pusillimonas sp. 5hp degrading 5-hydroxypicolinic acid
TRANSCRIPT
ORIGINAL PAPER
Pusillimonas sp. 5HP degrading 5-hydroxypicolinic acid
Laimonas Karvelis • Renata Gasparaviciut _e •
Algirdas Klimavicius • Regina Jancien _e •
Jonita Stankeviciut _e • Rolandas Meskys
Received: 27 September 2012 / Accepted: 25 March 2013
� Springer Science+Business Media Dordrecht 2013
Abstract A bacterial strain 5HP capable of degrading
and utilizing 5-hydroxypicolinic acid as the sole source
of carbon and energy was isolated from soil. In addition,
the isolate 5HP could also utilize 3-hydroxypyridine
and 3-cyanopyridine as well as nicotinic, benzoic and
p-hydroxybenzoic acids for growth in the basic salt media.
On the basis of 16S rRNA gene sequence analysis, the
isolate 5HP was shown to belong to the genus Pusilli-
monas. Both the bioconversion analysis using resting cells
and the enzymatic assay showed that the degradation of
5-hydroxypicolinic acid, 3-hydroxypyridine and nicotinic
acid was inducible and proceeded via formation of the
same metabolite, 2,5-dihydroxypyridine. The activity of a
novel enzyme, 5-hydroxypicolinate 2-monooxygenase,
was detected in the cell-free extracts prepared from
5-hydroxypicolinate-grown cells. The enzyme was par-
tially purified and was shown to catalyze the oxidative
decarboxylation of 5-hydroxypicolinate to 2,5-dihydr-
oxypyridine.Theactivity of 5-hydroxypicolinate2-mono-
oxygenase was dependent on O2, NADH and FAD.
Keywords 5-Hydroxypicolinic acid �3-Hydroxypyridine � Degradation �3-Hydroxypyridine � 5-Hydroxypicolinate
2-monooxygenase � Pusillimonas
Introduction
The pyridine ring is a major constituent of natural
compounds including plant alkaloids, coenzymes and
antibiotics. Pyridine and its derivatives are used as
dyes, industrial solvents, herbicides, and pesticides.
The biodegradation of pyridine-containing com-
pounds has been studied intensively (Houghton and
Cain 1972; Kaiser et al. 1996; Fetzner 1998; Brandsch
2006; Li et al. 2010).
Catabolism of pyridine, especially the initial steps
of hydroxylation of monocarboxylated pyridines such
as 2-carboxypyridine (picolinic acid) (Tate and
Ensign 1974; Siegmund et al. 1990; Kiener et al.
1993), 3-carboxypyridine (nicotinic acid) (Nagel and
Andreesen 1989; Jimenez et al. 2008), and 4-carb-
oxypyridine (isonicotinic acid) (Singh and Shukla
1986) have been studied in detail. Nicotinate dehy-
drogenases, enzymes that catalyze the hydroxylation
of nicotinate, were purified from Bacillus niacini
(Nagel and Andreesen 1990), Pseudomonas fluores-
cens TN5 (Hurh et al. 1994), Eubacterium barkeri
(Gladyshev et al. 1996) and Ralstonia/Burkholderia
strain DSM 6920 (Schrader et al. 2002). In addition,
such enzymes as isonicotinate dehydrogenase and
L. Karvelis � R. Gasparaviciut _e � J. Stankeviciut _e �R. Meskys (&)
Department of Molecular Microbiology and
Biotechnology, Institute of Biochemistry, Vilnius
University, Mokslininku 12, LT-08662 Vilnius, Lithuania
e-mail: [email protected]
A. Klimavicius � R. Jancien _eDepartment of Bioorganic Compounds Chemistry,
Institute of Biochemistry, Vilnius University,
Mokslininku 12, LT-08662 Vilnius, Lithuania
123
Biodegradation
DOI 10.1007/s10532-013-9636-3
picolinic acid 6-hydroxylase have been purified from
Mycobacterium sp. INA1 (Kretzer et al. 1993) and
Arthrobacter picolinophilus (Tate and Ensign 1974)
respectively. Moreover, it was shown that in Alcalig-
enes sp. strain UK21 6-hydroxypicolinic acid may be
also formed via conversion of quinolinic acid (Uchida
et al. 2003).
The microbial conversion of hydroxylated carb-
oxypyridines, particularly catabolism of hydroxypi-
colinic acids, has been less studied. The first step in the
degradation of nicotinic acid by both aerobic and
anaerobic organisms appears to be the same, i.e., the
formation of 6-hydroxynicotinic acid, but thereafter
the pathways diverge (Kaiser et al. 1996). The
anaerobic bacteria degrade 6-hydroxynicotinate by
reducing pyridine ring via formation of 1,4,5,6-
tetrahydro-6-oxonicotinate (Alhapel et al. 2006).
Bacillus and Pseudomonas spp. degrade 6-hydroxy-
nicotinate by an oxidative decarboxylation producing
2,5-dihydroxypyridine (Nagel and Andreesen 1990;
Nakano et al. 1999; Jimenez et al. 2008). The ring of
2,5-dihydroxypyridine is then cleaved oxidatively to
yield maleamic and formic acids (Jimenez et al. 2008).
The cells of the Bacillus sp. oxidize nicotinic acid via
6-hydroxynicotinic acid, 2,6-dihydroxynicotinic acid
and 2,3,6-trihydroxypyridine followed by ring cleav-
age and the formation of maleamic acid (Ensign and
Rittenberg 1964; Hirschberg and Ensign 1971). Such
compounds as 6-hydroxypicolinic, 3,6-dihydroxypi-
colinic acids and 2,5-dihydroxypyridine have been
detected as the main metabolites during picolinic acid
biodegradation by Bacillus sp. (Shukla 1975). How-
ever, the enzymes involved in conversion of 6-hy-
droxypicolinic acid have not been characterized so far.
The 5-hydroxypicolinic acid is a natural product
produced by Nocardia spp. (Makar’eva et al. 1989).
Some antibiotics, such as rubradirin and nikkomycin,
contain the fragment of 5-hydroxypicolinic acid (Kim
et al. 2008; Moon and van Lanen 2010). The hydroxy
derivatives of picolinic acid can be formed by
degradation of aminophenols (He and Spain 2000).
However, no data concerning microorganisms capable
to utilize 5-hydroxypicolinic acid or enzymes involved
in catabolism of this compound has been pub-
lished yet.
Oxidoreductases exhibiting the chemo- and regio-
selective hydroxylation of the pyridine ring represent a
perspective new and mild synthetic route to substi-
tuted pyridinols, many of which are potential drugs or
agrochemicals. (Yoshida and Nagasawa 2000; Wang
et al. 2005; Garrett et al. 2006). In this study, the
isolation and characterization of a new 5-hydroxypi-
colinic acid-degrading bacterium belonging to the
genus Pusillimonas is presented. A novel enzyme,
5-hydroxypicolinate 2-monooxygenase, catalyzing
the oxidative decarboxylation of 5-hydroxypicolinate
to 2,5-dihydroxypyridine is described.
Materials and methods
Chemicals
Picolinic, 3-hydroxypicolinic, 6-hydroxypicolinic,
nicotinic, 6-hydroxynicotinic acids, 5-hydroxy-2-
methylpyridine, 3-hydroxypyridine were obtained
from Merck. Phenazine methosulphate (PMS), 2,6-
dichloroindophenol (DCPIP), nitro blue tetrazole
(NBT) and cytochrome c were from Sigma-Aldrich.
5-Hydroxypicolinic acid was from Apollo Scientific.
5-Hydroxy-2-methylpyridine was synthesized accord-
ing to Iqbal et al. (2009). 2,5-Dihydroxypyridine was
synthesized according to Behrman and Pitt (1958).
Media and growth conditions
For the bacteria isolation, mineral salt medium (MSM)
was used: (grams per liter) 8.8 KH2PO4, 1.0
(NH4)2SO4, the final pH was adjusted to 7.2. After
autoclaving (121 �C, 30 min) and cooling, the med-
ium was supplemented with (grams per liter) 0.15
MgSO4�7H2O and salt solution (10 ml per liter). Salt
solution (g/l): CaCl2�2H2O 2.0, MnSO4�4H2O 1.0,
FeSO4�7H2O 0.5, Na2MoO4�2H2O 0.5, all compo-
nents were dissolved in 0.1 N HCl.
For enzyme assay and biodegradation studies the
bacteria were grown in MSMYP medium (MSM
supplemented with (grams per liter) 0.9 yeast extract,
1.0 peptone, 0.6 beef extract) containing 0.15 % of the
appropriate substrate. After cultivation biomass was
collected by centrifugation (6,0009g, 10 min),
washed with 0.9 % NaCl and frozen (-20 �C) until
further use.
Screening of bacterial strains
Samples of soils were cultivated aerobically in 125 ml
flask containing 30 ml of MSM supplemented with
Biodegradation
123
5-hydroxypicolinic acid (1.5 g/l). Samples were incu-
bated in orbital shaker (180 rpm) at 30 �C for at least
4 days. Then 1 ml of the dispersed soil suspension was
transferred to flasks containing the fresh medium
supplemented with the same substrate and incubated
for an additional 4 days under the same conditions.
After cultivation, the aliquots were diluted and spread
on the MSM agar plates containing 0.15 % of
5-hydroxypicolinic acid. Colonies were selected and
purified by streaking repeatedly on the Nutrient agar
medium and the MSM agar plates containing 0.15 %
of 5-hydroxypicolinic acid.
Identification of a 5-hydroxypicolinic acid
degrading strain
DNA was extracted according to Woo et al. (1992).
The gene for 16S rRNA was amplified using universal
primers w001 and w002 (Godon et al. 1997). The PCR
product was purified using a DNA purification kit and
cloned into pTZ57R/T plasmid (Thermo Fisher Sci-
entific, Lithuania). The cloned DNA fragment was
sequenced at the Sequencing Centre of Institute of
Biotechnology, Vilnius University Lithuania.
Bioconversion using whole cells
The strain 5HP was grown in MSM medium supple-
mented with 0.15 % of an appropriate substrate
aerobically at 30 �C for 4 days. Cells were harvested
(6,0009g, 10 min), washed twice in 0.9 % NaCl.
Bioconversion was performed in 50 mM potassium
phosphate buffer, pH 7.2, containing 0.15 mM of
substrate. The cells were suspended in this solution and
the suspension was incubated aerobically at 25 �C. The
buffer solution containing the appropriate compound
without cells and a cell suspension without the
compound served as controls. Following the centrifu-
gation to remove the cells, the bioconversion was
estimated by recording absorbance at 220–360 nm at
regular time intervals.
Enzyme assays
The cell-free extracts were prepared by suspending cell
paste in 50 mM potassium phosphate buffer, pH 7.2. The
cells were broken by ultrasonic treatment 30 s at 22 kHz.
The cell debris was removed by centrifugation (13,0009g,
5 min). 2,5-Dihydroxypyridine 5,6-dioxygenase activity
was measured at 30 �C spectrophotometrically at 320 nm
(e320 = 5,200 cm-1 M-1) as described previously
(Jimenez et al. 2008) with modifications. The reaction
mixture contained: 50 mM potassium phosphate buffer
(pH 7.2), 0.05 mM 2,5-dihydroxypyridine, 0.005 mM
FeSO4, and an appropriate amount of protein or cell-free
extract in a total volume of 1 ml. One unit of activity was
defined as the amount of enzyme that catalyzed the
disappearance of 1 lmol of 2,5-dihydroxypyridine in
1 min. Activities of nicotinate dehydrogenase and
6-hydroxynicotinic acid 3-hydroxylase were analyzed as
described previously (Jimenez et al. 2008). One unit of
activity was defined as the amount of enzyme necessary to
oxidize 1 lmol of substrate per min. Activity of 5-hy-
droxypicolinate 2-monooxygenase was analyzed spectro-
photometrically at 340 nm (e340 = 6,200 cm-1 M-1) in
50 mM potassium phosphate buffer, pH 7.2 containing
1 mM FAD and 0.15 mM NADH at 30 �C. One unit of
activity was defined as the amount of enzyme necessary to
oxidize 1 lmol of NADH per min.
Purification of 5-hydroxypicolinate
2-monooxygenase
The cells were harvested by centrifugation and
suspended in 20 mM potassium phosphate buffer pH
7.0, and the cell extracts were prepared by ultrasonic
treatment as described previously. The cell extracts
from a 100-ml culture were purified using ToyoSreen
AF-Blue-650 M 5 ml column. The column was
equilibrated with 20 mM potassium phosphate buffer,
pH 7.0, and the proteins were adsorbed with the same
buffer. Elution was performed in two steps. Initially,
the column was washed with 10 ml of binding buffer
containing 20 % of sucrose. Then proteins were eluted
with 5 ml of binding buffer. The fractions containing
the active enzyme were pooled, concentrated by
ultrafiltration and applied to a 5 9 200 mm column
containing Source 15PHE resin (GE Healthcare). The
enzyme was eluted with a linear gradient of 0–0.5 M
of NaCl in 20 mM potassium phosphate buffer pH 7.2.
The fractions containing the active enzyme were
pooled and concentrated by ultrafiltration.
Zymography analysis
The samples were resolved by gel electrophoresis
at room temperature on a 10 % non-denaturing
polyacrylamide gel. After electrophoresis, the gels
Biodegradation
123
were washed with 20 mM potassium phosphate buffer
pH 7.2. Then 20 mM potassium phosphate buffer pH
7.2 containing 0.2 mM 5-hydroxypicolinic acid,
0.01 mM NADH, 0.005 mM PMS and 0.3 mM NBT
was poured onto the gel. The results were recorded
after incubation at 25 �C for 3 h. The reaction mixture
without 5-hydroxypicolinic acid served as a control.
De novo sequencing of proteins
Protein bands were visualized by staining the gel with
Coommassie Blue R250 and excised from the gel
using a razor blade. Each sample was purified as
described previously (Hellman et al. 1995). Tryptic-
digest from each gel slice was analyzed by 4000
QTRAP (AB SCIEX) mass spectrometry in linear ion
trap mode using information dependent acquisition
(IDA) and dynamic exclusion protocol. The acquisi-
tion method consisted of an IDA scan cycle including
the enhanced mass scan (EMS) as the survey scan,
enhanced resolution scan (ER) to confirm charge state
and six dependent enhanced product ion (EPI) scans
(MS/MS). With the threshold of the ion intensity at
100,000 counts per second (cps), the IDA criteria were
set to allow the most abundant ions in the EMS scan to
trigger EPI scans. Survey MS scan was set to mass
range from 400 to 1,400 m/z. Dynamic ion exclusion
was set to exclude precursor ions after their two
occurrences during 60s interval. Peak lists were
generated using Analyst software 1.4.2 (AB/Sciex,
USA).
LC–MS analysis
To the samples of medium or enzymatic reaction the
same volume of acetonitrile was added. The insoluble
particles were removed by centrifugation (15,0009g,
15 min). Liquid chromatography-mass spectrometry
(LC–MS) analyses were performed using HPLC
system (CBM-20A controller, two LC-2020AD
pumps, SIL-30AC auto sampler and CTO-20AC
column oven; Shimadzu, Japan) equipped with pho-
todiode array (PDA) detector (SPD-M20A Promi-
nence diode array detector; Shimadzu, Japan) and
mass spectrometer (LCMS-2020, Shimadzu, Japan)
equipped with an ESI source. The chromatographic
separation was conducted using a Hydrosphere C18
column, 4 9 150 mm2 (YMC, Japan) at 40 �C and a
mobile phase that consisted of 0.1 % formic acid
(solvent A) and methanol (solvent B) delivered in
gradient elution mode at a flow rate of 0.6 mL min-1.
The elution programme used was as follows: isocratic
0 % B for 0.5 min, from 0 to 60 % B over 4.5 min,
isocratic 60 % B for 0.1 min, from 60 to 0 % B over
0.1 min, isocratic 0 % B for 5 min. Mass scans were
measured from m/z 10 up to 500, at 350 �C interface
temperature, 250 �C DL temperature, ±4,500 V
interface voltage, neutral DL/Qarray, using N2 as
nebulizing and drying gas. Mass spectrometry data
was acquired in both the positive and in the negative
ionization mode. The data was analyzed using Lab-
Solutions LCMS software.
Nucleotide sequence accession number
and bioinformatical analysis
Phylogenetic and molecular evolutionary analyses
were conducted using MEGA version 5.05 (Tamura
et al. 2011). The DNA sequence has been deposited in
GenBank and can be accessed via the accession
number KC602498.
Results
Isolation and identification of bacterium capable
of utilizing 5-hydroxypicolinic acid
Several bacterial isolates from different soil samples
were screened for their ability to grow on a mineral
medium supplemented with 5-hydroxypicolinic acid.
The isolate 5HP producing a dark pigment when
grown on solid medium containing 5-hydroxypicoli-
nic acid was selected for further studies. The analysis
of 16S rRNA gene sequence revealed that the strain
5HP was related to Pusillimonas species and, together
with Pusillimonas noertemannii BN9 and Pusillimon-
as sp. N11, formed a distinct branch on a phylogenetic
tree (Fig. 1).
To determine the substrate range capability of
Pusillimonas sp. 5HP, a number of aromatic com-
pounds were tested as potential growth substrates. The
growth was analyzed both on solid and in liquid
media. The growth test revealed that the strain utilized
5-hydroxypicolinic acid as the single carbon and
energy source (Fig. 2). LC–MS analysis confirmed the
depletion of 5-hydroxypicolinic acid, and \15 % of
the initial substrate concentration was detected in the
Biodegradation
123
medium after 86 h of cultivation. Nicotinic, 6-hydroxy-
nicotinic, benzoic and p-hydroxybenzoic acids as
well as 3-hydroxypyridine, 2,5-dihydroxypyridine and
3-cyanopyridine also served as growth substrates for
Pusillimonas sp. 5HP. The other tested pyridine deriv-
atives, such as 5-hydroxy-2-methylpyridine, 5-hydroxy-
2-hydroxymethylpyridine, 5-hydroxy-2-cyanopyridine
or picolinic, 3-hydroxypicolinic, 6-hydroxypicolinic,
2-hydroxynicotinic, and isocinchomeronic acids, did not
support the growth of Pusillimonas sp. 5HP. The growth
of Pusillimonas sp. 5HP on 5-hydroxypicolinate and
3-hydroxypyridine containing media was accompanied by
an accumulation of a green pigment, which gradually
turned dark brown suggesting the formation of 2,5-
dihydroxypyridine and its subsequent spontaneous auto-
oxidation (Khanna and Shukla 1977; Karvelis and Meskys
2004).
Bioconversions using the whole cells
The conversion of 5-hydroxypicolinic acid, 3-hydroxy-
pyridine, nicotinic acid and 2,5-dihydroxypyridine by
the resting cells of Pusillimonas sp. 5HP pre-grown in
the presence of the appropriate compound was observed.
In contrast, no bioconversion was detected in non-
induced control cells under the same conditions and
time. The 5-hydroxypicolinic acid-induced cells pre-
cultivated for 40–86 h catabolized 5-hydroxypicolinic
acid (18.2 mmol h-1 mg-1 of biomass) and 2,5-dihydr-
oxypyridine (12.7 mmol h-1 mg-1 of biomass) but did
not convert nicotinic acid. The 3-cyanopyridine-induced
cells could metabolize 3-cyanopyridine, nicotinamide,
nicotinic and 6-hydroxynicotinic acids and 2,5-dihydr-
oxypyridine without a lag period by the rate of 1.85,
1.68, 1.06, 1.04 and 0.9 mmol h-1 mg-1 of biomass,
respectively. The nicotinic acid-induced cells con-
verted the same compounds, except 3-cyanopyridine.
Pusillimonas sp. 5HP pre-grown in the presence of
3-hydroxypyridine could utilize 3-hydroxypyridine and
2,5-dihydroxypyridine only by the rate of 0.6 and 0.9
mmol h-1 mg-1 of biomass, respectively. These results
showed that the induction of enzymes catalyzing
utilization of pyridine compounds requires the presence
of the appropriate substrate. Since 3-hydroxypyridine,
3-cyanopyridine, 5-hydroxypicolinate and nicotinate-
Fig. 1 Unrooted tree
showing the phylogenetic
relationships between 5HP
and related Pusillimonasspecies. The tree was
constructed using the
neighbour-joining method
based on a comparison of
*1,600 nucleotides. The
bar represents difference in
one nucleotide per 200 bp
Fig. 2 Growth of Pusillimonas sp. strain 5HP in MSMYP
medium with (closed circles) and without 5-hydroxypicolinic
acid (open circles). Squares concentration of 5-hydroxypicol-
inic acid in the cultivation medium
Biodegradation
123
grown cells consumed 2,5-dihydroxypyridine, it was
proposed that this compound is an intermediate metab-
olite generated during the degradation pathways of
pyridine derivatives listed above.
Enzyme assay
2,5-Dihydroxypyridine 5,6-dioxygenase, which is
crucial for catabolism of 2,5-dihydroxypyridine, had
been previously detected in various pyridine deriva-
tives-degrading bacteria (Gauthier and Rittenberg
1971a, b; Kaiser et al. 1996; Jimenez et al. 2008;
Tang et al. 2012). To test the ability of Pusillimonas
sp. 5HP to induce the production of the analogous
enzyme, the cell-free extracts obtained from 5-hy-
droxypicolinate, 3-hydroxypyridine, 3-cyanopyridine,
and nicotinate-grown-Pusillimonas sp. 5HP were
analyzed for their ability to oxidize 2,5-dihydroxy-
pyridine in the presence of Fe(II) ions. The test
revealed that 2,5-dihydroxypyridine was consumed by
all crude extracts, and the highest activity of 2,5-
dihydroxypyridine 5,6-dioxygenase was detected in
the nicotinic acid-induced cells (Table 1). The cells
grown in the presence of nicotinic acid and 3-cyano-
pyridine also showed the activity of nicotinate dehy-
drogenase, but only if potassium ferricyanide, PMS
(DCPIP), NBT or cytochrome c was used as an
electron acceptor. The activity of 6-hydroxynicotinic
acid 3-hydroxylase was also detected in these cell-free
extracts. However, no conversion of 3-hydroxypyri-
dine to 2,5-dihydroxypyridine was detected in the cells
of Pusillimonas sp. 5HP cultivated in the presence of
3-hydroxypyridine.
The 5-hydroxypicolinate-dependent oxidation of
NADH was observed in the cell-free extracts of the
cells grown in the medium containing 5-hydroxypi-
colinic acid. The zymogram of the cell-free extracts is
shown in Fig. 3. The activity of the enzyme increased
by *25 % after addition of FAD, but not FMN. No
activity was detected under anaerobic conditions, in
the presence of NADPH or in the cells cultivated
without 5-hydroxypicolinic acid. Since the synthesis
of 2,5-dihydroxypyridine 5,6-dioxygenase was
induced in the cells of Pusillimonas sp. 5HP during
growth on 5-hydroxypicolinic acid, it was proposed
that 2,5-dihydroxypyridine may be a conversion
product of 5-hydroxypicolinic acid. To confirm this
hypothesis, the purified 2,5-dihydroxypyridine 5,6-
dioxygenase from Sinorhizobium sp. L1 (Karvelis and
Meskys 2004) was added into the reaction mixture
after completion of 5-hydroxypicolinic acid-depen-
dent NADH oxidation. A decrease in absorbance at
320 nm, the maximum of absorbance of 2,5-dihydr-
oxypyridine, was observed. In addition, an LC–MS
analysis of the reaction products was carried out as
described in Materials and methods. A new compound
(retention time–5.26 min,absorbtion maxima (nm)—
225 and 320, mass of ([M?H]?—112.10) that was
detected after the enzymatic conversion of 5-hydrox-
ypicolinic acid exactly matched to the authentic
2,5-dihydroxypyridine. Hence, it was assumed that
5-hydroxypicolinate 2-monooxygenase (decarboxy-
lating) was the enzyme involved at the initial stage
of catabolism of 5-hydroxypicolinic acid in Pusilli-
monas sp. 5HP cells.
The 5-hydroxypicolinate 2-monooxygenase selec-
tivity to FAD and NADH suggested that the protein
could specifically bind to Cibacron Blue F3GA dye.
The enzyme was purified from cell-free extract using
the affinity Blue and anion exchange resin. The
partially purified enzyme (fivefold purification; spe-
cific activity 0.5 U/mg of protein) was obtained
(Fig. 4). The enzyme was unstable and further
attempts to improve the purification procedure were
unsuccessful. The protein, after PAGE fractionation
(Fig. 4), was subjected to de novo sequencing. One
peptide with the amino acid sequence VGFL(I)PEA-
L(I)VGR was identified. BLAST analysis revealed
that the peptide has sequence homology to various
salicylate 1-monooxygenase related proteins, and
shows the highest similarity to a putative salicylate
1-monooxygenase from Burkholderia xenovorans
LB400 (YP_555487).
Discussion
2,5-Dihydroxypyridine was identified as an interme-
diate in the microbial degradation of nicotinate more
than six decades ago (Behrman and Stanier 1957). At
least four different degradation pathways, including
catabolism of 2-hydroxypyridine, 3-hydroxypyridine,
picolinic acid and nicotinic acid depends on formation
of this intermediate (Kaiser et al. 1996). Here, a new
degradation pathway found in Pusillimonas sp. 5HP is
described. These bacteria are capable to utilize
5-hydroxypicolinate via 2,5-dihydroxypyridine for-
mation. In addition, Pusillimonas sp. 5HP can utilize
Biodegradation
123
3-hydroxypyridine and nicotinic acid as a single
carbon and energy source. In all three cases, the
activity of an inducible 2,5-dihydroxypyridine 5,6-
dioxygenase has been observed. Hence, the catabolism
of these compounds proceeds through formation of
2,5-dihydroxypyridine (Fig. 5). It has been reported
that Achromobacter and Sinorhizobium spp. can
transform 3-hydroxypyridine to 2,5-dihydroxypyri-
dine, however a corresponding enzymatic activity has
not been detected in the induced cells (Houghton and
Cain 1972; Karvelis and Meskys 2004). Repeated
attempts to register oxidation of 3-hydroxypyridine by
adding NADP(H), NAD(H), methylene Blue, DCPIP,
NBT, FAD, FMN or their combination into the cell-
free extracts or membrane fraction of Pusillimonas sp.
5HP have been unsuccessful. However, the activity of
NADH-dependent 5-hydroxypicolinate 2-monooxy-
genase has been detected in 5-hydroxypicolinate-
induced cells of Pusillimonas sp. 5HP. The analogous
oxidative decarboxylation is catalyzed by salicylate
1-monooxygenase (Yamamoto et al. 1965) and 6-hy-
droxynicotinate 3-monooxygenases (Nakano et al.
1999; Jimenez et al. 2008). De novo sequencing of the
partially purified 5-hydroxypicolinate 2-monooxygen-
ase allowed identification of a single peptide which
shows sequence similarity to various enzymes belong-
ing to the group of salicylate 1-monooxygenases.
Hence, we demonstrate that5-hydroxypicolinate 2-mono-
oxygenase is a novel decarboxylating monooxygenase.
Conclusion
This is the first report of the biological conversion of
5-hydroxypicolinic acid. A 5-hydroxypicolinic acid-
degrading bacterium Pusillimonas sp. 5HP has been
isolated from the soil. The strain 5HP displays a broad-
Table 1 The enzyme activities in the cell-free extracts of Pusillimonas sp. 5HP
Substrate Enzyme activity, mU/mg of protein
5-Hydroxypicolinate
2-monooxygenase
2,5-Dihydroxypyridine
5,6-dioxygenase
Nicotinate
dehydrogenase
6-Hydroxynicotinic
acid 3-hydroxylase
Succinate \1 \1 \1 \1
5-Hydroxypicolinic acid 93 ± 9 687 ± 23 \1 \1
3-Hydroxypyridine \1 527 ± 61 \1 \1
3-Cyanopyridine \1 1416 ± 87 1423 ± 108 37 ± 5
Nicotinic acid \1 1872 ± 78 2364 ± 144 45 ± 13
The cells were grown in the MSMYP medium supplemented with 0.15 % of the appropriate substrate for 84 h. The activity of
5-hydroxypicolinate 2-monooxygenase was measured in the presence of NADH without addition of FAD. The activity of nicotinate
dehydrogenase was analysed using potassium ferricyanide
Fig. 3 Non-denaturing
PAGE (10 %) of cell-free
extracts of Pusillimonas sp.
5HP grown in the presence
of 5-hydroxypicolinic acid
and zymography of a
5-hydroxypicolinic acid-
oxidizing enzyme. Lane 1staining mixture without
5-hydroxypicolinic acid
(control), lane 2 staining
mixture with
5-hydroxypicolinic acid,
lane 3 protein molecular
mass marker
Fig. 4 SDS PAGE analysis of partially purified 5-hydroxypi-
colinate 2-monooxygenase. Lane 1 protein molecular mass
markers, lane 2 10 lg of partially purified 5-hydroxypicolinate
2-monooxygenase. Asterisk marks the protein band applied for
de novo sequencing
Biodegradation
123
spectrum degradation ability, it not only has the
enzymes participating in catabolism of 5-hydroxypi-
colinic acid but it can also consume 3-hydroxypyri-
dine and 3-cyanopyridine as well as nicotinic, benzoic
and p-hydroxybenzoic acids as a single carbon and
energy source. A novel enzyme catalyzing the oxida-
tive decarboxylation of 5-hydroxypicolinate to 2,5-
dihydroxypyridine has been identified.
Acknowledgments This research was funded by a Grant (No.
MIP-076/2011) from the Research Council of Lithuania. Authors
thanks dr. M. Ger for assisting with de novo sequencing and dr.
L. Kaliniene for critical reading of the manuscript.
References
Alhapel A, Darley DJ, Wagener N, Eckel E, Elsner N, Pierik AJ
(2006) Molecular and functional analysis of nicotinate
catabolism in Eubacterium barkeri. Proc Natl Acad Sci
USA 103:12341–12346
Behrman EJ, Pitt BM (1958) The Elbs peroxydisulfate oxidation
in the pyridine series: a new synthesis of 2,5-dihydroxy-
pyridine. J Am Chem Soc 80:3717–3718
Behrman EJ, Stanier RY (1957) The bacterial oxidation of
nicotinic acid. J Biol Chem 228:923–945
Brandsch R (2006) Microbiology and biochemistry of nicotine
degradation. Appl Microbiol Biotechnol 69:493–498
Ensign JC, Rittenberg SC (1964) The pathway of nicotinic acid
oxidation by a Bacillus species. J Biol Chem 239:2285–2291
Fetzner S (1998) Bacterial degradation of pyridine, indole,
quinoline, and their derivatives under different redox
conditions. Appl Microbiol Biotechnol 49:237–250
Garrett MD, Scott R, Sheldrake GN, Dalton H, Goode P (2006)
Biotransformation of substituted pyridines with dioxy-
genase-containing microorganisms. Org Biomol Chem
4:2710–2715
Gauthier JJ, Rittenberg SC (1971a) The metabolism of nicotinic
acid. I. Purification and properties of 2,5-dihydroxypyri-
dine oxygenase from Pseudomonas putida N-9. J Biol
Chem 246:3737–3742
Gauthier JJ, Rittenberg SC (1971b) The metabolism of nicotinic
acid. II. 2,5-dihydroxypyridine oxidation, product forma-
tion, and oxygen 18 incorporation. J Biol Chem 246:
3743–3748
Gladyshev VN, Khangulov SV, Stadtman TC (1996) Properties
of the selenium- and molybdenum-containing nicotinic
acid hydroxylase from Clostridium barkeri. Biochemistry
35:212–223
Godon JJ, Zumstein E, Dabert P, Habouzit F, Moletta R (1997)
Molecular microbial diversity of an anaerobic digestor as
determined by small-subunit rDNA sequence analysis.
Appl Environ Microbiol 63:2802–2813
He Z, Spain JC (2000) One-step production of picolinic acids
from 2-aminophenols catalyzed by 2-aminophenol 1,6-
dioxygenase. J Ind Microbiol Biotechnol 25:25–28
Hellman U, Wernstedt C, Gonez J, Heldin CH (1995)
Improvement of an ‘‘in-gel’’ digestion procedure for the
micropreparation of internal protein fragments for amino
acid sequencing. Anal Biochem 224:451–455
Hirschberg R, Ensign JC (1971) Oxidation of nicotinic acid by a
Bacillus species: purification and properties of nicotinic
acid and 6-hydroxynicotinic acid hydroxylases. J Bacteriol
108:751–756
Houghton C, Cain RB (1972) Microbial metabolism of the
pyridine ring. Formation of pyridinediols (dihydroxypyri-
dines) as intermediates in the degradation of pyridine
compounds by micro-organisms. Biochem J 130:879–893
Hurh B, Yamane T, Nagasawa T (1994) Purification and char-
acterization of nicotinic acid dehydrogenase from Pseu-domonas fluorescens TN5. J Ferment Bioeng 78:19–26
Iqbal P, Mayanditheuar M, Childs LJ, Michael J, Hannon MJ,
Spencer N, Ashton PR, Preece JA (2009) Preparation of
novel banana-shaped triple helical liquid crystals by metal
coordination. Materials 2:146–168
Jimenez JI, Canales A, Barbero JJ, Ginalski K, Rychlewski L,
Garcia JL, Diaz E (2008) Deciphering the genetic deter-
minants for aerobic nicotinic acid degradation: the nic
cluster from Pseudomonas putida KT2440. Proc Natl Acad
Sci USA 105:11329–11334
Kaiser JP, Feng Y, Bollag JM (1996) Microbial metabolism of
pyridine, quinoline, acridine, and their derivatives under
aerobic and anaerobic conditions. Microbiol Rev 60:
483–498
Karvelis L, Meskys R (2004) New Rhizobium strain degrading
3-hydroxypyridine. Biologija 2:98–101
Khanna M, Shukla OP (1977) Microbiol metabolism of
3-hydroxypyridine. Indian J Biochem Biophys 14:301–302
Kiener A, Glockler R, Heinzmann K (1993) Preparation of
6-oxo-1,6-dihydropyridine-2-carboxylic acid by microbial
hydroxylation of pyridine-2-carboxylic acid. J Chem Soc
Perkin Trans 1:1201–1202
Kim CG, Lamichhane J, Song KI, Nguyen VD, Kim DH, Jeong
TS, Kang SH, Kim KW, Maharjan J, Hong YS, Kang JS,
Fig. 5 Proposed biodegradation pathways in Pusillimonas sp.
5HP. 1 3-cyanopyridine, 2 nicotinic acid, 3 6-hydroxynicotinic
acid, 4 5-hydroxypicolinic acid, 5 3-hydroxypyridine, 6 2,5-
dihydroxypyridine, 7 N-formylmaleamic acid; a a putative
nitrilase, b nicotinic acid dehydrogenase, c 5-hydroxypicolinate
2-monooxygenase, d hypothetical 3-hydroxypyridine 6-hydrox-
ylase, e 6-hydroxynicotinic acid 3-hydroxylase, f 2,5-dihydr-
oxypyridine 5,6-dioxygenase
Biodegradation
123
Yoo JC, Lee JJ, Oh TJ, Liou K, Sohng JK (2008) Bio-
synthesis of rubradirin as an ansamycin antibiotic from
Streptomyces achromogenes var. rubradiris NRRL3061.
Arch Microbiol 189:463–473
Kretzer A, Frunzke K, Andreesen JR (1993) Catabolism of
isonicotinate by Mycobacterium sp. INA1: extended
description of the pathway and purification of the molyb-
doenzyme isonicotinate dehydogenase. J Gen Microbiol
139:2763–2772
Li H, Li X, Duan Y, Zhang KQ, Yang J (2010) Biotransfor-
mation of nicotine by microorganism: the case of Pseu-domonas spp. Appl Microbiol Biotechnol 86:11–27
Makar’eva TN, Kalinovskii AI, Stonik VA, Vakhrusheva EV
(1989) Identification of 5-hydroxypicolinic acid among the
products biosynthesized by Nocardia sp. Chem Nat Compd
25:125–126
Moon M, Van Lanen SG (2010) Characterization of a dual
specificity aryl acid adenylation enzyme enzyme with dual
function in nikkomycin biosynthesis. Biopolymers 93:
791–801
Nagel M, Andreesen JR (1989) Molybdenum-dependent deg-
radation of nicotinic acid by Bacillus sp. DSM 2923. FEMS
Microbiol Lett 59:147–152
Nagel M, Andreesen JR (1990) Purification and characterization
of the molybdoenzymes nicotinate dehydrogenase and
6-hydroxynicotinate dehydrogenase from Bacillus niacini.Arch Microbiol 154:605–613
Nakano H, Wieser M, Hurh B, Kawai T, Yoshida T, Yamane T,
Nagasawa T (1999) Purification, characterization and gene
cloning of 6-hydroxynicotinate 3-monooxygenase from
Pseudomonas fluorescens TN5. Eur J Biochem 260:
120–126
Schrader T, Thiemer B, Andreesen JR (2002) A molybdenum-
containing dehydrogenase catalyzing an unusual
2-hydroxylation of nicotinic acid. Appl Microbiol Bio-
technol 58:612–617
Shukla OP (1975) Isolation, characterization and metabolic
activities of a Bacillus sp. metabolizing alpha-picolinate.
Indian J Exp Biol 13:80–82
Siegmund I, Koenig K, Andreesen JR (1990) Molybdenum
involvement in aerobic degradation of picolinic acid by
Arthrobacter picolinophilus. FEMS Microbiol Lett 67:
281–284
Singh RP, Shukla OP (1986) Isolation, characterization and
metabolic activities of Bacillus brevis degrading isonicot-
inic acid. J Ferment Technol 64:109–111
Tamura K, Peterson D, Peterson N, Stecher G, Nei M, Kumar S
(2011) MEGA5: molecular evolutionary genetics analysis
using maximum likelihood, evolutionary distance, and
maximum parsimony methods. Mol Biol Evol 28:
2731–2739
Tang H, Yao Y, Wang L, Yu H, Ren Y, Wu G, Xu P (2012)
Genomic analysis of Pseudomonas putida: genes in a
genome island are crucial for nicotine degradation. Sci Rep
2:377
Tate RL, Ensign JC (1974) Picolinic acid hydroxylase of
Arthrobacter picolinophilus. Can J Microbiol 20:695–702
Uchida A, Ogawa M, Yoshida T, Nagasawa T (2003) Quino-
linate dehydrogenase and 6-hydroxyquinolinate decar-
boxylase involved in the conversion of quinolinic acid to
6-hydroxypicolinic acid by Alcaligenes sp. strain UK21.
Arch Microbiol 180:81–87
Wang SN, Xu P, Tang HZ, Meng J, Liu XL, Ma CQ (2005)
‘‘Green’’ route to 6-hydroxy-3-succinoyl-pyridine from
(S)-nicotine of tobacco waste by whole cells of a Pseudo-monas sp. Environ Sci Technol 39:6877–6880
Woo THS, Cheng AF, Ling JM (1992) An application of a
simple method for the preparation of bacterial DNA. Bio-
techniques 13:696–698
Yamamoto S, Katagiri M, Haeno H, Hayashi O (1965) Salicy-
late hydroxylase, a monooxygenase requiring flavin ade-
nine dinucleotide. J Biol Chem 240:3408–3413
Yoshida T, Nagasawa T (2000) Enzymatic functionalization of
aromatic N-heterocycles: hydroxylation and carboxylation.
J Biosci Bioeng 89:111–118
Biodegradation
123