Production of lipopeptide biosurfactants by Bacillus atrophaeus 5-2a and their potential use in microbial enhanced oil recovery
© The Author(s) 2016
Received: 25 April 2016
Accepted: 28 September 2016
Published: 3 October 2016
Lipopeptides are known as promising microbial surfactants and have been successfully used in enhancing oil recovery in extreme environmental conditions. A biosurfactant-producing strain, Bacillus atrophaeus 5-2a, was recently isolated from an oil-contaminated soil in the Ansai oilfield, Northwest China. In this study, we evaluated the crude oil removal efficiency of lipopeptide biosurfactants produced by B. atrophaeus 5-2a and their feasibility for use in microbial enhanced oil recovery.
The production of biosurfactants by B. atrophaeus 5-2a was tested in culture media containing eight carbon sources and nitrogen sources. The production of a crude biosurfactant was 0.77 g L−1 and its surface tension was 26.52 ± 0.057 mN m−1 in a basal medium containing brown sugar (carbon source) and urea (nitrogen source). The biosurfactants produced by the strain 5-2a demonstrated excellent oil spreading activity and created a stable emulsion with paraffin oil. The stability of the biosurfactants was assessed under a wide range of environmental conditions, including temperature (up to 120 °C), pH (2–13), and salinity (0–50 %, w/v). The biosurfactants were found to retain surface-active properties under the extreme conditions. Additionally, the biosurfactants were successful in a test to simulate microbial enhanced oil recovery, removing 90.0 and 93.9 % of crude oil adsorbed on sand and filter paper, respectively. Fourier transform infrared spectroscopy showed that the biosurfactants were a mixture of lipopeptides, which are powerful biosurfactants commonly produced by Bacillus species.
The study highlights the usefulness of optimization of carbon and nitrogen sources and their effects on the biosurfactants production and further emphasizes on the potential of lipopeptide biosurfactants produced by B. atrophaeus 5-2a for crude oil removal. The favorable properties of the lipopeptide biosurfactants make them good candidates for application in the bioremediation of oil-contaminated sites and microbial enhanced oil recovery process.
Biosurfactants are a heterogeneous group of surface-active molecules produced by microorganisms, such as bacteria, fungi, and yeasts . The molecular structures of biosurfactants include a hydrophilic moiety, comprising an amino acid or peptide, anions or cations, mono-, di-, or polysaccharides; and a hydrophobic moiety of unsaturated, saturated, or hydrocarbon fatty acids . Therefore, biosurfactants reduce surface tension and interfacial tension in both aqueous solutions and hydrocarbon mixtures and form micelles and microemulsions between the two phases [2, 3]. Such surface properties make biosurfactants good candidates for enhancing oil recovery [4, 5]. Bailey et al.  reported that a biosurfactant flooding process, using a low concentration (35–41 ppm) of biosurfactants produced by Bacillus mojavensis strain JF-2, resulted in high oil recovery, of up to 35–45 %. In recent years, an increase in concern about environmental protection has caused the development of cost-effective bioprocesses for biosurfactants production . The use of biosurfactants that have a comparable enhanced oil recovery performance is preferable .
Based on the types of biosurfactant-producing microbial species and the nature of their chemical structures, biosurfactants can be roughly divided into four groups: lipopeptides and lipoproteins, glycolipids, phospholipids, and polymeric surfactants . Among these four groups, the best-known compounds are lipopeptides, produced by Bacillus species, and glycolipids, produced by Pseudomonas species . In general, mixtures of cyclic lipopeptides are built from variants of heptapeptides and hydroxy fatty acid chains , while glycolipids are mixtures of rhamnolipid homologs, composed of one or two rhamnose molecules linked to one or two hydroxy fatty acid chains . The two types of biosurfactants improve oil recovery by reducing the interfacial tension and altering the wettability of reservoir rock . Glycolipids have been extensively studied in microbial enhanced oil recovery (MEOR) experiments and lipopeptides, such as surfactin and iturins, have also been found effective in similar studies . Surfactin is known as a powerful microbial surfactant with high surface activities and has been successfully used in enhancing oil recovery [12–14].
Biosurfactants MEOR represents a promising method to recover a substantial proportion of the residual oil from marginal oil fields [15, 16]. Biosurfactants can be implemented in two ways: they can be produced either ex situ to be injected into the reservoir or in situ by indigenous or injected microorganisms . The first approach involves the production of biosurfactants above ground by fermentation and therefore requires expensive equipment, including bioreactor and purification systems . The second method is more favorable from an economic point of view, but the indigenous microorganisms need to be identified and their capacity to grow and produce sufficient amounts of biosurfactants in oil reservoirs assessed. Unfortunately, this process cannot be completely manipulated and this places limitations on the reservoirs where microorganisms can be used for in situ treatment .
There have been several successful studies into the application of biosurfactants during in situ or ex situ field tests ; Recently, a field study demonstrated that approximately nine times the minimum concentration of biosurfactants required to mobilize oil was produced in situ by a consortium of Bacillus strains, resulting in the recovery of substantial amount of oil entrapped in the limestone reservoir of the Bebee field, Pontotoc City, Oklahoma, USA . Additionally, a study tested the interaction of biosurfactant produced by B. subtilis W19 with porous media in coreflooding experiments as a tertiary-recovery stage. B. subtilis W19 showed high potential of oil extraction during ex situ MEOR applications in which a total of 23 % of residual oil was extracted produced after biosurfactant and concentrated-biosurfactant injection . The main drawbacks of lipopeptide biosurfactants for MEOR are low yields and high production costs .
The aims of this work were to: (1) improve lipopeptide biosurfactant production yields, through selection of an appropriate bacteria strain and optimization of the carbon and nitrogen sources in the culture media; (2) characterize the biosurfactants produced by the bacteria selected; (3) assess the surface activities and potential of the biosurfactants produced; and (4) determine the feasibility for their use in MEOR.
Results and discussion
Effect of carbon source on biosurfactant production
Dry cell weight (g L−1), crude biosurfactant yield (g L−1), oil spreading (cm), emulsification index (%), and surface tension (mN m−1) obtained for Bacillus atrophaeus 5-2a grown in mineral salt solution with different carbon sources at 30 °C for 5 days
Dry cell weight (g L−1)
Crude biosurfactant yield (g L−1)
Oil spreading (cm)
Emulsification index (%)
Surface tension (mN m−1)
0.56 ± 0.0071c
0.95 ± 0.071b
18.4 ± 0.10b
61.81 ± 0.98a
26.12 ± 0.085c
0.37 ± 0.028e
0.74 ± 0.085c
18.1 ± 0.16c
56.76 ± 0.25c
26.32 ± 0.035b
0.33 ± 0.021e
0.53 ± 0.071d
17.2 ± 0.12e
58.34 ± 0.33b
26.38 ± 0.035b
0.86 ± 0.035a
0.82 ± 0.085bc
18.2 ± 0.10bc
54.80 ± 0.18d
26.11 ± 0.028c
0.51 ± 0.014cd
0.71 ± 0.071c
17.7 ± 0.12d
56.85 ± 0.13c
26.39 ± 0.099b
0.48 ± 0.0071d
1.11 ± 0.042a
19.6 ± 0.071a
54.11 ± 0.085d
25.82 ± 0.028d
0.80 ± 0.014b
0.72 ± 0.028c
17.8 ± 0.12d
57.43 ± 0.14bc
26.32 ± 0.057b
0.14 ± 0.028f
0.06 ± 0.028e
8.2 ± 0.16f
0.00 ± 0.00e
40.49 ± 0.057a
The highest dry cell weights (0.86 and 0.80 g L−1, respectively) were obtained using maltose and glycerol as the carbon source. The lowest surface tension (ST) of the culture supernatant (25.82 mN m−1) was obtained when mannitol was the sole carbon source. However, the other carbohydrate sources tested also decreased ST in the range of 26.11–26.39 mN m−1, except paraffin. Glucose, molasses, and palm oil have been found to be the best carbon sources for the growth of Bacillus isolates [9, 14]. Additionally, Bacillus strains were reported to grow utilizing glycerol and sucrose as the sole carbon sources and the STs of the culture broths were 27.1 and 27.9 mN m−1, respectively [16, 23].
The highest emulsifying activity of the culture was obtained using brown sugar as the carbon source (61.81 %), followed by glucose (58.34 %), glycerol (57.43 %), starch (56.85 %), sucrose (56.76 %), maltose (54.80 %) and mannitol (54.11 %). Raw glycerol from the biodiesel industry has previously been identified as a potential low-cost carbon source for biosurfactant production, with an emulsification efficiency of 67.6 % against crude oil . Furthermore, Al-Wahaibi et al.  found that the biosurfactants produced by Bacillus subtilis B30 had a high emulsifying activity against various hydrocarbons when glucose and molasses were used as the carbon sources.
The amount of biosurfactants produced varied from 0.53 to 1.11 g L−1 and the diameter of oil spreading ranged from 17.2 to 19.6 cm, depending on the carbon source used (Table 1). The highest crude biosurfactant yield and diameter of oil spreading were obtained when mannitol was used as the carbon source. In the second place, the crude biosurfactant yield and diameter of oil spreading reached 0.95 g L−1 and 18.4 cm, respectively, with brown sugar as the carbon source. These results are in agreement with the ST results obtained for B. atrophaeus 5-2a, but in contrast with the highest emulsifying activity (achieved with brown sugar). This indicates that various types of biosurfactants with different properties were synthesized by this strain, depending on the carbon source used.
Effect of nitrogen source on biosurfactant production
Dry cell weight (g L−1), crude biosurfactant yield (g L−1), oil spreading (cm), emulsification index (%), and surface tension (mNm−1) obtained for Bacillus atrophaeus 5-2a grown in mineral salt solution with different nitrogen sources at 30 °C for 5 days
Dry cell weight (g L−1)
Crude biosurfactant yield (g L−1)
Oil spreading (cm)
Emulsification index (%)
Surface tension (mN m−1)
0.64 ± 0.021e
0.47 ± 0.014c
16.5 ± 0.10f
59.50 ± 0.34c
27.64 ± 0.028b
0.87 ± 0.057d
0.66 ± 0.028ab
18.8 ± 0.10b
59.47 ± 0.36c
26.65 ± 0.057d
Corn steep liquor
0.63 ± 0.028e
0.42 ± 0.085c
14.2 ± 0.16 g
10.41 ± 0.57d
29.51 ± 0.035a
0.99 ± 0.028c
0.78 ± 0.028a
19.2 ± 0.10a
60.54 ± 0.38ab
26.43 ± 0.021e
1.41 ± 0.014a
0.55 ± 0.071bc
16.9 ± 0.10e
59.34 ± 0.18c
27.64 ± 0.014b
1.22 ± 0.014b
0.66 ± 0.085ab
17.2 ± 0.12d
61.16 ± 0.25a
27.42 ± 0.092c
0.85 ± 0.0071d
0.73 ± 0.042a
17.6 ± 0.12c
61.23 ± 0.59a
27.38 ± 0.099c
0.47 ± 0.014f
0.53 ± 0.099bc
16.7 ± 0.16e
60.14 ± 0.19bc
27.60 ± 0.057b
The lowest ST, which corresponded to the highest crude biosurfactant yield and the biggest the diameter of oil spreading, was obtained when urea was used as the sole nitrogen source (26.43 mN m−1). The other nitrogen sources tested also offered good results in terms of ST (26.65–29.51 mN m−1), crude biosurfactant yield (0.42–0.73 g L−1) and diameter of oil spreading (14.2–19.2 cm) for the culture supernatant. These results agree with Makkar and Cameotra  who reported that the maximum amount of biosurfactant, and ST values between 29 and 29.5 mN m−1, were produced by a thermophilic B. subtilis when urea or nitrate ions were supplied as the nitrogen sources.
The highest emulsifying activity was observed when (NH4)2SO4 and NaNO3 were used (61.16 and 61.23 %, respectively), followed by KNO3 (61.14 %), urea (60.54 %), beef extract (59.50 %), peptone (59.47 %) and NH4Cl (59.34 %). This is in agreement with the results reported by Dastgheib et al. , in which sodium nitrate was the best substrate for emulsifier production, followed by urea, yeast extract and peptone.
Among all of the carbon and nitrogen sources tested, brown sugar and urea were found to be the most suitable carbon and nitrogen sources regarding the amounts of crude biosurfactant, diameter of oil spreading, emulsifying activity and ST. They are also inexpensive and easily available, making their potential application in MEOR economically feasible. Therefore, brown sugar and urea were selected as the carbon and nitrogen sources for the remaining experiments.
Comparison of the optimal media for biosurfactant production
The potential use of Bacillus strains for biosurfactant production has been widely described in the literature [14, 16, 20]. To the authors’ knowledge, however, no studies have examined the production of biosurfactants by B. atrophaeus. In the study, B. atrophaeus 5-2a demonstrated a higher ability to produce biosurfactants in the BB medium than the BU medium. Its production of biosurfactants in the BU medium was assessed to ascertain its potential to ferment cheaper raw materials (i.e., urea and brown sugar).
Biosurfactant yield and surface tension
Dry cell weight (g L−1), crude biosurfactant yield (g L−1), oil spreading (cm), emulsification index (%), and surface tension (mN m−1) obtained from Bacillus atrophaeus 5-2a in BB and BU media
Dry cell weight (gL−1)
Crude biosurfactant yield (gL−1)
Oil spreading (cm)
Emulsification index (%)
Surface tension (mN m−1)
Yield (g g−1)
1.34 ± 0.014a
1.01 ± 0.016a
19.9 ± 0.071a
54.73 ± 0.085b
25.47 ± 0.042b
0.95 ± 0.028b
0.77 ± 0.014b
19.1 ± 0.10b
59.49 ± 0.33a
26.52 ± 0.057a
The biosurfactants produced using the BB and BU media were able to create low STs of the supernatant, at 25.47 and 26.52 mN m−1, respectively (Table 3). The results show that urea is an efficient nitrogen source. There is evidence that the nitrogen source plays an essential part in the biosurfactant production process . Elazzazy et al.  showed that urea and NaNO3 were the most efficient nitrogen sources for Virgibacillus salarius KSA-T; their culture produced a biosurfactant with minimal ST (29.5 mN m−1) and maximum emulsifying activity (82 %). Additionally, Ghribi and Ellouze-Chaabouni  found that biosurfactant production in their culture was highest using urea. Although there was no significant difference between sodium nitrate, ammonium nitrate, yeast extract, peptone or urea on biosurfactant production, urea was chosen as the cheaper nitrogen source, in comparison to sodium nitrate [21, 25].
The emulsifying activity of the biosurfactants produced using the BB and BU media was appreciable, against paraffin oil (Table 3). A significantly higher emulsification index (E24, 59.49 %) was obtained using the BU medium compared to the BB medium (E24, 54.73 %) (P < 0.05). The emulsification properties of a biosurfactant are of practical importance; good emulsification properties increase the potential environmental and industrial applications of biosurfactants . Formation of an oil-in-water emulsion often leads to an improvement in the effective mobility ratio . The cell-free broth produced by the BU medium could probably enhance oil recovery, based on the results observed with paraffin oil.
Chemical characteristics of the biosurfactants
TLC showed four compounds with Rf values of 0.47, 0.57, 0.75 and 0.8, respectively, when ninhydrin reagent was sprayed, indicating the presence of amino acids. No compounds were observed when sprayed with phenol–sulfuric acid, confirming the absence of sugar moiety. The above results confirm the lipopeptide nature of the biosurfactants. Similar results for other lipopeptide biosurfactants, produced by B. subtilis, have been reported [5, 24].
There were minimum deviations in the diameter of oil spreading and ST over the pH range of 6–13, and the emulsification activities of the biosurfactants were stable above pH 7.0. Higher stability was observed under alkaline compared to acidic conditions and the minimum ST was obtained at pH 6.0 (Fig. 2b). Under an acidic pH (pH 2.0 and 5.0) the biosurfactants showed much less activity; the diameter of oil spreading and emulsification index decreased, and the ST increased, due to precipitation of the biosurfactants. These results indicate that increased pH has a positive effect on surface activity and stability of the biosurfactants. Some reports have confirmed the stability of biosurfactants produced by Bacillus strains at different pH values, but mostly under alkaline conditions [5, 14].
The surface activity of the biosurfactants produced using both the BB and BU media varied with salinity of 0–50 % (w/v); when the salinity was lower than 9 %, the diameter of oil spreading, emulsification index and ST of the cell-free supernatants were constant. The diameter of oil spreading and emulsification index decreased, and the ST increased, with higher salt concentrations; however, the activity remained high at a salinity of 15 % (w/v). Even at the highest salt concentration (50 %, w/v), the biosurfactants produced in the BB and BU media still had reasonable oil spreading activity and the STs were 36.84 mN m−1 and 38.65 mN m−1, respectively (Fig. 2c). Overall, relatively high stability, with respect to salinity, was observed in comparison with other studies that used B. subtilis, Nocardiopsis sp. B4 and Serratia marscecens [14, 31, 32].
The biosurfactants produced by B. atrophaeus 5-2a were stable over a range of environmental factors and maintained their surface activities. Oil reservoirs are harsh environments, with the potential of high salinity and a wide range of pH values; the observed stability of the biosurfactants assessed in this study, over the pH range of 6–13 and salinity concentrations of 0–15 %, indicates that they would be suitable for oil recovery in most reservoirs. These results show that the biosurfactants from B. atrophaeus 5-2a are good candidates for application in MEOR.
Removal of crude oil from filter papers and sand
Crude oil removal efficiencies of fermentation both containing biosurfactants from BB and BU media
Crude oil removal
Removal efficiency (RE p %)
RE p /RE Ctrl
Removal efficiency (RE s %)
RE s /RE Ctrl
12.8 ± 0.19c
9.3 ± 0.042c
94.3 ± 0.049a
94.0 ± 0.092a
93.1 ± 0.12b
90.0 ± 0.057b
Bacillus atrophaeus 5-2a produced a potent biosurfactant with high surface activity and emulsification property, when using a cheap mineral salt medium containing brown sugar and urea as the carbon and nitrogen sources, respectively. The biosurfactant was able to reduce the surface tension of the culture supernatant to 26.52 mN m−1, and exhibited appreciable emulsification activity against paraffin oil (E24, 59.49 %). The biosurfactants produced by the strain 5-2a from both the BB and BU media remained stable under harsh conditions, including wide ranges of pH, temperature, and salinity. They removed ≥90 % of crude oil from artificially contaminated filter paper and sand. TLC and Fourier transform infrared spectroscopy showed that the biosurfactants produced were a mixture of lipopeptides. This study demonstrated the potential and feasibility of the lipopeptides produced by B. atrophaeus 5-2a for application in MEOR. Investigations by laboratory-scale sand-pack columns are warranted to further assess the applicability of the lipopeptides in field applications.
Bacteria, media and oil
Several bacteria were isolated from oil-contaminated surface soils near kowtow machines and oil tanks, adjacent to wells Hua-119 and Hao-129 in Ansai oilfield, Shaanxi province, Northwest China . The oil spreading method was used to select the potential biosurfactant-producing strains, as described by Youssef et al. , with minor modifications. Based on its oil spreading activity, Bacillus atrophaeus 5-2a was selected for further study; it was identified as Bacillus atrophaeus KP314029 by 16S rRNA gene sequencing  and was used for the present work. The purified culture was maintained on beef extract peptone agar medium and deposited in the China Center for Type Culture Collection (CCTCC; strain number CCTCC M 2014673).
The basal mineral salt solution (MSS; pH 7.0) used contained (g L−1): MgSO4·7H2O, 0.3; KH2PO4, 5.0; K2HPO4·3H2O, 5.0; and NaCl, 5.0. The fermentation medium (BB; pH 7.0) used contained (g L−1): beef extract, 3.0; peptone, 10.0; NaCl, 5.0; and brown sugar, 10.0.
Crude oil was obtained from a depleted oil well (Hua-20-4) in Ansai oilfield. The oil sample was taken at 1208 m depth in a low-permeability reservoir called Chang 6 (37°04′38 N, 109°02′58 E). The temperature in the reservoir was approximately 40 °C and the well depth reached 1283–1286 m. The oil sample was stored in a plastic bucket at 4 °C until use.
Effects of carbon and nitrogen sources on biosurfactant production
Biosurfactant production by the culture of Bacillus atrophaeus 5-2a was evaluated using a MSS with different carbon and nitrogen sources. Eight carbon source treatments (brown sugar, sucrose, glucose, maltose, starch, mannitol, glycerol and paraffin) were analyzed at final concentrations of 10.0 g L−1 in the MSS media, which contained NaNO3 (2.0 g L−1) and (NH4)2SO4 (1.0 g L−1) as the nitrogen sources. Eight nitrogen source treatments were assessed: beef extract, peptone, corn steep liquor, urea, NaNO3, NH4Cl, (NH4)2SO4 and KNO3; each was added to create a final concentration of 3.0 g L−1 in the MSS media and brown sugar (10.0 g L−1) was used as the carbon source. The initial pH of the media during each treatment was adjusted to 7.0.
To obtain a seed inoculum, the pure culture of B. atrophaeus 5-2a was transferred to 100 mL of BB medium and incubated at 30 °C with shaking (120 rpm) for 3 d, creating a cell density of 1010 colony-forming units m L−1. For each treatment, 5 % seed inoculum was transferred to 600 mL tissue culture vessels containing 100 mL of the treatment medium. The cultures were incubated at 30 °C, with shaking (120 rpm), for 5 days. After fermentation, the samples were collected and the dry cell weight, crude biosurfactant yield, oil spreading, emulsification index and surface tension (ST) were analyzed.
Effects of the optimal media on biosurfactant production
The ability of the Bacillus atrophaeus 5-2a culture to produce biosurfactants was further evaluated using two media. The first was the BB medium, in which the culture presented the best results regarding biosurfactant production. The second medium (hereafter known as BU) used brown sugar and inorganic nitrogen urea as the carbon and nitrogen sources, and was pH 7.0 (g L−1): MgSO4·7H2O, 0.3; KH2PO4, 5.0; K2HPO4·3H2O, 10.0; NaCl, 5.0; urea, 3.0; and brown sugar, 10.0. The brown sugar and urea as the carbon and nitrogen sources were used to assess the biosurfactant production with an economically viable medium, to test its potential application in MEOR. The cultures were incubated at 30 °C, with shaking (120 rpm), for 5 days. Then, the dry cell weight, crude biosurfactant yield, oil spreading, emulsion index (E24) and ST were analyzed.
Bacterial cells were harvested by centrifuging (10,000×g) for 10 min at 4 °C (Eppendorf, 5804R, Germany) and the dry cell weight (g L−1) was determined after drying at 110 °C for 24 h. The cell-free supernatant was taken for the crude biosurfactant yield, oil spreading, emulsion index and ST analyses. Data are expressed as the mean ± standard deviation (n = 3). Comparison of group means was conducted using Duncan’s multiple range test (considered significant at P < 0.05). The analyses were performed using SAS 9.2 (SAS Institute Inc, Cary, NC, USA). The experiments were performed in triplicate.
Oil spreading analysis
Oil spreading analysis tested the displacement activity of the fermentation broth, measured using the method of Youssef et al. , with minor modifications. A large plastic tub (25 cm diameter) was filled up with 3000 mL of clean water and two drops of paraffin oil were added to the surface of the water. Then, one drop of fermentation broth was added to the surface of the liquid paraffin. The diameter of the clear zone created on the paraffin oil surface was measured. The larger the diameter of the clear zone, the higher the surface activity of the test solution.
ST of the culture supernatants was measured with a digital surface tensiometer (JYW-200A, Chengde, Shandong, China), using the ring method previously described . For calibration, the ST of distilled water was first measured. All ST readings were taken in triplicate and an average value was used to express the ST of each sample.
Dried weight measurement of biosurfactants
The biosurfactants were extracted using the acid precipitation method described by Nitschke and Pastore . Briefly, the cell-free supernatant was adjusted to pH 2.0 using 6 M HCl and left overnight at 4 °C for complete precipitation of the biosurfactants. The precipitate was collected by centrifugation (10,000×g) for 10 min at 4 °C and washed twice with acidified water (pH 2.0). The crude biosurfactants were oven-dried at 110 °C for 24 h and weighed.
Characterization of the biosurfactants
Thin layer chromatography
The biosurfactants were preliminarily characterized by thin layer chromatography (TLC). The biosurfactant extract (5 mg) was hydrolyzed with 6 M HCl in sealed tubes, maintained at 110 °C for 24 h. The hydrolysate was separated on home-made silica gel plates using CH3CH2CH2CH2OH:CH3COOH:H2O (4:1:1, v/v/v) as the developing solvent system. The compounds separated by TLC were visualized by spraying with ninhydrin 0.5 % (w/v, in water) to identify those with free amino groups. Phenol–sulfuric acid (prepared by mixing 95 mL ethanol, 5 mL of sulfuric acid and 3 g of phenol) was used to identify the sugar moieties. The plates were heated at 110 °C for 5 min until the appearance of the respective colors .
Fourier transform infrared spectroscopy
The structural groups of the biosurfactants were identified using fourier transform infrared (FT-IR) spectroscopy analysis. The FT-IR spectrum of the dried biosurfactants was recorded on a TENSOR 27 FT-IR spectrometer, equipped with a DLATGS detector (Bruker, Germany); for this, 1 mg of dried biosurfactants was mixed with 100 mg of KBr and pressed down with 7500 kg for 30 s to obtain translucent pellets. The FT-IR spectra, with a resolution of 4 cm−1, were acquired between 400 and 4000 wave numbers (cm−1).
The stability (activity) of the biosurfactants was studied under a wide range of temperatures, pH and salt concentrations . The stability studies were performed using the cell-free supernatant (obtained by centrifugation at 10,000×g for 10 min at 4 °C). In the first set of tests, the supernatant was maintained at different constant temperatures, in the range of 20–100 °C for 3 h, and then allowed to cool to ambient temperature. In addition, the supernatant was subjected to autoclave conditions (121 °C, 15 psi for 30 min) as another temperature treatment. In the second set of tests, the pH of the supernatant was adjusted to various pH values, ranging from pH 2 to 13, using HCl (1 N) and NaOH (1 N). In the final set of tests, NaCl was added to the supernatant at different concentrations 0–50 % (w/v). In each series of tests, the diameter of the clear zone, the emulsification index and ST were measured.
Removal of crude oil from filter paper and sand
where m is the mass (g) of crude oil removed from the artificially contaminated sand after the fermentation broth treatment, and 10 is the original mass of the crude oil.
JHZ carried out the experiments, analyzed the data and drafted the manuscript. QHX conceived and supervised the study and reviewed the final manuscript. HG assisted in bacterial isolation and identification experiments. HXL and PW took oil-contaminated soils and crude oil samples, and participated in the design of the study and coordination. All authors read and approved the final manuscript.
The study was supported by the Boqin Biological Engineering Co., Ltd. (Sanyuan, Shaanxi Province, China). FT-IR data were collected at the Laboratory of the College of Natural Resources and Environment, Northwest A & F University (Yangling, Shaanxi Province, China). We thank Dr. Hong-hong Zhang for technical assistance.
The authors declare that they have no competing interests.
Availability of data and materials
The datasets supporting the conclusions of this article are included within the article.
The study was supported by the Boqin Biological Engineering Co., Ltd. (Sanyuan, Shaanxi Province, China).
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- Chakraborty S, Ghosh M, Chakraborti S, Jana S, Sen KK, Kokare C, Zhang L. Biosurfactant produced from Actinomycetes nocardiopsis A17: characterization and its biological evaluation. Int J Biol Macromol. 2015;79:405–12.View ArticleGoogle Scholar
- Georgiou G, Lin SC, Sharma MM. Surface active compounds from microorganism. Bio/Technology. 1992;10:60–5.View ArticleGoogle Scholar
- Neu TR. Significance of bacterial surface-active compounds in interaction of bacteria with interfaces. Microbiol Rev. 1996;60:151–66.Google Scholar
- Souayeh M, Al-Wahaibi Y, Al-Bahry S, Elshafie A, Al-Bemani A, Joshi S, Al-Hashmi A, Al-Mandhari M. Optimization of a low-concentration Bacillus subtilis strain biosurfactant toward microbial enhanced oil recovery. Energy Fuel. 2014;28:5606–11.View ArticleGoogle Scholar
- Bezza FA, Chirwa EMN. Production and applications of lipopeptide biosurfactant for bioremediation and oil recovery by Bacillus subtilis CN2. Biochem Eng J. 2015;101:168–78.View ArticleGoogle Scholar
- Bailey SA, Kenney TM, Schneider D. Microbial enhanced oil recovery: diverse successful applications of biotechnology in the oil field. SPE 72129, Proceedings of SPE Asia Pacific improved oil recovery conference. Society of petroleum engineers, Richardson. 2001.Google Scholar
- Gudiña EJ, Fernandes EC, Rodrigues AI, Teixeira JA, Rodrigues LR. Biosurfactant production by Bacillus subtilis using corns steep liquor as culture medium. Front Microbiol. 2015;59:1–7.Google Scholar
- Gudiña EJ, Rangarajan V, Sen R, Rodrigues LR. Potential therapeutic applications of biosurfactants. Trends Pharmacol Sci. 2013;34:667–75.View ArticleGoogle Scholar
- Pornsunthorntawee O, Arttaweeporn N, Paisanjit S, Somboonthanate P, Abe M, Rujiravanit R, Chavadej S. Isolation and comparison of biosurfactants produced by Bacillus subtilis PT2 and Pseudomonas aeruginosa SP4 for microbial surfactant-enhanced oil recovery. Biochem Eng J. 2008;42:172–9.View ArticleGoogle Scholar
- Aparna A, Srinikethana G, Smithab H. Production and characterization of biosurfactant produced by a novel Pseudomonas sp. 2B. Colloids Surf B. 2012;95:23–9.View ArticleGoogle Scholar
- Al-Sulaimani H, Al-Wahaibi Y, Al-Bahry S, Elshafie A, Al-Bemani A, Joshi S, Ayatollahi S. Residual-oil recovery through injection of biosurfactant, chemical surfactant, and mixtures of both under reservoir temperatures: induced-wettability and interfacial tension effects. SPE Reservoir Eval Eng. 2012;15:210–7.View ArticleGoogle Scholar
- Sen R. Biotechnology in petroleum recovery: the microbial EOR. Prog Energy Combust. 2008;34:714–24.View ArticleGoogle Scholar
- Schaller KD, Fox SL, Bruhn DF, Noah KS, Bala GA. Characterization of surfactin from Bacillus subtilis for application as an agent for enhanced oil recovery. Appl Biochem Biotechnol. 2004;113–116:827–36.View ArticleGoogle Scholar
- Al-Wahaibi Y, Joshib S, Al-Bahry S, Elshafie A, Al-Bemania A, Shibulal B. Biosurfactant production by Bacillus subtilis B30 and its application in enhancing oil recovery. Colloids Surf B. 2014;114:324–33.View ArticleGoogle Scholar
- Banat IM, Franzetti A, Gandolfi I, Bestetti G, Martinotti MG, Fracchia L, Smyth TJ, Marchant R. Microbial biosurfactants production, applications and future potential. Appl Microbiol Biotechnol. 2010;87:427–44.View ArticleGoogle Scholar
- Pereira JFB, Gudiña EJ, Costa R, Vitorino R, Teixeira JA, Coutinho JAP, Rodrigues LR. Optimization and characterization of biosurfactant production by Bacillus subtilis isolates towards microbial enhanced oil recovery applications. Fuel. 2013;111:259–68.View ArticleGoogle Scholar
- Al-Bahry SN, Elshafie AE, Al-Wahaibi YM, Al-Bemani AS, Joshi SJ, Al-Maaini RA, Al-Alawi WJ, Sugai Y, Al-Mandhari M. Microbial consortia in Oman oil fields: a possible use in enhanced oil recovery. J Microbiol Biotechnol. 2013;81:141–6.Google Scholar
- Youssef N, Simpson DR, Duncan KE, McInerney MJ, Folmsbee M, Fincher T, Knapp R. In-situ biosurfactant production by Bacillus strains injected into a limestone petroleum reservoir. Appl Environ Microbiol. 2007;73:1239–47.View ArticleGoogle Scholar
- Al-Sulaimani H, Al-Wahaibi Y, Al-Bahry SN, Elshafie A, Al-Bemani A, Joshi S, Zargari S. Optimization and partial characterization of biosurfactants produced by Bacillus species and their potential for ex situ enhanced oil recovery. SPE J. 2011;16:672–83.View ArticleGoogle Scholar
- Gurjar J, Sengupta B. Production of surfactin from rice mill polishing residue by submerged fermentation using Bacillus subtilis MTCC 2423. Bioresour Technol. 2015;189:243–9.View ArticleGoogle Scholar
- Abdel-Mawgoud AM, Aboulwafa MM, Hassouna NAH. Optimization of surfactin production by Bacillus subtilis isolate BS5. Appl Biochem Biotechnol. 2008;150:305–25.View ArticleGoogle Scholar
- Dastgheib SMM, Amoozegar MA, Elahi E, Asad S, Banat IM. Bioemulsifier production by a halothermophilic Bacillus strain with potential applications in microbially enhanced oil recovery. Biotechnol Lett. 2008;30:263–70.View ArticleGoogle Scholar
- Sousa M, Melo VMM, Rodrigues S. Sant’ana HB, Gonçalves LRB. Screening of biosurfactant-producing Bacillus strains using glycerol from the biodiesel synthesis as main carbon source. Bioprocess Biosyst Eng. 2012;35:897–906.View ArticleGoogle Scholar
- Faria AF, Teodoro-Martinez DS, Barbosa GNO, Vaz BG, Silva IS, Garcia JS, Tótola MR, Eberlin MN, Grossman M, Alves OL, Durrant LR. Production and structural characterization of surfactin (C14/Leu7) produced by Bacillus subtilis isolate LSFM-05 grown on raw glycerol from the biodiesel industry. Process Biochem. 2011;46:1951–7.View ArticleGoogle Scholar
- Makkar RS, Cameotra SS. Biosurfactant production by a thermophilic Bacillus subtilis strain. J Ind Microbiol Biotechnol. 1997;18:37–42.View ArticleGoogle Scholar
- Wu JY, Yeh KL, Lu WB, Lin CL, Chang JS. Rhamnolipid production with indigenous Pseudomonas aeruginosa EM1 isolated from oil-contaminated site. Bioresour Technol. 2008;99:1157–64.View ArticleGoogle Scholar
- Elazzazy AM, Abdelmoneim TS, Almaghrabi OA. Isolation and characterization of biosurfactant production under extreme environmental conditions by alkali-halo-thermophilic bacteria from Saudi Arabia. Saudi J Biol Sci. 2015;22:466–75.View ArticleGoogle Scholar
- Ghribi D, Ellouze-Chaabouni S. Enhancement of Bacillus subtilis lipopeptide biosurfactants production through optimization of medium composition and adequate control of aeration. Biotechnol Res Int. 2011;2090–3138:653–4.Google Scholar
- Gudiña EJ, Pereira JFB, Rodrigues LR, Coutinho JAP, Teixeira JA. Isolation and study of microorganisms from oil samples for application in microbial enhanced oil recovery. Int Biodeterior Biodegrad. 2012;68:56–64.View ArticleGoogle Scholar
- Ghojavand H, Vahabzadeh F, Roayaei E, Shahraki AK. Production and properties of a biosurfactant obtained from a member of the Bacillus subtilis group (PTCC 1696). J Colloid Interf Sci. 2008;324:172–6.View ArticleGoogle Scholar
- Khopade A, Biao R, Liu X, Mahadik K, Zhang L, Kokare C. Production and stability studies of the biosurfactant isolated from marine Nocardiopsis sp. B4. Desalination. 2012;285:198–204.View ArticleGoogle Scholar
- Ibrahim ML, Ijah UJJ, Manga SB, Bilbis LS, Umar S. Production and partial characterization of biosurfactant produced by crude oil degrading bacteria. Int Biodeterior Biodegrad. 2013;81:28–34.View ArticleGoogle Scholar
- Zhang JH, Xue QH, Gao H, Lai HX, Wang P. Bacterial degradation of crude oil using solid formulations of Bacillus strains isolated from oil-contaminated soil towards microbial enhanced oil recovery application. RSC Adv. 2016;6:5566–74.View ArticleGoogle Scholar
- Youssef NH, Duncan KE, Nagle DP, Savage KN, Knapp RM, Mclnerney MJ. Comparison of methods to detect biosurfactant production by diverse microorganisms. J Microbiol Method. 2004;56:339–47.View ArticleGoogle Scholar
- Jadhav VV, Yadav A, Shouche YS, Aphale S, Moghe A, Pillai S, Arora A, Bhadekar RK. Studies on biosurfactant from Oceanobacillus sp. BRI 10 isolated from Antarctic sea water. Desalination. 2013;318:64–71.View ArticleGoogle Scholar
- Xia WJ, Dong HP, Yu L, Yu DF. Comparative study of biosurfactant produced by microorganisms isolated from formation water of petroleum reservoir. Colloid Surface A. 2011;392:124–30.View ArticleGoogle Scholar
- Nitschke M, Pastore GM. Production and properties of a surfactant obtained from Bacillus subtilis grown on cassava wastewater. Bioresour Technol. 2006;97:336–41.View ArticleGoogle Scholar
- Zhang JH, Xue QH, Gao H, Ma X, Wang P. Biodegradation of crude oil by fungal enzyme preparations from Aspergillus spp for potential use in enhanced oil recovery. J Chem Technol Biotechnol. 2016;91:865–75.View ArticleGoogle Scholar