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i n t e r n a t i o n a l j o u r n a l o f h y d r o g e n en e r g y 3 7 ( 2 0 1 2 ) 4 9 1 5e4 9 2 4
Available online at w
journal homepage: www.elsevier .com/locate/he
Relationship between PHA and hydrogen metabolismin the purple sulfur phototrophic bacterium Thiocapsaroseopersicina BBS
Andras Fulop a, Rita Beres a, Roland Tengolics a, Gabor Rakhely a,b,*, Kornel L. Kovacs a,b
aDepartment of Biotechnology, University of Szeged, Kozep Fasor 52, Szeged 6726, Hungaryb Institute of Biophysics, Biological Research Center, Hungarian Academy of Sciences, Temesvari krt 62, Szeged 6726, Hungary
a r t i c l e i n f o
Article history:
Received 27 September 2011
Received in revised form
30 November 2011
Accepted 3 December 2011
Available online 29 December 2011
Keywords:
Hydrogen
Polyhydroxy alkanoates
Nitrogenase
Thiocapsa roseopersicina
Metabolic versatility
Purple sulfur bacteria
* Corresponding author. Department of Biotefax: þ36 62 544352.
E-mail address: [email protected] (G. Rakh0360-3199/$ e see front matter Copyright ªdoi:10.1016/j.ijhydene.2011.12.019
a b s t r a c t
Purple sulfur phototrophic bacteria accumulate various storage materials, such as sulfur
globules, glycogen or polyhydroxy alkanoates (PHAs) under appropriate conditions. The
formation of these materials requires reducing power which might be recovered upon their
breakdown. This work aims at the understanding of the metabolism of PHA and its link to
the nitrogenase mediated in vivo H2 evolution in Thiocapsa roseopersicina BBS. The strain
could accumulate 30% of the dry cell weight in the form of PHAs. Analysis of the genome
sequence revealed the loci involved in PHAs synthesis and degradation. Phylogenetic
analysis indicated independent evolution of the anabolic and catabolic proteins. A mutant
carrying deleted PHA biosynthesis genes has been created in a host containing nitrogenase
but none of the hydrogenases. Determination of the H2 evolving capacity of the mutant
revealed significantly reduced H2 production in PHA deficient cells. Addition of excess
electron sources such as thiosulfate stimulated the H2 production via multiple effects.
Copyright ª 2011, Hydrogen Energy Publications, LLC. Published by Elsevier Ltd. All rights
reserved.
1. Introduction metabolic processes, the quinone pool, NADH or directly from
Hydrogen is aneconomically soundenergy carrierwhichcanbe
produced by various biological pathways [1]. Hydrogenases are
the dedicated enzymes for hydrogen metabolism; they can
produce or oxidize H2. Nitrogenases can also produce substan-
tial amountofH2as thebyproduct ofnitrogenfixationand these
are practically unidirectional enzymes. In purple sulfur photo-
trophic bacteria, both enzyme systems can be involved in bio-
hydrogen evolution while in the case of non-sulfur phototophs
no H2 evolving hydrogenase has been identified so far.
H2 formation involving either enzyme systems requires
excess electrons, which may derive from the central
chnology, University of S
ely).2011, Hydrogen Energy P
the oxidation of organic/inorganic compounds, such as
formate or reduced sulfur compounds [1]. Most microorgan-
isms utilize reducing power also for the accumulation of
various storage materials, i.e. glycogen, PHA or globules of
elementary sulfur [2]. Accumulation of such excess materials
constitutes a widespread strategy, which enables the adap-
tation of microorganisms to the changing environment and
substrate fluctuations. The capability to conserve energy and
carbon source endows the microbes with a selective advan-
tage under nutrient limitations over those lacking this capa-
bility. The production of the storage materials competes for
the electrons with the H2 evolving enzymes, but upon their
zeged, Kozep fasor 52, Szeged 6726, Hungary. Tel.: þ36 62 546940;
ublications, LLC. Published by Elsevier Ltd. All rights reserved.
i n t e rn a t i o n a l j o u r n a l o f h y d r o g e n en e r g y 3 7 ( 2 0 1 2 ) 4 9 1 5e4 9 2 44916
consumption electrons can be provided for the hydrogenases
and/or nitrogenases.
PHAs are linear polyesters, which are synthesized in large
quantities when there is plenty of carbon supply in the envi-
ronment but cell proliferation is limited by the availability
of important nutrients such as phosphorus, nitrogen or
sulfur [3]. In Rhodospirillum rubrum, Rhodobacter sphaeroides
and Rhodopseudomonas palustris the switch between the PHB
accumulation and hydrogen production is mediated by the
S-nutrients availability in the growing medium [4]. The prop-
erties of PHAs vary with the producing microbial strain. The
PHAs are ideal reserve materials because they are insoluble in
water, chemically and osmotically inert and can be readily
decomposed to acetate by a series of enzymatic reactions. The
polymers have been classified according to the carbon atom
number of the 3-hydroxyalkanoate units: short chain length
PHAs (PHASCL) contain 3e5 carbon atoms/monomer while
medium chain length PHAs (PHAMCL) are made of 6e15 carbon
atoms/monomer [2].
Although, polyesters are made of more than 150 various
monomermoleculesareknown, themost typicalmonomerunit
is 3-hydroxybutyrate [3]. The ability to produce poly(3-
hydroxybutyrate) (PHB) is common in many bacteria, however
copolymers with other alkanoates, such as 3-hydroxyvalerate,
also frequently occur. The physicochemical properties and the
practical applications of PHAs vary with polymer composition.
The expression enzymes involved in PHA biosynthesis can
be induced and usually nutrient limitation upregulates the
expression of the components involved in the anabolic route.
The following enzymes are involved in the process: a keto-
thiolase (PhbA), which catalyzes the dimerization of acetyl-
CoA, to acetoacetyl-CoA, a reductase (PhbB), which catalyzes
the hydrogenation of the latter to [R]-3-hydroxybutyryl-CoA,
which is further polymerized to PHB by a PHA synthase (PhbC,
PhbE) [3].
In Paracoccus denitrificans, the intracellular PHB granules are
covered by a lipoprotein layer consisting of phasins, PHA
synthase, PHA depolymerase, other proteins and phospho-
lipids [5]. The phasin proteins (PhaP) form a boundary layer on
the PHB granule surface separating the hydrophobic polymer
from the other cytoplasmic constituents [5e7]. The phaR
encodes a repressor regulating the expression of phaP gene
and itself. PhaR can sense the presence of PHB via interacting
with the nascent PHB granules and derepresses the PhaP
expression [8,9].
There are intracellular and extracellular depolymerases
involved in PHA degradation. Since the intracellular PHA
depolymerases hydrolyze the native PHA granules, while the
extracellular PHA depolymerases degrade denaturedmaterial,
they are named as nPHA and dPHA depolymerases, respec-
tively [10,11]. Moreover, both types of depolymerase might act
either on short ormedium length PHAs, therefore four types of
depolymerases are known: n/dPHASCL and n/dPHAMCL depo-
lymerases [10,11].
Depending on the growth conditions, purple phototrophic
bacteria are also able to preserve energy in various forms
including PHA [12]. In the purple non-sulfur bacterium R.
sphaeroides cultivated on acetate, high PHB content was
observed [13]. It was later shown that the produced PHB could
be used for H2 production in the absence of external substrate
in Rhodovalum sulfidophilum [14]. The PHB could be converted
slightly more efficiently to H2 than succinate, which was one
of the best substrates for this strain [15]. In R. palustris, R.
sphaeroides and R. rubrum [16,17], a competition for the
reducing equivalents between H2 production and PHB accu-
mulation was pointed out. It should be noted that these
strains harbor only H2 uptake hydrogenases (if any) and
nitrogenase(s).
Our model organism, Thiocapsa roseopersicina BBS is
a photosynthetic purple sulfur bacterium (PSB) which can be
propagated photochemolitoautotrophically on reduced sulfur
compounds and simple organic substrates such as acetate,
succinate, pyruvate, glucose, etc. It contains four active [NiFe]
hydrogenases: two of them aremembrane-associated (HupSL,
HynSL) [18,19], and Hox1 [20] and the recently described Hox2
[21] are soluble hydrogenases. This microbe is able to fix
molecular nitrogen in the absence of alternative nitrogen
sources.
In this work, we studied the PHA and H2 metabolism of T.
roseopersicina BBS. It has been found that e depending on the
growth conditions e the cells synthesize PHB/PHV (poly-
hydroxyvalerate) copolymers of medium chain length. Based
on the genomic DNA sequence data available, the putative
metabolic pathways of PHA synthesis and degradation were
identified and phylogenetically analyzed. In order to disclose
the potential linkage between PHA and hydrogenmetabolism,
a mutant in PHA biosynthesis (PH12B) has been created on
hydrogenase minus background (DC12B) [22]. Comparing the
hydrogen production capacity of the control and pha mutant
strains revealed that PHA could supply reducing power for the
nitrogenase. Addition of electron rich substrates increased
both the PHA degradation rate and the H2 production.
2. Materials and methods
2.1. Bacterial strains and plasmids
Strains and plasmids are listed in Table 1.
Thiocapsa roseopersicina BBS strains were maintained in
Pfennig’s mineral medium (for 1000 ml: 20 g NaCl, 1 g KH2PO4,
1 g MgCl2, 1 g KCl, 1 g NH4Cl, 2 g Na2S2O3, 200 ml) B12 vitamin
(100 mg ml�1), 1 ml Fe-EDTA (3.3 g L�1), 1 ml micro elements
solution (2975 mg Na2-EDTA, 300 mg H3BO4, 200 mg
CaCl2 � 6H2O, 100 mg ZnSO4 � 7H2O, 30 mg MnCl2 � 4H2O,
30 mg Na2MoO4 � 2H2O, 20 mg NiCl2 � 6H2O, 10 mg
CuCl2 � 2H2O in 1000 ml) [23]. The other parameters of culti-
vation in liquid culture or on solid surface are given in [22].
Antibiotics were used in the following concentrations
(mg ml�1): for Escherichia coli: ampicillin (100), kanamycin (25);
for T. roseopersicina: gentamicin (5), kanamycin (25), strepto-
mycin (5), erythromycin (50).
In order to study PHA accumulation and H2 production,
two-stage cultivation conditions were used: (A) For the PHA
accumulating condition, NH4Cl was omitted from the Pfen-
nig’s mineral medium and sodium glutamate was added as
nitrogen source (optimally: 0.17 g/l). The sodium thiosulfate
content was reduced to 2 g/l and sodium acetate concentra-
tion was varied between 2 and 10 g/l. The hypovials were
flushed for 10 min with Ar gas. The cultures were first grown
Table 1 e Strains used in this study.
Strain/plasmid Relevant genotype or phenotype Reference or source
Thiocapsa roseopersicina
BBS wild type [56]
DC12B hypC1D, hypC2D, wild type [22]
PH12B DphbBPRAEC, DC12B This work
E. coli
S17-1(lpir) 294 (recA pro res mod) Tpr, Smr (pRP4-2-Tc::Mu-Km::Tn7), lpir [57]
XL1-Blue MRF’ D(mcrA)183, D(mcrCB-hsdSMR-mrr)173, endA1, supE44,
thi-1, recA1, gyrA96, relA1 lac [F0 proAB lacIqZDM15 Tn10 (Tcr)]cStratagene
Vectors
pBluescript SK (þ) Cloning vector, Ampr Stratagene
pK18mobsacB sacB, RP4 oriT, ColE1 ori, Kmr [28]
pPHA2_2 up- and downstream regions (PHDo7 and PHDo8) of phb biosynthetic
locus in pK18mobsacB, Kmr
This work
pPHA2_1 1069 bp downstream region (PHDo1 and PHDo2) in pK18mobsacB, Kmr This work
i n t e r n a t i o n a l j o u r n a l o f h y d r o g e n en e r g y 3 7 ( 2 0 1 2 ) 4 9 1 5e4 9 2 4 4917
in 500 ml hypovials at 25 �C under a photon flux of approxi-
mately 58 mm s�1 m�2. (B) H2-producing condition: The cells
were grown under PHA accumulation conditions for 5 days
(exponential growth phase) and were collected by centrifu-
gation. The pellet was resuspended in nitrogen free medium
(for 1000ml: 20 g NaCl, 1 g KH2PO4, 1 gMgCl2, 1 g KCl and, 200 ml
B12 vitamin (100 mg ml�1), 1 ml Fe-EDTA (3.3 g L�1), 1 ml micro
elements solution) and the transmittance was adjusted to
0.50e0.65 (at 772 nm). In some cases, the growth mediumwas
supplemented with 5 g L�1 sodium succinate and/or 2 g L�1
sodium thiosulfate. 60 ml aliquots were dispensed in 125 ml
hypovials and were flushed for 10 min with Ar gas before
illumination as above.
2.2. Isolation of the pha genes in T. roseopersicina
The Allochromatium vinosum phbC and phbZ genes were used as
query sequence in a TBLAST search in our local T. rose-
opersicina genome data bank.
2.3. Nucleotid sequence accession numbers
The DNA sequences presented in this studywere submitted to
Genbank under accession no. JN244736 ( phaARPBCE locus) and
JN244737 ( phaZ locus).
2.4. DNA and protein manipulation
DNA manipulations were performed using standard tech-
niques [24,25] or according to themanufacturers’ instructions.
Protein quantification was performed byNon-Interfering Protein
Assay� kit (Calbiochem) according to the manufacturer’s
instructions.
2.5. Computational analysis, phylogenetic treeconstruction
Protein sequences in the various databases were compared
with the BLAST (P, X) programs (www.ncbi.nih.nlm.gov).
Multiple alignment of the sequences was performed by T-
COFFEE in regular mode [26]. The results of multiple
alignments were saved in phylip format and used as input for
PhyML (http://www.atgc-montpellier.fr/phyml/) [27], where
LG substitution model was applied and the SH-like method
was used to assess the support of the data for internal
branches of a phylogeny. The phylogenetic trees were visu-
alized by the Figtree v1.3.1. software (http://tree.bio.ed.ac.uk/
software/figtree/).
2.6. Deletion of the PHA biosynthetic locus
The pK18mobsacB vector [28] was used for making construct
for deleting the pha biosynthetic genes. The upstream and
downstream regions of the phb biosynthetic locus were
amplified from genomic DNA with the PHADo1 (50
TCCTGCGCCGCTTACGTCTT 30), PHADo2 (50 CATCGCTGCC-
GACGTGTCT 30) upstream primers and with the PHADo7 (50
CTGATCGACGTAGCAGTACC 30), PHADo8 (50 GAGCCACTCTA-CAACCACAT 30) downstream primers (see also Fig. 1). The
upstream1.069 bp PCR productwas inserted into pK18mobsacB
digested by SmaI (pPHA2_1). The downstream 1.162 bp frag-
ment was put into pPHA2_1 previously cleaved by XbaI and
polished (pPHA2_2). This plasmid was conjugated into
a mutant T. roseopersicina strain (DC12B) [22] lacking active
hydrogenase. Single and double recombinants were selected
based on kanamycin resistance and the sacB positive selection
system, respectively [28] (Table 1.). The genotype of the
mutants was further confirmed by sequencing the 1631 bp
fragment amplified by the PHBMo5 (50 CCA-
CATCGGCATCTATGTCA 30) and PHBMo6 (50 TCATCACCGAC-GACAACTTC 30) primers (see also Fig. 1).
2.7. Measurement of thiosulfate and succinate
The thiosulfate concentration was determined spectrophoto-
metrically as described earlier in Ref. [21].
The concentration of succinate was measured using HPLC
(Elite LaChrom, Hitachi) fittedwith an ICsep ICE-COREGAL 64H
organic acid analysis column and equipped with a L-2490
Refractive Index Detector. The temperature of the column and
RI detector was set at 50 �C and 41 �C, respectively. The elution
was performed by a 0.01M H2SO4 solution with the constant
1kbp
PHAD 1
phaB
PHAD 2
phaP phaR phaA phaE phaC
PHAD 7
rsam
PHAD 8PHADo1 PHADo2 PHADo7 PHADo8
PHBMo5 PHBMo6
Fig. 1 e The physical and genetic map of T. roseopersicina pha biosynthetic locus. The rsam gene is coding a protein for
radical S-adenosylmethionin superfamily. For the other genes see text. PCR primers PHADo1 and PHADo2 (upstream
homologous region) PHADo7 and PHADo8 (downstream homologous region) used for deleting the PHA biosynthetic genes
are also indicated. The PHBMo5 and PHBMo6 are PCR primers used for confirmation of the genotype of the strains (details in
Materials and Methods).
i n t e rn a t i o n a l j o u r n a l o f h y d r o g e n en e r g y 3 7 ( 2 0 1 2 ) 4 9 1 5e4 9 2 44918
flow of 0.8 ml min�1. Preceding the measurements, the
samples were filtered on a 0.2 mm pores size filter to avoid
column contamination.
2.8. PHA analysis
PHAwas quantified by a slightly modified acidic methanolysis
method of Braunegg et al. [29] using commercial PHB as
standard. PHB, methyl(S )-3-hydroxybutyrate (Me-3HB) (99%),
and benzoic acid (99.5%) were purchased from SigmaeAldrich
(St. Louis, USA). Chloroform was from Scharlau Chemia S.A.
(Sentmenat, Spain), methanol (HPLC grade) and sulfuric acid
96% was from Carlo Erba (Rodano, Italy).
The freeze dried cells were suspended in a mixture of 2 ml
methanol acidified with 10% sulfuric acid containing benzoic
acid (0.5 g L�1) as the internal standard.Themixturewasheated
in 10 ml hypovials sealed with PTFE caps at 100 �C for 4 h. The
sampleswere vortexed for 2min every hour, then cooled down
to room temperature and supplemented with 1 ml deionized
water and 1 ml chloroform. Finally, samples were vortexed
again for 2min and the organic phasewas used for subsequent
GC analysis [30]. 1 ml of the previously esterified sample was
loaded onto a Supelco Equity-1 capillary GC column. The inlet
and flame ionization detector temperatureswere set at 265 and
250 �C, respectively. The oven temperature program was the
following: the initial temperature was 50 �C, then it was
increased at a rate of 30 �C min�1 until 170 �C, followed by
a 99 �C min�1 temperature raise rate to 270 �C and kept the
temperature for 3 min. The inlet was operated in split mode at
265 �C, the constant flow rate was 11.8 ml min�1 with helium
carrier. Under these conditions, the retention times for the PHB
derivative (methyl 3-hydroxybutyric acid) and the benzoic acid
internal standard were 2.63 and 4.08 min, respectively. Cali-
bration curve for methyl(S )-3-hydroxybutyrate ester was
determined in the concentration range: 0.13e5.22 mg ml�1. The
PHA content of the samples was determined in 4 independent
parallel measurements.
2.9. Determination of in vivo hydrogen evolutionactivity
After changing the media to H2 production conditions, the T.
roseopersicina cultures (60 ml) were incubated in various
Pfennig media under argon atmosphere in sealed 125 ml
Hypo-Vial flasks. H2 production was followed by gas chro-
matography (Agilent 6890, capillarymolecular sieve 5 column,
TCD detector). Four replicates were done for each in vivo H2
evolution measurement.
2.10. Nitrogenase activity measurements in vitro
A modified acetylene reduction method was used [31]. Acety-
lene (up to 13% of the gas phase) was injected into a hypovial
bottle (60 ml) containing 30 ml of cells and flushed with Ar.
Then, N2 (up to 3% of the gas phase) was injected and the
hypovialswere incubated under light for 4 h. The ethylene and
acetylene content of the gas phase was determined by gas
chromatography (Shimadzu GC-2010 equipped with a HP-
PlotQ column and TCD detector. The inlet was operated at
200 �Candsplitmode (0.5:1)with 23.5mlmin�1 total flow.Oven
temperature was kept at 55 �C during the operation). Three
replicaswereused for eachnitrogenase activitymeasurement.
3. Results and discussion
3.1. PHA accumulation
Various photosynthetic bacteria are able to accumulate
considerable amounts of PHAs [12e17,32e34]. Similarly to the
heterotrophic bacteria [3,12], accumulation of PHAs in
photosynthetic bacteria is reversibly associated with nitrogen
availability in the growth medium [12,16].
Inorder to find theoptimalmediumfor PHAaccumulation in
T. roseopersicina, the concentrations of several small organic
compounds and thiosulfate have been varied in media con-
taining limited amounts of glutamate as nitrogen source (data
not shown). Acetatewas found as the best substrate similarly to
several other purple bacteria [12,13,34]. Analysis of the
biopolymers revealed that PHAs produced by T. roseopersicina
are copolymers composed of 3-hydroxybutyrate and 3-
hydroxyvalerate. The mol% of 3-hydroxyvalerate varied
between 5 and 41% depending on the growth conditions. The
highest yield of PHA was achieved in cells propagated on 10 g/l
of sodium acetate and 0.17 g/l sodium glutamate: T. rose-
opersicinaaccumulated30.5� 4%ofPHAofdry cellweight (DCW)
and the ratioof3-hydroxybutyrateand3-hydroxyvalerate in the
polymer was 84:16. This yield puts T. roseopersicina BBS into
i n t e r n a t i o n a l j o u r n a l o f h y d r o g e n en e r g y 3 7 ( 2 0 1 2 ) 4 9 1 5e4 9 2 4 4919
group of the best PHAproducing purple photosynthetic bacteria
grown on acetate [12]. No PHA accumulation was observed in
the presence of succinate, pyruvate and glucose.
3.2. Genes involved in PHA synthesis and degradation inT. roseopersicina
A genomic locus containing six genes coding for enzymes
involved in PHA biosynthesis was identified in the genome
sequence database of T. roseopersicina (unpublished data)
using the A. vinosum PhbC protein as query sequence (Fig. 1.).
All genes required for PHA biosynthesis in T. roseopersicina
were found in this locus. The genomic organization of these
genes was similar to that of A. vinosum [35]. A similar strategy
was used to find the gene coding for PHA depolymerase
( phaZ ) located in a distinct genomic locus.
In the PHA biosynthetic locus, the genes are localized in
two e oppositely oriented e gene clusters (Fig. 1). One cluster
consists of the phaARPB genes, which encode for b-ketothio-
lase (PhaA), P(3HA) synthesis regulatory protein (PhaR), P(3HA)
granule associated phasin (PhaP) and NADPH-dependent
acetoacetyl-CoA reductase (PhaB), respectively. There are
two inversely oriented genes: phaC- phaE which encode for
a two component P (3HB) synthase.
The deduced protein sequences of the phaARPB and phaCE
genes were compared to the corresponding protein sequences
in the Genbank. All gene products significantly resembled the
corresponding enzymes of various species (see below).
Generally, the similarity was highest to the corresponding
proteins of A. vinosum (Fig. 1).
The central enzymes involved the polyester formation are
the PHA synthases (PHASs) polymerizing the b-hydroxy fatty
acids into PHA biopolyesters. These enzymes are grouped into
four classes (classes IeIV) based on their subunit composition
and substrate specificity [36e38]. T. roseopersicina apparently
has a class III type heterodimer PHA synthase composed of
a polymerase and an “additional” subunit. These enzymes
dominantly occurring in g-Proteobacteria and in cyanobac-
teria prefer CoA thioesters of (R)-3-hydroxy fatty acids
comprising 3 to 5 carbon atoms [39,40].
Site directed mutagenesis of the A. vinosum PHA synthase
revelealed Cys-149, Asp-302 and His-331 are involved in
enzyme catalysis [41]. Moreover, substitution of the highly
conserved Trp425 by alanine strongly reduced the enzyme
activity in Ralstonia eutropha [42]. Trp425 has been suggested to
play a role in the dimerization of the PhaC subunits. These e
and many other conserved e residues could be clearly iden-
tified in T. rosepersicina PhaC protein, as well.
InA. vinosum, the functional type-III PHA synthase requires
both the PhaE and PhaC subunits [43], neither of the subunits
is active alone. In bacteria possessing a class III PHA synthase,
phaC and phaE are jointly organized in the genomes and most
probably constitute a single operon. This is likely in T. rose-
opersicina, as well. The resemblance among PhaC proteins was
more pronounced than among the PhaE proteins. The latter
“additional” subunit was dissimilar in the various PHA poly-
merases. However, they contained a C-terminal element
similar to the phasins suggesting that PhaE had a role in
binding the PHA synthases to the surface of PHA granules [44].
However, the exact function of PhaE is still ambiguous.
The second PHA related locus contains only the PHB
depolymerase gene ( phaZ ). PHA depolymerases are carbox-
ylesterases belonging to the a/b-hydrolase fold family [11].
Majority of the PHA depolymerases have few conserved
regions, such as the Ser-His-Asp catalytic triad, a GxSxG
sequence motif (known as ‘lipase box’) and a non-catalytic
histidine [11,45]. In addition to these regions, a so-called
oxyanion hole can be easily recognized, which might be
located N- or C-terminally relative to the lipase box (type I and
type II catalytic domains) [45,46]. The in silico analysis of the T.
roseopersicina PhaZ protein identified all conserved regions
listed above. The PHA Depolymerase Engineering Database
(DED, http://www.ded.uni-stuttgart.de; [47]) classified T. rose-
opersicina PhaZ as an extracellular dPHASCL depolymerasewith
a catalytic domain type 1, where the oxyanion hole was
located N-terminally from the lipase box. Sequence compar-
ison of PhaZ proteins showed that the T. roseopersicina enzyme
had the highest identity to the Xanthobacter autotrophicus Py2
(53%), Methylobacterium extorquens species (52%), Azotobacter
vinelandii DJ (48%) and A. vinosum DSMZ 180 (38%).
A careful search in the T. roseopersicina genome did not
identify any additional putative gene(s) involved in PHAs
synthesis and degradation.
3.3. Phylogeny of PhaC and PhaZ
The identity level of the PhaC and PhaE proteins of T. rose-
opersicina and A. vinosum involved in PHA biosynthesis (90 and
70%, see Fig. 1) was more pronounced than that of the PhaZ
enzymes (38%). This observation prompted us to further
investigate the codon usage and phylogeny of the related
genes/proteins. The PHA polymerase PhaC subunit and the
depolymerase PhaZ proteins were used as model sequences.
Codon adaptation index (CAI) provides information about
the age of a gene in the genome of a given organism. If a gene
is young in a given host (the gene acquiring event happened
relatively short time ago) it’s codon usage had no time to be
adapted to the preferred codon usage of the strain. Therefore,
these genes should have relatively lower CAI values. CAI
calculation for the phaC and phaZ did not reveal significant
differences in CAI value/the codon usage of these two genes,
therefore conclusions on the timing of potential gene transfer
events could not be made.
Phylogenetic trees were constructed for the PhaC and PhaZ
proteins. Representative sequences from each class of PHA
synthases were chosen according to Ref. [37] and the PhaZ
sequences were extracted from the same or closely related
strains. Phylogenetic trees were constructed for both proteins
following the protocol described in theMaterials andMethods.
Fig. 2A shows that the PhaC protein of T. roseopersicina forms
a branch with the following photosynthetic bacteria: A. vino-
sum, Thiocystis violacea and Thiorhodococcus drewsii. In the case
of the PhaZ proteins, the T. roseopersicina enzyme has the
closest relationship to the PhaZ of the non-photosynthesizing
Xanthobacter autotrophicus, M. extorquens and there are 4
branching points between the A. vinosum and T. roseoperscina
enzymes (Fig. 2B). The best identities values are much smaller
for the PhaZ (around 52e53%) than for the PhaC proteins
(86e90%). Moreover, the T. roseopersicina group of PhaC
proteins is branchedmuch earlier than that of the PhaZ group
Fig. 2 e Phylogenetic tree of PhaC (A) and PhaZ (B) proteins. Aerhyd: Aeromonas hydrophila, Agrotum: Agrobacterium
tumefaciens, Alvin: Allochromatium vinosum, Avine: Azotobacter vinelandii, Bameg: Bacillus megaterium, BacINT005: Bacillus sp.
INT005, Burcar: Burkholderia caryophylli, Caucre: Caulobacter crescentus CB15, Cauvib: Caulobacter vibrioides Chromovi:
Chromobacterium violaceum, Metex: Methylobacterium extorquens, Paden: Paracoccus denitrificans, PseaerC1, PseaerC2:
Pseudomonas aeruginosa PcaC1, PcaC2, PsepuC1, PsepuC2: Pseudomonas putida PcaC1, PcaC2, PsestuC2: Pseudomonas stutzeri
PcaC2, Raleu: Ralstonia eutropha, RaleuZ1, RaleuZ2, RaleuZ3, RaleuZ4,: Ralstonia eutropha PcaZ1,Z2,Z3,Z4, Rhocap:
Rhodobacter capsulatus, Rhospha: Rhodobacter sphaeroides, Rhodru: Rhodococcus ruber, Rhode: Rhodococcus equi, Rhoru:
Rhodospirillum rubrum, SynPCC6803: Synechocystis sp. PCC 6803, Thiro: Thiocapsa roseopersicina, Thivio: Thiocystis violacea,
Thiodr: Thiorhodococcus drewsii, Vibcho: Vibrio cholerae V51, Xauto: Xanthobacter autotrophicus.
i n t e rn a t i o n a l j o u r n a l o f h y d r o g e n en e r g y 3 7 ( 2 0 1 2 ) 4 9 1 5e4 9 2 44920
which is a very last branch on the rooted phylogenetic trees.
These observations clearly indicate the independent evolution
of the PHA anabolic and catabolic genes/enzymes.
3.4. Mutant analysis
Deletion of the locus ( phaARPB and phaCE genes) involved in
the alkanoate biosynthesis in. T. roseopersicina (PH12B strain)
was performed on a genetic background lacking all active
hydrogenases [22], whichwas named as DC12B strain, in order
to find out if the reducing power coming from PHB degrada-
tion can lead to nitrogen fixation coupled hydrogen produc-
tion (see Materials and Methods).
In T. roseopersicina, the removal of the PHA biosynthetic
locus totally eliminated the polyester from the cells. Under
PHA accumulation conditions both PH12B and DC12B strains
were able to grow in the presence of high concentration of
acetate (10 g/l sodium acetate) and the PH12B strain reached
even higher cell densities relative to the DC12B strain.
3.5. Hydrogen production from PHA
In order to study the PHA driven and nitrogenase mediated H2
production, it is reasonable to choose a strain lacking hydrog-
enases capable to take up hydrogen [48e50]. PHA degradation
was examined in DC12B and PH12B cell suspensions in the
absence of any additional external substrate (Fig. 3A.). First, the
cells were cultivated under PHA accumulating conditions then
themedia were replaced by carbon freemedia and the amount
of evolved H2 was analyzed after 5 days (see Materials and
Methods). Analysis of the H2 producing capacities of the cell
suspensions revealed approximately two times higher H2
production by the hydrogenase deficient DC12B cells relative to
the PH12B strain, which lacks both hydrogenase and PHA syn-
thase activity. In DC12B, about 50% of the H2 production is
clearly associated with the PHA degradation and it was most
accentuated during the first 48 h of the H2 production growth
mode (Fig. 3B). After 48 h the PHA decomposition stopped
(Fig. 3B open circle) and the biohydrogen production was
similar to that of the PH12B strain (Fig. 3A). PHA was not
detectable in the PH12B strain under the same conditions.
The nitrogenase activities of DC12B and PH12B were prac-
tically identical, indicating that nitrogenase activity was not
affected by the deletion of the PHA biosynthetic locus (Fig. 4,
open triangles and lozenges). Interestingly, the acetylene
reduction assay of the T. roseopersicina Mo-nitrogenase could
be performed only in the presence of N2. It should be noted
that there is no clear reason why N2 is required for acetylene
reduction. This is in contrast to the previous findings stating
that N2 and acetylene compete for a common or shared
binding site [51].
Therefore, the lower hydrogen evolving capacity of the
PHA biosynthesis mutant PH12B strain, relative to the corre-
sponding parental strain, might be attributed to the lack of
PHA in the PH12B strain. It is to be noted that this strain could
still produce some H2 although in the H2 production medium
Fig. 3 e The comparison of the nitrogenase catalyzed
hydrogen evolution and PHA consumption of the pha
containing (DC12B) and Dphastrains (PH12B) in the absence
and presence of thiosulphate. (A) Cumulative normalized
hydrogen production. (B) The normalized cellular PHB
content as a function of time during hydrogen production.
PHB extracted from PH12B was undetectable during
cultivation period. “DT” indicates the addition of
thiosulphate to the hydrogen producing medium.
Fig. 4 eNitrogenase activities of the pha containing (DC12B)
and Dphastrains (PH12B) in the absence and presence of
thiosulphate. “DT” indicates the addition of thiosulphate
to the hydrogen producing medium.
Fig. 5 e Thiosulfate consumption of the pha containing
(DC12B) and Dphastrains (PH12B) in the presence or
absence of succinate. “DS” and “DT” indicates the
addition of succinate and thiosulphate to the solution,
respectively.
i n t e r n a t i o n a l j o u r n a l o f h y d r o g e n en e r g y 3 7 ( 2 0 1 2 ) 4 9 1 5e4 9 2 4 4921
there are no external carbon and nitrogen sources available.
This residual H2 formation is most probably linked to the
utilization of other storage material(s), like glycogen or
elementary sulfur (S0).
Light dependence of the in vivo nitrogenase mediated H2
production was also tested. After the PHA accumulation step
half of the bottles were wrapped in aluminum foil and were
further incubated in the dark. Both DC12B and PH12B could
evolve H2 only under continuous illumination, no hydrogen
production was observed in the dark (data not shown).
3.6. Effect of thiosulfate and succinate on PHAconsumption and H2 production
In the purple nonsulphur bacterium, R. sulfidophilum succinate
was found as one of the best substrate for H2 production [52].
Later, it was also demonstrated that the conversion to H2 is
a little bit more efficient from PHB than from succinate [15].
These observations prompted us to investigate the effect of
succinate on PHA metabolism and nitrogenase mediated H2
production.
In T. roseopersicina, thiosulfate is the primary electron
source and it is one of the key compounds connected to
central redox pool and H2 metabolism [53,54]. Upon addition
of Na-thiosulfate, the thiosulfate utilization by DC12B was
significantly (around 40%) higher as compared to that of the
PH12B strain (Fig. 5, open squares and circles). Interestingly,
thiosulfate could stimulate the PHA utilization after 48 h
incubation and almost all PHA was consumed after 5 days
(Fig. 3B). The presence of thiosulfate substantially e but to
similar extente increased the acetylene reduction activities in
both strains which were diminished to the basic level at the
late incubation period. Finally, the H2 production was also
elevated by addition of thiosulfate in both strains. This effect
might be due to the following reasons: thiosulfate could
i n t e rn a t i o n a l j o u r n a l o f h y d r o g e n en e r g y 3 7 ( 2 0 1 2 ) 4 9 1 5e4 9 2 44922
(i) feed electrons to the nitrogenase via the quinone pool,
(ii) increase the in vitro nitrogenase activity and (iii) accelerate
the PHA decomposition yielding more electrons for H2 evolu-
tion. The molecular background of the interaction between
thiosulfate and PHA utilization is still unclear.
Addition of succinate to the PHA containing and Dpha cell
suspensions indicated that the nitrogenase mediated H2
production can be driven by succinate (Fig. 3A vs Fig. 6A,
open squares and triangles). Addition of succinate practi-
cally doubled the H2 evolution in both the DC12B and PH12B
T. roseopersicina strains, which was significantly weaker
effect than that of thiosulfate (>4x, see Fig. 3A). Supple-
mentation of succinate had moderate effect on thiosulfate
utilization (Fig. 5, compare filled squares to open ones and
filled circles to open ones) and PHA degradation (Fig. 6B, see
also Fig. 3B).
Fig. 6 e The comparison of the nitrogenase catalyzed
hydrogen evolution and PHA consumption of the pha
containing (DC12B) and Dphastrains (PH12B) in the
presence or absence of thiosulfate. (A) Cumulative
hydrogen evolution normalized to the cellular proteins. (B)
Specific PHB content as a function of time during hydrogen
production. PHB extracted from PH12B was undetectable
during hydrogen production period. “DS” and “DT”
indicates the addition of succinate and thiosulphate to the
solution, respectively.
Combined addition of thiosulfate and succinate had
proportional effect on H2 production which was around 7e8
times higher in these cultures than in the samples incubated
in carbon and thiosulfate free media (Fig. 6A, vs Fig. 3A).
From these experiments it can be concluded that e among
the compounds studied e thiosulfate is the best substrate for
biohydrogen production in T. roseopersicina. The strain still can
use both PHA and succinate for H2 evolution with similar
efficacy. Moreover, an interaction between the thiosulfate and
PHA metabolism could be observed which had a further
positive effect on H2 production.
4. Conclusions
T. roseopersicina BBS is suitable for studies of energy metabo-
lism in purple bacteria due to its metabolic versatility. Mining
in the genome sequence database of T. roseopersicina revealed
the presence of orfs coding for putative proteins showing
significant homology to the subunits of the gene products
involved in PHAs biosynthesis and degradation.
Both PHB accumulation and H2 evolution represent alter-
native ways for discharging excess reducing power and both
take place under unbalanced growth conditions [16,55]. The
results obtained in this study confirm that the T. roseopersicina
BBS (i) has the genes involved in PHAs biosynthesis and
degradation; (ii) the phylogeny of the PhaC and PhaZ proteins
is apparently distinct and indicates their different evolu-
tionary history; (iii) the strain is able to accumulate PHA (30.5%
of DCW); (iv) the stored PHA is good substrate for H2 produc-
tion in a two-stage process where the H2-producing phase is
separated from the PHA accumulating growth condition; (v) in
contrast to purple non-sulfur bacteria, this H2 evolution is
strictly light dependent; there is no PHA driven hydrogen
evolution in the dark (vi) addition of electron rich substrates,
e.g. thiosulphate, succinate to the H2-producing medium
substantially increases the H2 production by donating elec-
trons, by increasing the nitrogenase activity and via acceler-
ating the PHA degradation.
Acknowledgments
ThisworkwassupportedbyEUprojectsHyVolutionFP6-IP-SES6
019825 and FP7 Collaborative Project SOLAR-H2 FP7-Energy-
212508, and by domestic funds (GOP-1.1.2.-07/1-2008-0007,
TAMOP-4.2.1/B-09/1/KONV-2010-0005,Baross_DA07_DA_TECH-
07-2008-0012, andKN-RET-07/2005).TheSTSMfinancial support
for A. Fulop by COST 868 Action is appreciated.
r e f e r e n c e s
[1] Benemann JR. Hydrogen biotechnology: progress andprospects. Nat Biotechnol 1996;14:1101e3.
[2] Dawes EA. Storage polymers in prokaryotes. In: Mohan S,Daw C, Cole J, editors. Prokaryotic structure and function:a new perspective. Cambridge: University Press; 1992. p.81e122.
i n t e r n a t i o n a l j o u r n a l o f h y d r o g e n en e r g y 3 7 ( 2 0 1 2 ) 4 9 1 5e4 9 2 4 4923
[3] Anderson AJ, Dawes EA. Occurrence, metabolism, metabolicrole and industrial uses of bacterial polyhydroxyalkanoates.Microbiol Rev 1990;54:450e72.
[4] Melnicki MR, Eroglu E, Melis A. Changes in hydrogenproduction and polymer accumulation upon sulfur-deprivation in purple photosynthetic bacteria. Int J HydrogenEnergy 2009;34(15):6157e70.
[5] Steinbuchel A, Aerts K, Babel W, Follner C, Liebergesell M,Madkour MH, et al. Consideration on the structure andbiochemistry of bacterial polyhydroxyalkanoic acidinclusions. Can J Microbiol 1995;41:94e105.
[6] Pieper-Furst U, Madkour MH, Mayer F, Steinbuchel A.Purification and characterization of a 14-kilodalton proteinthat is bound to the surface of polyhydroxyalkanoic acidgranules in Rhodococcus ruber. J Bacteriol 1994;176:4328e37.
[7] Maehara A, Ueda S, Nakano H, Yamane T. Analyses ofa polyhydroxyalkanoic acid granule-associated 16-kilodaltonprotein and its putative regulator in the pha locus ofParacoccus denitrificans. J Bacteriol 1999;181:2914e21.
[8] Maehara A, Doi Y, Nishiyama T, Takagi Y, Ueda S, Nakano H,et al. PhaR, a protein of unknown function conserved amongshort-chain-length polyhydroxyalkanoic acid-producingbacteria, is a DNA binding protein and represses Paracoccusdenitrificans phaP expression in vitro. FEMS Microbiol Lett2001;200:9e15.
[9] Maehara A, Taguchi S, Nishiyama T, Yamane T, Doi Y. Arepressor protein, PhaR, regulates polyhydroxyalkanoate(PHA) synthesis via its direct interaction with PHA. J Bacteriol2002;184:3992e4002.
[10] Tokiwa Y, Calabia BP. Degradation of microbial polyesters.Biotechnol Lett 2004;26:1181e9.
[11] Jendrossek D, Handrick R. Microbial degradation ofpolyhydroxyalkanoates. Annu Rev Microbiol 2002;56:403e32.
[12] Liebergesell M, Hustede E, Timm A, Steinbuchel A, ClintonFuller R, Lenz RW, et al. Formation of poly(3-hydroxyalkanoates) by phototrophic and chemolithotrophicbacteria. Arch Microbiol 1991;155:415e21.
[13] Brandl H, Gross RA, Lenz RW, Lloyd R, Clinton Fuller R. Theaccumulation of poly (3-hydroxyalkanoates) in Rhodobactersphaeroides. Arch Microbiol 1991;155:337e40.
[14] Maeda I, Idehara K, Okayama N, Miura Y, Yagi K,Mizoguchi T. Poly(3-hydroxybutyrate) as an endogeneoussubstrate for H2 evolution in Rhodovulum sulfidophilum.Biotechnol Lett 1997;19:1209e12.
[15] Maeda I, Miyasaka H, Umeda F, Kawase M, Yagi K.Maximization of hydrogen production ability in high-Densitysuspension of Rhodovulum sulfidiphilum cells usingintracellular poly (3-hydroxybutyrate) as sole substrate.Biotechnol Bioeng 2002;81:474e81.
[16] De Philippis R, Ena A, Guastini M, Sili C, Vincenzini M.Factors affecting poly-b-hydroxybutyrate accumulation incyanobacteria and in purple non-sulfur bacteria. FEMSMicrobiol Rev 1992;103:187e94.
[17] Hustede E, Steinbuchel A, Schlegel HG. Relationship betweenthe photoproduction of hydrogen and the accumulation ofPHB in nonsulphur purple bacteria. Appl MicrobiolBiotechnol 1993;39:87e93.
[18] Colbeau A, Kovacs KL, Chabert J, Vignais PM. Cloning andsequencing of the structural (hupSLC ) and accessory(hupDHI ) genes for hydrogenase biosynthesis in Thiocapsaroseopersicina. Gene 1994;140:25e31.
[19] Rakhely G, Colbeau A, Garin J, Vignais PM, Kovacs KL.Unusual organization of the genes coding for HydSL, thestable [NiFe] hydrogenase in the photosynthetic bacteriumThiocapsa roseopersicina BBS. J Bacteriol 1998;180:1460e5.
[20] Rakhely G, Kovacs AT, Maroti G, Fodor BD, Csanadi G,Latinovics D, et al. Cyanobacterial type, heteropentameric,NADþ reducing [NiFe] hydrogenase in the purple sulfur
photosynthetic bacterium, Thiocapsa roseopersicina. ApplEnviron Microbiol 2004;70:722e8.
[21] Maroti J, Farkas A, Nagy IK, Maroti G, Kondorosi E, Rakhely G,et al. A second soluble Hox-type NiFe enzyme complete thehydrogenase set in Thiocapsa roseopersicina BBS. Appl EnvironMicrobiol 2010;76(15):5113e23.
[22] Maroti G, Fodor BD, Rakhely G, Kovacs AT, Arvani S,Kovacs KL. Accessory proteins functioning selectively andpleiotropically in the biosynthesis of [NiFe] hydrogenases inThiocapsa roseopersicina. Eur J Biochem 2003;270:2218e27.
[23] Pfennig N, Truper HG. The family Chromatiaceae. In:Balows A, Truper HG, Dworkin MW, Harder, Schleifer KH,editors. The prokaryotes. Berlin: Springer; 1991. p. 3200e21.
[24] Sambrook J, Fritsch EF, Maniatis T. Molecular cloning:a laboratory manual. 2nd ed. New York: Cold Spring Harbor;1989.
[25] Ausubel FM, Brent R, Kingston RE, Moore DD, Seidman JG,Smith JA, et al. Current protocols in molecular biology. NewYork: Wiley; 1996.
[26] Notredame C, Higgins D, Heringa. T-Coffee: a novel methodfor multiple sequence alignments. J Mol Biol 2000;302(1):205e17.
[27] Guindon S, Dufayard JF, Lefort V, Anisimova M, Hordijk W,Gascuel O. New algorithms and methods to estimatemaximum-likelihood phylogenies: assessing theperformance of PhyML 3.0. Syst Biol 2010;59:307e21.
[28] Schafer A, Tauch A, Jager W, Kalinowski J, Thierbach G,Puhler A. Small mobilizable multi-purpose cloning vectorsderived from the Escherichia coli plasmids pK18 and pK19:selection of defined deletions in the chromosome ofCorynebacterium glutamicum. Gene 1994;145:69e73.
[29] Braunegg G, Sonnleitner B, Lafferty RM. A rapid gaschromatographic method for the determination of poly-b-hydroxybutyric acid in microbial biomass. Eur J ApplMicrobiol Biotechnol 1978;6:29e37.
[30] Betancourt A, Yezza A, Halasz A, Trea HV, Hawari J. Rapidmicrowave assisted esterification method for the analysis ofpoly-3-hydroxybutyrate in Alcaligenes latus by gaschromatography. J Chrom 2007;1154:473e6.
[31] Stewart WDP, Fitzgerald GP, Burris RH. In situ studies on N2
fixation using the acetylene reduction technique. Proc NatlAcad Sci USA 1967;58:2071e8.
[32] Kranz RG, Gabbert KK, Locke TA, Madigan MT.Polyhydroxyalkanoate production in Rhodobacter capsulatus:genes, mutants, expression, and physiology. Appl EnvironMicrobiol 1997;63:3003e9.
[33] Mas J, Van Gemerden H. Storage products in purple andgreen sulfur bacteria. In: Blankenship R, Madigan M, Bauer C,editors. Anoxygenic photosynthetic bacteria. Dordrecht:Kluwer; 1995. p. 973e90.
[34] Khatipov E, Miyake J, Asada Y. Accumulation of poly-b-hydroxybutyrate by Rhodopseudomonas sphaeroides on variouscarbon and nitrogen substrates. FEMS Microbiol Lett 1998;162:39e45.
[35] Liebergesell M, Steinbuchel A. Cloning and nucleotidesequence of genes relevant for biosynthesis ofpolyhydroxyalkanoic acid in Chromatium vinosum strain D.Eur J Biochem 1992;209:135e50.
[36] Rehm BHA, Steinbuchel A. Biochemical and genetic analysisof PHA synthases and other proteins required for PHAsynthesis. Int J Biol Macromol 1999;25:3e19.
[37] Rehm BHA. Polyester synthases: natural catalysts forplastics. Biochem J 2003;376:15e33.
[38] Solaiman DKY, Ashby RD. Rapid genetic characterization ofpoly (hydroxyalkanoate) synthase and its applications.Biomacromolecules 2005;6:532e7.
[39] Yuan W, Jia Y, Tian J, Snell KD, Muh U, Sinskey AJ, et al. ClassI and III polyhydroxyalkanoate synthases from Ralstonia
i n t e rn a t i o n a l j o u r n a l o f h y d r o g e n en e r g y 3 7 ( 2 0 1 2 ) 4 9 1 5e4 9 2 44924
eutropha and Allochromatium vinosum: characterization andsubstrate specificity studies. Arch Biochem Biophys 2001;394:87e98.
[40] Hai T, Hein S, Steinbuchel A. Multiple evidence forwidespread and general occurrence of type-III PHAsynthases in cyanobacteria and molecular characterizationof the PHA synthases from two thermophilic cyanobacteria:Chlorogloeopsis fritschii PCC 6912 and Synechococcus sp. strainMA19. Microbiology 2001;147:3047e60.
[41] Jia Y, Kappock TJ, Frick T, Sinskey AJ, Stubbe J. Lipasesprovide a new mechanistic model for polyhydroxybutyrate(PHB) synthases: characterization of the functional residuesin Chromatium vinosum PHB synthase. Biochemistry 2000;39:3927e36.
[42] Gerngross TU, Snell KD, Peoples OP, Sinskey AJ, Csuhai E,Masamune S, et al. Overexpression and purification of thesoluble polyhydroxyalkanoate synthase from Alcaligeneseutrophus: evidence for a required posttranslationalmodification for catalytic activity. Biochemistry 1994;33:9311e20.
[43] Muh U, Sinskey AJ, Kirby DP, Lane WS, Stubbe J. PHAsynthase from Chromatium vinosum: Cys 149 is involved incovalent catalysis. Biochemistry 1999;38:826e37.
[44] Liebergesell M, Rahalkar S, Steinbuchel A. Analysis of theThiocapsa pfennigiipolyhydroxyalkanoate synthase: subcloning,molecular characterization and generation of hybrid synthaseswith the corresponding Chromatium vinosum enzyme. ApplMicrobiol Biotechnol 2000;54:186e94.
[45] Jaeger KE, Steinbuchel A, Jendrossek D. Substratespecificities of bacterial polyhydroxyalkanoatedepolymerases and lipases: bacterial lipases hydrolyze poly(omega-hydroxyalkanoates). Appl Environ Microbiol 1995;61:3113e8.
[46] BehrendsA,Klingbeil B, JendrossekD.Poly (3-hydroxybutyrate)depolymerases bind to their substrate by a C-terminal locatedsubstrate binding site. FEMSMicrobiol Lett 1996;143:191e4.
[47] Knoll M, Hamm TM, Wagner F, Martinez V, Pleiss J. The PHAdepolymerase engineering database: a systematic analysistool for the diverse family of polyhydroxyalkanoate (PHA)depolymerases. BMC Bioinform 2009;10:89.
[48] Kars G, Gunduz U, Rakhely G, Ycel M, Ero�glu _I, Kovacs LK.Improved hydrogen production by hydrogenase deficientmutant strain of Rhodobacter sphaeroides O.U.001. Int JHydrogen Energy 2008;33:3056e60.
[49] Kars G, Gunduz U, Yucel M, Rakhely G, Kovacs LK, Ero�glu _I.Evaluation of hydrogen production by Rhodobacter sphaeroidesO.U.001 and its hupSL deficient mutant using acetate andmalate as carbon sources. Int J Hydrogen Energy 2009;34:2184e90.
[50] Kars G, Gunduz U. Towards a super H2 producer:improvements in photofermentative biohydrogenproduction by genetic manipulations. 2010;35:6646e6656.
[51] Kim CH, Newton WE, Dean DR. Role of the MoFe proteinalpha-subunit histidine-195 residue in FeMo-cofactorbinding and nitrogenase catalysis. Biochemistry 1995;34:2798e808.
[52] Maeda I, Chowdhury WQ, Idehara K, Yagi K, Mizoguchi T,Akano T, et al. Improvement of substrate conversion tomolecular hydrogen by three-stage cultivation ofa photosynthetic bacterium, Rhodovulum sulfidophilum.Appl Biochem Biotechnol 1998;70e72:301e10.
[53] Rakhely G, Laurinavichene TV, Tsygankov AA, Kovacs KL.The role of Hox hydrogenase in the H2 metabolism ofThiocapsa roseopersicina. Biochim Biophys Acta 2007;1767:671e6.
[54] Laurinavichene TV, Rakhely G, Kovacs KL, Tsygankov AA.The effect of sulfur compounds on H2 evolution/consumption reactions, mediated by various hydrogenases,in the purple sulfur bacterium, Thiocapsa roseopersicina. ArchMicrobiol 2007;188:403e10.
[55] Steinbuchel A. Polyhydroxyalkanoaic acids. In: Byrom D,editor. Biomaterials: novel materials from biological sources.New York: Stockton Press; 1991. p. 124e213.
[56] Bogorov LV. The properties of Thiocapsa roseopersicina, strainBBS, isolated from an estuary of the White Sea.Mikrobiologija 1974;43:326e32.
[57] Herrero M, Lorenzo V, Timmis KN. Transposon vectorscontaining non-antibiotic resistance selection markers forcloning and stable chromosomal insertion of foreign genesin gram-negative bacteria. J Bacteriol 1990;172:6557e67.