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REVIEW ARTICLE
Glutathione transferases in bacteria
Nerino Allocati
1
, Luca Federici
1,2
, Michele Masulli
1
and Carmine Di Ilio
1,2
1 Dipartimento di Scienze Biomediche, Universita
`‘G. d’Annunzio’, Chieti, Italy
2 Ce.S.I. Centro Studi per l’Invecchiamento, Universita
`‘G. d’Annunzio’, Chieti, Italy
Introduction
Glutathione transferases (GSTs; EC 2.5.1.18) consti-
tute a protein superfamily that is involved in cellular
detoxification against harmful xenobiotics and endo-
biotics [1–3]. One common feature of all GSTs is their
ability to catalyse nucleophilic attack by the tripeptide
glutathione (GSH) on the electrophilic groups of a
wide range of hydrophobic toxic compounds, thus pro-
moting their excretion from the cell [1]. GSTs are also
involved in several other cell functions, and are capa-
ble of binding a large number of endogenous and
exogenous compounds non-catalytically [1]. GSTs are
widely distributed in nature and are found in both
eukaryotes and prokaryotes. GSTs are divided into
at least four major families of proteins, namely cyto-
solic GSTs, mitochondrial GSTs, microsomal GSTs
and bacterial fosfomycin-resistance proteins [1,4]. The
cytosolic GSTs (cGSTs) have been subgrouped into
numerous divergent classes on the basis of their chemi-
cal, physical and structural properties [1,2]. The mito-
chondrial GSTs, also known as kappa class GSTs, are
soluble enzymes that have been characterized in
eukaryotes [5]. The third GST family comprises mem-
brane-bound transferases called membrane-associated
proteins involved in ecosanoid and glutathione metab-
olism (MAPEG), but these bear no similarity to solu-
ble GSTs [6]. Representatives of all three families are
also present in prokaryotes. The fourth family is found
exclusively in bacteria.
Keywords
bacterial glutathione transferase; chemical
stress; DCM dehalogenase; detoxification;
drug resistance; fosfomycin resistance
proteins; glutathione; HCCA isomerase;
oxidative stress; TCHQ dehalogenase
Correspondence
N. Allocati, Dipartimento di Scienze
Biomediche, Universita’ ‘G. d’Annunzio’, Via
dei Vestini 31, I-66013 Chieti, Italy
Fax: +39 0871 355 5282
Tel: +39 0871 355 5281
E-mail: allocati@unich.it
(Received 25 July 2008, revised 8 October
2008, accepted 14 October 2008)
doi:10.1111/j.1742-4658.2008.06743.x
Bacterial glutathione transferases (GSTs) are part of a superfamily of
enzymes that play a key role in cellular detoxification. GSTs are widely dis-
tributed in prokaryotes and are grouped into several classes. Bacterial
GSTs are implicated in a variety of distinct processes such as the biodegra-
dation of xenobiotics, protection against chemical and oxidative stresses
and antimicrobial drug resistance. In addition to their role in detoxifica-
tion, bacterial GSTs are also involved in a variety of distinct metabolic
processes such as the biotransformation of dichloromethane, the degrada-
tion of lignin and atrazine, and the reductive dechlorination of pentachloro-
phenol. This review article summarizes the current status of knowledge
regarding the functional and structural properties of bacterial GSTs.
Abbreviations
BxGST, Burkholderia xenovorans GST; CDNB, 1-chloro-2,4-dinitrobenzene; cGST, cytosolic GST; DCM, dichloromethane; EcGST,
Escherichia coli GST; GSH, glutathione; GST, glutathione transferase; HCCA, 2-hydroxychromene-2-carboxylic acid; MAPEG, membrane-
associated proteins involved in ecosanoid and glutathione metabolism; OaGST, Ochrobactrum anthropi GST; PmGST, Proteus mirabilis GST;
TCHQ, tetrachlorohydroquinone.
58 FEBS Journal 276 (2009) 58–75 ª2008 The Authors Journal compilation ª2008 FEBS
The first evidence for the presence of GSTs in bacteria
was reported more 25 years ago by Takashi Shishido
who showed the presence of GST activity in a strain of
Escherichia coli [7]. Since then, GSTs have been found
to be broadly distributed in aerobic prokaryotes, includ-
ing human and plant pathogens and soil bacteria. Con-
versely, GSTs have not been identified to date in
anaerobic bacteria [8] or in Archaea, the other domain
of prokaryotes. The absence of the enzyme in these
microorganisms is consistent with the lack of GSH [9].
This review summarizes current knowledge on the
functional and structural properties of bacterial GSTs
and the potential biotechnological applications of these
enzymes.
Classification and phylogenetic
relationships
cGSTs, also termed canonical GSTs, are homo- or hete-
rodimeric enzymes found in aerobic forms of life. cGSTs
metabolize a broad range of electrophilic substrates via
GSH conjugation. They are involved in protecting cells
against oxidative stresses, have peroxidase and isomer-
ase activities and are implicated in the development of
drug resistance [1,2]. In mammalian species they are well
characterized and have been grouped into seven classes:
alpha, mu, pi, sigma, theta, omega and zeta [1]. Several
other classes are restricted to non-mammalian species:
beta, chi, delta, epsilon, lambda, phi and tau [1,2,10]. To
assign a cGST to a class, it is generally accepted that
proteins with > 40% sequence identity belong to the
same class, whereas GSTs of different classes share
< 25% sequence identity. The identity increases if the
N-terminal region only is considered. This region com-
prises part of the active site, with residues that interact
with GSH, and it is evolutionarily conserved [1,2,11].
Besides amino acid sequence identity, immunological
properties, kinetic features as well as similarity of the
crystal structures provide additional supporting data
[1,2].
In bacteria, four different classes of cGSTs have
been identified: beta, chi, theta and zeta [2,10,12,13].
Beta class cGSTs have been purified and characterized
from several bacteria [14–25]. They are able to conju-
gate the model substrate 1-chloro-2,4-dinitrobenzene
(CDNB) and bind to the GSH–affinity matrix. All beta
class enzymes are characterized by the presence of a
cysteine residue at the GSH site [12]. The first cGST of
this class was characterized from a Proteus mirabilis
strain (PmGST). PmGST displayed biochemical and
structural properties that distinguish it from the GSTs
of other families and it was identified as the prototype
of the beta class [14,26–36].
Three other orthologues of the beta class were also
functionally and structurally characterized, from
E. coli (EcGST) and from two soil bacteria, Ochrobac-
trum anthropi (OaGST) and Burkholderia xenovorans
(BxGST, also known as BphK), respectively
[20,21,24,37–47].
Theta class enzymes in bacteria are represented by
two dichloromethane (DCM) dehalogenases produced
by facultative methylotrophic bacteria [48–52]. They
exhibit high amino acid sequence similarity to eukar-
yotic theta class GSTs and also share some properties
of these enzymes such as their reactivity with DCM,
their lack of activity with CDNB and their inability to
bind to GSH affinity matrices [50].
Tetrachlorohydroquinone (TCHQ) dehalogenase
was reported by Anandarajah et al. [53] to belong to
the zeta class on the basis of multiple sequence align-
ments. In particular, this enzyme is characterized, in
the GSH site, by the distinctive motif of zeta class
enzymes including two serine and a cysteine residues.
TCHQ dehalogenase is involved in two steps of the
biodegradation of pentachlorophenol and it also has
isomerase activity [53–56].
Recently a novel class of cGSTs, called chi class,
was proposed [10]. Two cyanobacterial cGSTs have
been purified and characterized from Thermosynechoc-
cus elongatus BP-1 (TeGST) and Synechoccus elongatus
PCC 6301 (SeGST). Although TeGST and SeGST
showed typical structural features of cGSTs, the results
presented here argued against their incorporation into
the beta class. In particular, these enzymes lack cyste-
ines completely indicating a possible different evolu-
tionary pathway for the cyanobacterial GSTs from the
beta class GSTs.
Like eukaryotic organisms, bacteria are character-
ized by multiple GST genes of widely divergent
sequences and unknown function [57]. In the E. coli
genome, in addition to the beta class GST [37] and to
Stringent starvation protein A, a RNA polymerase
with fold similarity to cGSTs [3], six GST homologues
have been identified [58]. The products of two of these
genes, YfcF and YfcG, exhibited GST- and GSH-
dependent peroxidase activities and were involved in
the defence against oxidative stress [59]. Pseudomonads
possess more than 10 GST genes [57]. In P. mirabilis
as well as in Proteus vulgaris three and four different
GSTs were identified, respectively [14,60]. Recently,
genomic analysis of the Gram-negative Shewanella
oneidensis revealed the presence of six GST-like genes
[61]. Two of these GST products showed high
sequence similarities to DCM dehalogenases.
Bacterial 2-hydroxychromene-2-carboxylic acid (HCCA)
isomerase is a GSH-dependent enzyme that is impli-
N. Allocati et al. Bacterial GSTs
FEBS Journal 276 (2009) 58–75 ª2008 The Authors Journal compilation ª2008 FEBS 59
cated in the naphtahalene degradation pathway
[5,62,63]. HCCA isomerase shares strong similarity
with kappa class enzymes, has a conserved serine resi-
due in the GSH site and displays catalytic activity
against CDNB [63]. Kappa class GSTs are soluble
dimeric proteins isolated and characterized from mam-
malian mitochondria [1,5]. In humans, hGSTK1 was
also located in the peroxisomal fraction suggesting a
new role for this class [1]. They are structurally distinct
from cGSTs, exhibit GSH activity towards haloarenes
and reduce cumene hydroperoxide and tert-butyl
hydroperoxide [1,5].
The MAPEG family are a wide and ubiquitous
group with diverse biological functions [6,64]. The
eukaryotic MAPEG family comprises at least six mem-
bers: 5-lipoxigenase activating protein (FLAP) and leu-
kotriene C
4
synthase (LTC
4
) involved in leukotriene
biosynthesis, MGST1, MGST2 and MGST3 with GST
and peroxidase activity and prostaglandin E synthase
(PGES) which catalyses the formation of prostaglan-
din E
2
from prostaglandin H
2
[6,64,65]. Recently,
crystallographic studies on different MAPEG members
clearly demonstrated that they are arranged into
trimers [66].
MAPEG members were also identified in several
bacteria such as E. coli,Vibrio cholerae and Synecho-
cystis sp. [6]. Some of them contained multiple MA-
PEG paralogues. They showed distant evolutionarily
relationships compared with eukaryotic mammalian
and non-mammalian forms. Bacterial MAPEG pro-
teins have been grouped in two distinct subfamilies,
one of which comprises E. coli and V. cholerae pro-
teins and the other the Synechocystis sp. protein which
more closely resembles enzymes belonging to the
MGST2/FLAP/LTC
4
subgroup [65]. Genes encoding
MAPEG proteins from E. coli and Synechocystis sp.
have been cloned and overexpressed. Membrane frac-
tions from cells overproducing E. coli MGST as well
as SynMGST showed GST activity with CDNB as sec-
ond substrate [65]. To date, no information about their
physiological role in bacteria is available.
A phylogenetic analysis using representative
prokaryotic and eukaryotic members of the GST
superfamily is shown in Fig. 1. The phylogenetic rela-
tionships among bacterial GSTs are consistent with
their known functional and structural features, show-
ing that they are distributed in different classes. The
beta class comprises the majority of bacterial GSTs
and enzymes belonging to the chi class are closely
related to this class. The two DCM dehalogenases are
clustered together with mammalian theta class
enzymes. TCHQ dehalogenases are closely related to
the zeta class. Agrobacterium tumefaciens GST shows
closer evolutionary relationship with mammalian alpha
class than with bacterial GSTs as reported previously
[67]. Sphingomonas paucimobilis LigF and LigG group
together and are distant from the Sph. paucimobilis
LigE enzyme which is more closely related to the zeta
class enzymes. Finally, Rhodococcus AD45 form a new
branch and it is not grouped with any other class.
Fig. 1. Evolutionary relationship between representative bacterial and eukaryotic GSTs. Multiple sequence alignment was produced by using
CLUSTAL W2 [143] and improved manually. The unrooted phylogenetic trees were constructed by the neighbour-joining method, based on the
distances derived from the Dayhoff matrix, with MEGA 4.0 software [144]. The robustness of the branches was assessed by the bootstrap
method with 1000 replications. Only nodes with a bootstrap value > 25% are reported. The scale bar represents a distance of 0.5 substitu-
tions per site. The sequences have the following accession numbers: epsilon class: Anopheles gambiae (XP_319972), Drosophila melanogas-
ter (CG5164); delta class: An. gambiae (Q93113), Anopheles dirus (AF273039); theta class: D. melanogaster (Q9VG96), An. gambiae
(Q94999), Bos taurus (Q2NL00), Homo sapiens (P30712); Methylobacterium sp. DM4 (P21161); Methylophilus sp. DM11 (P43387); phi class:
Arabidopsis thaliana (P42769), Zea mays GSTF3 (Q9ZP62), Z. mays GSTF1 (P12653), Triticum aestivum (P30111); Sph. paucimobilis LigF
(P30347); Sph. paucimobilis LigG (BAA77216); lambda class: A. thaliana (Q9LZ07), Z. mays (P49248), A. thaliana GSTL2 (Q9M2W2); omega
class: H. sapiens (P78417), Rattus norvegicus (Q9Z339), Caenorhabditis elegans (AAA27959); tau class: Aegilops tauschii (O04941), Z. mays
GSTU1 (Y12862), Z. mays GSTU2 (AJ010439); Agrobacterium tumefaciens (Q8UJG9); alpha class: H. sapiens GSTA1 (P08263), Mus muscu-
lus, GSTA2 (P10648); R. norvegicus (P04904), Gallus gallus GSTA1 (Q08392), G. gallus GSTA2 (Q08393), Bos taurus (Q5E9G0); sigma class:
H. sapiens (O60760), R. norvegicus (O35543), C. elegans (O16116), Manduca sexta (P46429), Ommastrephes sloanei (P46088); mu class:
H. sapiens (P09488), M. musculus (P10649), G. gallus (P20136), Dermatophagoides pteronyssinus (P46419); pi class: Onchocerca volvulus
(P46427), Bufo bufo (P81942), H. sapiens (P09211), R. norvegicus (P04906); Rhodococcus AD45 (AJ249207); chi class: T. elongatus
(NP_680998), S. elongatus (YP_171005), beta class: Haemophilus influenzae (P44521), Xylella fastidiosa (Q9PE18), Xanthomonas campestris
(P45875), O. anthropi (P81065), Magnetospirillum magnetotacticum (ZP_00054555), B. xenovorans LB400 (Q9RAFO), P. mirabilis (P15214),
E. coli (P39100); Sph. paucimobilis LigE (BAA02032); zeta class: H. sapiens (O43708), M. musculus (Q9WVL0), T. aestivum (O04437), A. tha-
liana (Q9ZVQ3); Sphingobium chlorophenolicum (Q03520); Sphingomonas spUG30 (AY057901); rho class: Pleuronectes platessa (X63761),
Pagrus major (AB158412), Micropterus salmoides (AY335905), Branchiostoma belcheri tsingtaunese (AY279519); kappa class: H. sapiens
(Q9Y2Q3), R. norvegicus (P24473), Xenopus tropicalis (AAH87819), G. gallus (XP_416525), Ps. putida (Q51948). MAPEG: H. sapiens
(P10620), B. taurus (Q64L89), D. melanogaster (AAN85305), Tetraodon nigroviridis (CAF97117), Synechocystis sp. (P73795), Acaryochl-
oris marina (YP_001518348), E. coli (P64515), V. cholerae (NP_232423).
Bacterial GSTs N. Allocati et al.
60 FEBS Journal 276 (2009) 58–75 ª2008 The Authors Journal compilation ª2008 FEBS
Because kappa class and MAPEG proteins are evolu-
tionarily distant from cGSTs two separate trees are
presented as insets in the Fig. 1. Bacterial MAPEG
proteins group with eukaryotic members, whereas
Pseudomonas putida HCCA isomerase groups with
mammalian kappa class members. Fosfomycin
resistance proteins show high divergence in primary
sequence and in structure, thus they were not
considered.
This classification is in agreement with the evolu-
tionary model proposed by Frova [11]. According to
this model, the ancestor from which GSTs originated
N. Allocati et al. Bacterial GSTs
FEBS Journal 276 (2009) 58–75 ª2008 The Authors Journal compilation ª2008 FEBS 61
is thioredoxin. The first phase of the evolution of
GSTs from thioredoxins saw the addition at the
C-terminus, or the insertion between the thioredoxin
fold, of an all-helical domain to produce two inter-
mediates: bacterial glutaredoxin 2 (GRX2), which
evolved into the cGSTs; and bacterial disulfide-bond-
forming oxidoreductase A (DsbA), which evolved
into the kappa GSTs. In a second phase, cGSTs fur-
ther diversified into different classes. Beta class
enzymes evolved after the dimerization of GRX2.
This model is supported by the ability of beta class
enzymes to act as thiol disulfide oxidoreductases as
well as GSH-conjugating enzymes and by the pres-
ence of a cysteine residue in the GSH site [14,68,69].
Finally, a shift from cysteine to serine chemistry
resulted in the theta class, followed by the zeta class
and then by all others classes. To date, there have
are no clear hypotheses about the evolution of
MAPEG family members [11].
Structures
Most of the bacterial GSTs identified to date belong
to the bacterial-specific beta class and since 1998 the
crystal structures of four representatives of this class
have been determined, i.e. P. mirabilis GST (PmGST)
[12], E. coli GST (EcGST) [37], B. xenovorans BphK
(BxGST) [47] and O. anthropi GST (OaGST) [41].
This, together with extensive site-directed mutagenesis
analysis, has allowed us to dissect in detail the
structural and catalytic properties of beta class
enzymes.
Beta class GSTs are homodimers with a chain length
of 201–203 residues. They display the canonical
GST fold with a thioredoxin-like N-terminal domain
followed by an all-helical C-terminal domain separated
by a short linker (Fig. 2A).
Comparative analysis of the crystal structures reveals
that the overall fold in beta class GSTs is remarkably
well conserved. Root mean square deviations among
equivalent Cas are generally < 1.5 A
˚when protein
monomers are superimposed, even though sequence
identities can be < 35–40%. When beta class monomers
are superimposed onto cGSTs belonging to other classes
rmsd values increase, ranging from 1.85 to 2.67 A
˚; these
values indicate that the canonical fold has been substan-
tially maintained from bacteria to mammals. Also the
monomers’ orientation in the different dimers is remark-
ably conserved (Fig. 2B). For example, when superim-
posing the OaGST dimer to the PmGST, EcGST and
BxGST dimers, rmsd values of 1.614, 1.418 and 1.54 A
˚,
respectively, are obtained [41]. These values are very
close to those obtained by superimposing the monomers
alone suggesting that strict conservation of the relative
orientation of the monomers in the dimer is required for
function.
Although the monomer fold in beta class GSTs
closely resembles that of other cGSTs, the dimer inter-
face is quite different. In fact, in contrast to other
GST classes, there is no open V-shaped interface,
although a close-packed arrangement is found, shaped
by the presence of stabilizing contacts at both the base
and top of the helical pairing that builds the interface
[12]. Furthermore, the interface in the majority of GST
classes is mainly hydrophobic in nature, whereas in
beta class GSTs it is markedly polar. As a conse-
quence, the well-known lock-and-key motif of alpha,
pi and mu class GSTs, comprising a protruding aro-
matic residue of one monomer that fits into a hydro-
phobic pocket in the other, is absent in beta class
GSTs [12,41]. Conversely, other structural motifs origi-
nally identified in mammalian GSTs are conserved in
beta class GSTs indicating their ancient origin. Among
them, an important stabilizing role is played by the
so-called N-capping box and hydrophobic staple motifs
at the N-terminus of the sixth helix in the C-terminal
domain that contribute to the interaction with the N-
terminal thioredoxin-like domain [36]. An additional
structural motif has been identified in beta class GSTs
that appears to be restricted to this class. This motif is
formed by a network of hydrogen bonds, located in
the proximity of the G-site, which zippers the terminal
helix of the C-terminal domain to the starting helix of
the thioredoxin-like domain. Partial disruption of this
motif has been shown to have dramatic consequences
on the both the stability and the functionality of
OaGST [41].
GSH binds to beta class GSTs in an extended fash-
ion consistent with what is observed in other classes.
Several interactions, both polar and hydrophobic, con-
tribute to its stabilization, including a hydrogen bond
with an aspartate residue from the other monomer
[12,41].
All beta class GSTs are characterized by the pres-
ence of a conserved cysteine residue located close to
the GSH sulfydryl group. Notably a mixed disulfide
bond was found in the structure of PmGST, with the
two sulfurs located at a distance of 2.2 A
˚(Fig. 2C)
[12]. This oxidized state, however, was not found in
the structures of OaGST [41] and BxGST [47], where
the average distance between sulfur atoms is 3.3 A
˚,
consistent with GSH being in the thiolate form and
sharing a hydrogen with the cysteine sulfur of the pro-
tein. In PmGST, two other residues are at hydrogen
bond distance from the GSH sulfydryl group, a
histidine (His106) and a serine (Ser9) (Fig. 2C). The
Bacterial GSTs N. Allocati et al.
62 FEBS Journal 276 (2009) 58–75 ª2008 The Authors Journal compilation ª2008 FEBS
histidine is conserved in other beta class GSTs,
whereas Ser9 is not conserved in OaGST, BxGST and
EcGST [37,41,47]. Interestingly, mutagenesis data on
PmGST and EcGST indicated that none of the above-
mentioned residues (Ser9, Cys10 and His106) is strictly
required for the classical conjugating activity or is
solely responsible for the reduced pK
a
of GSH, sug-
gesting that, in contrast with mammalian GSTs, the
stabilization of the GSH thiolate is likely the result of
a network of interactions [31,33,70]. OaGST deviates
partly from this behaviour. In fact, in OaGST the
G-site histidine adopts a different orientation with
respect to the other enzymes and does not bind GSH
[41]. In OaGST, in contrast to what is observed with
PmGST and EcGST, mutation of the conserved cyste-
ine to alanine led to a marked decrease in specific
activity, due to a dramatic loss in affinity for GSH
[42]. Interestingly, it was shown that, in this mutant,
GSH preferentially binds in a non-canonical position,
occupying the H-site [42]. Another beta class enzyme,
BxGST, was also shown to be able to bind a GSH in
the H-site [47]. Remarkably this enzyme was crystal-
lized in the presence of two GSH molecules, one with
the canonical G-site orientation and the other bound
at the H-site (Fig. 2D). In this structure the G- and
H-site GSH sulfurs are close (4.5 A
˚). These struc-
tural data support a mechanism in which once a disul-
fide bond is formed between the G-site GSH and
Cys10 in the reduction of several substrates, a second
GSH enters the H-site and a disulfide bond exchange
takes place with the formation and release of an
oxidized glutathione (GSSG), thus restoring the
enzyme’s functionality [47].
Two bacterial proteins show significant sequence
identity with mitochondrial kappa class GSTs. They
are DsbA and the HCCA isomerase. Kappa class
enzymes are peculiar in that, although they contain a
thioredoxin domain and an all-helical domain, their
topology differs from that of cytosolic enzymes
because the all-helical domain is inserted into the
thioredoxin fold. DsbA is a structural but not a func-
tional homologue of kappa class GSTs because its
active site does not bind GSH and it contains a
CXXC motif to perform redox catalysis [71]. HCCA
isomerase is the fourth enzyme in the naphthalene
catabolic pathway of Ps. putida. It catalyses the
conversion of HCCA, derived from cis-o-hydroxyben-
zeylidene pyruvic acid, to the more stable trans-o-
hydroxybenzeylidene pyruvic acid (Fig. 3I). Recently,
this enzyme has been subjected to extensive structural
and functional characterization that has shed light on
its peculiarities [63]. HCCA isomerase is a bona fide
AB
CD
Fig. 2. Structural studies on beta class
GSTs. (A) Structure of OaGST shown with
the twofold symmetry axis perpendicular to
the page (pdb code: 2NTO). The N-terminal
thioredoxin domain and the C-terminal all
helical domain are highlighted with different
tonalities. GSH molecules are shown in
sticks. (B) Overlay of four different beta
class GSTs dimers shown as Catraces: Oa-
GST (red), BxGST (green, pdb code: 2GDR),
EcGST (magenta, pdb code: 1A0F) and
PmGST (cyan, pdb code: 1PMT). This repre-
sentation highlights the conservation of beta
class fold as well as of the monomers’ ori-
entation in the dimers. (C) GSH binding site
in PmGST. In this crystal structure, GSH
(green carbons) forms a mixed disulfide with
Cys10. His106 and Ser9 are also at hydro-
gen bond distance from the GSH sulfur. (D)
Structure of BxGST in complex with two
GSH molecules (green carbons), one at the
canonical G-site and the other bound at the
hydrophobic substrates binding site (H-site).
The two GSH sulfurs are at close distance
from each other. This figure was prepared
with PYMOL (DeLano Scientific).
N. Allocati et al. Bacterial GSTs
FEBS Journal 276 (2009) 58–75 ª2008 The Authors Journal compilation ª2008 FEBS 63
Bacterial GSTs N. Allocati et al.
64 FEBS Journal 276 (2009) 58–75 ª2008 The Authors Journal compilation ª2008 FEBS
kappa class GST: it conserves the same topology as
the mammalian enzyme, it is able to bind GSH,
which is activated through a conserved serine residue,
and it performs the classic conjugating reaction on
CDNB. Its structure superimposes well onto the
mammalian kappa class enzyme with only minor dif-
ferences and overall rmsd values among equivalent
Caof 2.2 A
˚. GSH is bound and stabilized in a
similar manner to mammalian kappa class GSTs but
more tightly, due to two additional interactions in
HCCA isomerase. A possible mechanism for the
HCCA isomerase reaction has been proposed in
which GSH performs a nucleophilic attack on the
HCCA ring and is then released thus behaving as a
cofactor (see later).
Structural genomics initiatives are increasing our
understanding of the protein-fold evolution and often
lead to the functional annotation of proteins whose
role was previously undetectable or merely hypotheti-
cal, based on sequence alignments alone. This is the
case of the Atu5508 gene product of Ag. tumefaciens
whose structure has recently been determined [67].
The protein has a dimeric organization, it binds GSH
and displays the canonical GST fold even though its
sequence identity is < 20% in pairwise comparisons
with any previously characterized cGSTs. The protein
is also a functional GST because it is able to conju-
gate GSH to p-benzyl chloride, a GST substrate.
Although coming from a bacterium, protein-fold anal-
ysis and structure superpositions suggest that this
protein is more closely related to mammalian GSTs
than to other bacterial GSTs. In particular, it lacks
the hallmarks of beta class GSTs, including absence
of the catalytic cysteine and histidine in the G-site
and the presence of a hydrophobic lock-and-key
motif at the dimer interface. For these reasons it has
been proposed that this protein is the prototype of a
new class of bacterial GSTs that includes several close
homologues found analysing a large set of environ-
mental sequences in the environmental sequencing
project [67].
Functions
Bacterial GSTs are specialized in several detoxification
processes. They are able to detoxify a large number of
molecules via GSH conjugation (an example with the
classic substrate CDNB is shown in Fig. 3A). They
have an active role in protecting against oxidative
stress and are involved in the detoxification of antimi-
crobial agents. Some are implicated in the basal
metabolism and supply bacterial cells with carbon
sources. Bacterial GSTs are also involved in the
degradation of several monocyclic aromatic com-
pounds such as toluene, xylenes, phenols and atrazine
[72]. They also take part in the degradation of poly-
cyclic aromatic hydrocarbons, a class of hazardous
chemicals to both environmental and human health
[21,73–78].
Oxidative and xenobiotic stress
Beta class cGSTs are involved in detoxication reactions
against toxic effects of several xenobiotics [39,40,
79–81].
In a modulation study it was reported that, in a
P. mirabilis strain, PmGST contributed to protect the
cells against oxidative stress induced by hydrogen per-
oxide [80]. Increases in the level of mRNA transcrip-
tion and in protein expression levels were observed
when the bacterial cells were exposed to hydrogen per-
oxide. This result was confirmed by the analysis of a
gstB gene knock-out in the same P. mirabilis strain
that was found to be much more sensitive to hydrogen
peroxide than the wild-type strain [80]. Similar results
were also obtained for E. coli GST [59].
The modulation of OaGST in O. anthropi in the
presence of different xenobiotics was also investigated.
Unlike PmGST, hydrogen peroxide did not influence
the induction of the enzyme. Atrazine caused an
increase in the expression of OaGST at low, non-toxic
concentrations, suggesting its involvement in atrazine
metabolism [39]. Instead, phenolic compounds induced
a marked dose-dependent enhancement of the enzy-
matic cellular levels correlated to the toxicity of the
molecules indicating a role of OaGST in cellular
protection [39]. These data were also corroborated by
the preponderant presence of the enzyme in the peri-
plasmic space when bacteria were exposed to 4-chloro-
phenol [40].
However, although OaGST was found in the peri-
plasm, no signal sequence for export by the general
secretory (Sec) pathway was found [40]. Recently, an
alternative pathway has also been described, the twin-
Fig. 3. Reactions catalysed by bacterial GSTs. (A) Canonical conjugation of CDNB as second substrate; (B) dehalogenation of DCM to form-
aldehyde; (C) reductive dehalogenation of TCHQ to trichlorohydroquinone and of trichlorohydroquinone to 2,6-dichlorohydroquinone; (D) cis–
trans isomerization of maleylacetoacetate; (E) dehalogenation of 3-chloro-HOPDA; (F) hypothetical metabolic route for atrazine; (G) opening
of epoxide ring and reductive removal of GSH in isoprene metabolism; (H) b-aryl ether cleavage pathway; (I) step 4 of naphthalene catabolic
pathway; (J) opening of the epoxide ring of fosfomycin.
N. Allocati et al. Bacterial GSTs
FEBS Journal 276 (2009) 58–75 ª2008 The Authors Journal compilation ª2008 FEBS 65
arginine translocation (Tat) system, which allows the
transfer of folded proteins into periplasmic space [82].
Proteins transported via Tat system possess a distinc-
tive motif (SRRXFLK) at their N-terminus. This motif
was also not present in the OaGST sequence [83]. Sim-
ilarly, no Sec or Tat signals were found in PmGST,
EcGST, BxGST and Atu5508 [83,84]. Therefore,
the mechanism of OaGST transport (and possibly that
of other GSTs) into the periplasm is uncharacterized
at present. Moreover, a prokaryotic GSH transporter
in E. coli has recently been identified [85]. This
strongly suggests the presence of GSH in the peri-
plasm, as hypothesized previously [86], and underlines
that bacterial GSTs also display activity in this
compartment.
PmGST is able to catalyse a glutaredoxin-like reac-
tion using cysteine S-sulfate and hydroxyethyl disulfide
as substrates [68]. The G-site cysteine residue is essen-
tial for this redox activity [68] and the mixed disulfide
observed in the PmGST crystal structure has been
suggested as an intermediate in glutaredoxin-like
reactions [68].
Bacterial GSTs in dehalogenation
Microbial dehalogenases play a key role in the biodeg-
radation of several chlorinated xenobiotics, both ali-
phatic and aromatic [87,88]. Halogenated compounds
are widely used in industry and constitute an impor-
tant group of environmental pollutants.
Bacterial GSTs catalyse different reactions using
GSH as a cofactor, i.e. DCM dehalogenases catalyse
the hydrolytic dechlorination of dichloromethane,
whereas TCHQ dehalogenase catalyses a reductive
dehalogenation reaction.
DCM dehalogenases
DCM dehalogenase is a GSH-dependent enzyme syn-
thesized by a number of facultative methylotrophic
bacteria that are able to utilize DCM as a sole carbon
and energy source [48]. In the first step of degradation,
the enzyme dechlorinates DCM to formaldeyde and
inorganic chloride (Fig. 3B). DCM, a significant envi-
ronmental contaminant, is widely used as an industrial
solvent. The properties of two DCMDs are well docu-
mented in Methylobacterium dichloromethanicum DM4
and in Methylophilus leisingeri DM11 [48–52]. Both de-
halogenases are closely related to eukaryotic theta class
GSTs (Fig. 1). In particular, like theta class GSTs,
DCMDs share a conserved serine residue at the N-ter-
minal domain that is essential for catalysis [89]. Never-
theless, on the basis of other criteria such as N-
terminal amino acid sequences, kinetic and immuno-
logical properties, they have been further subdivided
into two classes. One class is formed by group A
enzymes, including the DCM dehalogenases of Methy-
lobacterium dichloromethanicum DM4. By contrast,
M. leisingeri DM11 is the prototype for group B
enzymes. The most significant difference between the
two groups lies in their kinetic properties. Under con-
ditions of substrate saturation, DM11 is significantly
faster in dechlorination than DM4.
To date, no structure is known for DCMDs. A 3D
homology model of DCMD from the M. leisingeri
DM11 strain has been presented based on alignments
with GST members from the theta and the alpha class
[90].
TCHQ dehalogenase
TCHQ dehalogenase catalyses the reduction of TCHQ
to trichlorohydroquinone and then to dichlorohydro-
quinone during the biodegradation of pentachlorophe-
nol, a xenobiotic compound present in the
environment, utilized primarily as fungicide for wood
preservation [91–94]. The catalytic mechanism of the
reaction was exhaustively studied by Copley et al.
[54,56,95]. TCHQ dehalogenase was purified by
Sphingobium chlorophenolicum, a soil bacterium that
can grow on pentachlorophenol as a sole carbon
source [92,96]. TCHQ dehalogenase utilizes two GSH
molecules to reductively dechlorinate TCHQ to trichlo-
rohydroquinone and then dichlorohydroquinone
(Fig. 3C). First, TCHQ dehalogenase catalyses the
nucleophilic attack of GSH on the substrate forming a
GSH conjugate, and then converts the conjugate to
reduced products. A conserved cysteine is required to
this second step of the reaction through the formation
of a mixed disulfide with GSH [54,97].
TCHQ dehalogenase also has maleylacetoacetate
isomerase activity, and the conserved cysteine is also
required for this activity [53]. Maleylacetoacetate
isomerases are enzymes that catalyse the GSH-depen-
dent cis–trans isomerization of maleylacetoacetate to
fumarylacetoacetate during the catabolism of tyrosine
and phenylalanine (Fig. 3D). Although the overall
sequence identity between TCHQ dehalogenase and
maleylacetoacetate isomerase is low, the active site is
highly conserved and in both cases contains a catalytic
cysteine [53].
Because maleylacetoacetate isomerases are part of
an ancient degradation pathway, whereas TCHQ
dehalogenase is a more specialized enzyme, it was
supposed that TCHQ dehalogenases evolved from
maleylacetoacetate isomerases [53].
Bacterial GSTs N. Allocati et al.
66 FEBS Journal 276 (2009) 58–75 ª2008 The Authors Journal compilation ª2008 FEBS
Biphenyl/polychlorinated
biphenyldehalogenation
A cGST characterized from B. xenovorans strain
LB400, a biphenyl/polychlorinated biphenyl-degrading
microorganism, known as BphK or BxGST, is one of
the most extensively investigated bacterial GSTs
[21,43–47]. This enzyme, which belongs to the beta
class, is encoded by a gene (bphK) located within the
bph locus, which specifies the degradation pathway of
biphenyl and chlorobiphenyl compounds. B. xenovo-
rans LB400 is able to attack a broad spectrum of poly-
chlorinated biphenyl congeners and is able to grow on
biphenyl as sole carbon source [21,43]. Mutagenic
studies indicated that although the bphK gene is not
essential for utilization of this carbon source its expres-
sion gives advantage to the strain in the utilization of
biphenyls [43]. Subsequently, it has been established
that BphK catalyses efficiently the dehalogenation of
3-chloro-2-hydroxy-6-oxo-6-phenyl-2,4-dienoate com-
pounds that are produced by the co-metabolism of
polychlorinated biphenyls (Fig. 3E) [46]. The proposed
reaction mechanism is similar to that described for
TCHQ dehalogenase [56]. Although less efficient,
BphK enzyme also has dechlorination activity against
4-chlorobenzoate [44]. A bphK gene is also present in
Sphingomonas yanoikuyae B1 and its expression allows
Sph. yanoikuyae B1 to grow faster on m-toluate
[98,99].
Atrazine metabolism
GSTs are able to detoxify several classes of herbicides
including triazines, a class of compounds to which
atrazine, one of the most widely used herbicides,
belongs [100,101]. GSTs are involved in the first step
of atrazine biodegradation with the removal of the
chlorine atom produced by atrazine–GSH conjugation
[100,101]. Dechlorination is followed by the stepwise
removal of isopropylamine and ethylamine groups by
dealkylation [102]. In bacteria, atrazine can be degra-
dated either by a microbial consortium or by a single
microorganism [103,104]. For instance, in Pseudomonas
ADP, atrazine is metabolized to cyanuric acid by three
enzymatic steps. The first step is performed by atrazine
chlorohydrolase followed by two dealkylations [104].
O. anthropi is a soil bacterium that is able to grow
on atrazine utilizing it as source of carbon [105] and
which expresses a functional beta class GST [24]. In a
modulation study of OaGST in the presence of several
xenobiotics, Favaloro and co-workers also showed
an increase in the levels of enzyme when atrazine
was added to the exponentially growing cells of
O. anthropi, suggesting an involvement of OaGST in
atrazine conjugation with GSH [39]. A proposed atra-
zine degradation pathway by bacterial GSTs is showed
in Fig. 3F.
Isoprene metabolism
Two GSTs were purified from the isoprene-utilizing
bacterium Rhodococcus sp. strain AD45 and their func-
tional properties were characterized [106–108]. Both
enzymes are involved in the metabolism of isoprene, an
atmospheric reactive hydrocarbon that plays a role in
ozone, organic peroxides and carbonic monoxide for-
mation, and their genes are localized in the isoprene
degradation gene cluster [106,108]. The first GST,
encoded by the isoI gene, catalyses the GSH-dependent
ring opening of isoprene monoxide, the primary oxida-
tion product of isoprene (Fig. 3G). The GSH conjugate
1-hydroxy-2-glutathionyl-2-methyl-3-butene is then oxi-
dized in two consecutive steps to 2-glutathionyl-2-
methyl-3-butenoic acid by a dehydrogenase (IsoH). The
way in which isoprene degradation proceeds has not
been fully characterized. A convincing hypothesis is
that 2-glutathionyl-2-methyl-3-butenoic acid could be
converted to the corresponding CoA-thioester by a
racemase expressed by isoG gene, to allow the second
GST, which is encoded by the isoJ gene, to remove the
GSH molecule [108,109]. It is thought that IsoJ might
catalyse the reductive removal of GSH using a second
GSH molecule in a similar fashion as the TCHQ dehal-
ogenase (Fig. 3G) [54,91,108,109]. A relevant difference
from TCHQ dehalogenase is that the GSH conjugate is
formed several steps before its reduction, because the
removal of the GSH from 1-hydroxy-2-glutathionyl-2-
methyl-3-butene is energetically unfeasible [109]. More-
over, IsoI/GST is able to degrade halogen epoxides
such as 1,2-dichloroepoxyethanes and epichlorohydrin
[106,107]. In Rhodococcus AD45 a novel GST, namely
IsoILR1, was recently characterized with activity
towards cis-1,2-dichloroethylene epoxide and epoxypro-
pane [110].
Lignin degradation pathway
In Sph. paucimobilis SYK-6, the role of three tandemly
located genes, ligE,ligF and ligG, involved in the pro-
cess of lignin degradation, a fundamental step for the
earth’s carbon cycle, has been described [111–113].
Sph. paucimobilis is able to degrade a wide variety of
lignin compounds including b-aryl ether. The b-aryl
ether cleavage is a fundamental step in lignin degrada-
tion, because this intermolecular linkage is the most
abundant in lignin. LigE and LigF are enantioselective
N. Allocati et al. Bacterial GSTs
FEBS Journal 276 (2009) 58–75 ª2008 The Authors Journal compilation ª2008 FEBS 67
GSTs that cleave the b-aryl ether linkage with con-
sumption of GSH [113]. LigG is instead a GSH lyase
that catalyses the elimination of GSH from the conju-
gate produced by LigF (Fig. 3H) [112,113].
Naphthalene metabolism
HCCA isomerase is a GSH-dependent enzyme, struc-
turally related to mammalian kappa class enzymes,
involved in the naphthalene degradation pathway
[5,62,63]. HCCA isomerase is also involved in naph-
thalene sulfonates and anthracene catabolism
[114,115]. Naphthalene catabolism consists of an upper
pathway and a lower pathway. In the upper pathway,
naphthalene is metabolized to salycilate in six steps.
HCCA isomerase is the fourth enzyme of this pathway
and catalyses cis–trans isomerization between HCCA
and trans-o-hydroxybenzylidene pyruvic acid (Fig. 3I).
GSH is thought to be involved in this reaction by its
covalent addition of HCCA. The addition alters the
hybridization state at C7 promoting a rotation around
the C7–C8 double bond [63].
Interaction with antibiotics
Several studies on the interaction of PmGST with dif-
ferent classes of antibiotics have been performed and a
possible role for the enzyme in antibiotic-resistance
proposed [29,116].
First, it was observed that the efficiency of a number
of antimicrobial drugs decreased notably in the pres-
ence of the purified enzyme in the medium culture, as
shown by increased minimal inhibitory concentration
values [16,116]. By contrast, the presence of mamma-
lian GSTs had no effect on antibiotic efficiency [16].
Second, studies on the interaction of PmGST with sev-
eral antibiotics indicated that the enzyme sequesters
antimicrobial drugs with avidity [29]. The effect of 18
different antibiotics as inhibitors of PmGST activity
using CDNB and GSH as substrates, were also mea-
sured. Four of them, namely minocycline, tetracycline,
rifamycin and nitrofurantoin, were strong inhibitors
with IC
50
values between 49 and 140 lm. These drugs
produced a significant decrease in the k
cat
values of the
bacterial enzyme for both substrates [29]. Furthermore,
PmGST displays a protective action against antibiotics
also in vivo [80,117]. An increase in PmGST levels was
observed when bacteria were grown in the presence of
drugs [80]. Moreover, viability tests showed that a gst
null-mutant P. mirabilis strain was more sensitive to
antibiotics than the wild-type bacterium [80]. Finally,
crystallographic data highlighted the presence of a
hydrophobic cavity large enough to bind antibacterial
molecules located at the dimer interface [12]. These
results were strengthened by the preponderant periplas-
mic location of the enzyme in the periplasmic space
[81].
Fosfomycin resistance proteins
Fosfomycin ([1R,2S]-[1,2-epoxypropyl]-phosphonic acid)
is a bactericidal broad-spectrum antibiotic effective
against both Gram-negative and Gram-positive bacte-
ria. Fosfomycin inhibits the enzyme MurA (UDP-
NAG enolpyruvyl transferase), which catalyses the
transfer of enolpyruvate from phosphoenolpyruvate to
uridine diphospho-N-acetylglucosamine, the first com-
mitted step of bacterial cell-wall biosynthesis. Resis-
tance is mainly chromosomal but resistance genes have
also been found on transmissible plasmids [118]. Resis-
tance to fosfomycin can be achieved by several differ-
ent mechanisms, including decreased uptake of the
antibiotic, overexpression or mutation of MurA, and
enzymatic modification of the antibiotic [118,119].
FosA, FosB and FosX represent three mechanisti-
cally distinct classes of enzymes that confer resistance
to fosfomycin by adding GSH, l-cysteine or a hydro-
xyl group, respectively, to the oxirane ring of the
antibiotic, and inactivating it.
FosA was originally identified in strains carrying
fosfomycin-resistance plasmids obtained from clinical
isolates [120–122]. Suarez and co-workers described a
new mechanism of antibiotic resistance due to the
enzymatic modification of fosfomycin [121,122]. Inacti-
vation of fosfomycin occurred by the formation of an
adduct between its carbon 1 atom and the sulfydryl
group of the GSH cysteine resulting in the opening of
the epoxide ring of the antibiotic (Fig. 3J). The reac-
tion was catalysed by an enzyme that was referred to
as a GST. The enzyme was purified and characterized.
It did not bind to the GSH–agarose matrix and did
not catalyse the reaction between GSH and CDNB,
indicating that this protein had different properties
from the canonical GSTs. The enzyme is a homodimer
of 32 kDa and its activity is dependent on the addition
of the Mn
2+
cation [122]. In subsequent studies, Arm-
strong and co-workers demonstrated that FosA is a
metalloglutathione transferase related to glyoxalase I
and extradiol dioxygenases, members of the vicinal
oxygen chelate superfamily [4,123]. In addition, they
showed that each subunit of the homodimer contains a
mononuclear Mn
2+
centre that interacts strongly with
the antibiotic and also that the enzyme requires a
monovalent cation K
+
for optimal catalytic activity
[123]. FosA is also encoded in the bacterial genomes
and the 3D structure of a genomically encoded FosA
Bacterial GSTs N. Allocati et al.
68 FEBS Journal 276 (2009) 58–75 ª2008 The Authors Journal compilation ª2008 FEBS
from the pathogen Ps. aeruginosa was described [124].
The protein fold showed similarity to members of vici-
nal oxygen chelate superfamily and consists of paired
babbb motifs that form a cupped-shaped cavity for the
metal ion-binding site. The K
+
ion is accommodated
in a loop located 6.5 A
˚from the Mn
2+
cation [124].
The structure of FosA in complex with antiobiotic was
also obtained. Plasmid-encoded and genomically
encoded enzymes are very similar in structure. The
crystal structure of FosA from transposon Tn2921
maintains the same basic molecular arrangement
observed in genomically encoded FosA [125]. Recently,
based on structural data, the residues involved in the
binding of both fosfomycin and GSH substrates have
been identified and characterized by mutagenesis
[126,127].
FosB was originally identified in fosfomycin-resis-
tant Staphylococcus strains and the genes were encoded
by plasmids [128–130]. A second type of FosB was
identified in the genome of a Bacillus subtilis strain
and subsequently characterized [131]. The protein is a
dimeric metallothiol transferase related to FosA.
Unlike FosA, FosB utilizes Mg
2+
as metal cofactor.
In addition, FosB uses l-cysteine rather than GSH as
thiol donor and is less efficient than FosA [131]. This
is in agreement with previous studies because the GSH
molecule was not detectable in most of the Gram-posi-
tive bacteria tested, including Bacillus subtilis [132].
FosX is a Mn(II)-dependent fosfomycin specific
epoxide hydrolase. It catalyses the addition of a water
molecule to fosfomycin, thus inactivating it. The
enzyme is genomically encoded, it is found in several
microorganisms and it has been well characterized
in Mesorhizobium loti and Lysteria monocytogenes
[133,134]. The two enzymes showed significant func-
tional differences. Listeria FosX is a good catalyst and
is responsible for high resistance to fosfomycin [133].
By contrast, M. loti FosX produces modest resistance
to the antibiotic and, consistently, its kinetic costants
are lower than those of Listeria FosX. In addition,
M. loti FosX also catalyses the addition of GSH to
the antibiotic even if with low efficiency. It has been
suggested that M. loti FosX may be an intermediate in
the evolution of fosfomycin resistance proteins that
plays some yet to be identified role in the catabolism
of phosphonates. The structure of FosX was also
determined for both enzymes [133,134]. The FosX
structures are closely related and the overlay with
FosA from Ps. aeruginosa [124] shows a large degree
of similarity. Unlike FosA, the enzymes do not contain
aK
+
ion-binding site near the active site. The
most interesting aspect of these structures is the obser-
vation that fosfomycin binds to FosX enzymes in a
different orientation from that observed in the FosA
enzyme.
A new mechanism of fosfomycin inactivation was
described by Garcia et al. [135] in a fosfomycin-resis-
tant strain of Pseudomonas syringae. The bacterium
yielded an enzyme, FosC, that inactivated the anti-
biotic using ATP to phosphorylate fosfomycin in the
presence of Mg
2+
. This finding was corroborated by
sequence alignments highlighting a region of partial
homology between FosC and the Mg-ATP binding
domains of AMP–ATP phosphotransferases. To date,
no relationship between FosC and the other fosfo-
mycin resistance proteins is known.
Potential applications of bacterial
GSTs
As previously described, bacterial GSTs are involved
in several types of chemical transformations and may
represent a versatile tool with a variety of biotechno-
logical applications, for example, in the field of bio-
remediation, an economical alternative to conventional
physicochemical methods to clean up environmentally
contaminated sites. The relative ease of genetic manip-
ulations in bacteria and their ability to grow rapidly
constitute a further advantage.
Several studies have been carried out exploiting the
potential of GSTs using both purified proteins and
microorganism engineering, some of which are summa-
rized here.
An example of protein engineering using the DNA-
shuffling technique was shown by Mannervik et al.
[136]. They hybridized six alpha class GSTs of differing
mammalian origin obtaining chimeric enzymes with
improved catalytic properties and altered substrate
selectivity towards several noxious iodoalkanes.
Another example is in the engineering of fusion pro-
teins with several distinct enzymatic activities. For
example, a trifunctional enzyme with superoxide
dismutase, glutathione peroxidase and glutathione
transferase activities was recently generated [137]. This
recombinant chimeric enzyme was shown to be effec-
tive in scavenging reactive oxygen species, thus show-
ing that this approach may have several applications
in medicine as well as in environmental field.
Another potential application lies in the preparation
of biosensors. These are detection systems widely used
to check contaminated environments that combine a
biological component with a detector element. Biosen-
sors are competitive systems in comparison to conven-
tional methods being inexpensive, easy to use and
characterized by high sensitivity and selectivity. For
example, a mammalian GST was used to develop an
N. Allocati et al. Bacterial GSTs
FEBS Journal 276 (2009) 58–75 ª2008 The Authors Journal compilation ª2008 FEBS 69
optical biosensor for detection of captan in contami-
nated waters [138]. Captan is used to control a broad
spectrum of plant pathogenic microorganisms and it is
a strong inhibitor of GSTs [139].
A large number of bacterial species have developed
the ability to degrade xenobiotics previously considered
to be non-degradable [140]. Examples of microbial con-
sortia combining the ability of two or more bacterial
species to metabolize one or more noxious molecules
have been described [141]. An alternative route is to
engineer a single bacterial strain to carry a complete
metabolic pathway that efficiently eliminates environ-
mental toxic compounds [110]. For example, Wood
et al. [110] engineered in E. coli a metabolic pathway to
improve the degradation of chlorinated ethenes, which
constitute a large group of toxic environmental pollu-
tants [142]. The degradation of these molecules is limited
by the accumulation of reactive intermediates epoxides.
The authors constructed a recombinant E. coli strain in
which a toluene ortho-monooxygenase from Burkholde-
ria cepacia G4, obtained by DNA shuffling, and a GST
from Rhodococcus AD45 with activity towards cis-1,2,-
dichloroethylene epoxide and epoxypropane, were
co-expressed [110]. The ability of GST to transform
epoxides in E. coli strain increased the mineralization of
cis-1,2,-dichloroethylene.
The examples provided above highlight the potential
biotechnological applications of using engineered
proteins and bacterial strains. In this respect, bacterial
GSTs, which are characterized by high stability and by
a wide variety of catalysed reactions, undoubtedly,
constitute an effective resource for the future.
Acknowledgements
This work was supported in part by grants from
the Ministero dell’Istruzione, dell’Universita
`e della
Ricerca (MIUR) of Italy.
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