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Article

Characterization and Transcriptome Analysis of a Long-Chain n-Alkane-Degrading Strain Acinetobacter pittii SW-1

by
Weina Kong
1,†,
Cheng Zhao
1,†,
Xingwang Gao
2,
Liping Wang
1,
Qianqian Tian
1,
Yu Liu
1,
Shuwen Xue
1,
Zhuang Han
3,
Fulin Chen
1,* and
Shiwei Wang
1,*
1
Key Laboratory of Resources Biology and Biotechnology in Western China, School of Life Sciences, Northwest University, Ministry of Education, Xi’an 710069, China
2
Hulangmao Oil Production Area in No.3 Oil Production Plant of Changqing Oilfield Company, Yan’an 717500, China
3
Institute of Deep-Sea Science and Engineering, Chinese Academy of Sciences, Sanya 572000, China
*
Authors to whom correspondence should be addressed.
†
These authors contributed equally to this work.
Int. J. Environ. Res. Public Health 2021, 18(12), 6365; https://doi.org/10.3390/ijerph18126365
Submission received: 17 April 2021 / Revised: 4 June 2021 / Accepted: 8 June 2021 / Published: 11 June 2021
(This article belongs to the Section Environmental Microbiology)
Browse Figures
Versions Notes

Abstract

Strain sw-1, isolated from 7619-m seawater of the Mariana Trench, was identified as Acinetobacter pittii by 16S rRNA gene and whole-genome sequencing. A. pittii sw-1 was able to efficiently utilize long-chain n-alkanes (C18–C36), but not short- and medium-chain n-alkanes (C8–C16). The degradation rate of C20 was 91.25%, followed by C18, C22, C24, C32, and C36 with the degradation rates of 89.30%, 84.03%, 80.29%, 30.29%, and 13.37%, respectively. To investigate the degradation mechanisms of n-alkanes for this strain, the genome and the transcriptome analyses were performed. Four key alkane hydroxylase genes (alkB, almA, ladA1, and ladA2) were identified in the genome. Transcriptomes of strain sw-1 grown in C20 or CH3COONa (NaAc) as the sole carbon source were compared. The transcriptional levels of alkB and almA, respectively, increased 78.28- and 3.51-fold in C20 compared with NaAc, while ladA1 and ladA2 did not show obvious change. The expression levels of other genes involved in the synthesis of unsaturated fatty acids, permeases, membrane proteins, and sulfur metabolism were also upregulated, and they might be involved in n-alkane uptake. Reverse transcription quantitative polymerase chain reaction (RT-qPCR) confirmed that alkB expression was significantly induced by C20, C24, and C32, and almA induction extent by C24 and C32 was higher than that with C20. Furthermore, ladA2 expression was only induced by C32, and ladA1 expression was not induced by any of n-alkanes. In addition, A. pittii sw-1 could grow with 0%–3% NaCl or 8 out of 10 kinds of the tested heavy metals and degrade n-alkanes at 15 °C. Taken together, these results provide comprehensive insights into the degradation of long-chain n-alkanes by Acinetobacter isolated from the deep ocean environment.

1. Introduction

The problem of offshore oil leakage during exploitation and transportation has considerably impacted the balance of marine natural ecology and the survival of human beings. Alkanes are the main component of petroleum pollutants. Several microorganisms in nature can degrade alkanes. To date, bacteria [1,2,3], fungi [4,5], and algae [6,7] have been reported to play roles in the degradation of alkanes. Microbes can transform alkanes into less harmful or non-hazardous substrates that can participate in natural biogeochemical cycles [8], and therefore, bioremediation is more economically and environmentally friendly compared with chemical and physical remediation methods. Acinetobacter, which is widely found in nature, is one of the dominant bacteria in soil and marine environments [9,10]. Recently, many reports have shown that Acinetobacter strains can degrade alkanes [11,12,13], indicating that Acinetobacter is promising for application in the repair engineering of alkane pollution, and more Acinetobacter strains with a high degradation efficiency of petroleum hydrocarbons are expected to be isolated.
Thus, it is of considerable significance to study the alkane degradation mechanisms of Acinetobacter. Diverse alkane hydroxylases have been characterized in several bacterial species. Cytochrome P450 mediates the oxidation of shorter chain alkanes (C5–C18) [14,15]. Alkane-1-monooxygenase (AlkB) has a wide range of alkane degradation activities. AlkB in Pseudomonas putida GPo1 has been characterized, and its activity helped utilize alkanes ranging from C6 to C12 [16]. alkB1 and alkB2 were obtained from A. oleivorans DR1. alkB1 was responsible for long-chain (LC) alkane degradation (C24–C26), whereas alkB2 participated in mid-chain alkane (C12–C16) utilization [17]. Additionally, the flavin-binding LC-alkane hydroxylase (AlmA) was first identified in Acinetobacter sp. strain DSM 17,874. It is responsible for LC alkane (C32 and longer) degradation [18]. Interestingly, the homolog of almA from A. oleivorans DR1 shows negligible activity for alkane degradation [17]. The thermophilic soluble LC-alkane hydroxylase (LadA) was first reported in Geobacillus thermodenitrificans NG80-2 and could degrade LC alkanes with carbon atom number at least up to 36 (C36) [19].
In this study, A. pittii sw-1 was isolated from 7619-m seawater in the Mariana Trench. The degradation potential was examined using different types of LC n-alkanes under various conditions. The genes involved in alkane degradation were analyzed via whole-genome sequencing, homologous alignment, and transcriptome analysis. Additionally, reverse transcription quantitative polymerase chain reaction (RT-qPCR) was carried out to verify the transcriptome analysis. These results provided insights into the LC n-alkane degradation by Acinetobacter.

2. Materials and Methods

2.1. Strain, Media, and Chemicals

Seawater samples from the Mariana Trench were collected using Tianya Lander during the TS01 voyage of the ocean research vessel Discovery No. 1 from 25 to 26 July 2016 (142°08.6521′ E, 11°04.7131′ N). Strain sw-1 was isolated from the 7619-m seawater sample using 2216E agar and it displayed round, smooth, and white colony. Luria–Bertani (LB) medium and basal salt medium (BSM) [20] were also used in this study. LB agar was used to resuscitate strains from the −80 °C refrigerator and BSM was used to provide basal salt in alkane degradation experiments of strain sw-1. All n-alkanes including C8–C36 were of analytical grade and obtained from Sigma-Aldrich Shanghai Trading (Shanghai, China). Various n-alkanes were first dissolved in n-hexane to prepare 100 g/L n-alkane solutions. Then, 250 μL of these solutions was added to 50 mL of BSM liquid to obtain 500 mg/L n-alkanes for degradation examination.

2.2. 16S rRNA Gene Analysis and Phylogenic Tree Construction

The 16S rRNA gene of strain sw-1 was PCR-amplified using the eubacterial primers 27F and 1492R (Table S1). Phylogenetic and molecular evolutionary of strain sw-1 and other strains was analyzed with Molecular Evolutionary Genetics Analysis (MEGA 6.0) using the neighbor joining method with 1000 bootstrap value and visualized using the Interactive Tree of Life (iTOL v5) [21]. The 16S rRNA gene sequence was deposited in GenBank (accession no. MT367764.1).

2.3. Genome Sequencing and Comparative Genomics Analysis

A whole-genome shotgun strategy was adopted to construct the genome library, and sequencing was carried out using next-generation sequencing (NGS) supported by Illumina NovaSeq 6000 technology. FastQC (version v0.11.5, Babraham Institute, Cambridge, UK) and Trimmomatic (version 0.38, Institute of Bio- and Geosciences: Plant Sciences, Julich, Germany) were used for performing read quality control and for trimming and removal of joint sequences, respectively. Thereafter, high-quality reads were obtained and assembled using shovill (version 1.0.4, The University of Melbourne, Melbourne, Australia) to generate the draft genome sequence of strain sw-1. Data from the whole-genome shotgun analysis were deposited in GenBank under the accession no. JABBFA000000000. Sequence similarity analysis was performed by comparing homologous fragments between the genomes using Orthologous Average Nucleotide Identity (OrthoANI, Department of ChunLab, Seoul National University, Seoul, Republic of Korea) [22]. Based on 16S rRNA gene analysis result, 9 representative Acinetobacter strains with the most similarity or relativity with strain sw-1 were selected, and the data on the genomes of the 9 Acinetobacter strains were obtained from NCBI.

2.4. Growth and Biodegradation Rate of SW-1 in the Presence of Various n-Alkanes

The biodegradation of n-alkanes was performed in a liquid culture using washed cell suspensions. Briefly, a single colony of strain sw-1 was cultivated in 5 mL of LB broth overnight. The cells were then harvested and subjected to washing three times with PBS buffer and resuspended in PBS buffer to obtain an OD600 of approximately 1.0. Subsequently, 500 μL of the cell inoculum was inoculated into 50 mL of BSM containing 500 mg/L of various n-alkanes (C8–C36) [20]. Flasks containing cells but no n-alkanes and those containing n-alkanes, but no cells were both used as control groups. All flasks were incubated at 30 °C for 7 d. The growth of the strain was determined by measuring the OD600 of the cell cultures [23]. After cultivation, the flasks containing residual alkanes were placed in the 4 °C refrigerator, which made alkanes become solid. Ten-milliliter n-hexane was added to the flasks, followed by being shaken vigorously for 10 min and set for 10 min. Then, the mixed liquid was centrifuged for 10 min at 10,000 rpm and organic phases were collected as extracts. In addition, the flasks and tubes were washed with n-hexane and integrated into extracts. All extracts were collected and placed in a fume cupboard to vaporize the solvent with nitrogen to obtain solid alkanes and then dissolved in 5 mL of n-hexane [24]. The obtained n-hexane was passed through a 0.22-μm organic membrane filter and taken as detected samples for gas chromatograph analysis. Flasks containing n-alkanes without bacterial cells were treated with the same procedure and the corresponding samples were taken as initial mass. The samples were detected using a 7890A gas chromatograph (Agilent, Santa Clara, CA, USA) with FID using a capillary BP5 column (30 m × 0.32 mm × 0.25 μm). The injector temperature and detector temperature were 250 and 310 °C, and the oven temperature was kept at 80 °C for 5 min and then raised to 300 °C at a rate of 10 °C/min [25]. The degradation rate of alkanes was determined by deducting the mass of residual alkanes from the initial mass. All experiments were repeated three times, and the results have been represented as mean values.

2.5. RNA-Seq and Data Analysis

Strain sw-1 was grown in three independent samples using two different carbon sources, namely C20 (500 mg/L) and CH3COONa (NaAc) (2 g/L), and the cultured cells were collected at mid-log phase. Thereafter, the total RNA was extracted using the Trizol reagent (Invitrogen, Carlsbad, CA, USA), and DNase I was used to eliminate genomic DNA contamination. The RNA-seq strand-specific libraries were prepared according to the instructions of the RNA sample preparation kit (San Diego, CA, USA) using 5 μg of total RNA. Transcriptional abundance was used as an input to DESeq (version 1.18.0, University of Duisburg-Essen, Essen, Germany) to assess differential expression. Transcripts with |log2 fold change| > 1 and p < 0.05, were selected as remarkably induced genes. A volcano map was illustrated using the R language.

2.6. RT-qPCR

Strain sw-1 was grown in BSM with NaAc and n-alkanes, respectively. Approximately 108 cells were harvested and collected. Total RNA was extracted using the Total RNA Micro Kit (Magen, Guangzhou, China). Then, 1 μg of RNA was used to synthesize cDNA using the Prime Script TMRT Reagent Kit (TaKaRa, Dalian, China). Primers used in this study are listed in Table S1. RT-qPCR was performed using the BioRad CFX96 Real-Time PCR Detection System (Hercules, CA, USA). The reactions were conducted in a 10-μL reaction volume including the DNA template, 5 μL SYBR Green PCR Super mix, primers, and sterile water. RT-qPCR was performed under the following conditions: 5 min at 95 °C, 15 s at 95 °C, 30 s at 57 °C, and 30 s at 72 °C, with a total of 45 cycles. The expression levels of the investigated genes were normalized to those of rpoB gene [26]. The relative expression levels of target genes were determined using the 2−△△Ct method [27].

2.7. Effect of Rhamnolipid, NaCl, pH, and Temperature on C20 Utilization by Strain SW-1

Fermentation was conducted by adding rhamnolipids at final concentrations of 50, 100, 200, and 400 mg/L to study the effect on C20 degradation by strain sw-1. To investigate the tolerance of bacteria to low temperature, pH, and NaCl, different temperatures (15 °C and 30 °C), pH values (4, 5, 6, 7, 8, 9, and 10), and concentrations of NaCl (0%, 1%, 2%, 3%, 4%, and 5%) were considered to detect the effects on bacterial growth. Other culture conditions were the same as described in Section 2.4.

2.8. Heavy Metal Tolerance Assays

The tolerance of strain sw-1 was detected using ten types of heavy metal salts (Fe2+, Mn2+, Cr2+, Co2+, Ni2+, Cu2+, Pb2+, Sr2+, Al2+, and Zn2+) as previously reported [28]. The concentrations of the metal salts were 100 μM. Strain sw-1 was inoculated into BSM with 500 mg/L C20 containing the above-mentioned individual metal salts. Strain sw-1 grown with 500 mg/L C20 was used as a control group. The culture conditions were the same as described in Section 2.4.

2.9. Determination of the Surface Tension and Cell Surface Hydrophobicity

The surface tension of the fermentation broth and cell surface hydrophobicity was measured to study the uptake mechanism of alkanes in strain sw-1. The surface tension was measured using a tensiometer (JYW-200A Automatic Interface Tensiometer, Xiamen, China) according to the previous report [29]. Briefly, the fermentation broth was transferred to a 50 mL tube, centrifuged at 8000 rpm for 5 min, and the supernatant was obtained. A glass beaker (25 mL) containing 20 mL of cell-free supernatant was placed onto the tensiometer platform. A platinum plate was slowly touched to the liquid–air interface to measure the surface tension. The instrument was calibrated by measuring the surface tension of pure water prior to each experiment. The experiment was repeated three times. Cell surface hydrophobicity was determined by assessing microbial adherence to n-octane [30]. Briefly, the bacterial cells were subjected to washing twice with PUM buffer and suspended at an OD600 of 0.6; then, 1 mL of the suspension was mixed with 0.2 mL of n-octane. The water phase at the bottom was considered for the measurement of OD550 after allowing the mixture to stand for 1 h. The hydrophobicity was determined using the formula (1 − A/A0) × 100%. A represents the OD550 of the water phase after treatment, and A0 represents the OD550 of the bacterial suspension before treatment.

3. Results

3.1. Isolation and Identification of A. pittii Strain SW-1

The strain used in this study was isolated from 7619-m seawater in the Mariana Trench and named sw-1. The 16S rRNA gene sequence of sw-1 showed 100% identity with that of A. pittii PgBE252, and phylogenetic tree analysis showed a close relationship between sw-1 and other Acinetobacter strains (Figure 1). Orthologous Average Nucleotide Identity (OrthoANI) values were used to identify evolutionary relationships among strains by performing paired comparison of genes existing in all the strains. To determine the evolutionary relationship of strains at the genome level, nine Acinetobacter strains were selected for comparison. The similarity values between these strains ranged from 74.82%−99.84% (Figure S1). Species with the values above 95% can be considered as the same species [31], and therefore, sw-1 was classified as an A. pittii strain.

3.2. A. pittii SW-1 Degrades LC n-Alkanes

The degradation of n-alkanes by A. pittii sw-1 was assessed by detecting the growth of the strain within 7 d in BSM containing 500 mg/L of various n-alkanes (C8–C36). Among them, strain sw-1 showed the best growth under C20, followed by C22, C18, C24, C32, and C36 (Figure 2a). Strain sw-1 showed no growth in the presence of shorter n-alkanes (C8–C16) as the only carbon source. The alkanes degradation rate on the seventh day of C18–C24 was above 80%, and the degradation efficiency of C20 was as high as 91.25%, while the degradation rates of C32 and C36 were only 30.29% and 13.37%, respectively (Figure 2b).

3.3. Analysis of the Genes Involved in Alkane Degradation

To identify the alkane hydroxylase involved in alkane metabolism in A. pittii sw-1, after genome sequencing, sequence analysis was performed through homologous amino acid sequence alignment using CLUSTALW (available online: https://www.genome.jp/tools-bin/clustalw (accessed on 1 November 2019)). Four alkane hydroxylases, AlmA, AlkB, LadA1, and LadA2, that probably participated in the utilization of LC alkanes, were identified in A. pittii sw-1. We constructed phylogenetic trees of four alkane hydroxylases compared with homologous proteins in other bacteria (Figure 3). The protein AlkB displayed 95.58% and 61.04% amino acid identity with AlkB1 and AlkB2 in A. oleivorans DR1 (Table 1). AlmA showed 81.49% amino acid identity with the homologous gene in Acinetobacter sp. strain DSM 17874 (Table 1). LadA1 and LadA2 in A. pittii sw-1 displayed 45.44% and 49.78% amino acid identity with LadA from G. thermodenitrificans NG80-2, respectively (Table 1). It has been demonstrated that RubA and RubB are the main components of the electron transport chain for alkane degradation by Acinetobacter strain ADP1 [32]. Two homologous proteins, RubA and RubB, were also found in A. pittii sw-1, which showed 94.44% and 82.95% amino acid identity, respectively, with those in Acinetobacter sp. strain ADP1. An alkane utilization regulator, AlkR, was also found in the genome of A. pittii sw-1, which belongs to the AraC family transcriptional regulator.

3.4. Alkane Degradation-Related Genes Were Induced by C20

RNA-Seq was performed using C20 or NaAc as the sole carbon source. A total of 831 genes were found to be differentially expressed. Among them, the expression levels of 437 genes were upregulated (Figure 4a). The results showed that the expression of numerous alkane degradation-related genes was altered in the presence of C20. the expression levels of alkane hydroxylase genes, alkB and almA, were upregulated 78.28-fold and 3.51-fold in C20, respectively, while those of ladA1 and ladA2 were not significantly increased (Figure 4a) (Table S2). Higher alkB expression indicated that AlkB could be the main alkane hydroxylase involved in C20 degradation. Additionally, the expression of the alkane utilization regulator gene alkR was 2.66-fold upregulated, while the expression of rubA and rubB was not induced (Figure 4a) (Table S2). Furthermore, the expression of one alcohol dehydrogenase gene, dhaT, and two aldehyde dehydrogenase genes, calB and ald, was induced in the presence of C20 (Figure 4b) (Table S2). The fatty acids produced by alkane metabolism might act as energy sources for bacteria through β-oxidation. Indeed, the expression levels of the acyl-CoA dehydrogenase gene acadM and enoyl-CoA hydratase gene fadJ were also upregulated (Figure 4b) (Table S2).
Under conditions of C20-mediated induction, the expression levels of fatty acid desaturase and delta-9 acyl-lipid fatty acid desaturase, which participate in the synthesis of unsaturated fatty acids, were upregulated 17.95-fold and 3.34-fold, respectively (Table S2). The expression levels of genes des6 and hmp, responsible for catalyzing dehydrogenation from C9, were also significantly upregulated, and the expression levels of tesB and yciA converting palmitoyl-CoA into palmitic acid were downregulated (Table S2).
Transcriptome analysis also showed that the expression levels of 12 genes encoding membrane proteins and four genes encoding permeases were upregulated (Table S2). The expression levels of two sulfate transport-related genes, cysT and cysP, were upregulated 74.13-fold and 5.03-fold, respectively. The expression of the thioredoxin reductase gene was upregulated 22.93-fold, and the expression of sulfate adenylyl transferase gene cysD was upregulated 8.62-fold (Table S2).

3.5. Detection of the Expression of Alkane Degradation-Related Genes by RT-qPCR

RNA-Seq analysis revealed that the expression of several alkane degradation-related genes was induced by C20. To confirm the results of the transcriptome analysis, total RNA was extracted from sw-1 cells induced by different n-alkanes (C20, C24, and C32) and NaAc, and the expression levels of alkB, almA, ladA1, and ladA2 were determined by performing RT-qPCR. These results showed that alkB was remarkably induced by C20, C24, and C32 (Figure 5). almA was induced 5.03-fold and 3.17-fold in the presence of C24 and C32, respectively, and 1.40-fold in the presence of C20. ladA2 expression was upregulated 3.56-fold in the presence of C32, while it did not show remarkable change in the presence of C20 and C24 (Figure 5). ladA1 expression was not induced in the presence of any alkane (Figure 5). These results also suggested that alkane hydroxylase AlkB could play a predominant role in alkane degradation for A. pittii sw-1.

3.6. Effects of Rhamnolipids, NaCl, pH, Low Temperature, and Heavy Metals on A. pittii SW-1 Growth

Surfactants increase the solubility of hydrophobic substances in water, enabling microorganisms to metabolize these substances more efficiently [36]. Therefore, we examined the effects of rhamnolipids on the growth and degradation rates of A. pittii sw-1 with C20. When rhamnolipids were added at concentrations ranging from 50–100 mg/L, the growth of A. pittii sw-1 was promoted, while a concentration more than 200 mg/L inhibited its growth (Figure 6a). The degradation rate was also enhanced by adding 50–100 mg/L rhamnolipids, while the addition of 200–400 mg/L rhamnolipids inhibited the degradation of C20 (Figure 6b). The degradation efficiency increased from 18.47%–26.66% with 100 mg/L rhamnolipids on the first day, and from 75.57%–87.65% on the third day (Figure 6b).
A. pittii sw-1 was isolated from a deep ocean environment; hence, the influence of NaCl, pH, and low temperature on A. pittii sw-1 was assessed. A. pittii sw-1 showed obvious growth under the conditions of 0%–3% NaCl. When the concentration of NaCl was higher than 3%, the growth of strain sw-1 was inhibited, and 5% NaCl completely inhibited its growth (Figure 6c). The optimum pH range for its growth was 7~8 (Figure 6d). In addition, although the growth of A. pittii sw-1 appeared weaker at 15 °C than that at 30 °C, it still exhibited obvious growth and alkane degradation ability (Figure 6e). In order to examine the effects of heavy metals on A. pittii sw-1 degradation ability, the tolerance of A. pittii sw-1 to heavy metals was also evaluated. The results showed that Co2+ and Cr2+ obviously inhibited the growth of A. pittii sw-1, while the other heavy metals tested in the study had little effect on its growth (Figure 6f). Furthermore, we also identified several genes that might be involved in salt tolerance (Table S3) and cold adaption in A. pittii sw-1 (Table S4), consistent with the above-mentioned results. In general, A. pittii sw-1 exhibited tolerance to low temperatures (15 °C), eight of ten tested heavy metals, and 1%–3% NaCl.

3.7. Cell Surface Hydrophobicity Might Contribute to the Alkane Uptake in A. pittii SW-1

Alkanes are a class of hydrophobic organic compounds that cannot be easily dissolved in water [37]. Biological surfactants can be used to reduce the surface tension of liquids and emulsify alkanes, which facilitate alkane accessibility for bacteria. Bacteria also can utilize alkanes by absorbing them directly through cell surface hydrophobicity [38]. Therefore, low surface tension and high cell surface hydrophobicity are favorable for absorbing alkane. To investigate the uptake mechanism of alkanes in A. pittii sw-1, the surface tension of the fermentation broth and cell surface hydrophobicity were comparatively analyzed with the common alkane degradation strain Pseudomonas aeruginosa PAO1. The results showed that the liquid surface tension and the cell surface hydrophobicity of strain sw-1 were both higher compared with those of P. aeruginosa PAO1, indicating strain sw-1 might absorb alkane through cell surface hydrophobicity (Figure 7).

4. Discussion

Acinetobacter is an important genus that exhibits the excellent ability of alkane biodegradation in the environment. Several strains of this genus have been reported to be alkane utilizers. For example, previous studies showed that A. calcoaceticus S30 was able to degrade C17–C24 [39] and A. oleivorans DR1 degraded C12–C30 [17]. Strain sw-1 was isolated from seawater at a depth of 7619-m in the Mariana Trench and belonged to A. pittii. It could utilize LC n-alkanes (C18–C36) but not shorter chain n-alkanes (C8–C16). This might be attributable to the lack of the enzymes that are responsible for degrading short-chain alkanes, such as cytochrome P450. This was consistent with the genome analysis results. In addition, strain sw-1 displayed the highest utilization efficiency of C20 among the tested n-alkanes. It was different from the other reported A. pittii strains. For example, A. pittii strain ABC, isolated from oil sludge pits at Noonmati Refinery of India, showed the best growth in C16 [28], whereas strain sw-1 could not utilize C16 as the sole carbon source. The different alkane degradation characterization of these two strains might be due to different isolation environments and substrate bias of alkane hydroxylases.
Several alkane hydroxylases have been identified in Acinetobacter and other bacteria (Table 1). Among them, AlkB of strain sw-1 showed the most similarities to AlkB1 of Acinetobacter DR1 and AlkMa of Acinetobacter M-1 (Figure 3). Our data showed that the alkane degradation ability of AlkB in strain sw-1 was also similar with that observed in Acinetobacter DR1 and Acinetobacter M-1, and their expression was significantly induced by C20–C32 (Table 1) [17,33]. The LC alkane hydroxylase, AlmA, was first identified in Acinetobacter DSM 17,874 and could degrade n-alkanes with a carbon atom number more than 32 (>C32) [18]. The degradation profiles of AlmA display some small differences for various species. In Alcanivorax Hongdengensis A-11-3 AlmA was shown to be involved in C18–C36 degradation, especially with higher induced expression for C24–C36 [35], AlmA of A. dieselolei B-5 was only induced by C22–C36, especially with higher expression in the degradation of C28–C36 [40], in P. aeruginosa SJTD-1 AlmA was be induced by C18–C24 [20], and in P. aeruginosa DN1 AlmA was induced by C20 and longer chain n-alkanes but not shorter chain n-alkanes [23]. Phylogenetic tree analysis suggested that AlmA in strain sw-1 was close to that in Acinetobacter strains, far from those in Alcanivorax and Pseudomonas spp., and AlmA expression in strain sw-1 was induced by longer chain alkanes (C24 and C32). These results indicated that AlmA in diverse strains all played roles in the degradation of LC alkanes, although some small differences were found. Another LC alkane hydroxylase LadA, firstly isolated from in G. thermodenitrificans NG80-2, was able to oxidize C15–C36 alkanes [19]. Strain sw-1 has two LadA, LadA1 and LadA2. LadA2 expression was induced only by C32, while ladA1 expression was not obviously induced by any tested alkanes (Figure 5). In G. thermodenitrificans B23, three LadA-type alkane monooxygenases were found to utilize various alkanes from C12 to C23 [41]. LadA are also identified from other bacteria such as Octadecabacter antarcticus and Terroglobus saanensis [42], while the function of these proteins is yet to be examined.
Biosurfactants are environmentally friendly and can be easily degraded, which facilitates their application in the bioremediation of petroleum hydrocarbon pollution [43]. Rhamnolipids, as glycolipid biosurfactants, can be used to increase the solubility of hydrocarbons in the aqueous phase by reducing the interfacial tension [44], and have been shown to promote the dissolution of hydrocarbons and to improve their bioavailability [45,46]. Our results showed that a low concentration (50–100 mg/L) of rhamnolipids promoted the biodegradation of alkanes in strain sw-1, while higher concentrations of rhamnolipids inhibited the growth of sw-1 and subsequent alkane biodegradation (Figure 6a,b). This indicated that a high concentration of rhamnolipids might be toxic to strain sw-1, consistent with the antimicrobial activity reported in other bacteria [47].
The expression of unsaturated fatty acid genes and synthesis of unsaturated fatty acids were also induced by C20 (Table S2). These results suggested that the strain might enhance cell membrane fluidity by facilitating the synthesis of such fatty acids to absorb alkanes. When strain sw-1 utilizes C20, it might increase the cell demand for sulfur. Transcriptome analysis of A. oleivorans DR1 showed that the expression levels of sulfate transport genes cysAWUP were upregulated by C16 [48]. We obtained similar results for strain sw-1. Levels of two sulfate transport proteins, cysT and cysP, and a sulfate adenylyl transferase cysD, were upregulated by C20 in strain sw-1 (Table S2). Bacteria absorb alkanes through their cell membranes, and membrane permeability is of substantial significance for the utilization of alkanes [49]. Thus, permeases and membrane proteins play an important role in the process of alkane absorption, transport, and regulation of the cell’s corresponding external environment. Transcriptome analysis also showed that certain genes encoding membrane protein permeases were induced by C20 (Table S2).
Lastly, it is worth mentioning that strain sw-1 was isolated from 7619-m seawater of the Mariana Trench, an extreme environment with a low temperature, high salinities and high hydrostatic pressures [50]. In general, microorganisms cannot survive in the environment except some extreme microorganisms. When cultured in the common laboratory with atmospheric pressure strain, sw-1 showed obvious growth, indicating that some gene mutation might have occurred to adapt to the standard laboratory culture conditions. This phenomenon was frequently found when the microbes from deep-sea were cultured in the standard laboratory [51,52]. In addition, alkanes are less found in deep-sea environments, but serpentinization and biological processes may release alkanes to the deep waters especially in subduction zones [53]. Heavy oil fractions such as LC alkanes may attach to suspended sediments and be deposited to the seabed and deep-sea water [54]. Oil contamination enhances the exo-polysaccharide production of phytoplankton [55], and its amphiphilicity promoted the dissolution of oil in sea water [56,57]. These results may be the reasons that many alkane-degrading bacteria have been isolated from deep-sea environments [58,59,60]. Furthermore, some excellent characteristics were maintained by strain sw-1, and it was able to grow under conditions of 1%–3% NaCl and utilize alkanes at a low temperature of 15 °C (Figure 6c,e), indicating strain sw-1 is promising for application in high salt and low temperature environments.

5. Conclusions

In conclusion, we isolated a LC alkane-degrading bacterium, strain sw-1, from the Mariana Trench, which was identified as A. pittii. Four alkane hydroxylases were identified via whole-genome sequencing and homologous alignment. The transcriptome analysis and RT-qPCR results showed that AlkB performed a major function in the utilization of alkanes, and AlmA and LadA2 were probably involved in the utilization of longer chains alkanes. Furthermore, strain sw-1 exhibited tolerance to low temperatures, heavy metals, and higher salt, and might be utilized in oil pollution remediation processes in similar environments.

Supplementary Materials

The following are available online at https://www.mdpi.com/article/10.3390/ijerph18126365/s1, Figure S1: the phylogenetic tree analysis based on the whole genome sequences of Acinetobacter strains; Table S1: the 16s RNA and RT-qPCR primers for alkane hydroxylase gene expression detection; Table S2: the alkane-degrading-related genes that could be induced by C20; Table S3: the salt tolerance-related genes in A. pittii sw-1; Table S4: the cold tolerance-related genes in A. pittii sw-1.

Author Contributions

Conceptualization: W.K. and S.W.; methodology: C.Z.; validation, C.Z., L.W. and Q.T.; resources, Z.H.; data curation: Y.L.; writing—original draft preparation, W.K.; C.Z.; writing—review and editing, W.K.; S.W.; X.G.; visualization, S.X.; supervision: W.K.; S.W.; F.C.; funding acquisition: W.K.; S.W.; F.C. All authors have read and agreed to the published version of the manuscript.

Funding

This research was funded by National Natural Science Foundation of China, grant number 31500111, 31770152, and 31400094, the Nature Science Foundation of Shaanxi Province, China, grant number 2020JM-424.

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

The data presented in this study are available upon reasonable request from the corresponding author.

Acknowledgments

This project was funded by National Key Research & Development Program of China at Institute of Deep-sea Science and Engineering, Chinese Academy of Sciences, under grant number: 2018YFC0309800. The authors, therefore, acknowledge, with thanks, Institute of Deep-sea Science and Engineering for providing the strain used in this study.

Conflicts of Interest

The authors declare no conflict of interest. The funders had no role in the design of the study; in the collection, analyses, or interpretation of data; in the writing of the manuscript, or in the decision to publish the results.

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Figure 1. Phylogenetic tree analysis of Acinetobacter strains based on 16S rRNA gene sequencing. The gene sequence of strain sw-1 was compared with that of 23 Acinetobacter isolates to determine its evolutionary position. Data for all 16S rRNA genes were downloaded from NCBI. Phylogenetic and molecular evolutionary analysis was conducted at 1000 bootstrap value using the MEGA software and was visualized by using iTOL.
Figure 1. Phylogenetic tree analysis of Acinetobacter strains based on 16S rRNA gene sequencing. The gene sequence of strain sw-1 was compared with that of 23 Acinetobacter isolates to determine its evolutionary position. Data for all 16S rRNA genes were downloaded from NCBI. Phylogenetic and molecular evolutionary analysis was conducted at 1000 bootstrap value using the MEGA software and was visualized by using iTOL.
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Figure 2. (a) Growth curves of sw-1 in 500 mg/L of various n-alkanes (C18–C36). Strain sw-1 was inoculated in 50 mL of BSM containing 500 mg/L of n-alkanes. All flasks were incubated at 30 °C for 7 d. The strain growth was determined by estimating OD600 of cells every 12 h. (b) Degradation rate of various n-alkane. The residual alkanes in BSM were extracted using n-hexane and were detected using gas chromatograph, and the degradation rate of alkanes was determined by deducting the mass of residual alkanes from the initial mass.
Figure 2. (a) Growth curves of sw-1 in 500 mg/L of various n-alkanes (C18–C36). Strain sw-1 was inoculated in 50 mL of BSM containing 500 mg/L of n-alkanes. All flasks were incubated at 30 °C for 7 d. The strain growth was determined by estimating OD600 of cells every 12 h. (b) Degradation rate of various n-alkane. The residual alkanes in BSM were extracted using n-hexane and were detected using gas chromatograph, and the degradation rate of alkanes was determined by deducting the mass of residual alkanes from the initial mass.
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Figure 3. Phylogenetic analyses of AlkB, AlmA, LadA1, and LadA2 in A. pittii sw-1 compared with homologous proteins in other bacteria. Phylogenetic and molecular evolutionary analysis was conducted at a 1000 bootstrap value using the MEGA software. Data on the sequences of other genes were downloaded from NCBI.
Figure 3. Phylogenetic analyses of AlkB, AlmA, LadA1, and LadA2 in A. pittii sw-1 compared with homologous proteins in other bacteria. Phylogenetic and molecular evolutionary analysis was conducted at a 1000 bootstrap value using the MEGA software. Data on the sequences of other genes were downloaded from NCBI.
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Figure 4. (a) The volcano plot illustrating the expression levels of the genes with significant difference in alkane degradation. Several genes involved in alkane metabolism were labeled. alkB, alkane hydroxylase gene; alma, flavin-binding monooxygenase gene; adhT, alcohol dehydrogenase gene; ald, aldehyde dehydrogenase gene; alkR, alkane hydroxylase transcriptional regulator gene; rub, rubredoxin reductase gene. (b) Pathway of alkane metabolism and related genes involved in alkane oxidation and β-oxidation. calB, aldehyde dehydrogenase gene; fadD, acyl-CoA synthetase gene; acadM, enoyl-CoA hydratase gene; fadJ, 3-hydroxybutyryl-CoA epimerase gene; paaJ, beta-ketoadipyl CoA thiolase gene. Upregulated genes are marked in red, and the non-induced genes are indicated in gray. A deeper color used in the illustration represents stronger induction by C20.
Figure 4. (a) The volcano plot illustrating the expression levels of the genes with significant difference in alkane degradation. Several genes involved in alkane metabolism were labeled. alkB, alkane hydroxylase gene; alma, flavin-binding monooxygenase gene; adhT, alcohol dehydrogenase gene; ald, aldehyde dehydrogenase gene; alkR, alkane hydroxylase transcriptional regulator gene; rub, rubredoxin reductase gene. (b) Pathway of alkane metabolism and related genes involved in alkane oxidation and β-oxidation. calB, aldehyde dehydrogenase gene; fadD, acyl-CoA synthetase gene; acadM, enoyl-CoA hydratase gene; fadJ, 3-hydroxybutyryl-CoA epimerase gene; paaJ, beta-ketoadipyl CoA thiolase gene. Upregulated genes are marked in red, and the non-induced genes are indicated in gray. A deeper color used in the illustration represents stronger induction by C20.
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Figure 5. The relative expression levels of four alkane hydroxylase genes in C20 (a), C24 (b), and C32 (c) detected by RT-qPCR analysis. The relative expression levels of four alkane hydroxylase genes in diverse alkanes (C20, C24, C32) to the expression in AcNa were normalized by that of rpoB. The 2−△△Ct method was used to calculate the fold change of the normalized mRNA expression levels.
Figure 5. The relative expression levels of four alkane hydroxylase genes in C20 (a), C24 (b), and C32 (c) detected by RT-qPCR analysis. The relative expression levels of four alkane hydroxylase genes in diverse alkanes (C20, C24, C32) to the expression in AcNa were normalized by that of rpoB. The 2−△△Ct method was used to calculate the fold change of the normalized mRNA expression levels.
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Figure 6. The growth curves of A. pittii sw-1 under various conditions and its alkane degradation rate. (a) Growth of A. pittii sw-1 in 500 mg/L C20 with 0–400 mg/L rhamnolipids (RLs). Strain sw-1 was inoculated in 50 mL of BSM with 500 mg/L C20. All flasks were kept at 30 °C for 7 d. The growth was determined by examining OD600 every 12 h. The daily degradation rate of C20 for 3 d was measured after adding different concentrations of RLs, and then compared with the degradation rate of the control group without RLs. (b) Degradation rate of C20 with different concentrations of RLs. (c) Growth of A. pittii sw-1 in C20 with 0–5% NaCl. (d) Growth of A. pittii sw-1 in 500 mg/L C20 with various pH values (4–10) for 7 d. (e) Growth of A. pittii sw-1 in 500 mg/L C20 with two kinds of temperature (30 °C and 15 °C) for 7 d. (f). Growth of A. pittii sw-1 in 500 mg/L C20 with diverse heavy metals. The concentration of each heavy metal was 100 μM. Bacterial growth on 1st, 3rd, and 5th d was compared. All experiments were repeated three times. The error bars represent standard errors.
Figure 6. The growth curves of A. pittii sw-1 under various conditions and its alkane degradation rate. (a) Growth of A. pittii sw-1 in 500 mg/L C20 with 0–400 mg/L rhamnolipids (RLs). Strain sw-1 was inoculated in 50 mL of BSM with 500 mg/L C20. All flasks were kept at 30 °C for 7 d. The growth was determined by examining OD600 every 12 h. The daily degradation rate of C20 for 3 d was measured after adding different concentrations of RLs, and then compared with the degradation rate of the control group without RLs. (b) Degradation rate of C20 with different concentrations of RLs. (c) Growth of A. pittii sw-1 in C20 with 0–5% NaCl. (d) Growth of A. pittii sw-1 in 500 mg/L C20 with various pH values (4–10) for 7 d. (e) Growth of A. pittii sw-1 in 500 mg/L C20 with two kinds of temperature (30 °C and 15 °C) for 7 d. (f). Growth of A. pittii sw-1 in 500 mg/L C20 with diverse heavy metals. The concentration of each heavy metal was 100 μM. Bacterial growth on 1st, 3rd, and 5th d was compared. All experiments were repeated three times. The error bars represent standard errors.
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Figure 7. The difference between A. pittii sw-1 and P. aeruginosa PAO1 in terms of fermented liquid surface tension (a) and cell surface hydrophobicity (b). The determination of surface tension was conducted using a tensiometer. The measurement was performed once a day. The cell surface hydrophobicity was detected by assessing cell adherence to n-octane.
Figure 7. The difference between A. pittii sw-1 and P. aeruginosa PAO1 in terms of fermented liquid surface tension (a) and cell surface hydrophobicity (b). The determination of surface tension was conducted using a tensiometer. The measurement was performed once a day. The cell surface hydrophobicity was detected by assessing cell adherence to n-octane.
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Table 1. The homologous alignment of functional alkane hydroxylases between A. pittii sw-1 and other bacteria using BLASTP.
Table 1. The homologous alignment of functional alkane hydroxylases between A. pittii sw-1 and other bacteria using BLASTP.
Strain NameGene NameResponsible for Range of AlkanesAmino Acid Identity (%)References
Acinetobacter M-1alkMaC22–C3086.27 %[33]
Acinetobacter M-1alkMbC16–C2260.79 %[33]
Acinetobacter DR1alkB1C24–C2695.58 %[17]
Acinetobacter DR1alkB2C12–C1661.04 %[17]
Acinetobacter ADP1alkMC12–C1883.09 %[11]
Acinetobacter RAG-1alkMaC1261.04 %[34]
Acinetobacter RAG-1alkMbC1286.42 %[34]
Acinetobacter DSM 17,874almAC32 and longer81.49 %[18]
Alcanivorax Hongdengensis A-11-3almAC18–C3650.20 %[35]
P. aeruginosa SJTD-1almAC18–C2448.50 %[20]
G. thermodenitrificans NG80-2ladAC15–C3645.44% (with ladA1)
49.78% (with ladA2)		[19]
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Kong, W.; Zhao, C.; Gao, X.; Wang, L.; Tian, Q.; Liu, Y.; Xue, S.; Han, Z.; Chen, F.; Wang, S. Characterization and Transcriptome Analysis of a Long-Chain n-Alkane-Degrading Strain Acinetobacter pittii SW-1. Int. J. Environ. Res. Public Health 2021, 18, 6365. https://doi.org/10.3390/ijerph18126365

AMA Style

Kong W, Zhao C, Gao X, Wang L, Tian Q, Liu Y, Xue S, Han Z, Chen F, Wang S. Characterization and Transcriptome Analysis of a Long-Chain n-Alkane-Degrading Strain Acinetobacter pittii SW-1. International Journal of Environmental Research and Public Health. 2021; 18(12):6365. https://doi.org/10.3390/ijerph18126365

Chicago/Turabian Style

Kong, Weina, Cheng Zhao, Xingwang Gao, Liping Wang, Qianqian Tian, Yu Liu, Shuwen Xue, Zhuang Han, Fulin Chen, and Shiwei Wang. 2021. "Characterization and Transcriptome Analysis of a Long-Chain n-Alkane-Degrading Strain Acinetobacter pittii SW-1" International Journal of Environmental Research and Public Health 18, no. 12: 6365. https://doi.org/10.3390/ijerph18126365

APA Style

Kong, W., Zhao, C., Gao, X., Wang, L., Tian, Q., Liu, Y., Xue, S., Han, Z., Chen, F., & Wang, S. (2021). Characterization and Transcriptome Analysis of a Long-Chain n-Alkane-Degrading Strain Acinetobacter pittii SW-1. International Journal of Environmental Research and Public Health, 18(12), 6365. https://doi.org/10.3390/ijerph18126365

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