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Review

Variability in Assembly of Degradation Operons for Naphthalene and its derivative, Carbaryl, Suggests Mobilization through Horizontal Gene Transfer

by
Prashant S. Phale
*,
Bhavik A. Shah
and
Harshit Malhotra
Department of Biosciences and Bioengineering, Indian Institute of Technology-Bombay, Powai, Mumbai 400 076, India
*
Author to whom correspondence should be addressed.
Genes 2019, 10(8), 569; https://doi.org/10.3390/genes10080569
Submission received: 30 May 2019 / Revised: 11 July 2019 / Accepted: 11 July 2019 / Published: 27 July 2019
(This article belongs to the Special Issue Genetics of Biodegradation and Bioremediation)
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Abstract

:
In the biosphere, the largest biological laboratory, increased anthropogenic activities have led microbes to evolve and adapt to the changes occurring in the environment. Compounds, specifically xenobiotics, released due to such activities persist in nature and undergo bio-magnification in the food web. Some of these compounds act as potent endocrine disrupters, mutagens or carcinogens, and therefore their removal from the environment is essential. Due to their persistence, microbial communities have evolved to metabolize them partially or completely. Diverse biochemical pathways have evolved or been assembled by exchange of genetic material (horizontal gene transfer) through various mobile genetic elements like conjugative and non-conjugative plasmids, transposons, phages and prophages, genomic islands and integrative conjugative elements. These elements provide an unlimited opportunity for genetic material to be exchanged across various genera, thus accelerating the evolution of a new xenobiotic degrading phenotype. In this article, we illustrate examples of the assembly of metabolic pathways involved in the degradation of naphthalene and its derivative, Carbaryl, which are speculated to have evolved or adapted through the above-mentioned processes.

1. Introduction

Anthropogenic activities like manufacturing, industrialization and combustion of fossil fuels have led to the release of a large number of compounds in the environment, which were previously unknown to the biosphere. These compounds, known as xenobiotics, are toxic to various life forms and persist in the environment for a long period of time. Monocyclic and polycyclic aromatic hydrocarbons (PAHs) form a major group of xenobiotics. Due to the highly reduced nature, resonance stabilized structure, greater hydrophobicity, and lower aqueous solubility, they are resistant to biodegradation (recalcitrant). They act as metabolic inhibitors, endocrine disrupters [1] and further reactive epoxide formed due to metabolic activation of these compounds by microsomal enzymes interacts with DNA, causing mutation(s) or chromosomal damage [2,3,4] which may lead to cytotoxicity, genotoxicity and/or carcinogenicity [5]. Repeated application and release of these compounds in the environment has exerted a selection pressure onto the microbes, resulting in the evolution of novel/unique degradative pathways. Although processes such as volatilization, chemical oxidation and photo-oxidation contribute to degradation, bioremediation is the most efficient and cost-effective method for complete removal of these compounds [6,7]. In this review, we focus on the metabolism and various genetic elements involved in the assembly of the degradative pathways for naphthalene and its derivative, Carbaryl.
Naphthalene is ubiquitous in the environment and used extensively in the manufacture of various compounds including pesticides and plastics, as well as for domestic consumption (mothballs, insect repellent). Being hydrophobic, it partitions into the membranes [8] and gets accumulated in tissues of aquatic organisms, leading to toxicity [9,10]. In humans, exposure to naphthalene occurs via skin, oral ingestion or inhalation of fumes. Acute toxicity causes hemolytic anemia [11], whereas exposure to higher doses causes cerebral oedema and chronic renal failure [12]. Naphthalene has been classified as a potential human carcinogen based on the studies performed on experimental animals [13].
Carbaryl (1-naphthyl N-methylcarbamate), a derivative of naphthalene, is a broad-spectrum carbamate family insecticide that has been manufactured and used since 1960. It acts as a competitive inhibitor of the enzyme acetylcholine esterase of the central nervous system leading to paralysis [14]. It is highly toxic to aquatic invertebrates, amphibians, bees, earthworms and humans [15,16,17,18,19,20,21]. It has also been classified as a likely human carcinogen based on vascular tumour formation in mice [22]. In nature, various bacterial species belonging to genus Pseudomonas, Rhodococcus, Mycobacterium, Nocardia, Bacillus, Vibrio, Marinobacter, Micrococcus and Sphingomonas have been reported to degrade naphthalene and Carbaryl.

2. Microbial Adaptation to Aromatics and Xenobiotics

Aromatics including PAHs and xenobiotics like pesticides, being toxic and persistent, act as a selection force on the microbial community to evolve degradative pathways and possibly remove sensitive microorganisms from the population [23,24,25]. Microbes adapt to these environmental challenges and acquire the ability to degrade these compounds using the following strategies:
a) Quite a few bacterial isolates have the ability to completely degrade and utilize mono as well as polycyclic aromatics like benzoate, phthalate isomers and their esters, chlorobenzoate, naphthalene, biphenyls, etc. [23,26,27,28,29,30,31,32,33,34,35,36,37,38,39,40,41]. Such organisms harbor genes encoding all enzymes responsible for the complete metabolism of these compounds as a sole source of carbon and energy. Further, these genes could be arranged as operon(s) so as to finetune their expression to achieve optimum degradation efficiency. In a few organisms, both the carbon source as well as detoxification pathways are functional. For example, in Pseudomonas putida CSV86, 1-methylnaphthalene, which is highly toxic and used as insect repellent, is metabolized by two pathways. It is transformed and detoxified by side chain hydroxylation pathway to 1-naphthoic acid, a less toxic and more water-soluble metabolite, which is released into the medium as a dead-end product [29]. Whereas in other pathway, 1-methylnaphthalene is ring-hydroxylated and further metabolized to central carbon pathway intermediates, thus acting as sole source of carbon and energy [42].
b) In biosphere, microbial communities degrade a diverse range of pollutants. Also, specific consortia are constructed in the laboratory based on their metabolic properties and compatibility of organisms to degrade the pollutants. Members of such communities/consortia achieve complete mineralization by working together, which is mutually beneficial. Initial transformation of the parent compound by one member yields metabolite(s) which may be a dead-end product(s) for its metabolic machinery, which can then be subsequently used by other member(s). To list a few examples: consortia of Pseudomonas spp. 50552 and 50581 involved in complete degradation of Carbaryl [43]; EC20 consortia of Pseudomonas, Mesorhizobium, Achromobacter, Stenotrophomonas, and Halomonas involved in BTEX (benzene, toluene, ethylbenzene and xylene) degradation [44]; consortia of five fungal and eight bacterial isolates to degrade phenanthrene, pyrene, and benzo(a)pyrene [45]; ASDC consortia of Rhodococcus sp., Bacillus sp., and Burkholderia sp. degrading chrysene [46]. Several bacteria, algae and fungi have been reported to transform methylnaphthalene into naphthoic acid [47,48] which can then be metabolized by other microbes like Stenotrophomonas maltophilia CSV89 [49].
c) Efficient degradation of certain xenobiotics can be achieved by supplementing with specific nutrient(s). For example, isophthalate, which is used in the plastic and textile industry, acts as a competitive inhibitor for the enzyme glutamate dehydrogenase (GDH), involved in the C/N metabolism. When the growth medium is supplemented with glutamate, GDH is relieved from the competitive inhibition by isophthalate, thereby enhancing the degradation efficiency of isophthalate in Pseudomonas sp. [50]. On the other hand, soil isolate Acinetobacter lwofii ISP4 degrades isophthalate faster and more efficiently without any supplementation of glutamate by expressing GDH, which has less sensitivity to inhibition by isophthalate and is synthesized in more quantity [51]. These examples indicate the adaptation by the microbes at the metabolic level for their effective survival.

3. Horizontal Gene Transfer Elements Involved in Catabolism of Aromatics

Genetic variation in microorganisms is the major driving factor in adaptation to environmental conditions. The metabolic diversity observed in the organism(s) can be attributed to the plasticity of the genome which is acquired through various strategies, resulting in the generation of genetic variants and ultimately adaptation, as described by Arber [52]. These include: (i) small local change(s) in the nucleotide sequence, (ii) reshuffling of gene fragments within the genome, and/or iii) horizontal gene transfer (HGT). The third strategy allows for evolution in quantum leaps [53] and is mediated through mobile genetic elements (MGEs) like plasmids (conjugative and non-conjugative), transposons, integrative conjugative elements (ICEs) and genomic islands (GEIs), as well as phages and prophages. The association of MGEs with catabolic gene clusters, as well as high levels of similarity in gene organization and nucleotide sequences among phylogenetically and geographically distant microbial species suggest that HGT is the major player in acquisition and assembly of the degradative pathways in microorganisms [25,54,55,56,57]. The presence of PAH-degradation genes on MGEs is an indication of ease of mobilization of catabolic genes and hence better adaptability to the polluted environment [58].
Catabolic plasmids involved in the degradation of camphor, octane, naphthalene, salicylate, etc. were first discovered in the early 70s [59,60,61,62,63]. These plasmids can either be conjugative or non-conjugative in nature. Plasmid isolation and characterization, and plasmid curing by chemicals as well as by nutritional conditions, southern hybridization, conjugation and transformation experiments established the association of the degradative property to the plasmid(s) [64,65,66,67]. Advances in genomic techniques and approaches have further provided insights into the evolutionary aspects of degradation properties [68,69,70]. Presence of insertion elements harboring functional or non-functional transposase and integrase like features have been seen to be associated with degradative genes in large number of catabolic plasmids like pWW0 and NAH7 amongst others [71,72]. The ability of some of these plasmids to move across various genera and strains make them carriers of the degradative property. Plasmids play an important role in the evolution of metabolic diversity in Pseudomonads [73].
Catabolic transposons form the major group of MGEs involved in the transfer of xenobiotic degradation property [74,75,76]. Transposons can be grouped into three classes based on the nucleotide sequence homology, genetic organization and mechanistic properties [77]. Class-I elements include composite transposons and simple insertion sequences (ISs). Simple ISs only contain the elements essential for transposition and are flanked by inverted or direct repeats (DRs). Composite transposons have genes encoding features other than transposition and are flanked by very similar ISs in direct or inverted position. For example, catabolic transposon Tn5280, harboring genes encoding chlorobenzene dioxygenase and dehydrogenase, was found to be part of the plasmid pP51 in Pseudomonas sp. strain P51 [78]. Class II transposons, known to transpose by the formation of co-integrate, are known to carry gene fragments greater than 50 kb. Transposon Tn4651 which harbors the xyl operon, is a part of Tn4653 and is located on the plasmid pWW0 in P. putida mt-2 [71,79]. The third class of transposons is called as conjugative transposons.
Elements like ICEs refer to a group of MGEs which had earlier been classified under different groups like conjugative transposons, integrative plasmids and GEIs [25,80]. These elements are excised by site-specific recombination yielding circular intermediates which are then transferred by conjugation to other bacteria and can possibly re-integrate into the genome [25,80]. Elements like GEIs have been described as MGEs residing on the genome in close proximity to a gene for a tRNA and harbor a gene for integrase and/along with a short duplication of the insertion element at the other end [53,54,81].
Pathogenicity islands (PAIs), a class of GEIs associated with the virulence phenotype, were first discovered in E. coli [82] and since then a wide plethora has been uncovered. Various disease associated toxins [83,84], antibiotic resistance genes [85] and even superantigens [86] are harbored on these MGEs. The similarity between the insertion sites of PAIs and phages at tRNA loci suggests that these islands are acquired through phage mediated HGT [87]. Also, certain PAIs harbor open reading frames that show high similarity to integrase of bacteriophages [88]. In comparison, conjugative transposons contain multiple integration sites and are not confined to tRNA genes. A few ICEs/GEIs are also reported to harbor genes involved in the degradation of various aromatic compounds; for example: clc element, for the metabolism of chlorobenzoate in Pseudomonas sp. strain B13 [89]; ICEXTD for m-xylene, toluene and cumene degradation in Azoarcus sp. CIB [90]; ICECSV86 for naphthalene degradation in P. putida CSV86 [91]; ICEclc JB2 for metabolism of o-halobenzoate and o-hydroxybenzoate in P. aeroginosa JB2 [92]; ICEKKS1024677 for the metabolism of polychlorinated biphenyl/biphenyl in Acidovorax sp. strain KKS102 [93]; proposed ICE harboring Tn4371, for the metabolism of biphenyl and 4-chlorobiphenyl [94]; and phn island for the metabolism of phenanthrene in Delftia sp. Cs1-4 [95]. The features of ICEs involved in aromatic compound degradation are depicted in Figure 1.
The clc element is the first GEI, reported and characterized in detail from Pseudomonas sp. strain B13 and involved in the degradation of 3-chlorobenzoate [89]. ICEclcB13, ICEXTDand ICECSV86 are associated with tRNAGly having att site at the 3’ end of tRNA (72% identity among all three att and 94% among ICEXTD and ICECSV86, Figure 1G). In P. aeruginosa JB2, the att site was found to be absent. The phn island involved in phenanthrene degradation from Delftia sp. Cs1-4 is structurally distinct from the clc family ICEs as it is not associated with the tRNA gene and has an SXT/R391 type mobilization system [95]. ICEKKS1024677 harbors bph operon and shows similar arrangement as observed in clc of B13 and ICECSV86, consisting of direct repeats (9 bp, attL and attR region in ICEKKS1024677) with attL at the start, followed by integrase. Also, it has been found to be integrated with the chromosome and shows low conjugal transfer frequency as observed in the case of CSV86 [93,96]. Transposon Tn4371 consists of transposase (tnpA) and phage-like integrase (int) genes [94]. Tn4371 and ICEKKS1024677 are flanked by 8 bp and 9 bp direct repeats (55.6% identity), respectively, which are not associated with/in proximity to tRNAGly.

4. Assembly of Naphthalene Degradation Pathway

Naphthalene, the simplest PAH, is used as a model compound to understand aromatic degradation pathways, enzymes and genetics. The number of microbes has been reported to metabolize naphthalene (Table 1A). The degradation is initiated by hydroxylation of one of the aromatic rings to yield 1,2-dihydroxynaphthalene, which is subsequently metabolized to salicylic acid. Generated salicylic acid is metabolized either via catechol (meta or ortho ring-cleavage) or gentisic acid to yield central carbon pathway metabolites like organic acids (Figure 2, Table 1A). Apart from these well studied routes, isolate Bacillus thermoleovorans was reported to degrade naphthalene via phthalic acid [97]. Based on biochemical, enzyme induction and regulation studies, naphthalene degradation pathway is segmented into upper pathway (naphthalene to salicylate, nah operon) and lower pathway (salicylate to central carbon pathway either via catechol, sal operon or gentisate, gen/sgp operon).
Metabolic diversity observed in naphthalene degradation pathways (Figure 2) is possible due to acquisition or exchange of genetic material. Genes for naphthalene degradation were found to be present on plasmid, chromosome, transposon or ICE (Table 1). The arrangement of genes encoding enzymes involved in naphthalene degradation is depicted in Figure 3. The degradation genes are arranged as two inducible operons: upper pathway (nah) and lower pathway (sal or sgp/gen) operon [98,99,100]. These operons are induced by salicylic acid and its analogue like 2-aminobenzoate and 2-hydroxybenzyl alcohol [100]. Among naphthalene degrading strains, the function of nahR was found to be highly conserved [101].
In P. putida G7, the plasmid NAH7 is known to harbor naphthalene degradation genes which are proposed to be part of a defective transposon which requires Tn4653 transposase for mobilization [99]. In NAH7, the transcription for nah and sal operons is in the same direction. In P. putida strain NCIB9816-4, genes were found to be present on a conjugative plasmid pDTG1 as two operons (~15 kb apart) which are transcribed in opposite direction [102]. As compared to NAH7 and pDTG1, a non-conjugative pAK5 (IncP-7 group) from P. putida strain AK5 encodes naphthalene degradation via gentisate pathway as nah and gen/sgp operon [103]. In P. putida strain PMD-1, upper pathway genes (nah operon) were found to be located on the chromosome, while salicylate degradation genes (sal operon) were present on the conjugative plasmid pMWD-1 [104]. However, in P. stutzeri AN10, the naphthalene degradation genes (nah and sal operons) were found to be located on the chromosome and hypothesized to be recruited through transposition, recombination and rearrangement events [105,106]. Besides plasmids and chromosomes, naphthalene degradation genes were hypothesized to be present on ICE in P. putida CSV86 [91]. The draft genome analysis revealed that the nah operon is present next to tRNAGly(along with att region) and phage-like integrase [91], suggesting the involvement of a GEI, referred to as ICECSV86(Figure 3). This ICE is located on the chromosome and the degradation genes are arranged as nah and sal operons, which were transferred by conjugation at a very low frequency [96].
Interestingly, irrespective of the location of genes for naphthalene degradation either on plasmid, chromosome + plasmid, chromosome or ICE, the gene arrangement in nah and sal operon is almost conserved among various naphthalene degraders (Figure 3). Further, metabolic variations in isolates are generated through the regulation of operons and specificity of the enzyme(s), thus granting an advantage to the strain to metabolize naphthalene and other PAHs effectively [107,108].

5. Assembly of Carbaryl Degradation Pathway

Carbaryl has been used extensively in the agriculture sector since 1960. Repeated application has led microbes to adapt and utilize Carbaryl as the sole source of carbon and energy (Table 1B). The degradation pathway is initiated by hydrolyzing the ester bond by the enzyme Carbaryl hydrolase (CH) to yield 1-napthol. Generated 1-naphthol is ring-hydroxylated by the enzyme 1-naphthol hydroxylase (1NH) yielding 1,2-dihydroxynaphthalene, which is further metabolized via salicylic acid and gentisic acid. Few Carbaryl degraders also metabolize salicylic acid via catechol route [44] (Table 1B and Figure 2). The metabolic steps involved in the conversion of 1,2-dihydroxynaphthalene to salicylic acid are common for naphthalene and Carbaryl degradation (Figure 2). Interestingly, in naphthalene degraders salicylic acid is predominantly metabolized via catechol, whereas in Carbaryl degraders, it is metabolized mainly through the gentisic acid route (Table 1B and Figure 2).
A large number of genes involved in Carbaryl degradation have been proposed to be plasmid borne [121]. Arthrobacter sp. RC100 harbors three plasmids (pRC1, pRC2, and pRC300) of which conjugative plasmids, pRC1 and pRC2, encode enzymes for Carbaryl degradation up to gentisic acid. Enzymes involved in the conversion of gentisic acid to central carbon metabolites are encoded by genes located on the chromosome [115]. A Rhizobium sp. strain AC100, which transforms Carbaryl to 1-naphthol, harbors a plasmid pAC200 carrying gene cehA encoding CH as a part of Tnceh transposon flanked by insertion element-like sequence (istA and istB, Figure 4). istA and istB, which comprise the ISRsp3 element, showed homology to IS1600 element from A. eutrophus NH9 and of IS1326 from P. aeruginosa of the IS21 family. Treating cells with plasmid curing agents like mitomycin-C resulted in deletion of cehA from the Tnceh leaving behind the insertion elements as a part of plasmid pAC200d due to homologous recombination among ISRsp3 [116]. This depicts the instability of the system and loss of catabolic genes by the activation of IS elements. Sphingomonas sp. strain CF06, which degrades carbofuran and its derivatives (including Carbaryl), harbors five plasmids- pCF01, pCF02, pCF03, pCF04, and pCF05. Plasmid curing and conjugation experiments revealed that the degradation property was associated with plasmid(s). Southern hybridization studies revealed a high degree of sequence similarity among pCF01 and pCF02, and pCF03 and pCF04, indicating gene duplication, which could be due to lack of positive regulatory system. Various IS elements were found to be present on pCF01, pCF02 and pCF03. The presence of active IS elements as well as gene duplications indicate that the system is in an early stage of evolution [67]. In Carbaryl degrading consortia of two Pseudomonas spp., the strain 50581 harbors a conjugative plasmid, pCD1 (50 kb) which encodes for CH, while chromosomally located genes from strain 50552 encode enzymes for 1-naphthol degradation [43].
Soil isolates Pseudomonas spp. strains C4, C5pp and C6 utilizes Carbaryl via salicylic acid and gentisic acid (Figure 2, [30]). Based on metabolic studies like enzyme induction, cell respiration and biotransformation, the Carbaryl degradation pathway was hypothesized to be divided into upper, middle and lower segments; and genes are probably arranged as three distinct operons induced by respective carbon source [122]. The degradation property was found to be very stable and could not be cured by nutritional conditions or chemical agents. Southern hybridization analyses indicate genes encoding degradative enzymes are located on the host genome [122]. The draft genome sequence of Pseudomonas sp. C5pp, primer walking, and gap filling PCR studies yielded a 76.3 kb sequence, referred to as Supercontig-A, harboring all genes required for Carbaryl degradation (Figure 5), [123,124]. Genes encoding enzymes responsible for the conversion of Carbaryl to salicylic acid (upper operon), salicylic acid to gentisic acid (middle operon), and gentisic acid to central carbon metabolites (lower operon) are probably under the regulation of transcription regulators encoded by mcbG, mcbH and mcbN, respectively (Figure 5).
The draft genome (6.15 Mb) analysis revealed the presence of 42 MGEs and 36 GEIs, out of which 17 MGEs were located in Supercontig-A (76.3 kb), indicating this region could be a hotspot for genome alterations [123,124]. The upper and middle operon region showed lower G+C content (54%) compared to the genome (62.65%) of strain C5pp. Whereas, the lower operon region showed comparable (60%) G+C content. This skewing of G+C content suggests that genes of the upper and middle pathways probably have a different ancestral origin and have been acquired through HGT events and assembled in proximity to each other. This is evident from the fact that 40% of MGEs are located in the Supercontig A (which is 1% of the total genome) [123,124]. Of the 36 GEIs, 3 were found to be a part of Supercontig-A. The upper pathway genes, except the regulator mcbG constitute a single GEI (13.8 kb), whereas the middle (6.5 kb) and the lower (9.6 kb) pathway genes, including their respective regulators, were established to be parts of two distinct GEIs (Figure 5). Interestingly, P. putida XWY-1, isolated from waste water in Shangong, China, 4750 km away from the site of isolation of the strain C5pp (Mumbai, India), showed a similar gene arrangement and nucleotide sequence for the genes involved in Carbaryl mineralization; however, these genes were reported to be plasmid borne [120].
In Pseudomonas sp. strain C5pp, the upstream region of the upper pathway genes showed class-I integron features, which showed high identity (95–99%) with Tn6217 [124]. Other features present were transposase, 25 bp left-end repeat (92% homology to IRi), attI site, 5′ and 3′ conserved segment, resistance to streptomycin and two additional genes. The regulator mcbG is flanked by truncated transposases, which showed a similarity to ISPa20 of IS3 family at the left end and ISPst7 of IS5 family at the right end. The presence of partial transposase sequences indicate that their function has probably been lost due to decay linked recombination events and these might be the leftover sequences of previously functional ICE. The region consisting of middle pathway genes, mcbIJKL, flanked by IS21 family insertion repeats, exhibits class-I composite transposon like features and is referred to as the catabolic transposon TnC5ppsal [123]. Members belonging to class-I composite transposon have been known to harbor gene clusters involved in degradation of xenobiotics [25]. The transposases present at the 3’ end of the cluster show a high degree of similarity to the IS110 and IS5 family, reverse transcriptase, group-II intron D1-D4-2, and leucine-zipper class of integrase. As depicted in Figure 5, the insertion elements of the IS21 family are present in inverted orientation, which could be the reason for the stability of the catabolic transposon in the genome of strain C5pp. Also, it has been reported that the increase in size of the intervening sequence of the composite transposon lowers the transposition frequency [123,124]. The lower pathway genes encoding for catabolism of gentisic acid to central carbon metabolites, are hypothesized to be a part of class-I composite transposon, which is bordered by non-identical insertion elements showing sequence similarity with ISPa1635 and IS481 [123,124]. In addition to this, the prediction of the probable ancestral origin of the genes using the IMG-JGI server indicates that mcbBC, mcbEF, and mcbIJKL were probably derived from beta-proteobacteria; mcbA and mcbM from alpha-proteobacteria; and mcbD, mcbGH and mcbNOPQ from gamma-proteobacteria.
The steps involved in the conversion of 1,2-dihydroxynaphthalene to salicylate appears to be common in both naphthalene and Carbaryl degradation pathways. Pair-wise sequence alignment (nucleotide as well as amino acid) of genes nahC, nahD, nahE and nahF (encoding these metabolic steps) from various naphthalene degrading Pseudomonads (Figure 3) and genes mcbB, mcbD, mcbE, and mcbF from Carbaryl degrading Pseudomonas sp. C5pp (Figure 5) revealed higher (~90–100%) identity amongst 2-hydroxybenzylidene pyruvate hydratase-aldolase as well as salicylaldehyde dehydrogenase encoding genes while 2-hydroxychromene 2-carboxylate isomerase showed moderate (~44–52%) identity. The phylogenetic analysis of Carbaryl degradation genes has been described in detail by Trivedi et al. [123,124]. Interestingly, 1,2-Dihydroxynaphthalene dioxygenase (12DHNDO) from strain C5pp, which belongs to class-II extradiol dioxygenases displayed low (4–10%) identity with 12DHNDOs from naphthalene degraders (class-I) as compared to protocatechuate 3,4-dioxygenase from lignin degraders Pseudomonas humi (74%) and Burkholderia sp. LIG30 (73%) [123,124]. Among various naphthalene degraders, irrespective of location, these genes displayed high (86–98%) identity. In strain C5pp, genes encoding CH and 1NH were hypothesized to be acquired from other degraders. Phylogenetic analysis revealed that CH from C5pp belongs to a new family of esterase with new conserved motif [124]. Enzyme 1NH from strain C5pp, which showed 47% activity on 2,4-dichlorophenol as substrate, yielded 55% identity with 2,4-dichlorophenol 6-monoxygenase from Paraburkholderia zhejiangensis [123,124]. This suggests that the strain has probably acquired the relevant gene, followed by mutations to evolve the enzyme, which will now accept 1-naphthol as its primary substrate. All of these observations indicate that the Carbaryl degradation genes must have been acquired through HGT followed by multiple transposition events leading to integration into the genome, giving a stable degradation phenotype in Pseudomonas sp. strain C5pp even in the absence of selection pressure.
Besides HGT events and assembly of genes in the form of operons, Pseudomonas sp. C5pp shows cellular level adaptation by compartmentalization of enzymes to tackle the toxicity of 1-naphthol [125,126]. This adaptation helps in degradation of higher concentration of Carbaryl (1% tested so far). The ability to metabolize Carbaryl at high concentration can be attributed to the presence of a low affinity CH (Km, 100 μM) in the periplasm of the bacterium [126]. This enzyme catalyses the conversion of Carbaryl to 1-naphthol (more toxic and recalcitrant than Carbaryl) in the periplasm, minimizing the interaction of 1-naphthol with cytoplasmic components. 1-Naphthol, transported across the membrane through diffusion and partition processes into the cytoplasm, is ring-hydroxylated by high affinity cytosolic 1NH (Km, 10μM) to 1,2-dihydroxynaphthalene and subsequently metabolized to central carbon pathway intermediates. The compartmentalization of enzymes involved in the degradation suggests a successful strategy evolved by Pseudomonas sp. strain C5pp for efficient degradation of Carbaryl at high concentration.

6. Conclusions

Bacteria, which are present ubiquitously in nature, with a simple unicellular structure and ability to grow faster, have made their niches very dynamic, metabolically as well as genotypically plastic, and hence hot spots for the evolution of new trait(s). During the process of adaptation to strenuous conditions, microbes might acquire new genes and functions to enhance survivability. In addition, they might mutate already existing and/or acquired genes. The former approach is mediated through MGEs, which are the major players responsible for genome plasticity. Microbes evolve genes for novel pathways encoding xenobiotic degradation by the above mechanisms, which are further assembled as transcription unit(s)/operon(s), so as to finetune their regulation. Thus, only the required enzymes of the degradative pathway or segment of the pathway are activated by the respective carbon source. Further, the mutations in the acquired gene(s), shuffling/rearrangement of genes and compartmentalization of metabolic steps grant an additional advantage to the organism to adapt and utilize the compound more efficiently, as observed in the case of Carbaryl metabolism by Pseudomonas sp. C5pp. Apart from plasmids and transposons, the genes for aromatic degradation have also been found to be present as a part of GEIs/ICEs in the genome of various organisms including Pseudomonas. Integration of the degradation property into the host genome may impart additional stability to the phenotype, as generally the plasmids are lost in the absence of selection pressure. Therefore, by employing various strategies, microbes display an ability to adapt to challenging environments.

Author Contributions

All three authors contributed equally towards conceptualization, writing original draft, review and editing. P.S.P. acquired funds through various government agencies to support the research activities.

Funding

PP acknowledges research grants from BRNS, DBT and DST, Govt. of India.

Acknowledgments

Thanks to Sravanti Kasarlawar for suggestions and discussion. BAS thanks DST for project Junior Research Fellowship and HM thanks CSIR, Govt. of India for Junior Research Fellowship.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Danzo, B.J. Environmental xenobiotics may disrupt normal endocrine function by interfering with the binding of physiological ligands to steroid receptors and binding proteins. Environ. Health Perspect. 1997, 105, 294–301. [Google Scholar] [CrossRef] [PubMed]
  2. Ohnishi, S.; Kawanishi, S. Double base lesions of DNA by a metabolite of carcinogenic benzo[a]pyrene. Biochem. Biophys. Res. Commun. 2002, 290, 778–782. [Google Scholar] [CrossRef] [PubMed]
  3. Conney, A.H. Induction of microsomal enzymes by foreign chemicals and carcinogenesis by polycyclic aromatic hydrocarbons: GHA Clowes memorial lecture. Cancer Res. 1982, 42, 4875–4917. [Google Scholar]
  4. Stegeman, J.J.; Lech, J.J. Cytochrome P-450 monooxygenase systems in aquatic species: Carcinogen metabolism and biomarkers for carcinogen and pollutant exposure. Environ. Health Perspect. 1991, 90, 101–109. [Google Scholar] [PubMed]
  5. Pashin, Y.V.; Bakhitova, L.M. Mutagenic and carcinogenic properties of polycyclic aromatic hydrocarbons. Environ. Health Perspect. 1979, 30, 185–189. [Google Scholar] [CrossRef] [PubMed]
  6. Wild, S.R.; Jones, K.C. Polynuclear aromatic hydrocarbons in the United Kingdom environment: A preliminary source inventory and budget. Environ. Pollut. 1995, 88, 91–108. [Google Scholar] [CrossRef]
  7. Haritash, A.K.; Kaushik, C.P. Biodegradation aspects of polycyclic aromatic hydrocarbons (PAHs): A review. J. Hazard. Mater. 2009, 169, 1–15. [Google Scholar] [CrossRef] [PubMed]
  8. Sikkema, J.; de Bont, J.A.; Poolman, B. Interactions of cyclic hydrocarbons with biological membranes. J. Biol. Chem. 1994, 269, 8022–8028. [Google Scholar] [PubMed]
  9. Hansen, B.H.; Altin, D.; Vang, S.H.; Nordtug, T.; Olsen, A.J. Effects of naphthalene on gene transcription in Calanus finmarchicus (Crustacea: Copepoda). Aquat. Toxicol. 2008, 86, 157–165. [Google Scholar] [CrossRef] [PubMed]
  10. Elumalai, M.; Balasubramanian, M.P. Influence of naphthalene on esterase activity during vitellogenesis of marine edible crab, Scylla serrata. Bull. Environ. Contam. Toxicol. 1999, 62, 743–748. [Google Scholar] [CrossRef]
  11. Valaes, T.; Doxiadis, S.A.; Fessas, P. Acute hemolysis due to naphthalene inhalation. J. Pediatr. 1963, 63, 904–915. [Google Scholar] [CrossRef]
  12. Gupta, R.; Singhal, P.C.; Muthusethupathy, M.A.; Malik, A.K.; Chugh, K.S. Cerebral oedema and renal failure following naphthalene poisoning. J. Assoc. Phys. India 1979, 27, 347–348. [Google Scholar]
  13. National Toxicology Program. Toxicology and carcinogenesis studies of naphthalene (CAS No. 91-20-3) in F344/N rats (inhalation studies). Natl. Toxicol. Program Tech. Rep. Ser. 2000, 500, 1–173. [Google Scholar]
  14. Smulders, C.J.; Bueters, T.J.; Van Kleef, R.G.; Vijverberg, H.P. Selective effects of carbamate pesticides on rat neuronal nicotinic acetylcholine receptors and rat brain acetylcholinesterase. Toxicol. Appl. Pharmacol. 2003, 193, 139–146. [Google Scholar] [CrossRef] [PubMed]
  15. Moeller, F.E. Effect of pollen availability on poisoning of honey bees by Carbaryl applied to sweet corn. J. Econ. Entomol. 1971, 64, 1314–1315. [Google Scholar] [CrossRef] [PubMed]
  16. Kaur, K.; Dhawan, A. Effect of Carbaryl on tissue composition, maturation, and breeding potential of Cirrhina mrigala (Ham.). Bull. Environ. Contam. Toxicol. 1996, 57, 480–486. [Google Scholar] [CrossRef] [PubMed]
  17. Boone, M.D.; Semlitsch, R.D.; Little, E.E.; Doyle, M.C. Multiple stressors in amphibian communities: Effects of chemical contamination, bullfrogs, and fish. Ecol. Appl. 2007, 17, 291–301. [Google Scholar] [CrossRef]
  18. Eraslan, G.; Kanbur, M.; Silici, S. Effect of Carbaryl on some biochemical changes in rats: The ameliorative effect of bee pollen. Food Chem. Toxicol. 2009, 47, 86–91. [Google Scholar] [CrossRef]
  19. Bridges, C.M. Tadpole swimming performance and activity affected by acute exposure to sub lethal levels of Carbaryl. Environ. Toxicol. Chem. 1997, 16, 1935–1939. [Google Scholar] [CrossRef]
  20. Bulen, B.J.; Distel, C.A. Carbaryl concentration gradients in realistic environments and their influence on our understanding of the tadpole food web. Arch. Environ. Contam. Toxicol. 2011, 60, 343–350. [Google Scholar] [CrossRef]
  21. Lima, M.P.; Cardoso, D.N.; Soares, A.M.; Loureiro, S. Carbaryl toxicity prediction to soil organisms under high and low temperature regimes. Ecotoxicol. Environ. Saf. 2015, 114, 263–272. [Google Scholar] [CrossRef] [PubMed]
  22. USEPA/Office of Pesticides Programs. Interim Reregistration Eligibility Decision for Carbaryl. p.2. Available online: https://www3.epa.gov/pesticides/chemsearch/regactions/reregistration/iredPC-056801_22-Oct-04.pdf (accessed on 15 April 2019).
  23. Gibson, D.T.; Subramanian, V. Microbial degradation of aromatic hydrocarbons. In Microbial Degradation of Organic Compounds; Gibson, D.T., Ed.; Microbiology Series; Marcel Dekker Inc.: New York, NY, USA; Basel, Switzerland, 1984; Volume 13, pp. 181–252. [Google Scholar]
  24. Singleton, I. Microbial metabolism of xenobiotics: Fundamental and applied research. J. Chem. Technol. Biotech. Int. Res. Process Environ. Clean Technol. 1994, 59, 9–23. [Google Scholar] [CrossRef]
  25. Nojiri, H.; Shintani, M.; Omori, T. Divergence of mobile genetic elements involved in the distribution of xenobiotic-catabolic capacity. Appl. Microbiol. Biotechnol. 2004, 64, 154–174. [Google Scholar] [CrossRef]
  26. Furukawa, K.; Matsumura, F. Microbial metabolism of polychlorinated biphenyls. Relative degradability of polychlorinated biphenyl components by Alkaligenes species. J. Agric. Food Chem. 1976, 24, 251–256. [Google Scholar] [CrossRef]
  27. Chatterjee, D.K.; Kellogg, S.T.; Hamada, S.; Chakrabarty, A.M. Plasmid specifying total degradation of 3-chlorobenzoate by a modified ortho pathway. J. Bacteriol. 1981, 146, 639–646. [Google Scholar] [Green Version]
  28. Baggi, G.; Barbieri, P.; Galli, E.; Tollari, S. Isolation of a Pseudomonas stutzeri strain that degrades o-xylene. Appl. Environ. Microbiol. 1987, 53, 2129–2132. [Google Scholar]
  29. Mahajan, M.C.; Phale, P.S.; Vaidyanathan, C.S. Evidence for the involvement of multiple pathways in the biodegradation of 1-and 2-methylnaphthalene by Pseudomonas putida CSV86. Arch. Microbiol. 1994, 161, 425–433. [Google Scholar] [CrossRef] [PubMed]
  30. Swetha, V.P.; Phale, P.S. Metabolism of Carbaryl via 1,2-dihydroxynaphthalene by soil isolates Pseudomonas sp. strains C4, C5, and C6. Appl. Environ. Microbiol. 2005, 71, 5951–5956. [Google Scholar] [CrossRef] [PubMed]
  31. Vamsee-Krishna, C.; Mohan, Y.; Phale, P.S. Biodegradation of phthalate isomers by Pseudomonas aeruginosa PP4, Pseudomonas sp. PPD and Acinetobacter lwoffii ISP4. Appl. Microbiol. Biotechnol. 2006, 72, 1263–1269. [Google Scholar] [CrossRef] [PubMed]
  32. John, R.C.; Essien, J.P.; Akpan, S.B.; Okpokwasili, G.C. Polycyclic aromatic hydrocarbon-degrading bacteria from aviation fuel spill site at Ibeno, Nigeria. Bull. Environ. Contam. Toxicol. 2012, 88, 1014–1019. [Google Scholar] [CrossRef] [PubMed]
  33. Zhang, H.; Jiang, X.; Lu, L.; Xiao, W. Biodegradation of polychlorinated biphenyls (PCBs) by the novel identified cyanobacterium Anabaena PD-1. PLoS ONE 2015, 10, e0131450. [Google Scholar] [CrossRef] [PubMed]
  34. Kanaly, R.A.; Harayama, S. Biodegradation of high-molecular-weight polycyclic aromatic hydrocarbons by bacteria. J. Bacteriol. 2000, 182, 2059–2067. [Google Scholar] [CrossRef] [PubMed]
  35. Smith, M.R. The biodegradation of aromatic hydrocarbons by bacteria. Biodegradation 1990, 1, 191–206. [Google Scholar] [CrossRef] [PubMed]
  36. Samanta, S.K.; Singh, O.V.; Jain, R.K. Polycyclic aromatic hydrocarbons: Environmental pollution and bioremediation. Trends Biotechnol. 2002, 20, 243–248. [Google Scholar] [CrossRef]
  37. González-Gaya, B.; Martínez-Varela, A.; Vila-Costa, M.; Casal, P.; Cerro-Gálvez, E.; Berrojalbiz, N.; Jiménez, B. Biodegradation as an important sink of aromatic hydrocarbons in the oceans. Nat. Geosci. 2019, 12, 119. [Google Scholar] [CrossRef]
  38. Srivastava, S.; Kumar, M. Biodegradation of polycyclic aromatic hydrocarbons (PAHs): A sustainable approach. In Sustainable Green Technologies for Environmental Management; Shah, S., Ramanan, V., Prasad, R., Eds.; Springer: Singapore, 2019; pp. 111–139. [Google Scholar]
  39. Ladino-Orjuela, G.; Gomes, E.; da Silva, R.; Salt, C.; Parsons, J.R. Metabolic pathways for degradation of aromatic hydrocarbons by bacteria. In Reviews of Environmental Contamination and Toxicology; de Voogt, P., Ed.; Springer: Cham, Switzerland, 2016; Volume 237, pp. 105–121. [Google Scholar]
  40. Liang, D.W.; Zhang, T.; Fang, H.H.; He, J. Phthalates biodegradation in the environment. Appl. Microbiol. Biotechnol. 2008, 80, 183. [Google Scholar] [CrossRef]
  41. Kumar, V.; Sharma, N.; Maitra, S.S. Comparative study on the degradation of dibutyl phthalate by two newly isolated Pseudomonas sp. V21b and Comamonas sp. 51F. Biotechnol. Rep. 2017, 15, 1–10. [Google Scholar] [CrossRef]
  42. Basu, A.; Dixit, S.S.; Phale, P.S. Metabolism of benzyl alcohol via catechol ortho-pathway in methylnaphthalene-degrading Pseudomonas putida CSV86. Appl. Microbiol. Biotechnol. 2003, 62, 579–585. [Google Scholar] [CrossRef]
  43. Chapalamadugu, S.; Chaudhry, G.R. Hydrolysis of Carbaryl by a Pseudomonas sp. and construction of a microbial consortium that completely metabolizes Carbaryl. Appl. Environ. Microbiol. 1991, 57, 744–750. [Google Scholar]
  44. Deng, Y.; Yang, F.; Deng, C.; Yang, J.; Jia, J.; Yuan, H. Biodegradation of BTEX aromatics by a haloduric microbial consortium enriched from a sediment of Bohai Sea, China. Appl. Biochem. Biotechnol. 2017, 183, 893–905. [Google Scholar] [CrossRef]
  45. Zafra, G.; Absalón, Á.E.; Anducho-Reyes, M.Á.; Fernandez, F.J.; Cortés-Espinosa, D.V. Construction of PAH-degrading mixed microbial consortia by induced selection in soil. Chemosphere 2017, 172, 120–126. [Google Scholar] [CrossRef]
  46. Vaidya, S.; Devpura, N.; Jain, K.; Madamwar, D. Degradation of chrysene by enriched bacterial consortium. Front. Microbiol. 2018, 9, 1333. [Google Scholar] [CrossRef]
  47. Cerniglia, C.E.; Freeman, J.P.; Althaus, J.R.; van Baalen, C. Metabolism and toxicity of 1-and 2-methylnaphthalene and their derivatives in cyanobacteria. Arch. Microbiol. 1983, 136, 177–183. [Google Scholar] [CrossRef]
  48. Cerniglia, C.E. Microbial metabolism of polycyclic aromatic hydrocarbons. Adv. Appl. Microbiol. 1984, 30, 31–71. [Google Scholar]
  49. Phale, P.S.; Mahajan, M.C.; Vaidyanathan, C.S. A pathway for biodegradation of 1-naphthoic acid by Pseudomonas maltophilia CSV89. Arch. Microbiol. 1995, 163, 42–47. [Google Scholar] [CrossRef]
  50. Vamsee-Krishna, C.; Phale, P.S. Bacterial degradation of phthalate isomers and their esters. Indian J. Microbiol. 2008, 48, 19–34. [Google Scholar] [CrossRef] [Green Version]
  51. Vamsee-Krishna, C.; Phale, P.S. Bypassing isophthalate inhibition by modulating glutamate dehydrogenase (GDH): Purification and kinetic characterization of NADP-GDHs from isophthalate-degrading Pseudomonas aeruginosa strain PP4 and Acinetobacter lwoffii strain ISP4. J. Bacteriol. 2010, 192, 801–806. [Google Scholar] [CrossRef]
  52. Arber, W. Genetic variation: Molecular mechanisms and impact on microbial evolution. FEMS Microbiol. Rev. 2000, 24, 1–7. [Google Scholar] [CrossRef]
  53. Hacker, J.; Carniel, E. Ecological fitness, genomic islands and bacterial pathogenicity: A Darwinian view of the evolution of microbes. EMBO Rep. 2001, 2, 376–381. [Google Scholar] [CrossRef]
  54. van der Meer, J.R.; Sentchilo, V. Genomic islands and the evolution of catabolic pathways in bacteria. Curr. Opin. Biotechnol. 2003, 14, 248–254. [Google Scholar] [CrossRef]
  55. Springael, D.; Top, E.M. Horizontal gene transfer and microbial adaptation to xenobiotics: New types of mobile genetic elements and lessons from ecological studies. Trends Microbiol. 2004, 12, 53–58. [Google Scholar] [CrossRef]
  56. Van Der Meer, J.R.; De Vos, W.M.; Harayama, S.; Zehnder, A.J. Molecular mechanisms of genetic adaptation to xenobiotic compounds. Microbiol. Mol. Biol. Rev. 1992, 56, 677–694. [Google Scholar]
  57. Nagata, Y.; Kato, H.; Ohtsubo, Y.; Tsuda, M. Mobile genetic elements involved in the evolution of bacteria that degrade recalcitrant xenobiotic compounds. In DNA Traffic in the Environment; Hiromi, N., Taku, O., Eds.; Springer: Singapore, 2019; pp. 215–244. [Google Scholar]
  58. Johnsen, A.R.; Wick, L.Y.; Harms, H. Principles of microbial PAH-degradation in soil. Environ. Pollut. 2005, 133, 71–84. [Google Scholar] [CrossRef]
  59. Chakrabarty, A.M. Genetic basis of the biodegradation of salicylate in Pseudomonas. J. Bacteriol. 1972, 112, 815–823. [Google Scholar]
  60. Chakrabarty, A.M.; Chou, G.; Gunsalus, I.C. Genetic regulation and extra chromosomal nature of octane degradative pathway in Pseudomonas. Proc. Natl. Acad. Sci. USA 1973, 70, 1137–1140. [Google Scholar] [CrossRef]
  61. Dunn, N.W.; Gunsalus, I.C. Transmissible plasmid coding early enzymes of naphthalene oxidation in Pseudomonas putida. J. Bacteriol. 1973, 114, 974–979. [Google Scholar]
  62. Rheinwald, J.G.; Chakrabarty, A.M.; Gunsalus, I.C. A transmissible plasmid controlling camphor oxidation in Pseudomonas putida. Proc. Natl. Acad. Sci. USA 1973, 70, 885–889. [Google Scholar] [CrossRef]
  63. Worsey, M.J.; Williams, P.A. Metabolism of toluene and xylenes by Pseudomonas putida (arvilla) mt-2: Evidence for a new function of the TOL plasmid. J. Bacteriol. 1975, 124, 7–13. [Google Scholar]
  64. Mulbry, W.W.; Karns, J.S.; Kearney, P.C.; Nelson, J.O.; McDaniel, C.S.; Wild, J.R. Identification of a plasmid-borne parathion hydrolase gene from Flavobacterium sp. by southern hybridization with opd from Pseudomonas diminuta. Appl. Environ. Microbiol. 1986, 51, 926–930. [Google Scholar]
  65. Hayatsu, M.; Hirano, M.; Tokuda, S. Involvement of two plasmids in fenitrothion degradation by Burkholderia sp. strain NF100. Appl. Environ. Microbiol. 2000, 66, 1737–1740. [Google Scholar] [CrossRef]
  66. Wu, S.J.; Hu, Z.H.; Zhang, L.L.; Yu, X.; Chen, J.M. A novel dichloromethane-degrading Lysinibacillus sphaericus strain wh22 and its degradative plasmid. Appl. Microbiol. Biotechnol. 2009, 82, 731–740. [Google Scholar] [CrossRef]
  67. Feng, X.; Ou, L.T.; Ogram, A. Plasmid-mediated mineralization of carbofuran by Sphingomonas sp. strain CF06. Appl. Environ. Microbiol. 1997, 63, 1332–1337. [Google Scholar]
  68. Maeda, K.; Nojiri, H.; Shinatani, M.; Yoshida, T.; Habe, H.; Omori, T. Complete nucleotide sequence of carbazole/dioxin degrading plasmid pCAR1 in Pseudomonas resinovorans strain CA10 indicates its mosaicity and the presence of large catabolic transposon Tn4676. J. Mol. Biol. 2003, 326, 21–33. [Google Scholar] [CrossRef]
  69. Martinez, B.; Tomkins, J.; Wackett, L.P.; Wing, R.; Sadowsky, M.J. Complete nucleotide sequence and organization of the atrazine catabolic plasmid pADP-1 from Pseudomonas sp. strain ADP. J. Bacteriol. 2001, 183, 5684–5697. [Google Scholar] [CrossRef]
  70. Sota, M.; Kawasaki, H.; Tsuda, M. Structure of haloacetate catabolic IncP-1β plasmid pUO1 and genetic mobility of its residing haloacetate-catabolic transposon. J. Bacteriol. 2003, 185, 6741–6745. [Google Scholar] [CrossRef]
  71. Tsuda, M.; Iino, T. Identification and characterization of Tn4653, a transposon covering the toluene transposon Tn4651 on TOL plasmid pWW0. Mol. Gen. Genet. 1988, 213, 72–77. [Google Scholar] [CrossRef]
  72. Tsuda, M.; Iino, T. Naphthalene degrading genes on plasmid NAH7 are on a defective transposon. Mol. Gen. Genet. 1990, 223, 33–39. [Google Scholar] [CrossRef]
  73. Obayori, O.S.; Salam, L.B. Degradation of polycyclic aromatic hydrocarbons: Role of plasmids. Sci. Res. Essays 2010, 5, 4093–4106. [Google Scholar]
  74. Weightman, A.J.; Topping, A.W.; Hill, K.E.; Lee, L.L.; Sakai, K.; Slater, J.H.; Thomas, A.W. Transposition of DEH, a broad-host-range transposon flanked by ISPpu12, in Pseudomonas putida is associated with genomic rearrangements and dehalogenase gene silencing. J. Bacteriol. 2002, 184, 6581–6591. [Google Scholar] [CrossRef]
  75. Williams, P.A.; Jones, R.M.; Shaw, L.E. A third transposable element, ISPpu12, from the toluene-xylene catabolic plasmid pWW0 of Pseudomonas putida mt-2. J. Bacteriol. 2002, 184, 6572–6580. [Google Scholar] [CrossRef]
  76. Tsuda, M.; Genka, H. Identification and characterization of Tn4656, a novel class II transposon carrying a set of toluene degrading genes from TOL plasmid pWW53. J. Bacteriol. 2001, 183, 6215–6224. [Google Scholar] [CrossRef]
  77. Grindley, N.D.; Reed, R.R. Transpositional recombination in prokaryotes. Annu. Rev. Biochem. 1985, 54, 863–896. [Google Scholar] [CrossRef]
  78. van der Meer, J.R.; Zehnder, A.J.; de Vos, W.M. Identification of a novel composite transposable element, Tn5280, carrying chlorobenzene dioxygenase genes of Pseudomonas sp. strain P51. J. Bacteriol. 1991, 173, 7077–7083. [Google Scholar] [CrossRef]
  79. Tsuda, M.; Minegishi, K.I.; Iino, T. Toluene transposons Tn4651 and Tn4653 are class II transposons. J. Bacteriol. 1989, 171, 1386–1393. [Google Scholar] [CrossRef] [Green Version]
  80. Burrus, V.; Pavlovic, G.; Decaris, B.; Guédon, G. Conjugative transposons: The tip of the iceberg. Mol. Microbiol. 2002, 46, 601–610. [Google Scholar] [CrossRef]
  81. Hentschel, U.; Hacker, J. Pathogenicity islands: The tip of the iceberg. Microb. Infect. 2001, 3, 545–548. [Google Scholar] [CrossRef]
  82. Blum, G.; Ott, M.; Lischewski, A.; Ritter, A.; Imrich, H.; Tschäpe, H.; Hacker, J. Excision of large DNA regions termed pathogenicity islands from tRNA-specific loci in the chromosome of an Escherichia coli wild-type pathogen. Infect. Immun. 1994, 62, 606–614. [Google Scholar]
  83. Yamaguchi, T.; Nishifuji, K.; Sasaki, M.; Fudaba, Y.; Aepfelbacher, M.; Takata, T.; Ohara, M.; Komatsuzawa, H.; Amagai, M.; Sugai, M. Identification of the Staphylococcus aureus etd pathogenicity island which encodes a novel exfoliative toxin, ETD, and EDIN-B. Infect. Immun. 2002, 70, 5835–5845. [Google Scholar] [CrossRef]
  84. Parreira, V.R.; Gyles, C.L. A novel pathogenicity island integrated adjacent to the thrW tRNA gene of avian pathogenic Escherichia coli encodes a vacuolating autotransporter toxin. Infect. Immun. 2003, 71, 5087–5096. [Google Scholar] [CrossRef]
  85. Luck, S.N.; Turner, S.A.; Rajakumar, K.; Sakellaris, H.; Adler, B. Ferric dicitrate transport system (Fec) of Shigella flexneri 2a YSH6000 is encoded on a novel pathogenicity island carrying multiple antibiotic resistance genes. Infect. Immun. 2001, 69, 6012–6021. [Google Scholar] [CrossRef]
  86. Novick, R.P. Mobile genetic elements and bacterial toxinoses: The superantigen-encoding pathogenicity islands of Staphylococcus aureus. Plasmid 2003, 49, 93–105. [Google Scholar] [CrossRef]
  87. Inouye, S.; Sunshine, M.G.; Six, E.W.; Inouye, M. Retronphage phi R73: An E. coli phage that contains a retroelement and integrates into a tRNA gene. Science 1991, 252, 969–971. [Google Scholar] [CrossRef]
  88. Cheetham, B.F.; Katz, M.E. A role for bacteriophages in the evolution and transfer of bacterial virulence determinants. Mol. Microbiol. 1995, 18, 201–208. [Google Scholar] [CrossRef]
  89. Gaillard, M.; Vallaeys, T.; Vorhölter, F.J.; Minoia, M.; Werlen, C.; Sentchilo, V.; Pühler, A.; van der Meer, J.R. The clc element of Pseudomonas sp. strain B13, a genomic island with various catabolic properties. J. Bacteriol. 2006, 188, 1999–2013. [Google Scholar] [CrossRef]
  90. Zamarro, M.T.; Martín-Moldes, Z.; Díaz, E. The ICEXTD of Azoarcus sp. CIB, an integrative and conjugative element with aerobic and anaerobic catabolic properties. Environ. Microbiol. 2016, 18, 5018–5031. [Google Scholar] [CrossRef]
  91. Paliwal, V.; Raju, S.C.; Modak, A.; Phale, P.S.; Purohit, H.J. Pseudomonas putida CSV86: A candidate genome for genetic bioaugmentation. PLoS ONE 2014, 9, e84000. [Google Scholar] [CrossRef]
  92. Obi, C.C.; Vayla, S.; De Gannes, V.; Berres, M.E.; Walker, J.; Pavelec, D.; Hyman, J.; Hickey, W.J. The integrative conjugative element clc (ICEclc) of Pseudomonas aeruginosa JB2. Front. Microbiol. 2018, 9, 1532. [Google Scholar] [CrossRef]
  93. Ohtsubo, Y.; Ishibashi, Y.; Naganawa, H.; Hirokawa, S.; Atobe, S.; Nagata, Y.; Tsuda, M. Conjugal transfer of polychlorinated biphenyl/biphenyl degradation genes in Acidovorax sp. strain KKS102, which are located on an integrative and conjugative element. J. Bacteriol. 2012, 194, 4237–4248. [Google Scholar] [CrossRef]
  94. Toussaint, A.; Merlin, C.; Monchy, S.; Benotmane, M.A.; Leplae, R.; Mergeay, M.; Springael, D. The biphenyl-and 4-chlorobiphenyl-catabolic transposon Tn4371, a member of a new family of genomic islands related to IncP and Ti plasmids. Appl. Environ. Microbiol. 2003, 69, 4837–4845. [Google Scholar] [CrossRef]
  95. Hickey, W.J.; Chen, S.; Zhao, J. The phn island: A new genomic island encoding catabolism of polynuclear aromatic hydrocarbons. Front. Microbiol. 2012, 3, 125. [Google Scholar] [CrossRef]
  96. Basu, A.; Phale, P.S. Conjugative transfer of preferential utilization of aromatic compounds from Pseudomonas putida CSV86. Biodegradation 2008, 19, 83–92. [Google Scholar] [CrossRef]
  97. Annweiler, E.; Richnow, H.H.; Antranikian, G.; Hebenbrock, S.; Garms, C.; Franke, S.; Francke, W.; Michaelis, W. Naphthalene degradation and incorporation of naphthalene-derived carbon into biomass by the thermophile Bacillus thermoleovorans. Appl. Environ. Microbiol. 2000, 66, 518–523. [Google Scholar] [CrossRef]
  98. Yen, K.M.; Gunsalus, I.C. Regulation of naphthalene catabolic genes of plasmid NAH7. J. Bacteriol. 1985, 162, 1008–1013. [Google Scholar] [Green Version]
  99. Sota, M.; Yano, H.; Ono, A.; Miyazaki, R.; Ishii, H.; Genka, H.; Top, E.M.; Tsuda, M. Genomic and functional analysis of the IncP-9 naphthalene-catabolic plasmid NAH7 and its transposon Tn4655 suggests catabolic gene spread by a tyrosine recombinase. J. Bacteriol. 2006, 188, 4057–4067. [Google Scholar] [CrossRef]
  100. Shamsuzzaman, K.M.; Barnsley, E.A. The regulation of naphthalene oxygenase in pseudomonads. Microbiology 1974, 83, 165–170. [Google Scholar] [CrossRef]
  101. Park, W.; Padmanabhan, P.; Padmanabhan, S.; Zylstra, G.J.; Madsen, E.L. nahR, encoding a LysR-type transcriptional regulator, is highly conserved among naphthalene-degrading bacteria isolated from a coal tar waste-contaminated site and in extracted community DNA. Microbiology 2002, 148, 2319–2329. [Google Scholar] [CrossRef]
  102. Dennis, J.J.; Zylstra, G.J. Complete sequence and genetic organization of pDTG1, the 83 kilobase naphthalene degradation plasmid from Pseudomonas putida strain NCIB 9816-4. J. Mol. Biol. 2004, 341, 753–768. [Google Scholar] [CrossRef]
  103. Izmalkova, T.Y.; Sazonova, O.I.; Nagornih, M.O.; Sokolov, S.L.; Kosheleva, I.A.; Boronin, A.M. The organization of naphthalene degradation genes in Pseudomonas putida strain AK5. Res. Microbiol. 2013, 164, 244–253. [Google Scholar] [CrossRef]
  104. Zuniga, M.C.; Durham, D.R.; Welch, R.A. Plasmid-and chromosome-mediated dissimilation of naphthalene and salicylate in Pseudomonas putida PMD-1. J. Bacteriol. 1981, 147, 836–843. [Google Scholar]
  105. Bosch, R.; García-Valdés, E.; Moore, E.R. Genetic characterization and evolutionary implications of a chromosomally encoded naphthalene-degradation upper pathway from Pseudomonas stutzeri AN10. Gene 1999, 236, 149–157. [Google Scholar] [CrossRef]
  106. Bosch, R.; García-Valdés, E.; Moore, E.R. Complete nucleotide sequence and evolutionary significance of a chromosomally encoded naphthalene-degradation lower pathway from Pseudomonas stutzeri AN10. Gene 2000, 245, 65–74. [Google Scholar] [CrossRef]
  107. Connors, M.A.; Barnsley, E.A. Naphthalene plasmids in pseudomonads. J. Bacteriol. 1982, 149, 1096–1101. [Google Scholar] [Green Version]
  108. Foght, J.M.; Westlake, D.W. Transposon and spontaneous deletion mutants of plasmid-borne genes encoding polycyclic aromatic hydrocarbon degradation by a strain of Pseudomonas fluorescens. Biodegradation 1996, 7, 353–366. [Google Scholar] [CrossRef]
  109. Li, W.; Shi, J.; Wang, X.; Han, Y.; Tong, W.; Ma, L.; Liu, B.; Cai, B. Complete nucleotide sequence and organization of the naphthalene catabolic plasmid pND6-1 from Pseudomonas sp. strain ND6. Gene 2004, 336, 231–240. [Google Scholar] [CrossRef]
  110. Heinaru, E.; Vedler, E.; Jutkina, J.; Aava, M.; Heinaru, A. Conjugal transfer and mobilization capacity of the completely sequenced naphthalene plasmid pNAH20 from multi plasmid strain Pseudomonas fluorescens PC20. FEMS Microbiol. Ecol. 2009, 70, 563–574. [Google Scholar] [CrossRef]
  111. Kim, J.; Park, W. Genome analysis of naphthalene-degrading Pseudomonas sp. AS1 harboring the mega plasmid pAS1. J. Microbiol. Biotechnol. 2018, 28, 330–337. [Google Scholar] [CrossRef]
  112. Sud, R.K.; Sud, A.K.; Gupta, K.G. Degradation of Sevin (1-naphthyl N-methyl carbamate by Achromobacter sp. Arch. Mikrobiol. 1972, 87, 353–358. [Google Scholar] [CrossRef]
  113. Larkin, M.J.; Day, M.J. The metabolism of Carbaryl by three bacterial isolates, Pseudomonas spp. (NCIB 12042 & 12043) and Rhodococcus sp. (NCIB 12038) from garden soil. J. Appl. Bacteriol. 1986, 60, 233–242. [Google Scholar]
  114. Hayatsu, M.; Nagata, T. Purification and characterization of Carbaryl hydrolase from Blastobacter sp. strain M501. Appl. Environ. Microbiol. 1993, 59, 2121–2125. [Google Scholar]
  115. Hayatsu, M.; Hirano, M.; Nagata, T. Involvement of two plasmids in the degradation of Carbaryl by Arthrobacter sp. strain RC100. Appl. Environ. Microbiol. 1999, 65, 1015–1019. [Google Scholar]
  116. Hashimoto, M.; Fukui, M.; Hayano, K.; Hayatsu, M. Nucleotide sequence and genetic structure of a novel Carbaryl hydrolase gene (cehA) from Rhizobium sp. strain AC100. Appl. Environ. Microbiol. 2002, 68, 1220–1227. [Google Scholar] [CrossRef]
  117. Doddamani, H.P.; Ninnekar, H.Z. Biodegradation of Carbaryl by a Micrococcus species. Curr. Microbiol. 2001, 43, 69–73. [Google Scholar] [CrossRef]
  118. Seo, J.S.; Keum, Y.S.; Li, Q.X. Metabolomic and proteomic insights into Carbaryl catabolism by Burkholderia sp. C3 and degradation of ten N-methyl carbamates. Biodegradation 2013, 24, 795–811. [Google Scholar] [CrossRef]
  119. Trivedi, V.D.; Bharadwaj, A.; Varunjikar, M.S.; Singha, A.K.; Upadhyay, P.; Gautam, K.; Phale, P.S. Insights into metabolism and sodium chloride adaptability of Carbaryl degrading halotolerant Pseudomonas sp. strain C7. Arch. Microbiol. 2017, 199, 907–916. [Google Scholar] [CrossRef]
  120. Zhu, S.; Wang, H.; Jiang, W.; Yang, Z.; Zhou, Y.; He, J.; Hong, Q. Genome analysis of Carbaryl-degrading strain Pseudomonas putida XWY-1. Curr. Microbiol. 2019, 76, 927–929. [Google Scholar] [CrossRef]
  121. Cheesman, M.J.; Horne, I.; Weir, K.M.; Pandey, G.; Williams, M.R.; Scott, C.; Russell, R.J.; Oakeshott, J.G. Carbamate pesticides and their biological degradation: Prospects for enzymatic bioremediation. Ration. Environ. Manag. Agrochem. Risk Assess. Monit. Remedial Act. 2007, 966, 288–305. [Google Scholar]
  122. Singh, R.; Trivedi, V.D.; Phale, P.S. Metabolic regulation and chromosomal localization of Carbaryl degradation pathway in Pseudomonas sp. strains C4, C5 and C6. Arch. Microbiol. 2013, 195, 521–535. [Google Scholar] [CrossRef]
  123. Trivedi, V.D. Biochemical and Evolutionary Aspects of Carbaryl Metabolism in Pseudomonas sp. PhD Thesis, Indian Institute of Technology-Bombay, Mumbai, India, December 2016. [Google Scholar]
  124. Trivedi, V.D.; Jangir, P.K.; Sharma, R.; Phale, P.S. Insights into functional and evolutionary analysis of Carbaryl metabolic pathway from Pseudomonas sp. strain C5pp. Sci. Rep. 2016, 6, 38430. [Google Scholar] [CrossRef]
  125. Kamini; Sharma, R.; Punekar, N.S.; Phale, P.S. Carbaryl as a carbon and nitrogen source: An inducible methylamine metabolic pathway at the biochemical and molecular levels in Pseudomonas sp. strain C5pp. Appl. Environ. Microbiol. 2018, 84, e01866–e01918. [Google Scholar] [CrossRef]
  126. Kamini; Shetty, D.; Trivedi, V.D.; Varunjikar, M.; Phale, P.S. Compartmentalization of the Carbaryl degradation pathway: Molecular characterization of inducible periplasmic Carbaryl hydrolase from Pseudomonas spp. Appl. Environ. Microbiol. 2018, 84, e02115–e02117. [Google Scholar]
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Figure 1. The structural features of various integrative conjugative elements (ICEs) involved in aromatic compound metabolism from: (A) clc element of Pseudomonas sp. B13; (B) ICEXTDof Azoarcus sp. CIB; (C) ICECSV86element of Pseudomonas putida CSV86; (D) clc element of Pseudomonas aeruginosa JB2; (E) ICEKKS1024677 from Acidovorax sp. strain KKS102; and (F) Tn4371 transposon most likely to be an ICE from Cupriavidus oxalaticus. Panel (G) represents multiple sequence alignment of attachment site (‘att’) region of the 3’ end of tRNAGly of Pseudomonas sp.B13, as B13, Pseudomonas putida CSV86 as CSV86 and Azoarcus sp. CIB as ICEXTD. Question mark in panel C depicts the incomplete/unidentified downstream region and attR site. Figure is not to the scale. tRNA: Transfer-RNA.
Figure 1. The structural features of various integrative conjugative elements (ICEs) involved in aromatic compound metabolism from: (A) clc element of Pseudomonas sp. B13; (B) ICEXTDof Azoarcus sp. CIB; (C) ICECSV86element of Pseudomonas putida CSV86; (D) clc element of Pseudomonas aeruginosa JB2; (E) ICEKKS1024677 from Acidovorax sp. strain KKS102; and (F) Tn4371 transposon most likely to be an ICE from Cupriavidus oxalaticus. Panel (G) represents multiple sequence alignment of attachment site (‘att’) region of the 3’ end of tRNAGly of Pseudomonas sp.B13, as B13, Pseudomonas putida CSV86 as CSV86 and Azoarcus sp. CIB as ICEXTD. Question mark in panel C depicts the incomplete/unidentified downstream region and attR site. Figure is not to the scale. tRNA: Transfer-RNA.
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Figure 2. Metabolic diversity observed in naphthalene and Carbaryl degradation pathways from various soil bacterial isolates. Abbreviations are: NDO, naphthalene 1,2-dioxygenase; CH, Carbaryl hydrolase; 1NH, 1-naphthol 2-hydroxylase; S1H, salicylate 1-monoocxygenase; S5H, salicylate 5-hydroxylase; C12DO, catechol 1,2-dioxygenase; C23DO, catechol 2,3-dioxygenase; GDO, gentisate 1,2-dioxygenase. ortho and meta pathway indicates the mode of aromatic ring-cleavage by these enzymes.
Figure 2. Metabolic diversity observed in naphthalene and Carbaryl degradation pathways from various soil bacterial isolates. Abbreviations are: NDO, naphthalene 1,2-dioxygenase; CH, Carbaryl hydrolase; 1NH, 1-naphthol 2-hydroxylase; S1H, salicylate 1-monoocxygenase; S5H, salicylate 5-hydroxylase; C12DO, catechol 1,2-dioxygenase; C23DO, catechol 2,3-dioxygenase; GDO, gentisate 1,2-dioxygenase. ortho and meta pathway indicates the mode of aromatic ring-cleavage by these enzymes.
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Figure 3. The diversity observed with respect to location, transcription and arrangement of genes involved in naphthalene degradation from: (A) Pseudomonas putida G7 as Tn4655 transposon on plasmid NAH7 flanked by IR1 and IR6; (B) Pseudomonas putida strain NCIB9816-4 on conjugative plasmid pDTG1; (C) Pseudomonas putida AK5 on conjugative plasmid pAK5 via gentisate pathway; (D) Pseudomonas stutzeri AN10 on chromosome; (E) Pseudomonas putida CSV86 on ICE showing tRNAGly and integrase while the other end is still not known. Arrow indicates the direction of transcription. Genes responsible for upper pathway, ‘nah’ operon (naphthalene to salicylic acid metabolism) are depicted in green; lower pathway, ‘sal’ operon (salicylic acid to central carbon metabolites via catechol) are depicted in yellow; while those in pink are responsible for salicylate metabolism via gentisic acid, ‘sgp/gen’ operon. Genes depicted in cyan arrows indicates transposase or integrase, black boxes depict IR elements, while red box indicates tRNA gene with ‘att’ site, light green arrow represents the regulators of the operons and the black arrow represents the putative integral membrane transport protein. Figure is not to the scale. Genes and proteins encoded are: nahAa, 2Fe-2S iron-sulfur cluster binding domain-containing protein, reductase; nahAb, non-heme iron oxygenase ferredoxin subunit; nahAc, naphthalene 1,2-dioxygenase; nahAd, naphthalene 1,2-dioxygenase subunit beta; nahB, cis-naphthalene dihydrodiol dehydrogenase; nahF, salicylaldehyde dehydrogenase; nahC, 1,2-dihydroxynaphthalene dioxygenase (oxygenase); nahE, 2-hydroxybenzalpyruvate aldolase; nahD, 2-hydroxychromene-2-carboxylate isomerase; nahG, salicylate 1-monooxygenase; nahT, 2Fe-2S iron-sulfur cluster binding domain-containing protein (chloroplast-type ferredoxin); nahH, catechol 2,3-dioxygenase; nahI, 2-hydroxymuconic semialdehyde dehydrogenase; nahN, 2-hydroxymuconic semialdehyde dehydrogenase; nahL, 2-oxopent 4-enoate hydratase; nahO, 4-hydoxy-2-oxovalerate aldolase; nahM, acetaldehyde dehydrogenase; nahK, 4-oxalocrotonate decarboxylase/2-oxo 3-hexendioate decarboxylase; nahJ, 4-oxalocrotonate tautomerase family protein; nahY, methyl accepting chemotaxis protein; nahX, unknown; sgpA, reductase component of salicylate 5-hydroxylase; sgpI, gentisate 1,2-dioxygenase; sgpK, fumarylacetoacetate hydrolase/fumarylpyruvate hydrolase; sgpG, salicylate 5-hydroxylase large oxygenase subunit; sgpH, salicylate 5-hydroxylase small oxygenase subunit; sgpB, ferredoxin component of salicylate 5-hydroxylase; mpi, maleylacetoacetate isomerase; mct1, methyl-accepting chemotaxis sensory transducer; nahR and sgpR, LysR family transcriptional regulator.
Figure 3. The diversity observed with respect to location, transcription and arrangement of genes involved in naphthalene degradation from: (A) Pseudomonas putida G7 as Tn4655 transposon on plasmid NAH7 flanked by IR1 and IR6; (B) Pseudomonas putida strain NCIB9816-4 on conjugative plasmid pDTG1; (C) Pseudomonas putida AK5 on conjugative plasmid pAK5 via gentisate pathway; (D) Pseudomonas stutzeri AN10 on chromosome; (E) Pseudomonas putida CSV86 on ICE showing tRNAGly and integrase while the other end is still not known. Arrow indicates the direction of transcription. Genes responsible for upper pathway, ‘nah’ operon (naphthalene to salicylic acid metabolism) are depicted in green; lower pathway, ‘sal’ operon (salicylic acid to central carbon metabolites via catechol) are depicted in yellow; while those in pink are responsible for salicylate metabolism via gentisic acid, ‘sgp/gen’ operon. Genes depicted in cyan arrows indicates transposase or integrase, black boxes depict IR elements, while red box indicates tRNA gene with ‘att’ site, light green arrow represents the regulators of the operons and the black arrow represents the putative integral membrane transport protein. Figure is not to the scale. Genes and proteins encoded are: nahAa, 2Fe-2S iron-sulfur cluster binding domain-containing protein, reductase; nahAb, non-heme iron oxygenase ferredoxin subunit; nahAc, naphthalene 1,2-dioxygenase; nahAd, naphthalene 1,2-dioxygenase subunit beta; nahB, cis-naphthalene dihydrodiol dehydrogenase; nahF, salicylaldehyde dehydrogenase; nahC, 1,2-dihydroxynaphthalene dioxygenase (oxygenase); nahE, 2-hydroxybenzalpyruvate aldolase; nahD, 2-hydroxychromene-2-carboxylate isomerase; nahG, salicylate 1-monooxygenase; nahT, 2Fe-2S iron-sulfur cluster binding domain-containing protein (chloroplast-type ferredoxin); nahH, catechol 2,3-dioxygenase; nahI, 2-hydroxymuconic semialdehyde dehydrogenase; nahN, 2-hydroxymuconic semialdehyde dehydrogenase; nahL, 2-oxopent 4-enoate hydratase; nahO, 4-hydoxy-2-oxovalerate aldolase; nahM, acetaldehyde dehydrogenase; nahK, 4-oxalocrotonate decarboxylase/2-oxo 3-hexendioate decarboxylase; nahJ, 4-oxalocrotonate tautomerase family protein; nahY, methyl accepting chemotaxis protein; nahX, unknown; sgpA, reductase component of salicylate 5-hydroxylase; sgpI, gentisate 1,2-dioxygenase; sgpK, fumarylacetoacetate hydrolase/fumarylpyruvate hydrolase; sgpG, salicylate 5-hydroxylase large oxygenase subunit; sgpH, salicylate 5-hydroxylase small oxygenase subunit; sgpB, ferredoxin component of salicylate 5-hydroxylase; mpi, maleylacetoacetate isomerase; mct1, methyl-accepting chemotaxis sensory transducer; nahR and sgpR, LysR family transcriptional regulator.
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Figure 4. Organization of insertion elements observed in Carbaryl degrading Rhizobium sp. strain AC101 harboring gene cehA encoding Carbaryl hydrolase. Figure is not to scale.
Figure 4. Organization of insertion elements observed in Carbaryl degrading Rhizobium sp. strain AC101 harboring gene cehA encoding Carbaryl hydrolase. Figure is not to scale.
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Figure 5. The organization of genes encoding enzymes responsible for Carbaryl degradation as three distinct transposons in Pseudomonas sp. strain C5pp. Genes are located on 76.3 kb long Supercontig-A (Accession number: KU522233.1). Inverted repeats (IRs) are depicted in red and black boxes. Arrow direction indicates the probable transcription direction. Blue color arrows depict genes encoding the probable regulators. Figure is not to the scale. Genes and protein encoded are transposase (tnpA and tnpR); integrase; attI site; streptomycin resistance (Smr); dihydropterate synthetase (DHP); N-acetyl transferase (NAT); mcbA, Carbaryl hydrolase; metA, conserved protein; mcbB, 1,2-dihydroxynaphthalene dioxygenase; mcbC, 1-naphthol 2-hydoxylase; mcbD, 2-hydroxychromene 2-carboxylate isomerase; mcbE, trans-o-hydroxybenzylidene pyruvate hydratase-aldolase; mcbF, salicylaldehyde dehydrogenase; mcbG, LysR family regulator flanked by truncated transposons (depicted as dotted lines). IS21 insertion elements with inverted repeats; IS30 insertion element; mcbH, transcriptional regulator NahR; mcbI, ferredoxin reductase; mcbJ, salicylate 5-hydroxylase large oxygenase component; mcbK, salicylate 5-hydroxylase small oxygenase component; mcbL, ferredoxin; other transposase and insertion elements present downstream of the transposon. metA, conserved protein; tnpA, transposase; mcbS, TetR family transcriptional regulator; FAR, fusaric acid resistance; Hmlysn, hemolysin; Pms, permease; mcbR, LysR family transcriptional regulator; Cup, pirin and cupin2 superfamily related protein; mcbQ, maleylpyruvate isomerase; mcbP, fumaryl pyruvate hydrolase; mcbO, gentisate dioxygenase; mcbN, LysR family transcription regulator; transposase; STP, serine/threonine phosphatase; tnpA, transposase; In-Pase, inositol phosphatase; recombinase; HP, hypothetical protein.
Figure 5. The organization of genes encoding enzymes responsible for Carbaryl degradation as three distinct transposons in Pseudomonas sp. strain C5pp. Genes are located on 76.3 kb long Supercontig-A (Accession number: KU522233.1). Inverted repeats (IRs) are depicted in red and black boxes. Arrow direction indicates the probable transcription direction. Blue color arrows depict genes encoding the probable regulators. Figure is not to the scale. Genes and protein encoded are transposase (tnpA and tnpR); integrase; attI site; streptomycin resistance (Smr); dihydropterate synthetase (DHP); N-acetyl transferase (NAT); mcbA, Carbaryl hydrolase; metA, conserved protein; mcbB, 1,2-dihydroxynaphthalene dioxygenase; mcbC, 1-naphthol 2-hydoxylase; mcbD, 2-hydroxychromene 2-carboxylate isomerase; mcbE, trans-o-hydroxybenzylidene pyruvate hydratase-aldolase; mcbF, salicylaldehyde dehydrogenase; mcbG, LysR family regulator flanked by truncated transposons (depicted as dotted lines). IS21 insertion elements with inverted repeats; IS30 insertion element; mcbH, transcriptional regulator NahR; mcbI, ferredoxin reductase; mcbJ, salicylate 5-hydroxylase large oxygenase component; mcbK, salicylate 5-hydroxylase small oxygenase component; mcbL, ferredoxin; other transposase and insertion elements present downstream of the transposon. metA, conserved protein; tnpA, transposase; mcbS, TetR family transcriptional regulator; FAR, fusaric acid resistance; Hmlysn, hemolysin; Pms, permease; mcbR, LysR family transcriptional regulator; Cup, pirin and cupin2 superfamily related protein; mcbQ, maleylpyruvate isomerase; mcbP, fumaryl pyruvate hydrolase; mcbO, gentisate dioxygenase; mcbN, LysR family transcription regulator; transposase; STP, serine/threonine phosphatase; tnpA, transposase; In-Pase, inositol phosphatase; recombinase; HP, hypothetical protein.
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Table
Table 1. Naphthalene and Carbaryl degradation pathways and location of genes from various isolates.
Table 1. Naphthalene and Carbaryl degradation pathways and location of genes from various isolates.
OrganismPathway, ring-cleavage modeChromosome/plasmid (kb);
Operon size (kb)		References
A. Naphthalene degradation
Pseudomonas putida G7Catechol, metaPlasmid, NAH7 (82);
nah (10) and sal (8)		[99]
Pseudomonas putida strain NCIB 9816-4Catechol, metaPlasmid, pDTG1 (88);
nah (9.5) and sal (13.4)		[102]
Pseudomonas sp. strain ND6Catechol, metaPlasmid, pND6-1 (102);
nah (10) and sal (18)		[109]
Pseudomonas fluorescens strain PC20Catechol, metaPlasmid, pNAH20 (88);
nah (6) and sal (13)		[110]
Pseudomonas putida strain AK5Gentisic acidPlasmid, pAK5 (-);
nah (6.7) and sal (12.2)		[103]
Pseudomonas sp. AS1Catechol, orthoPlasmid, pAS1 (82)[111]
Pseudomonas putida strain PMD-1Catechol, metaChromosome and Plasmid, pMWD-1[104]
Pseudomonas stutzeri AN10Catechol, metaChromosome, nah (11.5) and sal (16)[105,106]
Pseudomonas putida CSV86Catechol, metaICE, nah (8.2) and sal (9.8)[91]
B. Carbaryl degradation
Achromobacter sp.Hydroquinone, Catechol,- *[112]
Pseudomonas sp. NCIB 12043Gentisic acid -[113]
Pseudomonas sp. NCIB 12042Catechol, meta-[113]
Rhodococcus sp. NCIB 12038Gentisic acid-[113]
Consortia Pseudomonas spp. isolate 50581 and 50552Catechol Plasmid, pCD1 (50) in isolate 50581 encodes Carbaryl hydrolase; Chromosome encodes degradative enzymes for 1-naphthol in isolate 50552[43]
Blastobacter sp. strain M501Hydrolysis
to 1-naphthol		-[114]
Sphingomonas sp. strain CF06Gentisic acidPlasmids pCF01, pCF02, pCF03, pCF04, and pCF05, role of each plasmid is not clear [67]
Arthrobacter sp. RC100Gentisic acidPlasmid, pRC1 (110) encodes Carbaryl hydrolase;
Plasmid, pRC2 (120) encodes enzymes for 1-naphthol to gentisic acid;
chromosome encodes enzymes for utilization of gentisic acid 		[115]
Rhizobium sp. strain AC100Partial hydrolysis
to 1-naphthol		Plasmid, pAC200 encodes Carbaryl hydrolase[116]
Micrococcus sp.Gentisic acid-[117]
Pseudomonas sp. strain C4Gentisic acidChromosome[30]
Pseudomonas sp. strain C5Gentisic acidChromosome[30]
Pseudomonas sp. strain C6Gentisic acidChromosome[30]
Burkholderia sp. C3Catechol and Gentisic acid-[118]
Pseudomonas sp. strain C7Gentisic acid-[119]
Pseudomonas putida XWY-1Gentisic acid Plasmid, pXWY (400) encoding all enzymes of Carbaryl degradation [120]
Note: *: -, Not known/reported

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Phale, P.S.; Shah, B.A.; Malhotra, H. Variability in Assembly of Degradation Operons for Naphthalene and its derivative, Carbaryl, Suggests Mobilization through Horizontal Gene Transfer. Genes 2019, 10, 569. https://doi.org/10.3390/genes10080569

AMA Style

Phale PS, Shah BA, Malhotra H. Variability in Assembly of Degradation Operons for Naphthalene and its derivative, Carbaryl, Suggests Mobilization through Horizontal Gene Transfer. Genes. 2019; 10(8):569. https://doi.org/10.3390/genes10080569

Chicago/Turabian Style

Phale, Prashant S., Bhavik A. Shah, and Harshit Malhotra. 2019. "Variability in Assembly of Degradation Operons for Naphthalene and its derivative, Carbaryl, Suggests Mobilization through Horizontal Gene Transfer" Genes 10, no. 8: 569. https://doi.org/10.3390/genes10080569

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