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Applied and Environmental Microbiology, April 2001, p. 1476-1483, Vol. 67, No. 4
Division of
Microbiology,1 Division of
Chemistry,2 and Division of Biochemical
Toxicology,3 National Center for Toxicological
Research, U.S. Food and Drug Administration, Jefferson, Arkansas 72079
Received 27 September 2000/Accepted 26 January 2001
Cultures of Mycobacterium sp. strain PYR-1 were
dosed with anthracene or phenanthrene and after 14 days of incubation
had degraded 92 and 90% of the added anthracene and phenanthrene, respectively. The metabolites were extracted and identified by UV-visible light absorption, high-pressure liquid chromatography retention times, mass spectrometry, 1H and 13C
nuclear magnetic resonance spectrometry, and comparison to authentic compounds and literature data. Neutral-pH ethyl acetate extracts from
anthracene-incubated cells showed four metabolites, identified as
cis-1,2-dihydroxy-1,2-dihydroanthracene,
6,7-benzocoumarin, 1-methoxy-2-hydroxyanthracene, and
9,10-anthraquinone. A novel anthracene ring fission product was
isolated from acidified culture media and was identified as
3-(2-carboxyvinyl)naphthalene-2-carboxylic acid. 6,7-Benzocoumarin was
also found in that extract. When Mycobacterium sp.
strain PYR-1 was grown in the presence of phenanthrene, three neutral
metabolites were identified as cis- and
trans-9,10-dihydroxy-9,10-dihydrophenanthrene and
cis-3,4-dihydroxy-3,4-dihydrophenanthrene. Phenanthrene
ring fission products, isolated from acid extracts, were identified as
2,2'-diphenic acid, 1-hydroxynaphthoic acid, and phthalic acid. The
data point to the existence, next to already known routes for both
gram-negative and gram-positive bacteria, of alternative pathways that
might be due to the presence of different dioxygenases or to a relaxed
specificity of the same dioxygenase for initial attack on polycyclic
aromatic hydrocarbons.
Anthracene and phenanthrene
are tricyclic aromatic hydrocarbons that are found in high
concentrations in polycyclic aromatic hydrocarbon (PAH)-contaminated
sediments, surface soils, and waste sites. These hydrophobic
contaminants are widely distributed in the environment, occurring as
natural constituents of fossil fuels and their anthropogenic pyrolysis
products (6, 24, 55). Unlike the higher-molecular-weight
PAHs, phenanthrene and anthracene do not pose a risk to human health,
since they exhibit no genotoxic or carcinogenic effects. However, they
have been shown to be toxic to fish and algae (45, 46).
Anthracene and phenanthrene are considered prototypic PAHs and serve as
signature compounds to detect PAH contamination, since their chemical
structures are found in carcinogenic PAHs, such as
benzo[a]pyrene and benz[a]anthracene. They
have also been used as model PAHs to determine factors that affect the
bioavailability, biodegradation potential, and rate of microbial
degradation of PAHs in the environment (5, 6, 24, 48).
A variety of bacterial species have been isolated that have the ability
to utilize anthracene or phenanthrene as the sole source of carbon and
energy (6, 33, 48). The initial reactions in the
degradation of anthracene and phenanthrene are catalyzed by
multicomponent dioxygenases that incorporate both atoms of molecular
oxygen into the PAH nucleus to produce cis-dihydrodiols (1, 22). Genes involved in PAH metabolism and its
regulation have been described for Pseudomonas,
Sphingomonas, and Nocardioides species (36,
42, 43, 56-58).
Pseudomonas spp. and Sphingomonas yanoikuyae B1
initially oxidize anthracene in the 1,2 position to form
(+)-(1R,2S)-cis-1,2-dihydroxy-1,2-dihydroanthracene, which is subsequently converted to 1,2-dihydroxyanthracene, which is
further metabolized to 2-hydroxy-3-naphthoic acid, salicylate, and
catechol by enzymes of the naphthalene pathway (1, 11, 12,
22).
Phenanthrene degradation by Pseudomonas species proceeds by
two different pathways (1, 11, 12, 22, 32, 36). One is via
dioxygenation at the C-3 and C-4 ring positions, to form (+)-(3S,4R)-cis-3,4-dihydroxy-3,4-dihydrophenanthrene
(phenanthrene cis-3,4-dihydrodiol). This dihydroxylated
intermediate is further metabolized to 1-hydroxy-2-naphthoic acid, with
subsequent degradation either through salicylate and catechol or
through phthalate and protocatechuate, depending upon the bacterial
species. The other pathway involves dioxygenation at the C-1 and C-2
positions to form
(+)-(1R,2S)-cis-1,2-dihydroxy-1,2-dihydrophenanthrene
(phenanthrene cis-1,2-dihydrodiol). The initial product of
enzymatic attack in the 9,10 position,
trans-9,10-dihydroxy-9,10-dihydrophenanthrene (phenanthrene
trans-9,10-dihydrodiol), has been reported to be produced by
Streptomyces flavovirens but not by Pseudomonas
spp. (45).
Various Mycobacterium, Nocardia, and
Rhodococcus species have the ability to degrade PAHs
containing more than two rings (4, 7, 9, 10, 13-17, 23, 25, 26,
34, 35, 40, 41, 44, 49, 51, 53, 54). However, detailed
metabolite structure elucidation and degradation pathways for
anthracene and phenanthrene catabolism by this group of microorganisms
are not well known (4, 16, 41, 50).
Mycobacterium species metabolize phenanthrene at different
sites of the molecule, presumably via both dioxygenase and
monooxygenase attacks on the aromatic nucleus. To our knowledge, the
catabolic pathway of anthracene degradation by Mycobacterium species has not been investigated.
Mycobacterium sp. strain PYR-1, which was originally
isolated in our laboratory from oil-contaminated estuarine
sediment, is capable of mineralizing naphthalene, pyrene,
1-nitropyrene, fluoranthene, phenanthrene, anthracene, and
benzo[a]pyrene (7, 17, 19, 21, 26, 27, 39,
52). Biodegradation pathways have been elucidated for the
metabolism of naphthalene, pyrene, 1-nitropyrene, and fluoranthene by
Mycobacterium sp. strain PYR-1 (6, 20, 21,
26-30). We now propose metabolic pathways for the
degradation of anthracene and phenanthrene by Mycobacterium sp. strain PYR-1, based on the identification of initial ring oxidation
and ring cleavage products.
Chemicals.
[9,10-14C]anthracene (58 mCi/mmol) with a radiochemical purity of >98% was purchased from
Chemsyn Science Laboratories (Lenexa, Kans.). Unlabeled anthracene
(97% pure) was purchased from Aldrich Chemical Co. (Milwaukee, Wis.).
Unlabeled phenanthrene and
[9,10-14C]phenanthrene (10.9 mCi/mmol) with a
radiochemical purity of >99% were purchased from Sigma Chemical Co.
(St. Louis, Mo.). Bacteriological media and reagents were purchased
from BD Biosciences, Difco Laboratories (Detroit, Mich.). Nuclear
magnetic resonance (NMR) solvents were purchased from Isotec, Inc.
(Miamisburg, Ohio). Other solvents were purchased from J. T. Baker, Inc. (Phillipsburg, N.J.) and were of the highest purity available.
Culture conditions.
Cultures of Mycobacterium sp.
strain PYR-1 were grown in 125-ml Erlenmeyer flasks containing 30 ml of
minimal basal salt medium supplemented with 0.38-g/ml concentrations of
peptone, yeast extract, and soluble starch. A 15-µl aliquot of
phenanthrene or anthracene in N, N-dimethylformamide (12 mg/ml) was added to each flask for enzyme induction. The cultures
(A500, 0.38) were incubated for 6 days
in the dark at 24°C with shaking at 150 rpm. Phenanthrene or
anthracene was dissolved in N, N-dimethylformamide and added to the cultures, making the final concentrations 0.15 and 0.075 mM,
respectively. The phenanthrene-dosed cultures were further incubated
for 6 h, and those with anthracene were incubated for 24 h.
0099-2240/01/$04.00+0 DOI: 10.1128/AEM.67.4.1476-1483.2001
Degradation of Phenanthrene and Anthracene by Cell
Suspensions of Mycobacterium sp. Strain PYR-1
ABSTRACT
Top
Abstract
Introduction
Materials and Methods
Results
Discussion
References
INTRODUCTION
Top
Abstract
Introduction
Materials and Methods
Results
Discussion
References
MATERIALS AND METHODS
Top
Abstract
Introduction
Materials and Methods
Results
Discussion
References
Radiolabel experiments. Experiments to determine the degree of mineralization of anthracene and phenanthrene, as evidenced by CO2 evolution, were carried out in 250-ml biometer flasks. A CO2 trap, consisting of 20 ml of 70% ethylene glycol and 30% monoethanolamine, was added to the side arm of each flask. PAH-induced Mycobacterium cells were added to 50 ml of minimal basal salt medium with nutrients. The optical density of the cells at 500 nm was determined immediately using a Beckman DU-7 spectrophotometer (Beckman Instrument Co., Berkeley, Calif.) with a cell-free control as the background. Fifty micrograms of unlabeled anthracene or phenanthrene and 1.0 µCi of either labeled anthracene or phenanthrene were added to each of three flasks. Each flask was immediately sampled for CO2 production by removing 1.0 ml of the trapping solution. This sample was added to 14 ml of Ultima Gold liquid scintillation fluid (Packard Instruments, Downers Grove, Ill.) and counted in a Packard Tri-Carb 2000A scintillation analyzer. A 2.0-ml aliquot of the aqueous portion was removed from each flask, and its optical density was determined. Each sample was extracted with 3 equal volumes of ethyl acetate, acidified to pH 2.5, and extracted three more times. Flasks were also sampled and extracted at 6, 24, 48, 72, 168, 192, and 312 h.
Each of the radiolabeled extracts from both experiments was dissolved in a small amount of methanol and analyzed by HPLC.Physical and chemical analysis. Anthracene, phenanthrene, and their metabolites were separated by HPLC using a Hewlett-Packard model 1050 pump system (Hewlett-Packard, Palo Alto, Calif.) with a Hewlett-Packard diode array model 1040A detector at 254 nm and a 4.6- by 250-mm 5-µm C18 Inertsil ODS-3 column (MetaChem Technologies, Torrance, Calif.) at a flow rate of 1 ml/min. UV absorbance spectra were obtained online. The compounds were eluted using a linear gradient of 40 to 95% methanol/water over 40 min. For collection of larger amounts of metabolites, a Beckman model 100A dual pump system equipped with a Beckman model 160 absorbance detector (Beckman Instruments, Inc., Fullerton, Calif.), a Waters 486 tunable UV absorbance detector (Waters Corp., Milford, Mass.), and an Inertsil ODS-3 10.0- by 250-mm column (MetaChem) were used. The mobile phase was the same as that described above but with a flow rate of 5 ml/min.
Probe mass spectra were obtained on a TSQ 700 triple-quadrupole mass spectrometer (Finnigan Corp., San Jose, Calif.) using a direct exposure probe and electron ionization (EI). Gas chromatography-mass spectrometry (MS) analyses were performed on a model 4500 quadrupole mass spectrometer (Finnigan Corp.) and model 3400 (Varian, Inc., Sunnyvale, Calif.) gas chromatograph. Chromatography was achieved on a DB-1 fused silica capillary column (J & W Scientific, Folsom, Calif.). Further MS experiments were performed using a Platform single-quadrupole instrument (Micromass, Manchester, United Kingdom) equipped with an atmospheric pressure chemical ionization (APCI) interface. The total liquid chromatography (LC) column effluent was delivered into the atmospheric pressure ion source through a heated nebulizer probe (450°C), using nitrogen as the probe and bath gas (275 liters/h) with an ion source temperature of 150°C. Positive or negative ion spectra were acquired in full-scan mode (m/z of 100 to 400, 1.0-s cycle time) in series with a UV detector at 254 nm. At low cone voltage (15 to 20 V), the positive and negative ion mass spectra of the PAH metabolites predominantly consisted of protonated and deprotonated molecules, respectively. When further fragmentation was required, a higher cone voltage was used (60 V). PAH metabolite sample extracts, dissolved in starting mobile phase and prepared as described above, were injected into the LC-MS system. NMR spectra were recorded at 500.13 MHz (1H) and 125.77 MHz (13C) on a Bruker AM500 spectrometer (Bruker Instruments, Billerica, Mass.). The metabolites were dissolved in 0.5 ml of deuterated acetone (99.96 atom% 2H), except where otherwise noted. 1H chemical shifts are reported on the
scale
(parts per million) by assigning the residual solvent peak to
2.04 ppm. Typical 1H data acquisition parameters
were as follows: data size, 32,000; sweep width, 7,042 Hz; filter
width, 8,900 Hz; acquisition time, 2.33 s; flip angle, 90°;
relaxation delay, 0 s; temperature, 298.5 K. For spectra recorded
under quantitative conditions, a 10- to 20-s relaxation delay was used.
For measurement of coupling constants, the free induction decay was
zero-filled to 64,000, resulting in a final data point resolution of
0.215 Hz per point. Coupling constants reported are first order. Those
that were non-first order and those of overlapping resonances were
omitted. Assignments were made from homonuclear decoupling experiments,
nuclear Overhauser effect (NOE) experiments, integration, analysis of
substituent effects, and comparison to spectra of authentic compounds.
A 13C NMR spectrum was obtained for one
metabolite (data not shown). The sample was dissolved in 0.5 ml of
deuterated methanol (99.96 atom% 2H), and the
residual methanol resonance was assigned as 49.0 ppm.
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RESULTS |
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Top
Abstract
Introduction
Materials and Methods
Results
Discussion
References
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Mineralization of anthracene and phenanthrene.
Mycobacterium sp. strain PYR-1, when grown in the presence
of anthracene and phenanthrene for 14 days, degraded 92 and 90% of
these tricyclic PAHs, respectively. Both PAHs were mineralized; the
amounts of CO2 evolved are shown in Fig.
1. The percentages of
[14C]anthracene and
[14C]phenanthrene evolved as
14CO2 were 45 and 52%,
respectively, after 6 days. A lag period of 48 h was observed
before significant mineralization of anthracene occurred (Fig. 1).
|
) and mineralization (
) of anthracene
(dashed line) and phenanthrene (solid line) by
Mycobacterium sp. strain PYR-1.
Identification of phenanthrene degradation products.
HPLC analysis of the neutral extract from phenanthrene
incubations produced two metabolites as shown in Fig.
2A. The EI mass spectrum of
compound I, eluting at 21.6 min with 
max of
202 and 278 nm, contained a base peak at an m/z of
212, the molecular ion [M+.]. Fragment
ions at m/z values of 194 [M-18]+,
166 [M-18-28]+, and 165 [M-18-29]+ are characteristic of a dihydrodiol.
A fragment ion at an m/z of 181 possibly indicated the loss
of CH2-OH from the molecular ion. The mass and
1H NMR spectra are consistent with those
previously reported for cis-9,10-dihydroxy-9,10-dihydrophenanthrene (phenanthrene
cis-9,10-dihydrodiol). The NMR assignments and coupling
constants are as follows: 7.57 (H1,8;
J1,2 =7.5 Hz,
J1,3 = 1.5 Hz), 7.31 (H2,7;
J2,3 = 7.5 Hz, J2,4 = 1.5 Hz), 7.37 (H3,6;
J3,4 = 8.0 Hz), 7.84 (H4,5), 4.75 (H9,10). The chemical shift of the H9,10 resonance showed that the
compound was the cis- rather than the
trans-isomer, because the resonance is at 4.60 ppm in the
trans-isomer (37).
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max = 202, 260, and 268 nm) had a molecular
ion at an m/z of 212 and characteristic dihydrodiol fragment
ions at m/z values of 194, 166, and 165. Additional fragment
ions at m/z values of 168 and 140 were present at lower
intensities than in the mass spectrum of metabolite I, indicating that
II was a different dihydrodiol. The aromatic region of the
1H NMR spectrum of the metabolite contained 10 resonances belonging to one compound, with four of the resonances
exhibiting large upfield shifts. NOE and homonuclear decoupling
experiments proved that the substitution was at C-3 and C-4. The
small coupling constant (J3,4 = 5.6 Hz) is
consistent with a cis conformation. Compound II was
identified as cis-3,4-dihydroxy-3,4-dihydrophenanthrene (phenanthrene cis-3,4-dihydrodiol). NMR assignments and
coupling constants were as follows: 6.51 (H1;
J1,2 = 9.6 Hz,
J1,3 = 2.8 Hz), 5.97 (H2;
J2,3 = 1.7 Hz,
J2,4 = 1.4 Hz), 4.63 (H3;
J3,4 = 5.2 Hz), 5.28 (H4), 8.24 (H5;
J5,6 = 8.7 Hz), 7.54 (H6;
J6,7 = 7.7 Hz,
J6,8 = 1.4 Hz), 7.45 (H7;
J7,8 = 8.3 Hz,
J7,9 = 1.2 Hz), 7.85 (H8), 7.83 (H9;
J9,10 = 8.3 Hz), and 7.31 (H10). A
second compound apparent in the NMR spectrum of compound II was
identified as trans-9,10-dihydroxy-9,10-dihydrophenanthrene
(phenanthrene trans-9,10-dihydrodiol) by comparing its
chemical shifts and coupling constants
7.70 (H1,8;
J1,2 = 6.7 Hz,
J1,3 = 2.2 Hz), 7.35 (H2,3,6,7; J2,4 = 1.7 Hz,
J3,4 = 7.1 Hz), 7.79 (H4,5), and 4.60 (H9,10)to those in the literature. The chemical shift of H9,10
was the basis for the trans determination (3, 37, 45,
47).
The phenanthrene cis-3,4-and 9,10-dihydrodiols were also
detected by online HPLC with APCI/MS, which gave negative ion mass spectra with [M-H-H2O]
at an m/z of 193 and LC retention times of 14.3 and
15.0 min, respectively. The amounts of both the cis-3,4-and
9,10-dihydrodiols increased following 4 to 8 h of incubation.
However, between 8 and 32 h of incubation, the compounds were
totally degraded.
One acid-extractable metabolite eluting at 23.3 min with a
max of 214 was detected by HPLC analysis (Fig.
2B). The EI mass spectrum of the metabolite consisted of a molecular
ion at an m/z of 242 and characteristic fragment ions at
m/z values of 197 and 153 resulting from consecutive losses
of CO2H and CO2. The 1H NMR spectrum7.72 (H1,8;
J1,2 = 7.5 Hz,
J1,3 = 1.7 Hz), 7.38 (H2,7;
J2,3 = 7.5 Hz,
J2,4 = 1.7 Hz), 7.40 (H3,6;
J3,4 = 7.5 Hz), 7.05 (H4,5)was the
same as that of authentic 2,2'-diphenic acid (3). The
metabolite began to accumulate at 8 h after incubation, and the
concentration remained essentially unchanged after 96 h.
The parent compound, phenanthrene, was eluted at 41.9 min.
Two other ring fission products were detected by gas
chromatography-mass spectrometry analysis of the acidified
aqueous-phase extracts. Gas chromatography-mass spectrometry analysis
of methyl esters of the acid-extractable material gave retention times
and EI mass spectra consistent with 1-hydroxynaphthoic acid (9.55 min,
M+· = m/z of 216) and
phthalic acid (4.15 min, M+· = m/z of 194).
Identification of anthracene degradation products.
HPLC
analysis of the neutral extract from anthracene incubation (Fig. 2C)
produced four metabolites that were eluted at 22.9, 27.6, 34.2, and
34.9 min. The EI mass spectrum of compound I (retention time = 22.9 min, max = 204, 252, 296, and 306 nm)
from the neutral extract of anthracene consisted of a molecular ion at
an m/z of 212 and characteristic fragment ions at
m/z values of 194, 166, and 165 resulting from losses of
H2O and then either CO or HCO. The fragment ions
at m/z values of 168 and 140 indicate substitution on the
first aromatic ring. The 1H NMR assignments and
coupling constants are as follows: 4.75 (H1;
J1,2 = 4.7 Hz), 4.35 (H2;
J2,3 = 4.5 Hz), 6.09 (H3;
J3,4 = 9.7 Hz), 6.69 (H4), 7.82 (H5,8), 7.44 (H6,7), 7.94 (H9), and 7.58 (H10). The H1 and H2
resonances of the 1H NMR spectrum had chemical
shifts that were characteristic of a dihydrodiol. NOE experiments were
performed to make resonance assignments by irradiating H1 and H4 to
produce enhancements at H9 and H10, respectively. The final NOE
experiments were performed on the two singlets at 7.94 and 7.58 ppm
(H9,10). They each produced an enhancement of the multiplet at 7.82 ppm
(H5,8). Homonuclear decoupling experiments showed that multiplet to be
coupled to the one at 7.44 ppm (H6,7). Further decoupling experiments
were used to assign H2 and H3. The metabolite was identified as
cis-1,2-dihydroxy-1,2-dihydroanthracene (anthracene
cis-1,2-dihydrodiol) by MS and 1H NMR
spectrometry and by comparison to data previously published (1,
8, 22, 46).
max
values of 202, 232, 274, 284, and 328 nm. Its EI mass spectrum
consisted of a molecular ion at an m/z of 196 and
fragment ions at m/z values of 168 and 140 resulting from
consecutive losses of CO. The 1H NMR assignments
and coupling constants were 6.47 (H3;
J3,4 = 9.7 Hz), 8.12 (H4;
J3,4 = 9.7 Hz), 8.03 (H5;
J5,6 = 8.4 Hz), 7.54 (H6;
J6,7 = 7.7 Hz,
J6,8 = 1.3 Hz), 7.62 (H7;
J7,8 = 8.6 Hz,
J7,9 = 1.3 Hz), 8.00 (H8), 7.79 (H9),
8.27 (H10). Homonuclear decoupling and NOE experiments allowed
resonance assignments and showed substitutions at C-1 and C-2.
Comparison of the H3 and H4 chemical shifts of compound II to those
reported for coumarin (38) indicated that the compound was
6,7-benzocoumarin. After 72 h of incubation, 6,7-benzocoumarin
could not be detected, suggesting that it is a transient intermediate
and a substrate for ring fission enzymes.
Compound III was eluted at 34.2 min with max
values of 204 and 266 nm. The EI mass spectrum of compound III had an
apparent molecular ion at an m/z of 224 and strong fragment
ions at m/z values of 209, 181, and 152 that may
be attributed to sequential losses of CH3 and CO
or to the loss of
C3H4O2.
The 1H NMR chemical shifts and coupling constants
were assigned as follows: 4.00 (CH3), 7.78 (H3;
J3,4 = 9.0 Hz), 7.26 (H4), 8.05 (H5;
J5,6 = 8.2 Hz,
J5,7 = 1.5 Hz), 7.46 (H6;
J6,7 = 7.3 Hz,
J6,8 = 1.5 Hz), 7.41 (H7;
J7,8 = 8.2 Hz), 8.00 (H8), 8.53 (H9),
and 8.45 (H10). The sharp singlet at 4.00 ppm in the NMR spectrum was
characteristic of a methoxyl group. When irradiated, the singlet produced an NOE to the aromatic singlet at 8.53 ppm (H9), indicating that the methoxyl group was attached to C-1. Other proton
assignments were made from NOE and homonuclear decoupling experiments.
When the metabolite was dissolved in deuterated methylene chloride, the
exchangeable hydroxyl proton was observed at 5.91 ppm. Metabolite III
was identified as 1-methoxy-2-hydroxyanthracene. The concentration of
1-methoxy-2-hydroxyanthracene remained constant during the incubation
period, suggesting that it is a dead-end metabolite.
Compound IV (retention time = 34.9 min,
max = 204, 260, and 334 nm) had an EI
molecular ion at an m/z of 208 and fragment ions
at m/z values of 180 and 152, representing
successive losses of CO. The 1H NMR spectrum
consisted of two resonances at 8.29 and 7.94 ppm, consistent with that
of authentic 9,10-anthraquinone (46), and compound IV was
identified as such.
Anthracene was eluted at 42.4 min.
Negative- and positive-ion APCI mass spectra and HPLC retention times
were consistent with the formation of anthracene
cis-1,2-dihydrodiol ([M-H-H2O],
m/z = 193, retention time = 7.3 min),
9,10-anthraquinone ([M·],
m/z = 208, retention time = 27.7 min),
and 6,7-benzocoumarin ([M+H]+,
m/z = 197, retention time = 17.8 min).
The acid extract from the aqueous phase yielded two ring fission
metabolites (Fig. 3D),
eluting at 27.1 and 27.9 min. Compound I was identified as
6,7-benzocoumarin by comparison of its NMR spectrum to that of
6,7-benzocoumarin collected from the neutral extract.
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max = 266 nm), with a coupling pattern consistent with either substitution or ring cleavage at the C-1 and C-2 positions. Assignments of proton resonances 3 through 10 were made from decoupling and NOE
measurements. The proton-decoupled 13C NMR
spectrum of the metabolite had 12 aromatic resonances; 4 of the
resonances were from quaternary carbons. The resonances at 170.32 and 177.59 ppm were consistent with the chemical shifts of carbons in
carboxylic acid groups.
Compound II was eluted with a retention time of 26.2 min using APCI/MS
to produce diagnostic fragment ions in addition to molecular species.
The negative-ion mass spectrum acquired at 25 V contained ions
corresponding to the deprotonated molecule (M-H) at an m/z of 241. Other
diagnostic ions present were
(M-CO2-H) at an
m/z of 197 and
(M-2CO2-H) at an
m/z of 153, indicating sequential losses of the acid
moieties. Based on the NMR and APCI/MS data, compound II was identified as 3-(2-carboxyvinyl)naphthalene-2-carboxylic acid. This compound was
formed after 8 h of incubation and remained constant throughout the incubation period. A minor metabolite that eluted at 20.8 min had
an identical mass spectrum, suggesting the presence of an isomer of
compound II also having two acid moieties. The isomer was not
characterized by NMR due to quantity limitations.
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DISCUSSION |
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Top
Abstract
Introduction
Materials and Methods
Results
Discussion
References
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The results show that Mycobacterium sp. strain PYR-1 extensively metabolized anthracene and phenanthrene. The isolation and characterization of the major initial oxidation and ring fission products indicated multiple routes of enzymatic attack. The degradation pathways of anthracene and phenanthrene by Mycobacterium sp. strain PYR-1 are proposed in Fig. 3.
Mycobacterium sp. strain PYR-1 oxidized anthracene to anthracene cis-1,2-dihydrodiol in a reaction similar to those previously reported for anthracene degradation by Pseudomonas and Sphingomonas species (1, 22). The enzymatic attack in the C-1 and C-2 positions of the anthracene moiety was similar to the naphthalene dioxygenase pathways previously reported in Mycobacterium sp. strain PYR-1 (28). The resulting anthracene cis-dihydrodiol was dehydrogenated to 1,2-dihydroxyanthracene. The accumulation of 1-methoxy-2-hydroxyanthracene provided further evidence for the dioxygenation of anthracene by Mycobacterium sp. strain PYR-1. This is a novel metabolite for anthracene biodegradation studies; however, methylation of a dihydroxylated PAH intermediate was found previously in Mycobacterium sp. strain PYR-1 with the formation of 8-hydroxy-7-methoxyfluoranthene during the metabolism of fluoranthene (30). Kinetic studies indicate that these methoxylated derivatives are dead-end metabolites. The isolation of 6,7-benzocoumarin suggests that (3Z)-4-[3-hydroxy(2-naphthyl)]-2-oxobut-3-enoic acid was formed as a ring fission product of 1,2-dihydroxyanthracene. Previously, scholars reported the identification of 6,7-benzocoumarin in the degradation of anthracene by S. yanoikuyae B1 (31). A novel ring fission product, 3-(2-carboxyvinyl)naphthalene-2-carboxylic acid, was also identified in the present investigation. ortho-Ring cleavage of 1,2-dihydroxyanthracene could lead to the formation of 3-(2-carboxyvinyl)naphthalene-2-carboxylic acid. A minor amount of an isomer of this ortho-ring cleavage product was also detected in cultures of Mycobacterium sp. strain PYR-1, which suggests that dioxygenation could also occur in the C-2 and C-3 positions of anthracene. The detection of these ortho-cleavage ring fission products is analogous to evidence in a recent report on naphthalene degradation in Bacillus thermoleovorans (2). An alternate route of enzymatic attack by Mycobacterium sp. strain PYR-1 is in the C-9 and C-10 positions of anthracene. The presence of the dead-end product 9,10-anthraquinone could be explained by the formation and nonenzymatic oxidation of 9,10-dihydroxyanthracene (Fig. 3).
Based on rigorous chemical structure determination for the identification of cis-3,4- and 9,10-dihydrodiols, trans-9,10-dihydrodiol, and ring fission products formed from phenanthrene by Mycobacterium sp. strain PYR-1, at least three pathways are evident in the degradation of phenanthrene. As shown in an earlier study on pyrene catabolism (20), phenanthrene was metabolized by Mycobacterium sp. strain PYR-1 with initial attack in the K region to form the cis- and trans-9,10-dihydrodiols. Furthermore, the formation of 2,2'-diphenic acid during phenanthrene degradation is analogous to the formation of 4,5-phenanthrene dicarboxylic acid during pyrene degradation (10, 20, 44). Therefore, it is likely that the same mono- and dioxygenases and ortho-cleavage enzymes are involved in initial K region attack and subsequent ring fission of the dihydroxylated intermediates of phenanthrene and pyrene. Interestingly, dioxygenase attack also occurred at the C-3 and C-4 positions of phenanthrene to form a cis-3,4-dihydrodiol. This was followed by dehydrogenation to form 3,4-dihydroxyphenanthrene and then by meta-cleavage to form 1-hydroxy-2-naphthoic acid. This degradation pathway is similar to the phthalate pathway in other bacterial strains (32, 42). The isolation of phenanthrene trans-9,10-dihydrodiol indicates a monooxygenase attack on the phenanthrene nucleus to form phenanthrene 9,10-epoxide, followed by epoxide hydrolase to form the trans-dihydrodiol. This mode of enzymatic attack is similar to what was found in previous studies on the naphthalene and pyrene degradation pathways (20, 28). This work confirms and extends the catabolic pathways previously proposed for phenanthrene degradation by Mycobacterium species. We note that Mycobacterium sp. strains BG1 and BB1 degrade phenanthrene via 1-hydroxy-2-naphthoic acid and then via the meta-cleavage of protocatechuate (4, 16); however, no data have been provided for the initial oxidation reactions.
Rehmann et al. (41) showed that Mycobacterium sp. strain KR2 metabolizes phenanthrene in the 3,4 and 9,10 positions to form cis-3,4- and 9,10-dihydrodiols. 1-Hydroxy-2-naphthoic acid, phthalic acid, and 2-carboxybenzaldehyde were isolated from the culture filtrate, suggesting that ring fission pathways in Mycobacterium sp. strain KR-2 are similar to those previously reported for gram-negative bacteria. The degradation pattern of Mycobacterium sp. strain PYR-1 was similar to that of Mycobacterium sp. strain KR-2, except that phenanthrene trans-9,10-dihydrodiol was not detected using KR-2.
Recently, Tongpim and Pickard (50) reported that Mycobacterium sp. strain S1 grown on commercial anthracene, which contained phenanthrene as an impurity, formed phenanthrene trans-9,10-dihydrodiol. NMR analysis was not conducted on the metabolite to rigorously confirm that the phenanthrene 9,10-dihydrodiol was the trans and not the cis-isomer, although the trans-isomer assignment was supported by cytochrome P450 inhibitor experiments. In the present investigation, we show that both the cis and trans-9,10-dihydrodiols were produced by Mycobacterium sp. strain PYR-1.
Data from this investigation and previous studies of the degradation of PAHs by Mycobacterium sp. strain PYR-1 suggest that both dioxygenases and monooxygenases catalyze the initial attack on the aromatic ring. Since positional isomers of cis-dihydrodiols are formed, it may also be suggested that several dioxygenases are present in Mycobacterium sp. strain PYR-1. The broad range of PAHs that are degraded by Mycobacterium sp. strain PYR-1 may also indicate a relaxed specificity of the same dioxygenase for initial attack on PAHs. It is interesting that the ortho- and meta-ring fission pathways have similarities to, but also differences from, those known for other bacterial strains. The identification of ortho-ring cleavage intermediates from the degradation of dihydroxylated metabolites of anthracene, phenanthrene, and pyrene (20) indicates alternative enzymatic routes in the degradation of PAHs by Mycobacterium sp. strain PYR-1. Since, to date, all evidence on the catabolic pathways has been based on the identification of initial aromatic ring oxidation and ring fission products, it would be speculative to conclude what the oxygenation mechanisms in Mycobacterium sp. strain PYR-1 are without biochemical and molecular genetic analysis of the biodegradation pathways.
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ACKNOWLEDGMENTS |
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We thank John B. Sutherland and Thomas M. Heinze for critical review of the manuscript. We also thank Pat Fleischer for clerical assistance and Mona I. Churchwell for technical assistance.
Part of this work was supported by Cooperative Agreement CR820773 from the U.S. Environmental Protection Agency.
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FOOTNOTES |
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* Corresponding author. Mailing address: Division of Microbiology, National Center for Toxicological Research, U.S. Food and Drug Administration, Jefferson, AR 72079-9502. Phone: (870)543-7341. Fax: (870)543-7307. E-mail: CCerniglia{at}nctr.fda.gov.
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REFERENCES |
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Top
Abstract
Introduction
Materials and Methods
Results
Discussion
References
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Applied and Environmental Microbiology, April 2001, p. 1476-1483, Vol. 67, No. 4
0099-2240/01/$04.00+0 DOI: 10.1128/AEM.67.4.1476-1483.2001
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