Journal of Biotechnology 104 (2003) 99 /122
www.elsevier.com/locate/jbiotec
Acetate metabolism and its regulation in
Corynebacterium glutamicum
Robert Gerstmeir a, Volker F. Wendisch b, Stephanie Schnicke a, Hong Ruan a,
Mike Farwick c, Dieter Reinscheid a, Bernhard J. Eikmanns a,*
a
Department of Microbiology and Biotechnology, University of Ulm, 89069 Ulm, Germany
b
Institute of Biotechnology 1, Forschungszentrum Jülich, 52425 Jülich, Germany
c
Degussa., Feed Additives, R&D Biotechnology, 33790 Halle, Germany
Received 16 December 2002; received in revised form 27 February 2003; accepted 14 March 2003
Abstract
The amino acid producing Corynebacterium glutamicum grows aerobically on a variety of carbohydrates and organic
acids as single or combined sources of carbon and energy. Among the substrates metabolized are glucose and acetate
which both can also serve as substrates for amino acid production. Based on biochemical, genetic and regulatory studies
and on quantitative determination of metabolic fluxes during utilization of acetate and/or glucose, this review
summarizes the present knowledge on the different steps of the fundamental pathways of acetate utilization in C.
glutamicum , namely, on acetate transport, acetate activation, tricarboxylic acid (TCA) cycle, glyoxylate cycle and
gluconeogenesis. It becomes evident that, although the pathways of acetate utilization follow the same theme in many
bacteria, important biochemical, genetic and regulatory peculiarities exist in C. glutamicum . Recent genome wide and
comparative expression analyses in C. glutamicum cells grown on glucose and on acetate substantiated previously
identified transcriptional regulation of acetate activating enzymes and of glyoxylate cycle enzymes. Additionally, a
variety of genes obviously also under transcriptional control in response to the presence or absence of acetate in the
growth medium were uncovered. These genes, thus also belonging to the acetate stimulon of C. glutamicum , include
genes coding for TCA cycle enzymes (e.g. aconitase and succinate dehydrogenase), for gluconeogenesis (phosphoenolpyruvate carboxykinase), for glycolysis (pyruvate dehydrogenase E1) and genes coding for proteins with hitherto
unknown function. Although the basic mechanism of transcriptional regulation of the enzymes involved in acetate
metabolism is not yet understood, some recent findings led to a better understanding of the adaptation of C.
glutamicum to acetate at the molecular level.
# 2003 Elsevier B.V. All rights reserved.
Keywords: Corynebacterium glutamicum ; Acetate metabolism; Acetate activation; Glyoxylate cycle; Carbon flux regulation;
Expression profiling
* Corresponding author. Fax: /49-731-502-2719.
E-mail address: bernhard.eikmanns@biologie.uni-ulm.de (B.J. Eikmanns).
0168-1656/03/$ - see front matter # 2003 Elsevier B.V. All rights reserved.
doi:10.1016/S0168-1656(03)00167-6
100
R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
1. Introduction
In their natural environment, microorganisms
often encounter situations that change frequently
and rapidly with respect to e.g. temperature, pH,
oxygen concentration and nutrient availability. To
cope with these different situations, microorganisms have evolved a variety of coordinated and
adaptive mechanisms and regulatory circuits by
which they adjust their physiology to allow
optimal growth. This is especially true concerning
the availability of different carbon and energy
sources, which have to be converted into metabolites of the central metabolism and then serve as
fuel for energy conservation or as precursors for
the synthesis of new cell material.
Many microorganisms are able to use a variety
of different carbon and energy substrates and
adapt their enzymatic equipment and thus their
metabolism specifically to the availability of a
given substrate or substrate mixture. This adaptation often is mediated by substrate-specific induction or derepression of catabolic genes. When a
mixture of different carbon and energy sources is
present instead of a single substrate, many organisms utilize one carbon source preferentially and
consume the additional carbon source(s) only
when the preferred one is exhausted. As already
shown by Monod (1949), the preferred substrate in
general supports the best growth rate and/or
growth yield and the successive utilization of
substrates is often represented by a biphasic
growth behavior (diauxic growth). The basis of
this phenomenon is the so-called carbon catabolite
repression by which the expression of genes coding
for enzymes involved in catabolism of a subordinate substrate is repressed by the presence of a
catabolite generated from the preferred carbon
and energy source (for reviews on catabolite
repression, inducer exclusion and induction prevention in Gram-negative and -positive bacteria
and in yeast see Bruckner and Titgemeyer, 2002;
Stülke and Hillen, 2000; Saier, 1998; Gancedo,
1998; Paulsen, 1996). On the other hand, when
grown on specific substrate mixtures, some microorganisms are known to use two or more carbon
sources in parallel. In these cases no catabolite
repression occurs and a monophasic growth is
observed (reviewed by Harder and Dijkhuizen,
1982; Kovarova-Kovar and Egli, 1998).
Corynebacterium glutamicum is a Gram-positive
bacterium widely used in the industrial production
of amino acids such as L-glutamate and L-lysine
(Leuchtenberger, 1996). The organism is able to
use a variety of carbohydrates, alcohols and
organic acids as single sources of carbon and
energy for growth and also for amino acid
production (reviewed in Kinoshita and Tanaka,
1972; Liebl, 1991). By analysis of growth and
carbon consumption, it was shown that C. glutamicum co-metabolizes glucose with other sugars
and with organic acids such as lactate, pyruvate,
acetate and propionate and shows monophasic
growth on these substrate mixtures (Cocaign et al.,
1993; Dominguez et al., 1993; Wendisch et al.,
2000; Claes et al., 2002). Diauxic growth of C.
glutamicum and sequential utilization of carbon
sources was described so far only for the mixture
of glucose and glutamate (Krämer et al., 1990) and
is obviously due to induction of the gluABCD gene
cluster encoding the binding protein-dependent
glutamate uptake system in the presence of glutamate (Kronemeyer et al., 1995). However, so far
there is no direct evidence for a carbon catabolite
repression system in this organism. Thus, the
adaptation of the C. glutamicum metabolism to
the presence of various carbon sources is clearly
different from that in other well studied bacteria
such as Escherichia coli or Bacillus subtilis (for
reviews see above).
Independent of the carbon and energy source
used, one of the main and central pathways in C.
glutamicum and in other aerobic bacteria is the
tricarboxylic acid (TCA) cycle which is responsible
for the complete oxidation of acetyl-CoA derived
from the different substrates and for the provision
of precursors for amino acid biosynthesis (Fig. 1).
During growth, and especially under amino acid
production conditions, the TCA cycle has to be
replenished continuously in order to maintain the
acceptor molecule oxaloacetate at a sufficient level
and thus to keep the cycle running. For this
purpose, the organisms possess the so-called
anaplerotic reactions. During growth on carbohydrates, the replenishment of the TCA cycle is
accomplished by carboxylation of either phos-
R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
101
malate from two molecules of acetyl-CoA. Malate
is then oxidized by malate dehydrogenase or, as
shown for C. glutamicum , by the membraneassociated malate:chinone oxidoreductase (van
der Rest et al., 2000; Molenaar et al., 1998,
2000). Organisms growing on acetate, fatty acids
or ethanol as sole carbon and energy source
additionally require gluconeogenesis to provide
the cells with sugar phosphates from intermediates
of the TCA cycle.
This review focuses on various aspects of acetate
metabolism of C. glutamicum . It will summarize
the present knowledge on the activity and regulation of the enzymes involved, the expression and
regulation of the respective genes, the carbon
fluxes within the central metabolic pathways and
some recent findings on expression profiling of
acetate-grown cells in order to understand the
acetate stimulon of this industrially important
organism.
Fig. 1. Diagram of the central metabolism of C. glutamicum
during growth on glucose and acetate. Dotted arrows represent
pathways consisting of several reactions, uninterrupted arrows
represent single reactions. AK, acetate kinase; PTA, phosphotransacetylase; ICD, isocitrate dehydrogenase; ICL, isocitrate
lyase; MS, malate synthase; PEPCk, phosphoenolpyruvate
carboxykinase; PCx, pyruvate carboxylase; PEPCx, phosphoenolpyruvate carboxylase.
phoenolpyruvate (PEP) or pyruvate to yield oxaloacetate. PEP and pyruvate are derived from
glycolysis. In C. glutamicum , both PEP carboxylase and pyruvate carboxylase have been shown
to be present although it is the latter enzyme that is
mainly responsible for the anaplerotic function
during growth on and amino acid production from
glucose (Peters-Wendisch et al., 1997, 1998, 2001).
During growth on substrates entering the central
metabolism at the level of acetyl-CoA, e.g. acetate,
fatty acids or ethanol, the glyoxylate cycle with its
key enzymes isocitrate lyase (ICL) and malate
synthase (MS) functions to provide oxaloacetate
and thus fulfils the anaplerotic function (Fig. 1).
This bypass of the TCA cycle avoids the oxidative
decarboxylation steps of isocitrate dehydrogenase
(ICD) and 2-oxoglutarate dehydrogenase and
finally leads to the formation of one molecule of
2. Growth on acetate and other short and long chain
fatty acids
The growth of C. glutamicum on acetate,
glucose plus acetate and glucose alone has been
comparatively studied by Wendisch et al. (2000)
and the growth rates, the biomass yields and the
specific substrate and carbon consumption rates
are summarized in Table 1. The growth rate and
the biomass yield on acetate are lower than on
glucose or acetate/glucose mixtures indicating an
increased energy metabolism. In case of the
experiment with both substrates, the carbon consumption rate resulted from the simultaneous
consumption of acetate and glucose. The overall
carbon consumption rate under the three conditions tested is similar which reflects the fact that
during growth on the acetate /glucose mixture the
consumption rate for each of the two carbon
sources is reduced to 50% of the rate observed
during growth on either acetate or glucose alone
[from 148 to 72 and from 540 to 270 nmol (mg
protein) 1 min 1 for glucose and acetate, respectively]. This result indicates that either the uptake
of the two substrates or the pathways leading from
glucose to acetyl-CoA or from acetate to acetyl-
102
a
The CGC minimal medium used was described by Eikmanns et al. (1991); the concentrations of the carbon and energy sources were 120 mM acetate, 120 mM
acetate/55 mM glucose, 110 mM glucose, 22 mM palmitate, 22 mM palmitate/55 mM glucose, 100 mM propionate and 100 mM propionate/55 mM glucose,
respectively.
b
n.d., not determined.
0.31
0.40
n.d.b
n.d.b
0.07
0.17
157
470
0.27
0.43
n.d.b
n.d.b
0.02
0.18
8
124
0.38
0.41
148
888
0.36
0.41
270/72
972
0.28
0.29
540
1080
Growth rate (h 1)
Biomass yield (g C in dry wt (g C in substrate) 1)
Substrate consumption rate (nmol (mg protein) 1 min 1)
Carbon consumption rate (nmol C (mg protein) 1 min1)
Acetate Acetate /glucose Glucose Palmitate Palmitate/glucose Propionate Propionate/glucose
Growth on minimal medium containing
Growth parameter
Table 1
Growth characteristics of C. glutamicum grown in minimal medium containing different carbon and energy sourcesa
R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
CoA are directly or indirectly regulated by the
carbon source. In contrast to C. glutamicum , E.
coli and also B. subtilis do not co-utilize glucose
and acetate but instead preferentially use glucose
(Brown et al., 1977; Grundy et al., 1994).
It should be noted here that the concentration of
acetate in the growth medium affects the growth of
C. glutamicum . At initial concentrations higher
than 180 mM, a concentration dependent lag
phase (4 h at 200 mM /2 days at 400 mM) was
observed and the growth rate decreased significantly (Wendisch et al., 2000). This effect might be
due to a detrimental effect of acetate functioning
as an uncoupler of the transmembrane pH gradient (Baronofsky et al., 1984) or, as shown recently
for E. coli , to the interference of acetate with
methionine biosynthesis (Roe et al., 2002).
Recently, we studied the growth of C. glutamicum on short and long chain fatty acids which
enter the central metabolism at the level of acetylCoA. We tested growth of C. glutamicum on C4,
C5, C6, C8, C10, C11, C12, C13, C14, C16, C18
and C20 fatty acids as sole carbon and energy
source, however, growth was only observed with
palmitate (C16). The growth on minimal medium
containing 0.2 /0.5% (w/v) palmitate started after a
lag phase of 2 /3 days, the biomass yield and
especially the growth rate were much lower than
during growth on any other substrate tested (Table
1). A relatively long lag period was also observed
for enterobacteria growing on long chain fatty
acids, however, in E. coli growth on these substrates seems to be energetically more favorable
than growth on acetate (Clark and Cronan, 1996).
As a co-substrate in addition to glucose, palmitate
had a negative effect on the growth rate but not on
the biomass yield of C. glutamicum .
C. glutamicum is also able to use propionate as
sole carbon and energy source. Claes et al. (2002)
recently identified in C. glutamicum a gene cluster
(prpD2B2C2 ) encoding enzymes involved in propionate degradation and found strong evidence for
the operation of the 2-methylcitrate cycle. By this
cycle, propionate is oxidized to pyruvate which
then can be further converted to acetyl-CoA or to
oxaloacetate (Textor et al., 1997). The growth
characteristics of C. glutamicum growing on propionate and on a mixture of propionate and
R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
glucose as carbon and energy sources are listed in
Table 1. It became evident that the additional
presence of propionate in glucose minimal medium
led to a decreased growth rate. A growth-inhibitory effect of propionate has been reported previously for a variety of microorganisms (e.g.
Cherrington et al., 1991; Rehberger and Glatz,
1998; Pronk et al., 1994).
3. Acetate uptake and activation
Growth on, and amino acid production from
acetate firstly requires its uptake and subsequent
activation to acetyl-CoA. It has been assumed that
acetate uptake in bacteria occurs predominantly
by unspecific diffusion of the undissociated acid
across the cytoplasmic membrane (Kell et al.,
1981; Baronofsky et al., 1984). However, Ebbighausen et al. (1991) could clearly show that acetate
uptake in C. glutamicum is catalyzed by a specific
secondary carrier according to an acetate/proton
symport mechanism and that there is no significant contribution by a passive diffusion process.
The carrier is dependent on the membrane potential and is highly specific. Aside from acetate only
propionate is accepted as a substrate for transport
while a variety of other monocarboxylates are not.
Such a specificity for acetate and propionate was
also found for uptake systems in enterobacteria
(Kay, 1978) and allows the growth of the respective bacteria on these substrates. However, the
maximal activity of 35 nmol acetate (mg dry
weight)1 min 1 [corresponding to about 70
nmol (mg protein) 1 min 1], measured in the
mid exponential growth phase of C. glutamicum
cells growing on glucose, is much lower than the
acetate consumption rate measured during growth
on acetate (see above). Therefore, it can be
speculated that the expression of the acetate
carrier gene is increased in acetate-grown and
also in propionate-grown cells, as are other genes
involved in acetate metabolism (see below) and
propionate degradation (Claes et al., 2002), respectively. However, a gene encoding an acetate/
propionate uptake carrier so far has not been
identified within the genome of C. glutamicum
(Burkowski and Krämer, personal communica-
103
tion) and further studies are necessary to clarify
the regulation of acetate and propionate uptake at
the genetic level.
Acetate activation to acetyl-CoA in C. glutamicum is accomplished by the combined activities of
acetate kinase (AK) and phosphotransacetylase
(PTA) (Shiio et al., 1969) (Fig. 1). AK activates
acetate in an ATP-dependent reaction to acetyl
phosphate which subsequently is converted to
acetyl-CoA by PTA. Recently, both enzymes
from C. glutamicum and their regulation were
intensively studied and also mutants defective in
either or both of the enzymes were constructed and
analyzed (Wendisch et al., 1997; Reinscheid et al.,
1999). The apparent Km values of AK were found
to be 7.9 mM for acetate and 0.23 mM for ATP
which roughly is in the same range as determined
for AK enzymes from other bacteria utilizing
acetate for growth (Fox and Roseman, 1986).
The apparent Km values of PTA were 0.13 mM
for acetyl phosphate and 0.4 mM for CoA and
thus slightly lower and higher, respectively, than
those of PTA enzymes from other bacteria (Shimizu et al., 1969; Rado and Hoch, 1973). As in the
case of the acetate carrier, the C. glutamicum AK
also accepts propionate aside from acetate as a
substrate, although with a lower affinity (Km /15
mM) and an about 25% lower Vmax (Reinscheid et
al., 1999). Together with the results that the PTA
accepts propionyl-CoA as a substrate in the
reverse reaction and that mutants defective in
either AK or PTA are not able to grow on
propionate (Rittmann and Wendisch, unpublished) it is evident that AK and PTA are not
only responsible for acetate but also for propionate activation in C. glutamicum . That propionate
activation might occur via AK and PTA was
already suggested by Claes et al. (2002) due to
the apparent lack of an homologue of the propionyl-CoA synthetase gene (prpE ) in C. glutamicum .
Isolation and analysis of the AK and PTA genes
(ack and pta , respectively; Table 2) revealed that
the two genes form an operon with pta upstream
of ack (Fig. 2A) and a single basepair overlap of
the pta stop codon with the first nucleotide of the
ack start codon (Reinscheid et al., 1999). Recent
primer extension experiments identified two transcriptional start sites 46 and 160 bp upstream of
104
66 874
610
80 091
739
As deduced from the respective nucleotide sequence.
Monocistronic
AJ269506
a
pck
Yes
Isocitrate dehydrogenase
PEP carboxykinase
Monocistronic
X71489
icd
No
82 262
739
Malate synthase
Monocistronic
X78491
aceB
Yes
47 228
432
Isocitrate lyase
Monocistronic
X75504
aceA
Yes
Bicistronic with ack
X89084
pta
Yes
Phosphotransacetylase
329
35 242
Reinscheid et al.
(1999)
Reinscheid et al.
(1999)
Reinscheid et al.
(1994a)
Reinscheid et al.
(1994b)
Eikmanns et al.
(1995)
Riedel et al. (2001)
43 098
397
Acetate kinase
Yes
Bicistronic with pta
X89084
Transcriptional organization
ack
Name
Name Accessionnumber
Transcriptional regulation in response to acetate
Protein
Gene
Table 2
Genes and proteins involved in acetate metabolism of C. glutamicum and some of their characteristics
Amino acids per
monomera
Mr of monomera
Reference
R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
the initiation codon of the pta gene (Fig. 2B;
unpublished). Centered 12 and 14 bp upstream of
the /35 regions we found a completely conserved
13-bp repeat with an internal dyad symmetry (Fig.
2B), possibly involved in induction or repression
of the operon. Further studies by Reinscheid et al.
(1999) showed that the expression of the pta /ack
operon is regulated at the transcriptional level,
resulting in high and low specific activities of both
enzymes in the presence and absence, respectively,
of acetate in the growth medium (Table 3). This is
in sharp contrast to the situation in enterobacteria,
in which the level of AK and PTA activities varies
only little in dependence on the carbon source and
expression of the ack and pta genes (i.e. the ack /
pta operon) is neither induced by acetate nor
repressed by glucose (Brown et al., 1977; Nyström,
1994; Clark and Cronan, 1996). In fact, Oh et al.
(2002) recently even observed an about 2-fold
reduced RNA level of the ack /pta operon in
acetate-grown cells of E. coli compared with
glucose-grown cells. According to all these findings, the AK/PTA pathway in enterobacteria is
suggested to operate in both directions and to be
functioning not only during growth on acetate but
also during anaerobic growth on carbohydrates
when acetate is excreted. Under the latter condition acetyl-CoA is converted via acetyl phosphate
to acetate with concomitant energy conservation
by substrate level phosphorylation (Thauer et al.,
1977). Additionally, cells of E. coli contain an
acetate-inducible acetyl-CoA synthetase which indicates that this enzyme might be mainly responsible for acetate activation during growth on this
substrate (Brown et al., 1977; Kumari et al., 2000;
Oh et al., 2002). In B. subtilis , the ack and pta
genes are under transcriptional control of the
catabolite control regulator protein CcpA
(Grundy et al., 1993a; Presecan-Siedel et al.,
1999; Shin et al., 1999), however, in contrast to
the situation in C. glutamicum , both genes are
induced in the presence of an excess of glucose.
This result and the analysis of mutants defective in
AK suggested that AK and PTA in B. subtilis are
not required for utilization of acetate but for its
formation when the cells are growing on glucose
(Grundy et al., 1993a). Accordingly, B. subtilis
also possesses an acetyl-CoA synthetase which has
105
R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
Fig. 2. Genomic locus of the C. glutamicum pta /ack operon and its flanking region (A) and nucleotide sequence of its promoter
region (B). The thick arrows represent the coding regions. The transcriptional start sites are underlined and indicated as TS1 pta and
TS2 pta . The respective /10 and /35 regions are underlined and putative regulatory sites are boxed. fprA and pknG represent genes
showing similarity to genes encoding ferredoxin NADP reductase and protein kinase G, respectively, from M. tuberculosis .
Table 3
Specific activities of enzymes involved in acetate metabolism of C. glutamicum cells grown in minimal media (MM)a containing 200
mM acetate, 100 mM acetate plus 55 mM glucose, 110 mM glucose, 22 mM palmitate and 22 mM palmitate plus 55 mM glucose. AK,
acetate kinase; PTA, phosphotransacetylase; ICL, isocitrate lyase; MS, malate synthase; PCK, phosphoenolpyruvate carboxykinase;
ICD, isocitrate dehydrogenase
Medium
MM/acetate
MM/acetate/glucose
MM/glucose
MM/palmitate
MM/palmitate/glucose
a
b
Specific activity (U (mg protein)1) of
AK
PTA
ICL
MS
PCK
ICD
0.81
0.43
0.21
0.17
0.11
2.95
1.87
0.66
0.36
0.21
2.07
1.40
0.02
0.97
0.61
1.77
1.19
0.04
1.39
1.03
0.08
0.05
0.04
n.d.b
n.d.b
1.10
1.05
1.07
0.85
0.91
The CGC minimal medium used was described by Eikmanns et al. (1991).
n.d., not determined.
106
R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
been shown to be essential for growth on acetate
and which is repressed in the presence of glucose in
the growth medium (Grundy et al., 1993b, 1994).
As shown by gene inactivation studies in C.
glutamicum , both the ack and the pta genes are
essential for growth on acetate but not on glucose
as the sole carbon source indicating that a functional AK/PTA pathway is necessary for growth of
this organism on acetate (Reinscheid et al., 1999).
So far, neither an acetyl-CoA synthetase activity
has been detected in C. glutamicum (Ozaki and
Shiio, 1968; Ebbighausen et al., 1991; Reinscheid
et al., 1999) nor a corresponding gene homologue
was found within the genome sequence (Acc.-No.
NC_003450). However, although defined ack and
pta mutants were not able to grow on acetate as
sole carbon and energy source, they are able to cometabolize acetate in the presence of glucose
(unpublished results). Thus, an alternative route
for acetate activation in C. glutamicum , possibly
via an hitherto unknown CoA transferase reaction
awaits investigations. In this context it is noteworthy to mention that the C. glutamicum genome
contains two genes annotated as acetyl-CoA
hydrolases (NP_601784 and NP_601767). One of
these genes shows similarity to the Clostridium
kluyveri cat1 gene which encodes a succinylCoA:CoA transferase. In C. kluyveri , this enzyme
catalyzes the reversible transfer of the CoA moiety
from acetyl-CoA to succinate and is involved in
the anaerobic succinate degradation (Söhling and
Gottschalk, 1996). Thus, it might be that C.
glutamicum is able to form acetyl-CoA from the
TCA cycle intermediate succinyl-CoA. However,
gene inactivation studies and analysis of respective
mutants have to be performed to unravel the
alternative route of acetate activation.
4. The glyoxylate cycle
When acetate or a carbon source entering the
metabolism at the level of acetyl-CoA is the only
carbon and energy source for an organism, catabolism occurs via the TCA cycle which does not
allow any net assimilation of carbon. To supply
the cell with C4 and C3 intermediates for the
biosynthesis of cell material, growth on these
substrates, therefore, requires the operation of
the glyoxylate cycle as anaplerotic pathway (Kornberg, 1966a; Fig. 1). This cycle consists of five of
the eight reactions of the TCA cycle and bypasses
the two decarboxylation steps by the additional
reactions of ICL and MS. Thus, a part of the TCA
cycle carbon flux is diverted at isocitrate (Kornberg, 1966a,b). ICL catalyzes the cleavage of
isocitrate to succinate and glyoxylate, and MS
condenses glyoxylate with acetyl-CoA to give
malate (for reviews on these enzymes see Clark
and Cronan, 1996; Cronan and LaPorte, 1996;
Cortay et al., 1989). Each turn of the glyoxylate
cycle results in the net formation of one molecule
of malate from two molecules of acetyl-CoA.
Malate is converted to oxaloacetate which then
can further be used either as precursor for amino
acids derived from TCA cycle intermediates (the
members of the aspartate and the glutamate family
of amino acids) or for gluconeogenesis. It has been
generally assumed that whenever more easily
metabolizable carbon sources than acetate or fatty
acids (e.g. glucose or other sugars) become available, the ICL and MS genes are repressed via
catabolite repression and thus, the glyoxylate
bypass is turned off (Cozzone, 1998; Clark and
Cronan, 1996).
In accordance with the ability of C. glutamicum
to grow on acetate and other substrates entering at
the level of acetyl-CoA, ICL and MS activities
have been found (Ozaki and Shiio, 1968; Shiio et
al., 1969) and, due to the key position in the
central metabolism, the enzymes as well as the
corresponding genes were subjects of intensive
investigations. Both enzymes of C. glutamicum
were purified and biochemically characterized and
it turned out that especially ICL is controlled by
allosteric regulation by a variety of intermediates
of the central metabolism (Reinscheid et al.,
1994a,b). ICL showed a moderate affinity for its
substrate isocitrate (Km /0.28 mM) and was
effectively inhibited by 3-phosphoglycerate, 6phosphogluconate, PEP, fructose-1,6-bisphosphate and succinate. The inhibition constants of
these metabolites were determined to be between
0.46 and 1.48 mM, which is in the range of the
intracellular concentrations of these metabolites in
bacterial cells (LaPorte and Koshland, 1982;
R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
Petersen et al., 2001; Buchholz et al., 2001) and
thus of physiological significance. MS showed high
affinities of 30 and 12 mM for the substrates
glyoxylate and acetyl-CoA, respectively, and was
found to be inhibited by oxalate, glycolate and
ATP, but not by any of the intermediates of the
glycolysis or the TCA cycle. However, since
oxalate and glycolate are probably not of importance within the central metabolism of C. glutamicum and the inhibition constant for ATP was
relatively high (4.3 mM), we assume that the
inhibition or activation of the MS plays only a
minor role in controlling the carbon flow in the
glyoxylate cycle.
The biochemical characterization of the corynebacterial MS and also the analysis of the MS gene
(see below) revealed that the enzyme from C.
glutamicum differs significantly both in size and
primary structure from MS enzymes used by other
organisms as glyoxylate cycle enzyme (Reinscheid
et al., 1994b). It turned out that the C. glutamicum
enzyme corresponds to an alternative MS of E.
coli , designated MS G, which is involved in
glycolate and glyoxylate utilization and accordingly, is strongly induced by glycolate but not by
acetate in the growth medium (Molina et al.,
1994). However, C. glutamicum is not able to
grow on glycolate or glyoxylate as sole carbon
sources (unpublished results) and it remains unclear why C. glutamicum has adopted a homologue of MS G for its glyoxylate cycle.
The C. glutamicum ICL and MS genes (aceA
and aceB , respectively; Table 2) have been isolated, their structure and genomic organization,
their expression and regulation were intensively
analyzed and, by gene inactivation studies, they
were shown to be essential for growth on acetate
as the sole carbon source (Reinscheid et al.,
1994a,b; Wendisch et al., 1997). The two genes
are clustered on the chromosome, separated by
597 bp and transcribed in divergent directions
(Fig. 3A). According to the C. glutamicum genome
map (Tauch et al., 2002), the aceA /aceB cluster is
not in the vicinity of the pta /ack operon. While
the deduced gene product of aceA shows significant identity (up to 79%) to ICL enzymes from
other organisms, the predicted aceB gene product
showed only weak similarity to all MS polypep-
107
tides known at that time. In the meantime, it
became evident that the C. glutamicum aceB gene
product is 54% identical to the MS G of E. coli
(Molina et al., 1994; see above) and 60% identical
to the MS of the closely related Mycobacterium
tuberculosis (Smith et al., 2003). In the intergenic
region between aceA and aceB , one transcriptional start site 112 bp upstream of the aceA gene
and two transcriptional start sites 466 and 468 bp
upstream of the aceB gene were recently identified
by primer extension experiments (Fig. 3B; unpublished). Thus, the /10 regions of the divergent
aceA and aceB promoters overlap. About 55 bp
upstream of the /35 region of the aceA gene and
about 72 bp downstream of the aceB transcriptional start, a motif was found (Fig. 3B) which is
identical in all but one bp with the motif observed
in front of the /35 regions of the pta /ack operon
(see above). This finding might indicate a common
regulator for the pta /ack operon and the aceA
and/or aceB gene. Further transcriptional studies
(Wendisch et al., 1997) showed that the expression
of aceA and aceB is regulated at the transcriptional level, resulting in quite different specific
activities of ICL and MS in the presence and
absence of acetate in the growth medium (Table 3).
The induction of the aceA and aceB genes (and
also that of the pta /ack operon) in the presence of
acetate occurs independent of the presence or
absence of an additional carbon and energy
source. This is in contrast to what has been
observed in E. coli and other organisms. In these
organisms, ICL and MS are only formed when
acetate or fatty acids are the sole carbon sources
and not formed on any other carbon source,
irrespective of the presence or absence of acetate
as a co-substrate (Kornberg, 1966b; Hillier and
Charnetzky, 1981; Blasco et al., 1991). In enterobacteria, the ICL and MS genes are organized as
an operon together with the aceK gene encoding
the ICD kinase/phosphatase (LaPorte et al., 1985;
Chung et al., 1988). The expression of the E. coli
aceB /aceA /aceK operon is positively controlled
by the pleiotropic transcriptional regulator FruR
(identical to Cra) and by the integration host
factor (IHF) and negatively controlled by the
IclR repressor which itself is under positive control
of the fatty acid degradation and synthesis reg-
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R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
Fig. 3. Genomic locus of the C. glutamicum aceA and aceB genes and the flanking region (A) and nucleotide sequence of the aceA /
aceB -intergenic promoter region (B). The thick arrows represent the coding regions. The transcriptional start sites are underlined and
indicated as TS aceA , TS1 aceB and TS2 aceB . The /10 and /35 regions of the aceA promoter are overlined, those of the aceB
promoter underlined and putative regulatory sites are boxed. thiX represents a gene which is necessary for thiamin biosynthesis
(Reinscheid et al., 1994a), orfY a hitherto unidentified gene.
ulator FadR (reviewed in Cozzone, 1998). Up to
now there is no evidence for the presence of
functional homologues of FruR, IHF or IclR in
C. glutamicum . In conclusion, all the data show
R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
remarkable differences in the regulation of the
aceA and aceB genes in C. glutamicum and other
organisms.
5. Gluconeogenesis
Growth on acetate and other carbon sources
entering the central metabolism at the level of
acetyl-CoA requires gluconeogenesis for providing
the cells with 3-phosphoglycerate and with hexose
and pentose sugars. The initial step in the gluconeogenic pathway is the conversion of a TCA cycle
intermediate to PEP. In most organisms, this
reaction is accomplished by a PEP carboxykinase
which catalyzes the decarboxylation and simultaneous ATP- or GTP-dependent phosphorylation
of oxaloacetate (Utter and Kolenbrander, 1972).
In some organisms, oxaloacetate or malate are
decarboxylated to pyruvate by oxaloacetate decarboxylase or malic enzyme, respectively (Hansen
and June, 1974) and in a second reaction, the
pyruvate formed is converted to PEP by PEP
synthetase or pyruvate:orthophosphate dikinase
(Cooper and Kornberg, 1967). PEP then is further
converted up to glucose-6-phosphate via reactions
of glycolysis. The irreversible step of glycolysis
leading from glucose-6-phosphate to PEP, i.e. the
phosphofructokinase reaction, is bypassed by
fructose-1,6-bisphosphatase.
C. glutamicum possesses PEP carboxykinase,
oxaloacetate decarboxylase and malic enzyme and
all three enzymes have been (partially) purified
and biochemically characterized (Jetten and Sinskey, 1993, 1995; Peters-Wendisch et al., 1993;
Gourdon et al., 2000). In contrast to all other
bacterial PEP carboxykinases studied so far, the C.
glutamicum enzyme shows a high specificity for
GTP and ITP instead of ATP, and is even
effectively inhibited by ATP (Jetten and Sinskey,
1993). The gluconeogenic function of PEP carboxykinase in C. glutamicum was shown by inactivation experiments. In contrast to the wild type
strain, a defined PEP carboxykinase-deficient
mutant was unable to grow on substrates which
require gluconeogenesis (Riedel et al., 2001). The
inability of this mutant to grow on acetate and
lactate additionally indicates that PEP carboxyki-
109
nase is the only enzyme responsible for PEP
synthesis and that it cannot be functionally
replaced by the combined activities of malic
enzyme or oxaloacetate decarboxylase and PEP
synthetase. Whereas the malic enzyme of C.
glutamicum has recently been proposed to be
involved in the generation of NADPH on substrates known to have a low flux through the
pentose pathway (Gourdon et al., 2000), the role
of oxaloacetate decarboxylase in C. glutamicum is
completely unclear and remains to be investigated.
According to the GTP-specificity of the C.
glutamicum PEP carboxykinase, the analysis of
the respective gene (pck ; Table 2) revealed, that the
deduced polypeptide showed no similarity to
known ATP-dependent but significant identity to
GTP-dependent eukaryotic PEP carboxykinases
(Riedel et al., 2001). The gene is monocistronic
and, according to the genome sequence (Acc.-No.
NC_003450), not linked to any other gene known
to be involved in acetate metabolism. The expression of the pck gene is weakly regulated by the
carbon source in the growth medium resulting in
about 2-fold higher specific activities of PEP
carboxykinase in cells grown on acetate (Table 3)
and about 3-fold higher activities in cells grown on
lactate when compared with cells grown in minimal medium containing glucose. Whereas the
regulation of pck expression in C. glutamicum
with respect to the carbon source is similar to that
in other bacteria, a growth phase dependent
regulation of pck , as observed in E. coli , Rhodopseudomans palustris and Rhizobium meliloti
(Goldie, 1984; Inui et al., 1999; Osteras et al.,
1995), seems very unlikely for C. glutamicum since
the specific PEP carboxykinase activities were
nearly identical throughout all stages of growth
(Riedel et al., 2001).
It is noteworthy to point out that there is
considerable PEP carboxykinase activity also present in cells grown in glucose minimal medium
(Table 3). This finding is in agreement with
observations made during labeling experiments
using 13C /glucose and subsequent nuclear magnetic resonance (NMR) analyses. Here a relatively
strong (backwards) flux from oxaloacetate/malate
to PEP/pyruvate was found to take place during
growth on and amino acid production from
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R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
glucose in addition to the carboxylating (forward)
flux from PEP/pyruvate to oxaloacetate/malate
(Sonntag et al., 1995; Marx et al., 1999; Wendisch
et al., 2000). Petersen et al. (2000, 2001) then
showed that the backwards flux is nearly completely due to oxaloacetate decarboxylation by PEP
carboxykinase. Thus, PEP carboxykinase, aside
from its function in gluconeogenesis, may have
physiological significance under glycolytic conditions as well.
The fructose-1,6-bisphosphatase of C. glutamicum has not yet been studied so far. Due to
sequence comparison, five genes have been annotated as putative or possible fructose-1,6-bisphosphatase genes within the genome sequence (Acc.No. NC_003450). However, further studies are
necessary to identify the functional gene(s) for this
gluconeogenic enzyme.
It is noteworthy that the genome sequence of C.
glutamicum contains in addition to the previously
characterized glyceraldehyde-3-phosphate dehydrogenase gene (Eikmanns, 1992; Schwinde et
al., 1993) a further gene (Acc.-No. AX121128)
most probably coding for a glyceraldehyde-3phosphate dehydrogenase isoenzyme. Since this
gene (designated gapB ) seems to be up-regulated
during growth of C. glutamicum on acetate (see
below), Hayashi et al. (2002) speculated the gapB
gene product to be involved in gluconeogenesis.
However, gene inactivation studies and validation
of the expression data on the level of enzyme
activity are necessary to confirm this hypothesis.
6. Metabolic fluxes during growth on acetate and/or
glucose
The regulation of the enzymes involved in
acetate metabolism of C. glutamicum suggested
significant differences of the carbon flux within the
central metabolism of this organism when acetate
instead of glucose is the sole carbon source. By
13
C-labeling experiments with subsequent NMR
analyses in combination with metabolite balancing, the in vivo activities for pathways or single
enzymes in the central metabolism of C. glutamicum were quantified for growth on acetate,
glucose and both carbon sources together (Wen-
disch et al., 2000). As shown in Table 4, the
metabolization of acetate is characterized by a
relatively high in vivo activity of the TCA cycle, a
high in vivo activity of the glyoxylate cycle as
anaplerotic sequence, and a high rate of PEP/
pyruvate formation from oxaloacetate/malate and
gluconeogenesis (as indicated by high backward
fluxes of PEP/pyruvate carboxylation and glycolysis). C. glutamicum cells grown on glucose show
a low activity of the TCA cycle (about 25% relative
to acetate-grown cells), the complete absence of
glyoxylate cycle activity, a high glycolytic flux and,
as expected, anaplerosis by carboxylation of PEP
or pyruvate. The higher TCA cycle activity in
acetate-grown cells (as compared with glucosegrown cells) at least partly compensates for the
lower amount of energy, which becomes available
per mol of acetate. The difference in the TCA cycle
activity between acetate- and glucose-grown cells
is probably brought about by (slight) induction of
several of the genes encoding TCA cycle enzymes
(citrate synthase, aconitase, fumarase and succinate dehydrogenase; gltA , acn , fum and sdhABCD
genes, respectively) in acetate-grown cells (see
below, Table 5) and by activity control of the
citrate synthase. This enzyme is inhibited by ATP
and cis- aconitate (Eikmanns et al., 1994). Additionally, the availability of the substrate acetylCoA may control the in vivo activities of citrate
synthase, as its substrate constant for acetyl-CoA
(51 mM; Eikmanns et al., 1994) is higher than the
intracellular concentration of acetyl CoA during
growth on glucose but lower than that during
growth on acetate (24 and 145 mM, respectively,
Wendisch et al., 1997).
In cells grown on glucose plus acetate, the
central metabolism of C. glutamicum is characterized by an about 2-fold reduction of the consumption of both carbon sources compared with growth
on either carbon source alone, an intermediate
activity of the TCA cycle and a relatively low rate
of glycolysis and acetyl-CoA formation by pyruvate dehydrogenase. Surprisingly, and in contrast
to what has been found in E. coli for growth on
glucose plus acetate (Walsh and Koshland, 1985),
the glyoxylate cycle of C. glutamicum completely
fulfills the anaplerotic function under these conditions. The glyoxylate cycle does not only replenish
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R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
Table 4
In vivo activities (metabolic fluxes) of selected pathways/reactions in the central metabolism of C. glutamicum during growth in
minimal medium containing different carbon sourcesa
Pathway/reaction
Acetate uptake
Glucose uptake
TCA cycle (citrate synthase)
TCA cycle (isocitrate dehydrogenase)
Glyoxylate cycle
Glycolysis (glyceraldehyde-3-phosphate to PEP)
Pyruvate dehydrogenase reaction
PEP/pyruvate carboxylation
Net carbon flux (mU (mg protein)1)b during growth on
Acetate
Glucose
Glucose/acetate
540
/
413
314
99
/42
0
/72
/
148
111
111
0
227
161
30
270
72
219
169
50
57
33
/15
a
The CGC minimal medium used was described by Eikmanns et al. (1991); the concentrations of the carbon and energy sources
were 120 mM acetate, 110 mM glucose and 120 mM acetate/55 mM glucose, respectively.
b
Negative values represent backward fluxes.
the TCA cycle for intermediates withdrawn for 2oxoglutarate- and oxaloacetate-derived biosyntheses, but additionally provides malate/oxaloacetate for the formation of PEP/pyruvate (as indicated by the backward flux of PEP/pyruvate
carboxylation). The difference between the carbon
flux into the glyoxylate cycle in E. coli and C.
glutamicum cannot be accounted for by the substrate affinities of the enzymes involved [i.e. ICL,
MS, and ICD] since these are comparable (Walsh
and Koshland, 1984; Reinscheid et al., 1994a,b;
Eikmanns et al., 1995). Instead, the differences are
most probably due to different regulatory control.
As mentioned above, the E. coli ICL and MS
genes are transcriptionally linked to the isocitrate
dehydrogenase kinase/phosphatase (ICD-KP)
gene and this aceB /aceA /ack operon is repressed
in the presence of glucose and derepressed during
growth on acetate (Clark and Cronan, 1996;
Cozzone, 1998). The ICD-KP controls the phosphorylation status of ICD (Garnak and Reeves,
1979; LaPorte and Koshland, 1982, reviewed in
Cozzone, 1998). During growth of E. coli on
acetate there are high levels of ICL and MS, and
ICD is predominantly in its phosphorylated,
inactive form. During growth on glucose /acetate
mixtures, much lower ICL and MS levels are
present and ICD is mostly in its active, unphosphorylated form. In C. glutamicum , however,
there is no evidence for a similar phosphorylation
control of ICD (Eikmanns et al., 1995) and, in
contrast to the situation in E. coli, transcription of
the ICL and MS genes is increased in the presence
of acetate regardless of the presence or absence of
glucose (see above). The relative metabolization of
isocitrate by ICD and ICL (about 75% vs. 25%
during growth of C. glutamicum in the presence of
acetate) is consistent with their KM values of 12
and 280 mM, respectively, and with allosteric
regulation by glyoxylate and oxaloacetate (Reinscheid et al., 1994a; Eikmanns et al., 1995).
7. Global expression profiling of acetate-grown
cells
The genome sequence of C. glutamicum has
been independently determined at least three times
by different companies and recently became available for the public (Acc.-No. NC_003450). This
made it possible to analyze the proteome and the
transcriptome of C. glutamicum cells in a systematic way and thus, to study expression patterns
under certain conditions. By a combination of
two-dimensional (2-D) gel electrophoresis (O’Farrell, 1975) and protein identification via microsequencing or mass spectrometry, proteome
analysis of C. glutamicum has been established
(Hermann et al., 2001) and a high-resolution
reference map for cytoplasmic and membrane-
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R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
Table 5
The -fold changes of gene expression in acetate- and in acetate/glucose-grown cells of C. glutamicum compared with glucose grown
cells
Accession number
Gene (protein)
Ratio Ac/
Glca
Ratio Mix/
Glca
X75504
X78491
X89084
X89084
AX122555
AX121783
AX121209
AX120498
AX120497
AX120496
X66112
AJ269506
AX121528
AX123545
AX121827
AX121826
AX121824
AX123567
AX122546
AX122209
AX123412
AX121169
X59404
AX121284
AX122267
AX122266
aceA (isocitrate lyase)
aceB (malate synthase)
pta (phosphotransacetylase)
ack (acetate kinase)
acp (acyl-carrier protein)
acn (aconitase)
fum (fumarase)
sdhB succinate dehydrogenase B
sdhA succinate dehydrogenase A
sdhCD succinate dehydrogenase C and D
gltA (citrate synthase)
pck (phosphoenolpyruvate carboxykinase)
malP (similarity to maltodextrin phosphorylase, E. coli )
ptsM (glucose-phosphotransferase-system enzyme II [glucose-permease])
zwf2 (glucose-6-phosphate-dehydrogenase)
tal (transaldolase)
tkt (transketolase)
pyk (pyruvate kinase)
aceE (pyruvat-dehydrogenase component E1)
fruA (fructose-specific phosphotransferase system II BC)
malE (malic enzyme)
eno (enolase)
gdh (glutamate dehydrogenase)
gluA (strong similarity to glutamate transport ATP-binding protein)
oppC (strong similarity to oligopeptide ABC transporter [permease] */B. subtilis )
oppB (strong similarity to oligopeptide transport system permease protein */B.
subtilis )
oppA (similarity to oligopeptide-binding protein-E. coli )
Strong similarity to fatty-acid synthase-Brevibacterium ammoniagenes
28.6
8.4
6.2
3.1
2.3
3.7
1.9
2.1
2.1
2.1
2.0
3.8
/4.2
/2.3
/2.0
/1.8
/2.0
/2.0
/3.1
/2.4
/2.8
/1.6
/2.7
/2.4
/2.2
/2.3
27.1
7.0
6.1
3.2
1.7
3.9
1.8
2.3
1.7
2.0
2.1
2.9
/2.8
/2.9
/1.7
/1.5
/1.8
/1.9
/2.5
/2.2
/2.7
/1.5
/2.6
/2.1
/1.5
/1.9
/2.4
/3.0
/1.5
/2.5
AX122265
AX122823
a
The data are presented as average fold change of four independent microarray experiments. Positive fold change indicates
increased expression on acetate or acetate /glucose mixture compared with the reference glucose. Negative fold change indicates
decreased expression on acetate or acetate /glucose mixture compared with the reference glucose. All P -values in paired t -test were
smaller than 0.02 thus giving proof of significance.
associated proteins (169 protein spots identified
out of 970 observed) of glucose-grown cells has
been presented (Schaffer et al., 2001). For transcriptome analysis, DNA microarray technology
with high density arrays of open reading framespecific DNA fragments (Schena et al., 1995;
Lucchini et al., 2001) has been established for C.
glutamicum (Loos et al., 2001) and very recently,
was applied to study differential transcription
profiles of this organism under different conditions
on a full genomic scale (Muffler et al., 2002;
Wendisch, 2003 and several other articles in this
issue of J. Biotech).
In a first approach to study the acetate stimulon
of C. glutamicum by proteome analysis, lysates
prepared from cells grown on acetate and on
glucose (and labeled with 35S-methionine in the
exponential growth phase) were subjected to 2-D
gel electrophoresis and the protein patterns were
compared (Fig. 4). Out of about 500 protein spots
observed with both cell lysates, 54 were present in
more than 2-fold higher and 26 in more than 2fold lower amounts in lysates of acetate-grown
cells, indicating a significant adaptation of the C.
glutamicum metabolism. So far, ten out of the 54
‘‘acetate-induced’’ proteins were identified, i.e.
R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
113
Fig. 4. Protein pattern of C. glutamicum cells grown on acetate (A) and on glucose (B) as determined by 2-D gel electrophoresis.
Highlighted by circles and numbers are protein spots present in higher amounts in acetate-grown cells and identified as ICL (1), MS (2),
citrate synthase (3), fumarase (4), malate:chinone oxidoreductase (5), a putative ABC transporter (6), cysteine synthase (7), glycin /
tRNA ligase (8), butyryl-CoA transferase (9) and aminotransferase (10).
ICL (55-fold higher amount), MS (18-fold), citrate
synthase (2.7-fold), fumarase (2.5-fold), malate:
chinone oxidoreductase (3.7-fold), a putative ABC
transporter (2.3-fold), cystein synthase (2.2-fold),
glycin/tRNA ligase (3.3-fold), butyryl-CoA transferase (2.6-fold) and an aminotransferase (5.4fold) (see Fig. 4). For the latter five proteins we
presently do not see any direct connection to
acetate metabolism whereas the differences observed for ICL, MS, citrate synthase and fumarase
correspond well with data obtained by microarray
analysis (see below) and are in agreement with the
higher activity of the TCA and glyoxylate cycles in
acetate-grown cells (see above).
DNA arrays based on PCR fragments representing 2720 annotated open reading frames of C.
glutamicum were used by Muffler et al. (2002) to
study differential transcription profiles of cells
grown on glucose and on acetate as the sole
carbon source. Using a ‘‘metabolic array’’ of 120
genes involved in central metabolism and amino
acid biosynthesis, Hayashi et al. (2002) studied the
expression of these genes under the same conditions. At the same time, our group compared
whole genome transcript profiles of C. glutamicum
cells grown on acetate and on acetate plus glucose
with that of cells grown on glucose. With respect
to genes with expression levels differing by a factor
of two or more, the main results of all three groups
were very similar: the most prominent genes upregulated in the presence of acetate encode for
enzymes of the acetate activating pathway (AK
and PTA), the glyoxylate cycle (ICL and MS), the
TCA cycle (citrate synthase, aconitase, succinate
dehydrogenase subunits A, B and CD, fumarase)
and for PEP carboxykinase (our results are shown
in Table 5). The down-regulated genes (or upregulated genes in glucose-grown cells) comprise
those for some enzymes involved in sugar metabolism (glucose- and fructose-phosphotransferasesystem enzymes II, glucose-6-phosphate dehydrogenase, transaldolase, transketolase, pyruvate kinase and the E1 subunit of the pyruvate
dehydrogenase complex) and malic enzyme (Table
5). Muffler et al. additionally found the lactate,
alcohol and acetaldehyde dehydrogenase genes
induced during growth on glucose and discussed
the formation of lactate and ethanol. However,
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R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
while these genes were not represented on the
array of Hayashi et al., our experiments did not
show significant expression differences under the
conditions tested and neither lactate nor ethanol is
formed during growth of C. glutamicum under our
conditions. In contrast to the results by Muffler et
al. and to those by our group, Hayashi et al. found
2 /4-fold decreased expression levels of many
biosynthetic genes during growth on acetate and
refer to the low growth rate under these conditions. As neither the absolute nor the relative
growth rates on acetate or glucose were given by
the authors, the different expression of the biosynthetic genes is difficult to interpret and might be
due to global regulatory mechanisms in response
to carbon sources or in response to quite different
growth rates. Interestingly, Hayashi et al. found
two glyceraldehyde-3-phosphate dehydrogenase
genes (gapA and gapB) inversely regulated: the
gapA expression was found to be 2-fold lower and
gapB expression 4-fold higher in acetate-grown
than in glucose-grown cells. The authors discuss
that the enzyme encoded by gapA might be
involved in glycolysis while the gapB product
might be involved in gluconeogenesis.
A variety of additional C. glutamicum genes
obviously also under transcriptional control in
response to the presence or absence of acetate in
the growth medium was uncovered. In total, 132
regulated genes were detected by Muffler et al.
(2002) and these included nearly all of the 60
regulated genes found by our group. The reason
for the difference might be a slightly different
stringency applied by the two groups and/or
slightly different signal to noise ratios. However,
Muffler et al. identified several genes with expression ratios clearly above 2.5 and below /2.5,
which were not detected by our approach. Aside
from the above mentioned lactate, alcohol and
acetaldehyde dehydrogenase genes, these genes
include those for catalase, trehalose/maltose binding protein, E2 of the 2-oxoglutarate dehydrogenase complex, malate and formate dehydrogenases
(all expressed higher during growth on acetate)
and thymidilate kinase, propionyl-CoA carboxylase and poly-ß-hydroxybutyrate polymerase (expressed lower during growth on acetate). Among
the regulated genes obtained by both groups were
many hypothetical open reading frames with
hitherto unknown function and further studies
are necessary to clarify a possible role in acetate or
glucose metabolism. The knowledge on differential
expression of these genes may hopefully facilitate
the study for their function.
With a subset of C. glutamicum genes showing
different expression levels during growth on acetate and glucose as obtained by the DNA microarray technique, we performed quantitative RTPCR and promoter fusion experiments. The gene
expression ratios obtained from these studies
(acetate- vs. glucose-grown cells) were approximately in the same range as the ratios obtained by
microarrays, except that the ratios of aceA and
aceB were significantly higher (Table 6). This
result may indicate a restriction of the array
experiment in the higher expression range, i.e.
the dynamic range might be too small. The
transcription ratios of a subset of genes also
corresponded well with the ratio of specific
activities of the respective enzymes, indicating
that C. glutamicum adjusts its metabolism to a
large part on the transcriptional level.
Recently, the transcript profile of E. coli during
balanced growth in acetate medium was monitored and compared with that of glucose-grown E.
coli cells (Oh et al., 2002). At a 99% confidence
level and out of 3649 open reading frames, the
RNA level of 185 genes was found to be higher
and that of 177 genes was found to be lower in
acetate-grown cells, indicating that, under the
conditions tested, in E. coli many more genes are
under transcriptional control than in C. glutamicum . A large part of the E. coli genes with
different transcript levels are hypothetical, unclassified, unknown or putative proteins/enzymes. The
genes with lower transcript levels on acetate
comprise many genes involved in cell replication,
transcription, translation and amino acid biosynthesis, which was attributed to growth rate
dependent regulation by the authors (Oh et al.,
2002). However, as in the case of C. glutamicum ,
the up-regulated set of genes in acetate-grown cells
includes those for enzymes of the glyoxylate cycle,
the TCA cycle and gluconeogenesis and the downregulated set of genes those for enzymes involved
in glycolysis, the phosphotransferase sugar trans-
R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
115
Table 6
Comparison of DNA array data with Northern blot hybridization, RT-PCR, transcriptional fusion and specific enzyme activity data
obtained with selected genes or enzymes, respectively
Gene
Microarraya
Qt-RT-PCRa
Promoter fusiona,b
Specific activitya,b
aceA
aceB
pta
ack
pck
acn
aceE
ptsM
malE
28.6
8.4
6.1
3.1
3.8
3.7
/3.1
/2.3
/2.8
/100
42
8.3
9.3
6.9
4.7
/4.5
/3.5
/2.8
90
45
3.6
3.6
n.d.
n.d.
n.d.
n.d.
n.d.
103
44
4.5
3.9
2.0
n.d.
n.d.
n.d.
n.d.
a
The data are presented as average fold change. Positive fold change indicates increased activity/expression on acetate compared
with the reference glucose. Negative fold change indicates decreased activity/expression on acetate compared with the reference
glucose.
b
Data are taken from Wendisch et al. (1997) and Reinscheid et al. (1999).
port system and the pyruvate dehydrogenase
complex. Surprisingly, and in contrast to what
has been observed for the pta /ack operon of C.
glutamicum , the E. coli ack /pta operon was found
to be down-regulated 2-fold in acetate-grown cells.
The additional finding that in these cells the acetylCoA synthetase gene was up-regulated 8-fold,
corroborates the hypothesis that this enzyme
rather than the AK-PTA pathway is of major
importance for acetate activation in E. coli .
8. Regulation of acetate metabolism
The data presented above make it quite obvious
that the carbon flux within the central metabolism
of C. glutamicum in the presence and absence of
acetate in the growth medium is quite different and
regulated by different mechanisms at various
levels. The most important and most economic
regulation certainly takes place at the RNA level.
As shown by classical methods, such as Northern
blot hybridization and transcriptional fusion experiments as well as by DNA microarray technology, the different specific activities of the key
enzymes of acetate metabolism (AK, PTA, ICL,
MS and PEP carboxykinase) during growth in the
presence and absence of acetate can be explained
almost completely by transcriptional regulation
and thus are most probably due to an induction
and/or derepression process. In accordance with
induction by an activator protein is the finding of
a highly conserved 13-bp motif with dyad symmetry upstream of the pta /ack operon and in the
intergenic region between the aceA and the aceB
gene (see Fig. 2B and Fig. 3B), which might act as
the binding site for the regulatory protein(s)
(Collado-Vides et al., 1991). Co-substrate experiments with glucose and with lactate in addition to
acetate (Wendisch et al., 1997) revealed that aside
from the positive effect of acetate in the growth
medium, there is a negative effect of glucose and of
lactate on the specific activities of the enzymes
mentioned above. This indicates an induction (or
derepression) of the respective genes in the presence of acetate and additionally, to a minor
extent, repression in the presence of a co-substrate.
In other words, an activator as well as a repressor
protein is proposed to be involved in the transcriptional control of the enzymes of acetate metabolism. This hypothesis of dual transcriptional
control is corroborated by the recent isolation
and analysis of a mutant (TMG25) which, in
comparison to the parental strain, showed about
4-fold higher specific activities of AK and PTA,
and 7 /10-fold higher specific activities of ICL and
MS when grown on glucose-medium (unpublished
results). In the presence of acetate, the specific AK,
PTA, ICL and MS activities in mutant TMG25
were even higher than on glucose-medium and
116
R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
comparable with those of the parental strain on
acetate-medium. These characteristics indicate
that the mutant is defective in the repression
mechanism but shows a functional induction of
the respective genes. Independent of the regulatory
mechanisms, the regulatory pattern of AK, PTA,
MS, ICL and PEP carboxykinase may suggest a
common and tightly linked transcriptional control
of the respective genes. The different strengths of
the induction of the aceA and aceB on the one
hand, and the pta /ack operon and the pck gene
on the other might be caused by different affinities
of the transcriptional regulators to the respective
operator regions or by differences in the promoter
region of the respective genes. However, during
growth of C. glutamicum on palmitate the specific
ICL and MS activities were much higher than
during growth on glucose whereas the AK and
PTA activities were not (see Table 3). This
observation indicates that in principle the cells
can uncouple the transcriptional regulation of the
pta /ack operon from that of the aceA and aceB
genes.
As indicated by the DNA microarray experiments, there are many other C. glutamicum genes
transcriptionally regulated positively and/or negatively in response to the presence or absence of
acetate in the growth medium and thus, there is a
large acetate stimulon in this organism. Among
these regulated genes we found those for several
TCA cycle enzymes (up-regulated) and those for
some enzymes of sugar metabolism (down-regulated), which explains at least partially the different fluxes within the TCA cycle (higher during
growth in the presence of acetate) and glycolysis
and pyruvate dehydrogenation (lower during
growth in the presence of acetate). At present
there is no direct experimental evidence for (a)
common superior regulatory mechanism(s), however, the presence of a global regulatory network
affecting many steps within the central metabolism
of C. glutamicum is very likely. Although it is clear
that acetate metabolism of C. glutamicum is to a
large extent regulated by transcriptional control,
there is no indication for any involvement of a
typical carbon catabolite repression mechanism in
this organism. A functional catabolite control
protein (CcpA) and typical catabolite-responsive
elements (CRE’s), the two typical regulatory
elements in carbon catabolite repression of lowGC Gram-positive bacteria (Hueck et al., 1994,
1995; Stülke and Hillen, 2000), as well as inducer
exclusion and induction prevention (Saier, 1996;
Stülke and Hillen, 2000) have not been identified
so far in C. glutamicum . There is also no indication
for cAMP-CRP or cra- controlled mechanisms of
catabolite repression, as typical for the Gramnegative enteric bacteria (Saier, 1996, 1998).
Furthermore, from the genome sequence of C.
glutamicum it can be deduced that this organism
probably does not possess the typical Fnr or the
Arc systems which in enterobacteria are known to
regulate the expression of some of the TCA cycle
genes (Cronan and LaPorte, 1996). With respect to
specific control mechanisms, in C. glutamicum
there is also no genetic or other evidence for the
presence of regulatory devices known to regulate
the expression of the acetate operon in enteric
bacteria, namely the negative control by the IclR
repressor and the FadR protein or the positive
control by the Cra (Fru) protein, the IHF or other
effectors (reviewed in Cozzone, 1998). Although
there are some candidate genes for these regulator
proteins within the genome, inactivation and overexpression studies so far did not lead to the
identification of homologous regulator proteins
functional in the regulation of the acetate metabolism of C. glutamicum . Thus, although much
progress in the elucidation of the acetate metabolism of C. glutamicum has been made during the
last years, the basic mechanism of the regulation of
the acetate metabolism is not yet understood and,
to unravel the molecular mechanism(s) of the
regulation and to identify the protein(s) involved
will be one of the major challenges in the near
future.
Another challenge for future research is the
unequivocal identification of the physiological
trigger(s) of the transcriptional regulation of the
acetate metabolism in C. glutamicum . As C.
glutamicum mutants defective in acetate activation
(either AK- or PTA-deficient) showed low specific
activities of ICL and MS irrespective of the
presence or absence of acetate in the growth
medium and since there was a correlation between
a high intracellular acetyl-CoA concentration with
R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
high specific activities of ICL, MS, AK and PTA
(Wendisch et al., 1997), it has been suggested that
acetyl-CoA or a derivative thereof is the physiological trigger of the genetic regulation of the four
enzymes. However, at present it cannot be excluded that additional or alternative factors (e.g.
intracellular NAD(P)H pool or ATP/ADP ratio,
or a combination of intracellular metabolites) are
involved in triggering the transcriptional response
to the presence and absence of acetate in the
growth medium.
Applied to the model of the central metabolism
of C. glutamicum , all of the transcriptional data
are in agreement with data obtained by quantitative determination of metabolic fluxes during
growth on acetate and/or glucose, indicating that
the central metabolism is to a large part governed
by transcriptional regulation. However, biochemical analysis of some of the enzymes of the C.
glutamicum central metabolism indicate additional
and very tight control of the main pathways by
inhibition and activation of key enzymes and by
the substrate affinities of some of these enzymes.
Whereas AK, PTA and MS of C. glutamicum do
not seem to be significantly affected in their
activities by central metabolic intermediates
(Ozaki and Shiio, 1968; Reinscheid et al., 1994b,
1999), citrate synthase, ICD, ICL and PEP carboxykinase are subject to (allosteric) regulation by
a variety of metabolites of glycolysis and the TCA
cycle (Shiio and Ozaki, 1968; Ozaki and Shiio,
1968; Reinscheid et al., 1994a,b; Jetten and
Sinskey, 1993; Eikmanns et al., 1994, 1995). These
regulations at the level of enzyme activities certainly contribute to the (fine) control of the carbon
flux into the TCA cycle, within the TCA and
glyoxylate cycles and into gluconeogenesis. In
general, glycolytic intermediates and succinate
inhibit the glyoxylate cycle activity, oxaloacetate
and glyoxylate inhibit the TCA cycle activity at the
level of ICD and a high level of ATP inhibits the
TCA cycle activity at the level of citrate synthase
and gluconeogenesis. Flux control at the entry of
the TCA cycle and at the isocitrate branchpoint is
additionally governed by the intracellular concentration of isocitrate, i.e. by the different affinities
of ICL and ICD towards their common substrate
(280 and 12 mM, respectively). At present, there
117
are no indications in C. glutamicum for a regulation of the carbon flux at the isocitrate level by
transcriptional regulation of the ICD gene (Tables
2 and 3) or by phosphorylation of the ICD
protein, as it has been shown for enteric bacteria
(reviewed in Cozzone, 1998). C. glutamicum possesses a monomeric ICD which is completely
different from and unrelated to the enzyme known
from most other bacteria (Eikmanns et al., 1995;
Chen and Yang, 2000). Although the monomeric
type of ICD to our knowledge has never been
shown to be phosphorylated or regulated by other
modifications, further studies are necessary to
definitely rule out this possibility in C. glutamicum . However, since protein phosphorylation as a
regulatory device is wide-spread among bacteria
(Cozzone, 1998; Kennelly and Potts, 1996) it
would be very interesting to study whether phosphoproteins are involved in acetate metabolism of
C. glutamicum .
9. Concluding remarks and perspectives
The analysis of acetate metabolism in C. glutamicum and its regulation is of particular interest
for several reasons. First, it gives us the chance to
understand the molecular mechanisms of adaptation of this industrially important organism to the
extracellular and intracellular nutritional environment. Second, it will provide us with information
on the regulation of the central metabolic pathways, i.e. of glycolysis, TCA cycle, glyoxylate cycle
and gluconeogenesis within this organism and this
will certainly allow us in the near future to govern
the carbon flux within the central metabolism of
C. glutamicum in desired directions. And third,
since global regulatory circuits controlling general
functions of the metabolism are likely to be
conserved among the members of the Corynebacterianeae , analysis of acetate metabolism and its
regulation in C. glutamicum might be very helpful
for the understanding of the finding that the
glyoxylate pathway in the close relative M. tuberculosis plays a pivotal role in the persistence in
immunocompetent hosts, and thus in the pathology of tuberculosis (McKinney et al., 2000; Höner
zu Bentrup and Russell, 2001). As outlined above,
118
R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
a lot of biochemical and genetic knowledge on the
acetate metabolism of C. glutamicum has been
accumulated and it becomes evident that the
characteristics of the enzymes and in particular
the regulation of the enzymes and pathways
involved are different when compared with other
model organisms such as E. coli or B. subtilis.
However, many questions about the molecular
mechanism of repression and/or activation within
the regulation of the acetate metabolism of C.
glutamicum and about the intracellular signal of
acetate availability remain to be answered. In
particular, the transcriptional regulator(s) and
their DNA binding motifs have to be identified
and characterized. The relevance of those putative
DNA binding motifs found in front of the pta /
ack operon and in the intergenic region between
the aceA and aceB genes needs to be proven by
mutation and deletion studies. Identified operator
regions can be used to isolate regulatory proteins
by employing DNA affinity chromatography. The
inductive and/or repressive function of such proteins can then be studied on the molecular level.
Further studies should aim at the nature of the
metabolites modulating the function of the regulatory proteins and to other potential target genes
of these proteins. One of the most interesting
questions remaining is the mechanism by which
acetate in the growth medium affects the expression of the large set of C. glutamicum genes
observed to be regulated at the transcriptional
level. The knowledge of the C. glutamicum genome
sequence and further comparative transcriptome
and proteome analyses with the wildtype and
mutants defective in acetate metabolism should
provide interesting information about this global
regulatory system which then may be also
exploited for the control and optimization of the
amino acid productivity of this industrially important organism.
Acknowledgements
We thank Jennifer Brehme, Katja Luigart and
Petra Dangel for excellent technical assistance,
Marcella Eikmanns for critically reading the
manuscript. The support of the EU (VALPAN,
QLK3-2000-00497), BMBF (Genome research on
bacteria relevant for agriculture, environment and
biotechnology; cluster IV: Corynebacteria) and
Degussa is gratefully acknowledged.
References
Blasco, R., Cardenas, J., Castillo, F., 1991. Regulation of
isocitrate lyase in Rhodobacter capsulatus E1F1. Curr.
Microbiol. 22, 73 /76.
Baronofsky, J.J., Schreurs, W.J.A., Kashket, E.R., 1984.
Uncoupling by acetic acid limits growth of and acetogenesis
by Clostridium thermoaceticum . Appl. Environ. Microbiol.
48, 1134 /1139.
Brown, T.D.K., Jones-Mortimer, M.C., Kornberg, H.L., 1977.
The enzymatic interconversion of acetate and acetyl-coenzyme A in Escherichia coli . J. Gen. Microbiol. 102, 327 /
336.
Bruckner, R., Titgemeyer, F., 2002. Carbon catabolite repression in bacteria: choice of the carbon source and autoregulatory limitation of sugar utilization. FEMS Microbiol.
Lett. 209, 141 /148.
Buchholz, A., Takors, R., Wandrey, C., 2001. Quantification of
intracellular metabolites in Escherichia coli K12 using liquid
chromatographic-electrospray ionization tandem mass spectrometric techniques. Anal. Biochem. 295, 129 /137.
Chen, R., Yang, H., 2000. A highly specific monomeric
isocitrate dehydrogenase from Corynebacterium glutamicum . Arch. Biochem. Biophys. 383, 238 /245.
Cherrington, C.A., Hinton, M., Pearson, G.R., Chopra, I.,
1991. Inhibition of Escherichia coli K12 by short-chain
organic acids: lack of evidence for induction of SOS
response. J. Appl. Bacteriol. 70, 156 /160.
Chung, T., Klumpp, D.J., LaPorte, D.C., 1988. Glyoxylate
bypass operon of Escherichia coli : cloning and determination of the functional map. J. Bacteriol. 170, 386 /392.
Claes, W.A., Pühler, A., Kalinowski, J., 2002. Identification of
two prpDBC gene clusters in Corynebacterium glutamicum
and their involvement in propionate degradation via the 2methylcitrate cycle. J. Bacteriol. 184, 2728 /2739.
Clark, D.P., Cronan, J.E., 1996. Two-carbon compounds and
fatty acids as carbon sources. In: Neidhardt, F.C., Curtiss,
R., Ingraham, J.L., Lin, E.C.C., Low, K.B., Magasanik, B.,
Reznikoff, W.S., Riley, M., Schaechte, M., Umbarger, H.E.
(Eds.), Escherichia coli and Salmonella typhimurium : Cellular and Molecular Biology, vol. 1. American Society for
Microbiology, Washington, DC, pp. 343 /357.
Cocaign, M., Monnet, C., Lindley, N.D., 1993. Batch kinetics
of Corynebacterium glutamicum during growth on various
substrates: use of substrate mixtures to localize metabolic
bottlenecks. Appl. Microbiol. Biotechnol. 40, 526 /530.
Collado-Vides, J., Magasanik, B., Gralla, J.D., 1991. Control
site localisation and transcriptional regulation in Escherichia coli . Microbiol. Rev. 55, 371 /394.
R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
Cooper, R.A., Kornberg, H.L., 1967. The direct synthesis of
phosphoenolpyruvate from pyruvate by Escherichia coli .
Proc. R. Soc. Lond. B Biol. Sci. 168, 263 /280.
Cortay, J.C., Bleicher, F., Duclos, B., Cenatiempo, Y., Gautier,
C., Prato, J.L., Cozzone, A.J., 1989. Utilization of acetate in
Escherichia coli : structural organization and differential
expression of the ace operon. Biochimie 71, 1043 /1049.
Cozzone, A.J., 1998. Regulation of acetate metabolism by
protein phosphorylation in enteric bacteria. Annu. Rev.
Microbiol. 52, 127 /164.
Cronan, J.E., Jr, LaPorte, D., 1996. Tricarboxylic acid cycle
and glyoxylate bypass. In: Neidhardt, F.C., Curtiss, R.,
Ingraham, J.L., Lin, E.C.C., Low, K.B., Magasanik, B.,
Reznikoff, W.S., Riley, M., Schaechte, M., Umbarger, H.E.
(Eds.), Escherichia coli and Salmonella typhimurium : Cellular and Molecular Biology, vol. 1. American Society for
Microbiology, Washington, DC, pp. 206 /216.
Dominguez, H., Cocaign-Bousquet, M., Lindley, N.D., 1993.
Simultaneous consumption of glucose and fructose from
sugar mixtures during batch growth of Corynebacterium
glutamicum . Appl. Microbiol. Biotechnol. 47, 600 /603.
Ebbighausen, H., Weil, B., Krämer, R., 1991. Carrier-mediated
acetate uptake in Corynebacterium glutamicum . Arch.
Microbiol. 155, 505 /510.
Eikmanns, B.J., 1992. Identification, sequence analysis, and
expression of a Corynebacterium glutamicum gene cluster
encoding the three glycolytic enzymes glyceraldehyde-3phosphate dehydrogenase, 3-phosphoglycerate kinase, and
triosephosphate isomerase. J. Bacteriol. 174, 6076 /6086.
Eikmanns, B.J., Metzger, M., Reinscheid, D., Kircher, M.,
Sahm, H., 1991. Amplification of three threonine biosynthesis genes in Corynebacterium glutamicum and its influence
on carbon flux in different strains. Appl. Microbiol.
Biotechnol. 34, 617 /622.
Eikmanns, B.J., Thum-Schmitz, N., Eggeling, L., Lüdtke, K.,
Sahm, H., 1994. Nucleotide sequence, expression and
transcriptional analysis of the Corynebacterium glutamicum
gltA gene encoding citrate synthase. Microbiology 140,
1817 /1828.
Eikmanns, B.J., Rittmann, D., Sahm, H., 1995. Cloning,
sequence analysis, expression, and inactivation of the
Corynebacterium glutamicum icd gene encoding isocitrate
dehydrogenase and biochemical characterization of the
enzyme. J. Bacteriol. 176, 774 /782.
Fox, D.K., Roseman, S., 1986. Isolation and characterization
of homogeneous acetate kinase from Salmonella typhimurium and Escherichia coli . J. Biol. Chem. 261, 13487 /13497.
Gancedo, J.M., 1998. Yeast carbon catabolite repression.
Microbiol. Mol. Biol. Rev. 62, 334 /361.
Garnak, M., Reeves, H.C., 1979. Phosphorylation of isocitrate
dehydrogenase of Escherichia coli . Science 203, 1111 /1112.
Goldie, H., 1984. Regulation of transcription of the Escherichia
coli phosphoenolpyruvate carboxykinase locus: studies with
pck /lacZ operon fusions. J. Bacteriol. 159, 832 /838.
Gourdon, P., Baucher, M.F., Lindley, N.D., Guyonvarch, A.,
2000. Cloning of the malic enzyme gene from Corynebacter-
119
ium glutamicum and role of the enzyme in lactate metabolism. Appl. Environ. Microbiol. 66, 2981 /2987.
Grundy, F., Waters, D.A., Allen, S.H., Henkin, T.M., 1993a.
Regulation of the Bacillus subtilis acetate kinase gene by
CcpA. J. Bacteriol. 175, 7348 /7355.
Grundy, F., Waters, D.A., Takova, T.Y., Henkin, T.M., 1993b.
Identification of genes involved in utilization of acetate and
acetoin in Bacillus subtilis . Mol. Microbiol. 10, 259 /271.
Grundy, F., Turinsky, A.J., Henkin, T.M., 1994. Catabolite
regulation of Bacillus subtilis acetate and acetoin utilization
genes by CcpA. J. Bacteriol. 176, 4527 /4533.
Hansen, E.J., June, E., 1974. Two routes for synthesis of
phosphoenolpyruvate from C4-dicarboxylic acids. Biochem.
Biophys. Res. Commun. 59, 1204 /1210.
Harder, W., Dijkhuizen, L., 1982. Strategies of mixed substrate
utilization in microorganisms. Phil. Trans. Soc. Lond. 297,
459 /480.
Hayashi, M., Mizogushi, H., Shiraishi, N., Obayashi, M.,
Nakagawa, S., Imai, J., Watanabe, S., Ota, T., Ikeda, M.,
2002. Transcriptome analysis of acetate metabolism in
Corynebacterium glutamicum using a newly developed
metabolic array. Biosci. Biotechnol. Biochem. 66, 1337 /
1344.
Hermann, T., Pfefferle, W., Baumann, C., Busker, E., Schaffer,
S., Bott, M., Sahm, H., Dusch, N., Kalinowski, J., Pühler,
A., Bendt, A.K., Krämer, R., Burkovski, A., 2001. Proteome analysis of Corynebacterium glutamicum . Electrophoresis 22, 1712 /1723.
Hillier, S., Charnetzky, W.T., 1981. Glyoxylate bypass enzymes
in Yersinia species and multiple forms of isocitrate lyase in
Y. pestis . J. Bacteriol. 145, 452 /458.
Höner zu Bentrup, K., Russell, D.G., 2001. Mycobacterial
persistence: adaptation to a changing environment. Trends
Microbiol. 9, 597 /605.
Hueck, C.J., Hillen, W., Saier, M.H., 1994. Analysis of a cisactive sequence mediating catabolite repression in grampositive bacteria. Res. Microbiol. 145, 503 /518.
Hueck, C.J., Kraus, A., Schmiedel, D., Hillen, W., 1995.
Cloning, expression and functional analyses of the catabolite control protein CcpA from Bacillus megaterium . Mol.
Microbiol. 16, 855 /864.
Inui, M., Nakata, K., Roh, J.H., Zahn, K., Yukawa, H., 1999.
Molecular and functional characterization of the Rhodopseudomonas palustris No.7 phosphoenolpyruvate carboxykinase gene. J. Bacteriol. 181, 2689 /2696.
Jetten, M.S.M., Sinskey, A.J., 1993. Characterization of
phosphoenolpyruvate carboxykinase from Corynebacterium
glutamicum . FEMS Microbiol. Lett. 111, 183 /188.
Jetten, M.S.M., Sinskey, A.J., 1995. Purification and properties
of oxaloacetate decarboxylase from Corynebacterium glutamicum . Antonie van Leeuwenhoek 67, 221 /227.
Kay, W.W., 1978. Transport of carboxylic acids. In: Rosen,
B.P. (Ed.), Bacterial Transport. Marcel Dekker, New York,
pp. 385 /411.
Kell, D.B., Peck, M.W., Rodger, G., Morris, J.G., 1981. On the
permeability of weak acids and bases of the cytoplasmic
120
R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
membrane of Clostridium pasteurianum . Biochem. Biophys.
Res. Commun. 99, 81 /88.
Kennelly, P.J., Potts, M., 1996. Fancy meeting you here! A
fresh look at ‘‘prokaryotic’’ protein phosphorylation. J.
Bacteriol. 178, 4759 /4764.
Kinoshita, S., Tanaka, K., 1972. Glutamic acid. In: Yamada,
K. (Ed.), The Microbial Production of Amino Acids. Wiley,
New York, pp. 263 /324.
Kornberg, H.L., 1966a. The role and control of the glyoxylate
cycle in Escherichia coli . Biochem. J. 99, 1 /11.
Kornberg, H.L., 1966b. Anaplerotic sequences and their role in
metabolism. In: Campbell, P.N., Greville, G.P. (Eds.),
Essays in Biochemistry, vol. 2. Academic Press, New
York, pp. 1 /31.
Kovarova-Kovar, K., Egli, T., 1998. Growth kinetics of
suspended microbial cells: from single-substrate-controlled
growth to mixed-substrate kinetics. Microbiol. Mol. Biol.
Rev. 62, 646 /666.
Krämer, R., Lambert, C., Hoischen, C., Ebbighausen, H., 1990.
Uptake of glutamate in Corynebacterium glutamicum . 1.
Kinetic properties and regulation by internal pH and
potassium. Eur. J. Biochem. 194, 929 /935.
Kronemeyer, W., Peekhaus, N., Krämer, R., Sahm, H.,
Eggeling, L., 1995. Structure of the gluABCD cluster
encoding the glutamate uptake system of Corynebacterium
glutamicum . J. Bacteriol. 177, 1152 /1158.
Kumari, S., Beatty, C.M., Browning, D.F., Busby, S.J., Simel,
E.J., Hovel-Miner, G., Wolfe, A.J., 2000. Regulation of
acetyl coenzyme A synthetase in Escherichia coli . J.
Bacteriol. 182, 4173 /4179.
LaPorte, D.C., Koshland, D.E., Jr, 1982. A protein with kinase
and phosphatase activities involved in regulation of tricarboxylic acid cycle. Nature 300, 458 /460.
LaPorte, D.C., Thorsness, P.E., Koshland, D.E., Jr, 1985.
Compensatory phosphorylation of isocitrate dehydrogenase, a mechanism for adaptation to the intracellular
environment. J. Biol. Chem. 260, 10563 /10568.
Leuchtenberger, W., 1996. Amino acids */technical production
and use. In: Rehm, H.J., Reed, G., Pühler, A., Stadler, P.,
Roehr, M. (Eds.), Biotechnology, vol. 6. VCH Verlagsgesellschaft, Weinheim, pp. 465 /502.
Liebl, W., 1991. The genus Corynebacterium */nonmedical. In:
Balows, A., Trüper, H.G., Dworkin, M., Harder, W.,
Schleifer, K.H. (Eds.), The Procaryotes, vol. 2. Springer,
New York, pp. 1157 /1171.
Loos, A., Glanemann, C., Willis, L.B., O’Brien, X.M., Lessard,
P.A., Gerstmeir, R., Guillouet, S., Sinskey, A., 2001.
Development and validation of Corynebacterium DNA
microarrays. Appl. Environ. Microbiol. 67, 2310 /2318.
Lucchini, S., Thompson, A., Hinton, J.C.D., 2001. Microarrays
for microbiologists. Microbiology 147, 1403 /1414.
Marx, A., Eikmanns, B.J., Sahm, H., de Graaf, A.A., 1999.
Response of the central metabolism in Corynebacterium
glutamicum to the use of an NADH-dependent glutamate
dehydrogenase. Metab. Eng. 1, 35 /48.
McKinney, J.D., Höner zu Bentrup, K., Munoz-Elias, E.J.,
Miczak, A., Chen, B., Chan, W.T., Swenson, D., Sacchetti,
J.C., Jacobs, W.R., Jr, Russell, D.G., 2000. Persistence of
Mycobacterium tuberculosis in macrophages and mice
requires the glyoxylate shunt enzyme isocitrate lyase.
Nature 406, 683 /685.
Molenaar, D., van der Rest, M.E., Petrovic, S., 1998. Biochemical and genetic characterization of the membrane
associated malate dehydrogenase (acceptor) from Corynebacterium glutamicum . Eur. J. Biochem. 254, 395 /403.
Molenaar, D., van der Rest, M.E., Drysch, A., Yucel, R., 2000.
Functions of the membrane-associated and cytoplasmic
malate dehydrogenases in the citric acid cycle of Corynebacterium glutamicum . J. Bacteriol. 182, 6884 /6891.
Molina, I., Pellicer, M.T., Badia, J., Aguilar, J., Baldoma, L.,
1994. Molecular characterization of Escherichia coli malate
synthase G: differentiation with the malate synthase A
isoenzyme. Eur. J. Biochem. 224, 541 /548.
Monod, J., 1949. The growth of bacterial cultures. Annu. Rev.
Microbiol. 3, 371 /394.
Muffler, A., Bettermann, S., Haushalter, M., Hörlein, A.,
Neveling, U., Schramm, M., Sorgenfrei, O., 2002. Genome-wide transcription profiling of Corynebacterium glutamicum after heat shock and during growth on acetate and
glucose. J. Biotechnol. 98, 255 /268.
Nyström, T., 1994. The glucose-starvation stimulon of Escherichia coli : induced and repressed synthesis of enzymes of
central metabolic pathways and role of acetyl phosphate in
gene expression and starvation survival. Mol. Microbiol. 12,
833 /843.
O’Farrell, P.H., 1975. High resolution two-dimensional electrophoresis of proteins. J. Biol. Chem. 250, 4007 /4021.
Oh, M.-K., Rohlin, L., Kao, K.C., Liao, J.C., 2002. Global
expression profiling of acetate-grown Escherichia coli . J.
Biol. Chem. 277, 13175 /13183.
Osteras, M., Driscoll, B.T., Finan, T.M., 1995. Molecular and
expression analysis of the Rhizobium meliloti phosphoenolpyruvate carboxykinase (pckA ) gene. J. Bacteriol. 177,
1452 /1460.
Ozaki, H., Shiio, I., 1968. Regulation of the TCA and
glyoxylate cycles in Brevibacterium flavum . J. Biochem. 66,
297 /311.
Paulsen, I.T., 1996. Carbon metabolism and its regulation in
Streptomyces and other high GC Gram-positive bacteria.
Res. Microbiol. 147, 535 /541.
Petersen, S., de Graaf, A.A., Eggeling, L., Möllney, M.,
Wiechert, W., Sahm, H., 2000. In vivo quantification of
parallel and bidirectional fluxes in the anaplerosis of
Corynebacterium glutamicum . J. Biol. Chem. 275, 35932 /
35941.
Petersen, S., Mack, C., de Graaf, A.A., Riedel, C., Eikmanns,
B.J., Sahm, H., 2001. Metabolic consequences of altered
phosphoenolpyruvate carboxykinase activity in Corynebacterium glutamicum reveal anaplerotic regulation in vivo.
Metab. Eng. 3, 344 /361.
Peters-Wendisch, P.G., Eikmanns, B.J., Thierbach, G., Bachmann, B., Sahm, H., 1993. Phosphoenolpyruvate carboxylase in Corynebacterium glutamicum is dispensable for
R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
growth and lysine production. FEMS Microbiol. Lett. 112,
269 /274.
Peters-Wendisch, P.G., Wendisch, V.F., Paul, S., Eikmanns,
B.J., Sahm, H., 1997. Pyruvate carboxylase as anaplerotic
enzyme in Corynebacterium glutamicum . Microbiology 143,
1095 /1103.
Peters-Wendisch, P.G., Kreutzer, C., Kalinowski, J., Patek, M.,
Sahm, H., Eikmanns, B.J., 1998. Pyruvate carboxylase from
Corynebacterium glutamicum : characterization, expression
and inactivation of the pyc gene. Microbiology 144, 915 /
927.
Peters-Wendisch, P., Schiel, B., Wendisch, V.F., Katsoulidis,
E., Möckel, B., Sahm, H., Eikmanns, B.J., 2001. Pyruvate
carboxylase as a major bottleneck for glutamate and lysine
production by Corynebacterium glutamicum . J. Mol. Microbiol. Biotechnol. 3, 295 /300.
Presecan-Siedel, E., Galinier, A., Longin, R., Deutscher, J.,
Danchin, A., Glaser, P., Martin-Verstraete, I., 1999. Catabolite regulation of the pta gene as part of carbon flow
pathways in Bacillus subtilis . J. Bacteriol. 181, 6889 /6897.
Pronk, J.T., van der Linden-Beuman, A., Verduyn, C.,
Scheffers, W.A., van Dijken, J.P., 1994. Propionate metabolism in Saccharomyces cerevisiae : implications for the
metabolon hypothesis. Microbiology 140, 717 /722.
Rado, T.A., Hoch, J.A., 1973. Phosphotransacetylase from
Bacillus subtilis : purification and physiological studies.
Biochim. Biophys. Acta 321, 114 /125.
Rehberger, J.L., Glatz, B.A., 1998. Response of cultures of
Propionibacterium to acid and low pH: tolerance and
inhibition. J. Food Prot. 61, 211 /216.
Reinscheid, D.J., Eikmanns, B.J., Sahm, H., 1994a. Characterization of the isocitrate lyase gene from Corynebacterium
glutamicum and biochemical analysis of the enzyme. J.
Bacteriol. 176, 3474 /3483.
Reinscheid, D.J., Eikmanns, B.J., Sahm, H., 1994b. Malate
synthase from Corynebacterium glutamicum : sequence analysis of the gene and biochemical characterization of the
enzyme. Microbiology 140, 3099 /3108.
Reinscheid, D.J., Schnicke, S., Rittmann, D., Zahnow, U.,
Sahm, H., Eikmanns, B.J., 1999. Cloning, sequence analysis, expression and inactivation of the Corynebacterium
glutamicum pta /ack operon encoding phosphotransacetylase and acetate kinase. Microbiology 145, 503 /513.
Riedel, C., Rittmann, D., Dangel, P., Möckel, B., Sahm, H.,
Eikmanns, B.J., 2001. Characterization, expression, and
inactivation of the phosphoenolpyruvate carboxykinase
gene from Corynebacterium glutamicum and significance of
the enzyme for growth and amino acid production. J. Mol.
Microbiol. Biotechnol. 3, 573 /583.
Roe, A.J., O’Byrne, C., McLaggan, D., Booth, I.R., 2002.
Inhibition of Escherichia coli growth by acetic acid: a
problem with methionine biosynthesis and homocysteine
toxicity. Microbiology 148, 2215 /2222.
Saier, M.H., Jr, 1996. Cyclic AMP-independent catabolite
repression in bacteria. FEMS Microbiol. Lett. 138, 97 /103.
Saier, M.H., Jr, 1998. Multiple mechanisms controlling carbon
metabolism in bacteria. Biotechnol. Bioeng. 58, 170 /174.
121
Schaffer, S., Weil, B., Nguyen, V.D., Dongmann, G., Gunther,
K., Nickolaus, M., Hermann, T., Bott, M., 2001. A high
resolution reference map for cytoplasmic and membraneassociated proteins of Corynebacterium glutamicum . Electrophoresis 22, 4404 /4422.
Schena, M., Shalon, D., Davis, R.W., Brown, P.O., 1995.
Quantitative monitoring of gene expression patterns with
complementary DNA microarray. Science 270, 467 /470.
Schwinde, J.W., Thum-Schmitz, N., Eikmanns, B.J., Sahm, H.,
1993. Transcriptional analysis of the gap /pgk /tpi /ppc
gene cluster of Corynebacterium glutamicum . J. Bacteriol.
175, 3905 /3908.
Shiio, I., Ozaki, H., 1968. Concerted inhibition of isocitrate
dehydrogenase by glyoxylate plus oxaloacetate. J. Biochem.
64, 45 /53.
Shiio, I., Momose, H., Oyama, A., 1969. Genetic and biochemical studies on bacterial formation of L-glutamate I.
Relationship between isocitrate lyase, acetate kinase, and
phosphate acetyltranferase levels and glutamate production
in Brevibacterium flavum . J. Gen. Appl. Microbiol. 15, 27 /
40.
Shimizu, M., Suzuki, T., Kameda, K.-Y., Abiko, Y., 1969.
Phosphotransacetylase of Escherichia coli B, purification
and properties. Biochim. Biophys. Acta 191, 550 /558.
Shin, B.S., Choi, S.K., Park, S.H., 1999. Regulation of the
Bacillus subtilis phosphotransacetylase gene. J. Biochem.
126, 333 /339.
Smith, C.V., Huang, C.C., Miczak, A., Russell, D.G., Sacchetti,
J.C., Höner zu Bentrup, K., 2003. Biochemical and structural studies of malate synthase from Mycobacterium
tuberculosis . J. Biol. Chem. 278, 1735 /1743.
Söhling, B., Gottschalk, G., 1996. Molecular analysis of the
anaerobic succinate degradation pathway in Clostridium
kluyveri . J. Bacteriol. 178, 871 /880.
Sonntag, K., Schwinde, J., de Graaf, A., Marx, A., Eikmanns,
B.J., Wiechert, W., Sahm, H., 1995. 13C NMR studies of the
fluxes in the central metabolism of Corynebacterium glutamicum during growth and overproduction of amino acids in
batch cultures. Appl. Microbiol. Biotechnol. 44, 489 /495.
Stülke, J., Hillen, W., 2000. Regulation of carbon catabolism in
Bacillus subtilis . Annu. Rev. Microbiol. 54, 849 /880.
Tauch, A., Homann, I., Mormann, S., Rüberg, S., Billault, A.,
Bathe, B., Brand, S., Brockmann-Gretza, O., Rückert, C.,
Schischka, N., Wrenger, C., Hoheisel, J., Möckel, B.,
Huthmacher, K., Pfefferle, W., Pühler, A., Kalinowski, J.,
2002. Strategy to sequence the genome of Corynebacterium
glutamicum ATCC 13032: use of a cosmid and a bacterial
artificial chromosome library. J. Biotechnol. 95, 25 /38.
Textor, S., Wendisch, V.F., de Graaf, A.A., Müller, U., Linder,
I., Linder, D., Buckel, W., 1997. Propionate oxidation in
Escherichia coli : evidence for operation of a methylcitrate
cycle in bacteria. Arch. Microbiol. 168, 428 /436.
Thauer, R.K., Jungermann, K., Decker, K., 1977. Energy
conservation in chemotrophic anaerobic bacteria. Bacteriol.
Rev. 41, 100 /180.
Utter, M.F., Kolenbrander, H.M., 1972. Formation of oxaloacetate by CO2 fixation on phosphoenolpyruvate. In: Boyer,
122
R. Gerstmeir et al. / Journal of Biotechnology 104 (2003) 99 /122
P.D. (Ed.), The Enzymes, vol. VI. Academic Press, New
York, pp. 117 /170.
van der Rest, M.E., Frank, C., Molenaar, D., 2000. Functions
of the membrane-associated and cytoplasmic malate dehydrogenases in the citric acid cycle of Escherichia coli . J.
Bacteriol. 182, 6892 /6899.
Walsh, K., Koshland, D.E., Jr, 1984. Determination of flux
through the branch point of two metabolic cycles. J. Biol.
Chem. 259, 9646 /9654.
Walsh, K., Koshland, D.E., Jr, 1985. Branch point control by
the phosphorylation state of isocitrate dehydrogenase. J.
Biol. Chem. 260, 8430 /8437.
Wendisch, V.F., 2003. Genome-wide expression analysis in
Corynebacterium glutamicum using DNA microarrays. J.
Biotechnol. 104, 273 /285.
Wendisch, V.F., Spies, M., Reinscheid, D.J., Schnicke, S.,
Sahm, H., Eikmanns, B.J., 1997. Regulation of acetate
metabolism in Corynebacterium glutamicum : transcriptional
control of the isocitrate lyase and malate synthase genes.
Arch. Microbiol. 168, 262 /269.
Wendisch, V.F., de Graaf, A.A., Sahm, H., Eikmanns, B.J.,
2000. Quantitative determination of metabolic fluxes during
coutilization of two carbon sources: comparative analyses
with Corynebacterium glutamicum during growth on acetate
and/or glucose. J. Bacteriol. 182, 3088 /3096.