cluster analysis of
SSCP profiles of microcosms in
system A at site #3: a SSCP
fingerprint, b cluster analysis
388 Bioprocess Biosyst Eng (2010) 33:383–391
123
and reached a steady state; the highest being found at site
#2, followed by site #3, and the lowest at sites #4 and #1.
Therefore, the decrease in DO from upstream to down-
stream can be attributed to the utilization of oxygen to the
bacteria, thereby increasing the bacterial population.
Figure 6 depicts the changes in cell density in systems A
(with added nitrogen) and B (without nitrogen). At
monitoring site #3, this value increased from 4.1 9 106
(day 5) to 1.3 9 107 CFU ml-1 (day 19) in both systems.
The remaining wells exhibited a similar pattern. At the
beginning of the second phase in system A, the DO tended
to decrease from 1.77 (day 21) to 0.86 mg l-1 (day 26) and
subsequently stabilize between approximately 0.75 and
1.13 mg l-1 (the value at site #4 was even lower at
(a)
(b)
Fig. 8 Cluster analysis of
SSCP profiles of microcosms in
system A at site #4: a SSCP
fingerprint, b cluster analysis
Bioprocess Biosyst Eng (2010) 33:383–391 389
123
0.11–0.35 mg l-1). Although the oxygen at site #2 was
continuously released from ORC, it was rapidly consumed
by a significant growth of bacteria, thus resulting in a
constant value of DO at 2.03–3.15 mg l-1.
Figure 6 also indicates that the CFU value at site #3
increased to 1.5 9 108 CFU ml-1 in the second phase, a
result caused by the addition of BTEX-degrading bacteria.
However, the microbial population was lower at site #4
near the end of the flow, indicating a possible washout of
microorganisms. Figure 6 also shows a higher CFU value
from days 3–45—particularly in days 10–20—in system A
in comparison with B because nitrogen, which can be
required for biomass construction, was added in only sys-
tem A.
Variations within microbial communities in monitoring
wells
PCR-SSCP was use to characterize the community distri-
bution in both systems at the monitoring wells (sites #3 and
#4) from the two-phase study. The removal efficiency, DO
and CFU were compared to assess the feasibility of this
method as well as the relationship between BTEX degra-
dation and the microbial growth or declination.
Figure 7 shows a UPGMA cluster analysis of the SSCP
profiles of microcosms at site #3 in system A. Three
biomarkers with highly similar sequences were used,
including Pseudomonas sp. (DQ211692), Pseudomonas
sp. (AF065166) and Pseudomonas putida (AY686638);
therefore, the three observed bands (c, d and e) were quite
similar. However, the Pseudomonas sp. (DQ124297) was
screened from a source different from that of the bacteria
mentioned earlier, and its bands (a, b, d and e) were slightly
different. The relative similarities indicated in Fig. 7b can
be classified into two phases for system A: (1) days 0, 5, 9,
12 and 19; and (2) days BA (bioaugmentation at day 20),
and days 22, 25, 28, 35, 40 and 45. Among the different
phase-tests, the diversity in the microbial community was
the greatest; therefore, and the least similarity (31%) was
exhibited. A low correlation between the groups for days 0
and 5 (about 0.65) was also indicated. The reasons appear
to be that the BTEX and COD removal efficiency was
gradually enhanced after bioaugmentation (10–20 days, as
plotted in Fig. 4A), and that the DO consumed by the
microorganisms resulted in an increase in the bacterial
population (as plotted in Fig. 5A). These possible reasons
led to a slight change in the microbial structure at site #3,
thereby tending to form the predominant bacteria as in the
first 19 days of this study. The results obtained from sys-
tem B were similar to those from A (data not shown). On
the basis of the analysis illustrated in Fig. 7a, the BA had a
correlation of 0.66 with the biomarker. The system con-
ditions gradually stabilized, thus becoming suitable for the
growth of bacteria. Days 22 and 25 paired had a similarity
of 0.66; days 28 and 35 had 1.0; days 40 and 45 had 0.89.
Since the supply of oxygen and substrate was adequate at
site #3, this site was more diversified than sites #1 and #4.
The results obtained from system B were similar to those
from A.
Figure 8 depicts a cluster analysis of the SSCP profiles
of the microcosms in system A at site #4. In both sys-
tems, the microcosms on day 22 and the marker were
highly similar (0.9 in A and 0.67 in B); whereas, on day
28, the similarities were reduced to 0.53 and 0.56 in
systems A and B, respectively. Because site #4 was
located near the outlet region and the supply of DO was
almost depleted at site #3, the bacterial structure at site
#4, including both aerobic and anaerobic bacteria, was
more complex than at site #3.
Conclusion
This study has demonstrated the use of ORRB to treat
BTEX-polluted groundwater. Both biostimulation and
bioaugmentation can accelerate the microbial activity and
degradation of pollutants. Moreover, the highest CFU value
and microbial diversity were found 15 cm downstream.
Both removal effects and stable CFUs were gradually
achieved. PCR-SSCP can be effectively used to explain the
changes in microbial structure, when CFU and environ-
mental information are provided. Determining the rela-
tionships among the BTEX removal efficiency, COD, DO,
bacteria densities and the microbial community structure
are the capable tools to assess the effectiveness of using
ORRB in BTEX-contaminated groundwater.
Acknowledgments This study was funded by the National Science
Council of the Republic of China under contract NO. NSC 96-2221-
E-224-093-MY3. The authors also wish to express their appreciation
to Dr. Cheryl J. Rutledge for her editorial assistance.
References
1. ATSDR (2001) Interaction profile for benzene, ethylbenzene,
toluene, and xylenes (BTEX). Agency for Toxic Substances and
Disease Registry, US Department of Health and Human Services,
Atlanta
2. Schreiber ME, Bahr JM (2002) Nitrate-enhanced bioremediation
of BTEX-contaminated groundwater: parameter estimation from
natural-gradient tracer experiments. J Contam Hydrol 55:29–56
3. Mater L, Sperb RM, Madureira LAS, Rosin AP, Correa AXR,
Radetski CM (2006) Proposal of a sequential treatment meth-
odology for the safe reuse of oil sludge-contaminated soil.
J Hazard Mater 136:967–971
4. Hristova K, Gebreyesus B, Mackay D, Scow KM (2003) Natu-
rally occurring bacteria similar to the methyl tert-butyl ether
(MTBE)-degrading strain PM1 are present in MTBE-contami-
nated groundwater. Appl Environ Microbiol 69:2616–2623
390 Bioprocess Biosyst Eng (2010) 33:383–391
123
5. Trindade POV, Sobral LG, Rizzo ACL, Leite SGF, Soriano AU
(2005) Bioremediation of a weathered and a recently oil-con-
taminated soils from Brazil: a comparison study. Chemosphere
58:515–522
6. Gavaskar AR (1999) Design and construction techniques for
permeable reactive barriers. J Hazard Mater 68:41–71
7. Kao CM, Chen SC, Wang JY, Chen YL, Lee SZ (2003) Reme-
diation of PCE-contaminated aquifer by an in situ two-layer bio-
barrier: laboratory batch and column studies. Water Res 37:27–38
8. Vezzulli L, Pruzzo C, Fabiano M (2004) Response of the bac-
terial community to in situ bioremediation of organic-rich sedi-
ments. Mar Pollut Bull 49:740–751
9. Liu SJ, Jiang B, Huang GQ, Li XG (2006) Laboratory column
study for remediation of MTBE-contaminated groundwater using a
biological two-layer permeable barrier. Water Res 40:3401–3408
10. van Cauwenberghe L, Diane PG, Roote S (1998) In situ biore-
mediation, Ground-Water Remediation Technologies Analysis
Center (GWRTAC), TO–98–01
11. Ruberto L, Vazquez SC, Mac Cormack WP (2003) Effectiveness
of the natural bacterial flora, biostimulation and bioaugmentation
on the bioremediation of a hydrocarbon contaminated Antarctic
soil. Int Biodeterior Biodegrad 52:115–125
12. Stallwood B, Shears J, Williams PA, Hughes KA (2005) Low
temperature bioremediation of oil-contaminated soil using bi-
ostimulation and bioaugmentation with a Pseudomonas sp. from
maritime Antarctica. J Appl Microbiol 99:794–802
13. Salanitro JP, Johnson PC, Spinnler GE, Maner PM, Wisniewski
HL, Bruce C (2000) Field-scale demonstration of enhanced
MTBE bioremediation through aquifer bioaugmentation and
oxygenation. Environ Sci Technol 34:4152–4162
14. Cunningham JA, Rahme H, Hopkins GD, Lebron C, Reinhard M
(2001) Enhanced in situ bioremediation of BTEX-contaminated
groundwater by combined injection of nitrate and sulfate. Envi-
ron Sci Technol 35:1663–1670
15. Oh JI, Lee SH, Yamamoto K (2004) Relationship between molar
volume and rejection of arsenic species in groundwater by a low-
pressure nanofiltration process. J Membr Sci 234:167–175
16. Lin CW, Lai CY, Chen LH, Chiang WF (2007) Microbial com-
munity structure during oxygen-stimulated bioremediation in
phenol-contaminated groundwater. J Hazard Mater 140:221–229
17. Lee DH, Zo YG, Kim SJ (1996) Nonradioactive method to study
genetic profiles of natural bacterial communities by PCR-single-
strand-conformation polymorphism. Appl Environ Microbiol
62:3112–3120
18. Schwieger F, Tebbe CC (1998) A new approach to utilize a PCR-
single-strand conformation polymorphism for 16S rRNA gene-
based microbial community analysis. Appl Environ Microbiol
64:4870–4876
19. Stach JE, Bathe S, Clapp JP, Burns RG (2001) PCR-SSCP
comparison of 16S rDNA sequence diversity in soil DNA
obtained using different isolation and purification methods.
FEMS Microbiol Ecol 36:139–151
20. Backman JSK, Hermansson A, Tebbe CT, Lindgren PE (2003)
Liming induces growth of diverse flora of ammonia-oxidising
bacteria in acid spruce forest soil as determined by SSCP and
DGGE. Soil Biol Biochem 35:1337–1347
21. Vacca G, Wand H, Nikolausz M, Kuschk P, Kastner M (2005)
Effect of plants and filter materials on bacteria removal in pilot-
scale constructed wetlands. Water Res 39:1361–1373
22. Bohan DG, Schlett WS (1999) Enhanced natural bioremediation
using a time release oxygen compound, in situ and on-site bio-
remediation. Battelle Press, Columbus 5:475–480
23. Lin CW, Chen LH (2007) The composition, structure, and use of
a set-up for an oxygen-release unit. Chinese patent M323474,
Taiwan, ROC
24. LaPara TM, Nakatsu CH, Pantea LM, Alleman JE (2001) Aerobic
biological treatment of pharmaceutical wastewater: effect of
temperature on COD removal and bacterial community devel-
opment. Water Res 35:4417–4425
25. White D, Schmidtke T, Woolard C (1999) Laboratory model of a
petroleum migration barrier in Arctic Alaska. J Hazard Mater
B67:313–323
26. Gallizia I, Vezzulli L, Fabiano M (2004) Oxygen supply for
biostimulation of enzymatic activity in organic-rich marine
ecosystems. Soil Biol Biochem 36:1645–1652
27. Dou JF, Liu X, Hu ZF, Deng D (2008) Anaerobic BTEX bio-
degradation linked to nitrate and sulfate reduction. J Hazard
Mater 151:720–729
28. Turlough FG, Stuart H, Terry M, Brent D (2002) An application
of permeable reactive barrier technology to petroleum hydro-
carbon-contaminated groundwater. Water Res 36:15–24
29. Vesela L, Nemecek J, Siglova M, Kubal M (2006) A biofiltration
permeable reactive barrier: practical experience from Synthesia.
Int Biodeterior Biodegrad 58:224–230
Bioprocess Biosyst Eng (2010) 33:383–391 391
123