Novel homologs of the multiple resistance regulator marA in antibiotic-contaminated environments
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Transcript of Novel homologs of the multiple resistance regulator marA in antibiotic-contaminated environments
w a t e r r e s e a r c h 4 2 ( 2 0 0 8 ) 4 2 7 1 – 4 2 8 0
Avai lab le a t www.sc iencedi rec t .com
journa l homepage : www.e lsev ie r . com/ loca te /wat res
Novel homologs of the multiple resistance regulator marAin antibiotic-contaminated environments
Sara Castiglionia,*, Francesco Pomatib, Kristin Millerb, Brendan P. Burnsb,Ettore Zuccatoa, Davide Calamaric, Brett A. Neilanb
aDepartment of Environmental Health Sciences, Mario Negri Institute for Pharmacological Research,
Via La Masa 19, 20156 Milano, ItalybSchool of Biotechnology and Biomolecular Sciences, The University of New South Wales, 2052 Sydney, AustraliacDepartment of Biotechnology and Molecular Sciences, University of Insubria, Via J.H. Dunant 3, 21100 Varese, Italy
a r t i c l e i n f o
Article history:
Received 15 April 2008
Received in revised form
2 July 2008
Accepted 4 July 2008
Available online 16 July 2008
Keywords:
Antibiotic resistance
Antibiotic contamination
Aquatic environment
marA
Bacillus
E. coli
* Corresponding author. Tel.: þ39 02 3901477E-mail address: [email protected]
0043-1354/$ – see front matter ª 2008 Elsevidoi:10.1016/j.watres.2008.07.004
a b s t r a c t
Antibiotics are commonly detected in the environment as contaminants. Exposure to
antibiotics may induce antimicrobial-resistance, as well as the horizontal transfer of
resistance genes in bacterial populations. We selected the resistance gene marA, mediating
resistance to multiple antibiotics, and explored its distribution in sediment and water
samples from surface and sewage treatment waters. Ciprofloxacin and ofloxacin (fluo-
roquinolones), sulphamethoxazole (sulphonamide), erythromycin, clarythromycin, and
spiramycin (macrolides), lincomycin (lincosamide), and oxytetracycline (tetracycline) were
measured in the same samples to determine antibiotic contamination. Bacterial pop-
ulations from environmental samples were challenged with antibiotics to identify resistant
isolates. The gene marA was found in almost all environmental samples and was
confirmed by PCR amplification in antibiotic-resistant colonies. 16S rDNA sequencing
revealed that the majority of resistant isolates belonged to the Gram-positive genus
Bacillus, not previously known to possess the regulator marA. We assayed the incidence of
marA in environmental bacterial populations of Escherichia coli and Bacillus by quantitative
real-time PCR in correlation with the levels of antibiotics. Phylogenetic analysis indicated
the possible lateral acquisition of marA by Bacillus from Gram-negative Enterobacteriaceae
revealing a novel marA homolog in Bacillus. Quantitative PCR assays indicate that the
frequency of this gene in antropised environments seems to be related to bacterial expo-
sure to water-borne antibiotics.
ª 2008 Elsevier Ltd. All rights reserved.
1. Introduction aquatic and soil ecosystems (Kummerer, 2004). Recently, Dan-
The aquatic and terrestrial ecosystems are the biggest known
reservoirs of antibiotic-resistant bacteria (D’Costa et al., 2006;
Biyela et al., 2004), and continuous exposure to antimicrobial
agents has the potential to enhance both the spread of resis-
tance genes and the selection for resistant bacterial strains in
6; fax: þ39 02 39014735.(S. Castiglioni).
er Ltd. All rights reserved
tas et al. (2008) showed that phylogenetically diverse soil
bacteria can grow using both natural and synthetic antibiotics
ascarbon sources,developing a veryhigh resistance level which
can be transferred also to closely related human pathogens.
Antibiotics normally used for therapeutic treatment may not be
completely metabolised and can therefore contaminate waste,
.
w a t e r r e s e a r c h 4 2 ( 2 0 0 8 ) 4 2 7 1 – 4 2 8 04272
surface and ground waters (Ternes, 1998; Hirsch et al., 1999;
Sacher etal., 2001; Calamarietal., 2003; Castiglioni etal., 2005). It
appears from the literature that environmental levels of anti-
biotics pose little environmental toxic risk, the greatest risk of
their presence being their potential to select for antibiotic
resistance amongst bacteria. Although antibiotics are found in
the environment at sub-inhibitory levels, relatively low
concentrations of antimicrobial agents can still promote
bacterial resistance (Kummerer, 2003; Cabello, 2006). Indeed,
antibiotic-resistant bacteria have been detected in sewage
(Iversen et al., 2002; Bertrand et al., 2005), surface (Ash et al.,
2002) and drinking water (Schwartz et al., 2003), soil (Burgos
et al., 2005; Nikolakopoulou et al., 2005), river sediment (Pei
et al., 2006) and marine aquaculture sites (Kim et al., 2004).
Exchange of resistance genes is optimal under conditions
of high nutrients, such as those found in aerobic and anaer-
obic treatments of wastewater, and high bacterial density,
such as in biofilms that are common in drinking water pipes,
soil and sediments. Hospital effluents and sewage treatment
plants (STPs) are major contributors to antibiotic resistance
spreading in the environment (Kummerer, 2004). Resistance
may be exchanged in the environment between distant
bacterial species and genera by horizontal gene transfer
(HGT) (Davidson, 1999), and eventually may reach human
pathogens through the food chain (Perreten et al., 1997) with
potential serious implications for human health. HGT can
also influence ecosystem stability changing the genetic code
of bacteria with possible alteration of their functionality and
ecological role.
The classical approach to study antibiotic resistance in the
environment is by cultivation and susceptibility testing. In
this study, we aimed to identify the presence of antibiotic-
resistant bacteria in selected environmental samples by
utilising standard cultivation methods and a molecular
approach, which represents a more direct means to search the
environment for bacteria and antimicrobial-resistance genes
(Schwartz et al., 2003). Recently, real-time PCR has been uti-
lised to quantify specific bacteria and associated genes in
environmental specimens (Volkmann et al., 2004; Smith et al.,
2004; Yu et al., 2005; Klomberg et al., 2005). As the environ-
ment is a reservoir of potential antibiotic resistance that can
be selected and transmitted to animals and humans, the
determination of sources and the quantification of occur-
rences relative to resistant bacteria and their relevant genes
are of paramount ecological and sanitary interest.
We targeted marA, a multiple antibiotic resistance regu-
lator, whose expression is sufficient to activate the marRAB
operon and produce a multidrug resistant phenotype (Gam-
bino et al., 1993; Martin et al., 1996; Alekshun and Levy, 1999).
The marA locus provides resistance to tetracycline, chloram-
phenicol, ampicillin, nalidixic acid, and ciprofloxacin, as well
as to other toxic chemicals such as household disinfectants
(Alekshun and Levy, 1999). Our objective was to investigate the
distribution of antibiotic resistance in association with this
antimicrobial-resistance regulator. The presence of a broad
array of antibiotics in the environment was measured by liquid
chromatography–tandem mass spectrometry and the possible
correlation with antibiotic resistance was investigated. We
used real-time PCR to directly ascertain a quantitative corre-
lation between high/low levels of antibiotic contamination at
selected sampling sites and the relative presence of the anti-
microbial-resistance regulator marA.
2. Materials and methods
2.1. Sampling of water and sediment
Seven samples of sediment and 10 samples of water were
collected from three rivers and a sewage treatment plant (STP)
in the north of Italy (Fig. 1). The sampling sites were chosen
along the Olona, Lambro and Po Rivers that receive wastes
from the most densely inhabited and industrialised areas of
Italy (Table 1). The Varese Olona STP was also studied in
Varese.
Influent (untreated) and effluent (treated wastewater)
samples were collected in the Varese Olona STP. Olona River
was sampled before and after the emission of discharges from
the Varese Olona STP. Site 1 was close to the river spring and
received few local urban wastes (Table 1). Sites 2 and 3, located
after the STP, were sampled to monitor the fate of antibiotics
in the river. Lambro River was sampled in Milan (site 4) and
immediately before connecting with Po River (site 5) to
monitor the contamination received from Milan and the
surrounding highly inhabited area. Po is the main Italian river,
with a length of 652 km (from the Alps to the Adriatic sea) and
an average flow rate of 1500 m3/s. It collects wastewater from
a catchment area of about 71,000 km2 in the north of Italy. The
sampling sites along the Po River (sites 6–8) were selected to
detect the contribution of the Lambro’s flow into the Po.
When sampling the Varese Olona STP, influent and effluent
were obtained by pooling water collected every 20 min by an
automatic sampler for 24 h (composite 24 h). Surface waters
were obtained by pooling samples collected every 20 min
during a limited period of 2 h (composite 2 h). Influent was
collected as a composite 24 h sample. Effluent was similarly
collected as a composite 24 h sample, starting from time 0þ RT
(retention time of the wastewater in the STP). Olona River
waters were collected as a composite 2 h sample starting from
time 0þ RTþ 12 h. Sediment samples were collected in all the
sampling sites along the rivers with the exception of site 5.
All water samples (2 L) were collected at the beginning of
September 2004, transferred to glass flasks, stored at þ4 �C,
and filtered on glass microfiber filters GF/D 1.6 mm (Whatman,
Kent, UK) prior to analysis. Sediment samples were trans-
ferred to sterile tubes (50 mL) and stored at �20 �C before
being lyophilised and analysed. Particulate and sediment
samples were lyophilised (Flexi-Dry� MP, Microprocessor
Control) and stored at �20 �C until DNA extraction.
Further details regarding the sampling procedure and sites
are reported in previous publications (Calamari et al., 2003;
Castiglioni et al., 2006).
2.2. Antibiotic measurement
We selected ciprofloxacin and ofloxacin (fluoroquinolones),
sulphamethoxazole (sulphonamide), erythromycin, clary-
thromycin, and spiramycin (macrolides), lincomycin (lincosa-
mide), and oxytetracycline (tetracycline) for the measurement
in surface and wastewater. Water samples were extracted
Fig. 1 – Sampling sites along the Olona, Lambro and Po Rivers, as well as the Varese Olona STP in the north of Italy.
w a t e r r e s e a r c h 4 2 ( 2 0 0 8 ) 4 2 7 1 – 4 2 8 0 4273
using solid phase extraction (SPE) and analysed by high-
pressure liquid chromatography–tandem mass spectrometry
(HPLC–MS–MS) using a specific multi-residue method recently
validated for the simultaneous determination of several
pharmaceuticals (Castiglioni et al., 2005, 2006). Briefly, samples
were extracted by two SPE columns, an Oasis MCX (60 mg,
Waters Corp., Milford, MA) at pH 2.0 and a Lichrolut EN (200 mg,
Table 1 – List of the sampling sites selected for thisinvestigation with the flow rate and the populationequivalents for each site
Sampling sites Flow rates (m3/s) Populationequivalents
STP (Varese Olona)
Influent and effluent 0.2 120,000
Olona River
Site 1 0.1 100
Site 2 0.5 120,000
Site 3 0.5 120,000
Lambro River
Site 4 5 1,500,000
Site 5 5 5,000,000
Po River
Site 6 932 5,400,000
Site 7 932 10,000,000
Site 8 1150 11,700,000
Merck, Darmstadt, Germany) at pH 7.0. A Luna C8 column
50 mm� 2 mm i.d., 3 mm particle size (Phenomenex, Torrance,
CA, USA) was used for chromatographic separation. An
Applied Biosystem–SCIEX API 3000 triple quadrupole (Q1q2Q3)
mass spectrometer, equipped with a turbo ion spray source
(Applied Biosystems–Sciex, Thornhill, Ontario, Canada), was
used for the analysis in the multiple reaction monitoring mode
(MRM). Deuterated internal standards were used for quantifi-
cation of the eight antibiotics investigated (Table 2).
2.3. Antibiotic sensitivity testing and isolatecharacterisation
Water samples were filtered and lyophilised together with
sediment samples according to the analytical procedures
mentioned above. The Kirby–Bauer method using Mueller–
Hinton Agar was employed to identify antibiotic-resistant
isolates (Hindler and Inderlied, 1985). Briefly, water and sedi-
ment samples were plated on Mueller–Hinton Agar before
overlaying antibiotic disks to test for bacterial strains suscep-
tibility to five antibiotics: tetracycline, chloramphenicol,
ampicillin, nalidixic acid and ciprofloxacin. Plates were incu-
bated aerobically for 24 h at 37 �C. Colonies that grew within the
zone of inhibition surrounding an antibiotic disk were
suspected resistant strains and were subcultured with that
antibiotic toconfirmresistance.Onplates, astandardMinimum
Inhibitory Concentration (MIC) was utilised for each antibiotic
(Table 3) as previously recommended (Cohen et al., 1993;
Table 2 – Antibiotic concentrations (ng/L) in water samples from rivers and wastewater
Varese Olona STP Olona River Lambro River Po River
Influent Effluent Site 1 Site 2 Site 3 Site 4 Site 5 Site 6 Site 7 Site 8
Ciprofloxacin 1674.20 626.50 nd 588.50 580.50 128.40 nd 24.50 17.40 nd
Clarythromycin nd 100.10 nd 114.80 80.50 73.51 46.64 4.30 4.50 3.04
Erythromycin nd nd nd nd nd nd nd nd nd nd
Lincomycin 3.90 3.70 nd 2.20 1.90 17.31 16.70 9.60 3.88 16.88
Ofloxacin 539.80 183.10 nd 177.40 157.30 306.10 19.31 23.11 36.91 nd
Oxytetracycline nd nd nd nd nd 105.10 nd nd nd 7.67
Spiramycin nd 118.70 nd 137.80 126.70 459.50 176.70 3.37 8.07 5.71
Sulphamethoxazole nd nd nd nd nd nd nd nd nd nd
nd¼Not detected.
w a t e r r e s e a r c h 4 2 ( 2 0 0 8 ) 4 2 7 1 – 4 2 8 04274
Goldman et al., 1996; Hooper et al., 1987). Isolates were cat-
egorised as resistant or sensitive according to their growth at
the MIC of the antibiotics tested.
The taxonomic identification of resistant strains was per-
formed by sequencing the amplification products obtained by
PCR with the 16S rDNA universal primers 27F and 1492R
(Neilan et al., 1997). marA primers were multiplexed with the
16S rDNA PCR to verify the presence of the resistance gene in
each isolate. Amplified DNA fragments were sequenced and
analysed as described below.
2.4. DNA extraction, amplification, and sequencing
Five hundred milliliters of filtered particulate or 0.3 g of the
sediment were resuspended in 500 mL of TNE buffer (50 mM
Tris–HCl, pH 8.0, 50 mM NaCl, 5 mM EDTA, pH 8.0), and
extracted for genomic DNA as reported elsewhere (Neilan et al.,
2002). DNA was ethanol precipitated, resuspended in 50 mL of
Table 3 – Antibiotic susceptibility of bacterial colonies from pla
Sampling sites
Waterparticulate
Presence ofmarA
Ampicillin(1.1 mg/mL)a
Tetracycline(2 mg/mL)a
STP influent þ R R
STP effluent þ R R
Site 1 � S R
Site 2 þ R R
Site 3 þ R R
Site 4 þ R R
Site 5 þ R R
Site 6 þ R R
Site 7 þ R R
Site 8 þ R R
Sediments
Site 1 þ R R
Site 2 þ R R
Site 3 � R R
Site 4 � R R
Site 6 þ R R
Site 7 þ R R
Site 8 þ R R
R, resistant; S, sensitive. The presence of marA (þ) in each sample is also
a Minimum Inhibitory Concentration (MIC).
sterile water, and quantified using an UV spectrophotometer
(NanoDrop, USA). The suitability of each extracted DNA for
amplification was initially checked with the universal bacterial
16S rDNA PCR (Neilan et al., 1997), and in case of polymerase
inhibition samples were diluted (1/10 and 1/100) to achieve
optimal amplification.
A set of two degenerate primers were designed, based on
sequences available from the literature, to amplify marA from
environmental samples. Sequences from strains of Escherichia
coli, Shigella, Enterobacter and Salmonella were obtained from
GenBank. The designed primers were: marAF (50-CTCCATA
CTAGAYTGGATHGARGA-30) and marAR (50-TGGTGGTACGT
CRAARTARTTYTT-30), with an expected amplification product
of 280 bp. PCR conditions were as follows: each 20 mL reaction
consisted of 1 mL of dNTPs mix (2 mM), 1 mL of MgCl2 (50 mM),
2 mL of 10� buffer, 1 mL of each primer (10 mM), 0.2 mL of Taq--
polymerase (1 U/mL) (Biotech International, Perth, Australia)
and 1 mL of the extracted DNA. Sterile filtered water was added
ted water and sediment samples
Antibiotic susceptibility
Ciprofloxacin(0.02 mg/mL)a
Chloramphenicol(7 mg/mL)a
Nalidixic acid(4.5 mg/mL)a
R R R
R R R
R R R
R R R
R R R
S R S
S R R
S R R
S S R
S R R
R R R
R R R
S R R
R R R
S R R
R R R
S R R
indicated.
w a t e r r e s e a r c h 4 2 ( 2 0 0 8 ) 4 2 7 1 – 4 2 8 0 4275
to 20 mL. The thermal cycling conditions for amplification were:
94 �C for 2 min, followed by 30 cycles of 94 �C for 10 s, 50 �C for
20 s, 72 �C for 25 s, with initial hot-start for 2 min at 94 �C before
the addition of 0.2 U Taq. A successive round of additional 30
PCR cycles, using 1 mL of amplified DNA as template, was
necessary to amplify marA from environmental samples.
Amplicons were analysed by 2% agarose gel electropho-
resis. Amplified DNA fragments for marA were extracted from
an agarose gel and purified by gel extraction (Promega
Corporation, Madison, WI) according to the manufacturer’s
instructions. Sequencing was performed using the Big Dye
Terminator method (ABI PRISM system, Applied Biosystems,
Foster City, CA). Sequence alignments and phylogenetic tree
constructions were performed using the ClustalX version 1.8
(Thompson et al., 1997). Homology searches were performed
using BLAST (Altschul et al., 1997).
2.5. Real-time PCR
Specific standard real-time PCR primer sets were designed
based on sequence alignments of marA homologs and 16S
rDNA using the Primer Express software 2.0.0 (Applied Bio-
systems). Alignment of sequences obtained from this study
along with those from GenBank allowed the design of specific
primers for marA from E. coli (EmarAF 50-ACGGAAATCGCG
CAAAAG-30 and EmarAR 30-CCAGATAGAGTATCGGCTCGTT
ACTT-50) and from Bacillus sp. (BmarAF 50-GCGCAAAAGCT
GAAGGAAAG-30, and BmarAR 30-TGTTGCGACTCGAAGC
CATA-50). This primer set specific for the novel marA homo-
logs in Bacillus was tested in silico versus known marA
sequences from the databases, and this indicated there was
no unspecific annealing during real-time PCR standard
conditions of two-step amplification (60 �C annealing and
extension). Similarly, 16S rDNA-based ColiF (50-CGCGTGTAT
GAAGAAGGCCT-30) and ColiR (30-TCCTCCCCGCTGAAAGTAC
TT-50), and BacillusF (50-CCTTGACGGTACCTAACCAGAAA-30),
and BacillusR (30-GATAACGCTTGCCAC CTACGTAT-50) were
produced for E. coli and Bacillus sp. taxonomic groups,
respectively. These primer sets were highly specific and did
not show any potential for cross-reactivity either in silico
(DNA alignment and primer testing) or in the laboratory (data
not shown). 16S rDNA specific primers were tested for speci-
ficity against the Ribosomal Database Project (http://rdp.cme.
msu.edu/index.jsp) and BLAST search (http://blast.ncbi.nlm.
nih.gov). While BacillusF/R primers were highly specific for
Bacillus species, ColiF/R appeared to recognise other entero-
bacterial species such as Shigella, Enterobacter and Salmonella.
In the laboratory, ColiF/R primers amplified E. coli DNA with
the highest efficiency compared to DNA from Salmonella as
assessed by serial dilution of genomic DNA from standard
strains (data not shown). No cross-reactivity was experimen-
tally detected between ColiF/R and Bacillus DNA, or between
BacillusF/R and E. coli DNA (data not shown).
Two representative samples were chosen for an exploratory
investigation by real-time PCR: a ‘‘blank’’ sample (site 1) with
no antibiotic contamination, and a contaminated sample (STP
influent) with high levels of antibiotics (Table 2). Real-time PCR
was carried out using total genomic DNA as templates with
samples extracted and purified as described in Section 2.4.
Reactions (25 mL) were performed using different dilutions
(1/10, 1/100) of samples, combined with the Sybr-Green�
Universal PCR Master Mix (Applied Biosystems). Reactions
were cycled using standard two-step real-time PCR protocol
and analysed using the ABI PRISM 7000 detection system and
software (version 1.1). The reactions were performed in tripli-
cate and blank (no-template) samples were added for each set
of primers in order to detect DNA contamination.
Our results were expressed using the comparative Ct
method following standard protocols (Livak and Schmittgen,
2001). This approach has the advantage of comparing target
genes directly to a control DNA sequence within the same
bacterium or bacterial population in order to obtain relative
quantitation.
To normalise for background contamination from E. coli
DNA in the Taq-polymerase mix (Bach et al., 2002), Ct values
from no-template PCR reactions (blank) were used as a refer-
ence for every 16S rDNA analysis; DCt values were obtained as
(Ctsample� Ctblank). Where no DNA contamination was detected
in blank amplification runs, such as for the Bacillus ribosomal
RNA gene primers, Ct values in no-template controls were set
arbitrarily to 45. Variations in this arbitrary Ct number did not
change the final ratio for the results expressed as 2�DDCt (data
not shown). The relative quantitation of marA in each DNA
sample was obtained by utilising 16S rDNA levels as internal
calibrators for quantitative DDCt calculation. DDCt quantita-
tions (marA DCt-16S DCt) were estimated for both E. coli and
Bacillus. Final 2�DDCt values were normalised using genomic 16S
rDNA copy numbers available for E. coli and Bacillus, respec-
tively (Klappenbach et al., 2001). Comparisons between
populations of E. coli and Bacillus by 16S rDNA quantitative
analysis used 2�DCt as the discriminant value.
2.6. Phylogenetic analysis
Sequences for the marA gene from isolates in this study and
from reference strains were used to infer a phylogeny,
reconstructing the phenogram from a pairwise distance
matrix (Jukes and Cantor, 1969) using the neighbor-joining
method (Saitou and Nei, 1987). All DNA sequences obtained in
this study have been submitted to the GenBank nucleotide
sequence database and assigned to accession numbers
DQ420170–DQ420219.
3. Results and discussion
3.1. Presence of antibiotics in surface and wastewater
We measured the concentrations of ciprofloxacin and ofloxacin
(fluoroquinolones), sulphamethoxazole (sulphonamide),
erythromycin, clarythromycin, and spiramycin (macrolides),
lincomycin (lincosamide), and oxytetracycline (tetracycline), in
surface and wastewater (Table 2). At the first sampling site
along the Olona River (site 1) no antibiotics were detected, while
concentrations at site 2 were comparable with those of the STP
effluent. Antibiotic levels were loweratsite 3, 1 kmdownstream
of the STP (Table 2). The effect of an STP on reducing antibiotic
concentrations has been previously described (Ternes, 1998;
Castiglioni et al., 2006). Spiramycin and clarythromycin were
detected in higher concentrations in the STP effluent possibly
Table 4 – Taxonomic identification of resistant isolatesand presence (D) of marA; nd [ not detected
Waterparticulate
Taxonomicalidentification
using 16S DNA
BLASTidentity
(%)
marA fromresistantcolonies
STP influent Enterococcus faecium 100 þSTP effluent Bacillus subtilis 97 þSite 1 Bacillus fusiformis 97 þSite 2 Bacillus fusiformis 97 þSite 3 Bacillus subtilis 95 þSite 4 Bacillus cereus 97 þSite 5 Bacillus sphaericus 96 þSite 6 Bacillus cereus 97 þSite 7 Bacillus subtilis 98 þSite 8 Bacillus pumilus 98 þ
Sediments
Site 1 Bacillus cereus 96 þSite 2 Bacillus cereus 97 þ
Bacillus fusiformis 97
Site 3 Bacillus cereus 97 þSite 4 Bacillus cereus 100 þSite 6 Bacillus cereus 96 nd
Site 7 Bacillus subtilis 96 þBacillus fusiformis 97
Site 8 Bacillus fusiformis 99 nd
w a t e r r e s e a r c h 4 2 ( 2 0 0 8 ) 4 2 7 1 – 4 2 8 04276
due to retention and successive release during the treatment
process or cleavage of the respective excretion conjugates
(Hirsch et al., 1999). Concentrations in the Lambro River were
approximately 10 times higher than in the Po River, with the
former receiving higher city loads from Milan and having
a lower dilution factor. Lincomycin was the only antibiotic that
was observed at the same concentration in all the samples.
Ciprofloxacin was the most abundant compound with
a maximum concentration of about 1.5 mg/L in the STP influent,
circa 600 ng/L in theSTP effluent and theriver Olona, 120 ng/L in
the Lambro, and 20 ng/L in the Po. This is consistent with
previous reports that identified ciprofloxacin as a ubiquitous
contaminant, detected at relevant concentrations in aquatic
habitats as well as in soil, sediment, and sludge (Golet et al.,
2002; Calamari et al., 2003; Castiglioni et al., 2005). We could not
detect erythromycin and sulphamethoxazole, possibly due to
the degradation of erythromycin to its main metabolite, dehy-
droerythromycin (Hirsch et al., 1999), and the summer decrease
in sulphamethoxazole use (Castiglioni et al., 2006). The veteri-
nary antibiotic oxytetracycline was detected only in Po and
Lambro Rivers, which receive animal farm wastes.
3.2. Antibiotic sensitivity testing
To evaluate the presence of antibiotic-resistant bacteria in our
water and sediment samples, we cultured environmental
specimens in the presence of ampicillin, tetracycline, cipro-
floxacin, chloramphenicol, and nalidixic acid. Under the
conditions tested, several isolates were obtained from each
sample and were classified as resistant or sensitive. Generally,
bacteria were resistant to at least three out of the five antibi-
otics tested at standard minimum inhibitory concentrations
(Table 3). All samples showed resistance to tetracycline,
ampicillin, chloramphenicol and nalidixic acid with few
exceptions (Table 3). Ciprofloxacin is the most recently intro-
duced antibiotic among those tested and, despite the fact that
bacteria can develop resistance to this drug in a short time
(Cunha, 2001), more sites contained isolates susceptible to this
antibiotic (8/17) compared to other compounds (Table 3).
3.3. Taxonomic identification and characterisation ofresistant bacterial colonies
Purified isolates from each sensitivity test-plate were identi-
fied by 16S rDNA amplification and sequencing. Resistant
bacterial strains obtained from antibiotic sensitivity tests
belonged to the genus Bacillus, with the exception of the
Enterococcus faecium isolates from the STP influent (Table 4,
GenBank accession numbers DQ420170–DQ420188).
The presence of marA in resistant colonies was probed by
PCR amplification and the corresponding DNA bands
sequenced. Amplicons obtained in this study, each associated
with the characterised bacterial isolates as reported in Table 4,
were revealed to be novel marA homologs (GenBank accession
numbers DQ420189–DQ420207). Homologs of the multiple
antibiotic resistance gene marA could not be found in any
known Bacillus genome present in the databases (GenBank) and
in the literature (Rasko et al., 2004). To our knowledge, this is the
first evidence of the multidrug resistance regulator marA iden-
tified in strains of the Gram-positive bacterial genus Bacillus.
Previously, the mar locus has been only identified in Gram-
negative bacteria (Cohen et al., 1993; Goldman et al., 1996), and
results from the present investigation suggest the novel
possibility of these genes being transferred to Gram-positive
microorganisms. Questions remain, however, regarding the
putative function in Gram-positive bacteria of marA, a global
regulator and not the actual protein product responsible for
drug resistance (Alekshun and Levy, 1999). In E. coli the MarA
protein can control the expression of multiple chromosomal
genes affecting resistance to antibiotics (Barbosa and Levy,
2000) and can also autoactivate marRAB operon transcription
(Martin et al., 1996). The resulting mechanism of resistance is
related to the influx decrease and efflux increase of toxic
chemicals from the cell (Alekshun and Levy, 1999).
All colonies recovered in this study after antibiotic sensi-
tivity testing possessed marA (Table 4), suggesting that this
regulator could potentially be involved in mechanisms associ-
ated with the observed resistance phenotypes. Species that
comprised our resistant bacterial colonies were mostly related
to inhabitants of soil or sediments of freshwater environments.
It is possible that our novel marA homologs could be involved in
the activation of certain endogenous drug or chemical export
systems, such as those that have been already described for
Bacillus (Grkovic et al., 2002). In any case, the present report of
potentially toxigenic and antibiotic-resistant Bacillus cereus
strains bearing the marA regulator may be of concern, as this
species is commonly responsible for food poisoning.
3.4. Detection of marA in environmental samples
The presence of marA was observed in all water samples except
site 1, and in all sediment samples except sites 3 and 4 (Table 3).
Every environmental sample appeared to be characterised by
w a t e r r e s e a r c h 4 2 ( 2 0 0 8 ) 4 2 7 1 – 4 2 8 0 4277
a single nucleotide sequence, each showing a homology of 97–
100% with other database entries for this multiple antibiotic
resistance regulator (accession numbers DQ420208–DQ420219).
Antibiotics were not detected in the surface water at site 1,
which is close to the river spring and receives little urban waste.
Organic compounds such as antibiotics and other contami-
nants can be adsorbed and concentrated in sediments (Golet
et al., 2002). It is possible that the occurrence of marA in
sediments at site 1 was associated with the presence of
accumulated antimicrobials or other local pollutants in this
matrix (Alekshun and Levy, 1999), which have not been ana-
lysed in this study.
3.5. Quantitative analysis of marA in environmentalsamples
The possible linkage between antibiotic environmental
contamination and the insurgence of bacterial resistance is
currently a topic of debate. Antibiotic susceptibility tests and
a marA specific PCR showed that the occurrence of resistance
genes or resistant phenotypes could not be clearly correlated
to the pattern of antibiotic contamination (Table 3). We
hypothesised that a quantitative analysis of resistance genes
could be useful to study the possible correlation between the
occurrence of antibiotics and the development of resistance in
the environment. Water-borne antibiotics may select for
a higher proportion of cells carrying resistance genes in
a bacterial population, rather than determining the presence
or absence of these genes in the community. Thus, real-time
quantitative PCR (q-PCR) was performed on two samples with
different antibiotic contamination profiles: site 1 and the STP
influent (Table 2).
We focused first on E. coli specific marA, and then on the
novel homolog found in our antibiotic-resistant Bacillus colo-
nies. E. coli specific marA was detected in both samples,
although the gene was observed at higher levels in the STP
influents relative to 16S rDNA (Table 5). E. coli and entero-
bacterial cells were more prevalent in the STP influent
compared to site 1 as assessed by 16S rDNA-based quantita-
tive analysis. marA specific for Bacillus was confirmed to be
present only in the STP influent and not at site 1 (Table 5),
although Bacillus strains were found at both sampling sites by
16S rDNA-based quantitative analysis (with a higher preva-
lence in the STP influent). These data suggested that the level
of bacterial resistance could be related to local pollutants
exposure among which antibiotics may represent a significant
Table 5 – Real-time PCR comparison for site 1 and the STP infl
E. coli
Raw valuea Norma
Site 1 16S rDNA 1.50� 0.16
marA 16.22� 5.49
STP influent 16S rDNA 1033.70� 73.46 1
marA 65.27� 4.96
a Values (average� standard error) correspond to 2�DCt (n¼ 3) and 2�DDCt
b Real-time PCR average raw-values adjusted for the 16S rDNA copy n
(Klappenbach et al., 2001).
selective pressure. Our initial data also revealed that marA
was borne mainly by Enterobacteriaceae in antibiotic-
contaminated environments. We observed that only 0.6% of
Bacillus cells in sewage water had genes that encoded for
multiple antibiotic resistance (Table 5). Enterobacteria do not
survive long in surface waters and may represent a health
hazard only in regions with local sewage discharge. On the
other hand, Bacillus strains bearing marA can be a long-term
vehicle for the spread of antibiotic resistance genes in the
environment.
3.6. Phylogeny of marA
With the aim of exploring the ancestor/descendant relation-
ships among our novel marA homologs, we constructed
a phylogenetic tree using sequences obtained from environ-
mental samples and antibiotic-resistant bacterial isolates,
together with known marA genes collected from databases
(Fig. 2). Sequences obtained from bacterial isolates and envi-
ronmental samples clustered into two distinct clades. The first
major clade contained marA sequences from the databases,
which branched into four sub-clades:Enterobacter (A), Salmonella
(B), E. coli and Shigella (C), and the DNA sequences obtained from
antibiotic-resistant colonies (D). marA sequences obtained from
environmental samples formed the second lineage of the
phylogenetic tree (E) (Fig. 2). According to this phylogenetic
analysis, marA sequences amplified from bacterial isolates
were different from those detected in the environment, and
more closely related to the marA from E. coli and Shigella (Fig. 2C
and D). Our phenogram suggested that both E. coli and Bacillus
acquired marA from an ancestral sequence found in Shigella.
The only marA sequence recovered in this study from E. faecium
(Table 4) also clustered with the Bacillus orthologs (Fig. 2D),
indicating the possibility of HGT between Enterococcus and
Bacillus.
In more general terms, our phylogenetic tree suggested
a delineation of marA sequences in Bacillus strains and
Enterobacteriaceae originating from an Enterobacter (Fig. 2).
Additionally, divergent bacterial and environmental DNA
sequences share a single early common ancestor. This indi-
cated that multiple antibiotic resistance and global regulators
such as marA could be more widespread among diverse
environmental bacterial populations than expected from
previous studies. D’Costa et al. (2006) and Dantas et al. (2008)
have recently highlighted the wealth of resistance strategies
that can be found in soil bacteria.
uent
Bacillus
lised valueb Raw valuea Normalised valueb
0.21 72.28� 47.3 8.12
2.32 Not detected –
47.67 2453.99� 403.31 275.73
9.32 0.0548� 0.0112 0.0062
(n¼ 6) for the 16S rDNA and marA analyses, respectively.
umber per genome (7 and 8.9 for E. coli and Bacillus, respectively)
Fig. 2 – Phylogenetic affiliations of marA homologs from bacterial isolates and environmental samples. The Bacillus
thuringiensis transcription regulator gene araC was included as a reference outgroup. The scale represents one substitution
per 100 base pair positions. Significant local bootstrapping values (1000 resampling cycles) are shown. (A) Enterobacter
strains; (B) Salmonella strains; (C) E. coli and Shigella strains; (D) antibiotic-resistant isolates from this study; (E)
environmental samples from this study. The number in the sequence designation refers to the different sampling sites,
while W and S indicate water and sediment, respectively.
w a t e r r e s e a r c h 4 2 ( 2 0 0 8 ) 4 2 7 1 – 4 2 8 04278
3.7. Methodological considerations
At the present stage, we can only speculate about the actual
diversity and distribution of marA and its associated resistance
in the environment, since the approach employed in this study
has several limitations. Our investigation on the bacterial
community present in aqueous samples was based on
membrane filtration, which may have selected only bacteria
with cell dimensions greater than 1.6 mm, both for total envi-
ronmental DNA extraction and plate culturing. The fact that
marA was borne mainly by Enterobacteriaceae in contami-
nated environments may explain the reason why we could
amplify only one dominant marA nucleotide sequence from
each of our water and sediment samples, which appeared
phylogenetically different from our cultured strains. The use of
nested PCR may also have increased this bias. Lyophilisation of
samples similarly could have biased our cultivation analyses
favouring bacteria of the Bacillus group, which can produce
endospores. Another bias could be introduced by the culture
media itself that would not be suitable for all soil organisms.
This signifies that data obtained from our extracted total DNA
and our cultivated strains may not be representative for the
total environmental bacterial community. The aim of our
q-PCR analysis was exploratory and suffered from challenges
associated with the quantitation of environmental bacterial
samples and the lack of more test samples. Future studies that
w a t e r r e s e a r c h 4 2 ( 2 0 0 8 ) 4 2 7 1 – 4 2 8 0 4279
will build on this present work include a larger area of study
and additional well-suited locations to conclusively support
a correlation between environmental levels of antibiotics and
multidrug resistance.
4. Conclusions
Our study shows that the multidrug resistance regulator marA
was widespread in environmental samples, but the presence/
absence of marA or associated resistant phenotypes was not
clearly correlated with the occurrence of antibiotic contami-
nation as we expected. Instead, preliminary q-PCR analysis of
marA in environmental samples suggested a possible relation
between antibiotic exposure and the level of bacterial resis-
tance, and suggested that the primary cause for the spread of
antibiotic resistance is anthropogenic (WWTP effluents).
Using a combination of different techniques we revealed
the presence of the multidrug resistance regulator marA in the
genus Bacillus, suggesting the acquisition of this novel
homolog by HGT and its putative origin in Enterobacteriaceae.
The approach employed was novel and the information pre-
sented is of topical environmental relevance. Most studies
investigating antibiotic-resistant bacteria have focused
strictly on faecally derived organisms and this is one of the
few studies that identify environmental bacteria as a target for
anthropogenic-induced antibiotic resistance. The identifica-
tion of multiple resistance genes in the toxic species B. cereus
may have implications for human health. Our results are
encouraging for further investigations to identify the origin
and distribution of antimicrobial-resistance in the environ-
ment. Antibiotic prescription and/or wastewater treatment
must adapt to face this increasing concern.
Acknowledgements
This work was partially supported by the Italian MIUR project
2002098317 (2002). The authors are grateful to C. Rossetti,
F. Goh and R. Cavaliere for the support in the experimental
work, and to T. Salmon for assistance in designing degenerate
primers. A special thanks to A. Infantino for assistance with
real-time PCR data analysis.
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