Submitted Successfully!
To reward your contribution, here is a gift for you: A free trial for our video production service.
Thank you for your contribution! You can also upload a video entry or images related to this topic.
Version Summary Created by Modification Content Size Created at Operation
1 -- 10243 2022-09-20 03:29:30 |
2 ver 1 -570 word(s) 9172 2022-09-27 03:45:07 |

Video Upload Options

Do you have a full video?


Are you sure to Delete?
If you have any further questions, please contact Encyclopedia Editorial Office.
Cho, W.Y.;  Ng, J.F.;  Yap, W.H.;  Goh, B.H. Sophorolipids—Bio-Based Antimicrobial Formulating Agents. Encyclopedia. Available online: (accessed on 13 April 2024).
Cho WY,  Ng JF,  Yap WH,  Goh BH. Sophorolipids—Bio-Based Antimicrobial Formulating Agents. Encyclopedia. Available at: Accessed April 13, 2024.
Cho, Wei Yan, Jeck Fei Ng, Wei Hsum Yap, Bey Hing Goh. "Sophorolipids—Bio-Based Antimicrobial Formulating Agents" Encyclopedia, (accessed April 13, 2024).
Cho, W.Y.,  Ng, J.F.,  Yap, W.H., & Goh, B.H. (2022, September 20). Sophorolipids—Bio-Based Antimicrobial Formulating Agents. In Encyclopedia.
Cho, Wei Yan, et al. "Sophorolipids—Bio-Based Antimicrobial Formulating Agents." Encyclopedia. Web. 20 September, 2022.
Sophorolipids—Bio-Based Antimicrobial Formulating Agents

Sophorolipids are well-known glycolipid biosurfactants, produced mainly by non-pathogenic yeast species such as Candida bombicola with high yield. Its unique environmental compatibility and high biodegradable properties have made them a focus in the present review for their promising applications in diverse areas.

sophorolipids biosurfactants glycolipid biosurfactants

1. Introduction

Biosurfactants are surface-active compounds that are produced by microorganisms such as bacteria and yeasts. The prominence of these biomolecules is reflected through their unique properties including biodegradation capacity, low toxicity, improved environmental compatibility, and enhanced specific activities under extreme pH, salinity, and temperature [1]. Therefore, biosurfactants produced by microbes have been shown to be involved in wide ranges of applications such as food, pharmaceutical, agriculture and cosmetics due to their diversity and remarkable functional properties [1]. Additionally, due to the amphiphilic nature of biosurfactants, it reduces the interfacial and surface tension between phases and results in micelle formation. With these features, biosurfactants can be used as emulsifiers, foaming agents, wetting agents, as well as detergents, thus making them potential agents in industrial sectors such as bioremediation and microbial enhanced oil recovery [2]. Based on Thakur et al. [3], biosurfactants have been divided into different categories such as polymers, lipopeptides, polypeptides, glycolipids, and many others [3]. Among all, glycolipid biosurfactants are currently one of the most broadly studied biomolecules with outstanding properties in applications for food and health (Figure 1).
Figure 1. Applications of sophorolipids in food and health. Sophorolipids are synthesized by non-pathogenic yeast species, and they have the potential to be used in wide range of applications including wound healing, cosmetic formulations, anticancer agents, antimicrobial agents, food preservation, food waste management, and agriculture practices.
Sophorolipids are glycolipid biosurfactants composed of a hydrophilic sophorose unit and a hydrophobic fatty acid tail. In general, crude sophorolipid consists of both lactonic and acidic forms of sophorolipid that are structurally different in terms of their length of the fatty acid chains, degree of unsaturation, and types of acetylation depending on the substrates used in the process of production [4]. The structural variation causes a marked discrepancy in biological and physicochemical properties [5]. Due to their low toxicity and high biodegradability properties, sophorolipids are currently explored to be applied as biosurfactant in various aspects such as reducing surface and interfacial tension, increasing the dissolution rate of hydrocarbons, facilitating solubilization and absorption of compounds [6]. Sophorolipids are one of the most attractive and promising biosurfactants found in nature and have been shown to have various biological activities such as antimicrobial, anticancer, antiviral, as well as immunomodulatory activities [7]. The production of sophorolipids from Starmerella bombicola yeast species has become an interest in the application of cosmetics, pharmaceuticals, food, and health industries due to their source of many active substances, for example, carbon sources such as glucose and fatty acids [7]. Additionally, sophorolipids are natural compounds, which can rarely cause undesirable side effects, making them a great attention focus in current research.
Sophorolipids that are synthesized by non-pathogenic yeast species have gained a lot of attention and interest in recent years, mainly due to their unique properties of an environmental-friendly nature. The demand for sophorolipids is increasing for various end-use sectors such as food and health industries, hence contributing to the rising market for sophorolipids [8]. As such, there is an increasing trend in the number of publications and research activities of sophorolipids related to its wide range of applications over the years. Moreover, the growth of the publications on sophorolipids has resulted in an increased number of review articles. Considering human health and the environment, the interest in the research on sophorolipids has increased and has developed a strong interest in the unique properties of sophorolipids and explores their vast potential applications.
According to Akubude et al. [9], the introduction of sophorolipids in the food industry has shown beneficial effects in food processing and food products because of their positive impacts on human wellness and the natural environment [9]. They appear to be promising compounds used in substituting the usage of chemical surfactants which will cause detrimental effects on human beings and the environment [9]. Further studies show the utilization of sophorolipids in the agriculture field to enhance crop yield and to protect against plant diseases [10]. From this review, sophorolipids serve as potential biopesticides as they exhibited strong antimicrobial activity against phytopathogens such as bacteria and fungi, making them useful in the agriculture field in recent years [10].

2. Overview of Sophorolipids

2.1. Origin and Structure of Sophorolipids

Sophorolipids were originally discovered by Gorin et al. in 1961 [11]. Sophorolipids are an extracellular glycolipid mixture which is produced by Torulopsis magnoliae [11]. In 1968, Tulloch et al. also reported that extracellular glycolipids were synthesized by the yeast Candida bogoriensis, later as renamed Rhodotorula bogoriensis [12]. Sophorolipids produced by Rhodotorula bogoriensis and Candida apicola have the same structure, but the ones synthesized by Rhodotorula bogoriensis have a sophorose unit attached to 13-hydroxydocosanoic acid [13]. Thereafter, the third yeast strain of sophorolipid was discovered by Spencer et al. from the species Candida bombicola and the properties and production of glycolipids of this yeast species were similar to those of Candida apicola [14]. Furthermore, yeast species Starmerella bombicola was found to synthesize sophorolipids and it was presented as the teleomorph of Candida apicola as they could generate ascospores through sexual reproduction based on the high 18S recombinant DNA (rDNA) identity between two yeast strains [15]. Additionally, Chen et al. [16] discovered that sophorolipids can also be produced by yeast strain Wickerhamiella domericqiae and the major glycolipids observed were nearly similar to those produced by Candida apicola and Candida bombicola [16]. Sophorolipids have been produced by various non-pathogenic yeasts, especially Candida species, including Candida bombicolaCandida batistaeCandida apicolaRhodotorula bogoriensis, and Wickeramiella domerquiae [17]. The formation of sophorolipids by non-pathogenic microorganisms makes them advantageous in the application of food and health-related industries [18].
Candida bombicola is the most intensively studied yeast strain that produces sophorolipids and it is widely known due to its high efficiency for sophorolipid production [19,20]. Sophorolipids are produced mainly by Candida bombicola ATCC 22214, which originated from genus Torulopsis. Yeast strain C. bombicola was originally isolated from bumblebee honey and it was termed as Torulopsis bombicola due to its close correlation with bumblebees [21]. Later in 2012, the yeast species was renamed Starmerella bombicola, which is the teleomorph of Candida bombicola [15]. Its strains were discovered worldwide, typically isolated from the samples of flowers and bumblebee honey [22]. According to Lachance et al., yeast strains of Starmerella bombicola were originally discovered in concentrated grape juice in South Africa, suggesting that nectar-feeding insects were most likely their dominant habitat of survival. Hence, yeast strain S. bombicola has high nutritional value because of their natural habitats of insects and plants [23]. Yeast S. bombicola can be defined as a species with potential to produce sophorolipids and cause no harm to human beings [22]. Due to alkane utilizing properties of yeast species, sophorolipids are mainly produced by S. bombicola with the use of first- and second-generation substrates. Solaiman et al. [24] reported that the utilization of second-generation substrates such as cheap waste stream substrates gave prominence to the production of sophorolipids in the recent decade, rather than the first-generation substrates such as vegetable oils and glucose [24]. Furthermore, in the study conducted by Cletus et al. [25], it was shown that sophorolipids can only be produced by S. bombicola subclade but not all species from the Starmerella clade can successfully synthesize sophorolipids. From this research, S. bombicola had the highest yield of sophorolipids after periods of incubation as compared with other Candida species such as Candida kuoi and Candida cellae [25].
Sophorolipids are glycolipid biosurfactants that are produced at relatively high yields by yeast strains [8]. Sophorolipids are glycolipids made up of a hydrophilic sophorose moiety coupled with a hydroxylated fatty acid tail of 16 or 18 carbon atoms and it is linked by a glycosidic bond [26]. The β-glycosidic bond is formed between anomeric carbon of the sophorose moiety (C1′) with the terminal or sub-terminal carbon of the hydroxylated fatty acids [8]. The carboxylic group of fatty acid can be in free (acidic) or internally esterified (lactonic) form (Figure 2).
Figure 2. Chemical structure of (A) acidic sophorolipid (B) lactonic sophorolipid.

2.2. Sophorolipids Biosynthesis

Sophorolipids production requires building blocks such as glucose and fatty acid. Both sources can be found in the production medium for the synthesis to take place [26]. Yeast strains such as Candida bombicola and Candida apicola have the essential enzymes to produce sophorolipids when growing on hydrophobic substrates such as alkanes, synthesizing fatty acids to be metabolized through the process of oxidation [26]. Hydroxylation of fatty acids by extracellular lipase will occur if there are fatty acids present in the culture medium. However, de novo synthesis of fatty acids from the acetyl-CoA produced by glycolysis will be done in the absence of fatty acids in the culture media [31]. Moreover, carbon sources such as a variety of sugars and oils can be used to synthesize sophorolipids effectively using Candida bombicola [32].
Sophorolipids are a glycolipid compound that is produced by a mixture of different molecules, which is commonly made up of glucose disaccharide sophorose and a hydroxylated fatty acid. The mixture of different congeners is susceptible to batch-to-batch variability of the compounds, resulting in discrepancy in the biological and physicochemical properties of the batches produced [33]. As such, in-product uniformity should be increased through production process and strain engineering to reduce batch-to-batch variation and ensure consistency. In contrast, the introduction of new types of natural producers can increase the inter-product variety of sophorolipids, which make them different from each batch [33]. Increasing attention on inter-product variation allows selection of compounds with differentiated configuration and performance to be applied in many diverse fields including food, pharmaceuticals, cosmetics, etcetera.
To ensure inter-product variation in synthesizing sophorolipids, genetic modification and process engineering can be introduced to increase and enhance product variability and uniformity during the production process [33]. Based on Van Bogaert et al. [34], through the approach of genetic engineering, one of the yeast strains’, Starmerella bombicola, lactone esterase gene (also known as sble) was knocked-out while another strain acetyltransferase gene was knocked-out [34]. The product that is supposed to be observed is non-acetylated acidic sophorolipids, but interestingly, bolaform sophorolipids were obtained as well [34]. Bolaform glycolipid is made up of a hydrophobic fatty acid molecule with a sophorose head attached on both sides. Due to this unique structure, bolaform sophorolipid is expected to show unique physicochemical properties and activities compared to native sophorolipids, making them a great potential for applications in various aspects [35].
For example, bolaform sophorolipid has the potential to be applied in the biomedical field due to its outstanding features to control the interaction with cell surface receptors in moderation [35] and to provide tools for DNA purification [36]. The production of bolaform sophorolipids are usually obtained in very low amounts in the wild type sophorolipids mixture and process development strategies can be used to improve the production yield [33]. Based on Roelants et al. [37], the method of genetic engineering has been shown to provide new production of glycolipids with unique properties and gives a better understanding on the regulation of sophorolipid production [37]. Such new types of compounds offer more opportunities for the potential applications of biosurfactants in various fields.

2.3. Natural Roles

Sophorolipids produced by Starmerella clade were found to have many natural roles due to the positive correlation of yeast strains with flowers and honey of bumblebees [45]. Firstly, sophorolipids can enhance the absorption of hydrophobic substrates such as alkanes and triglycerides. For example, the utilization of octadecane in the culture medium can give rise to the production of sophorolipids, resulting in reduced energy use of yeast species in the production process [46]. Moreover, Hommel et al. proved that sophorolipids can function as an extracellular storage compound for energy and carbon [46]. According to Garcia-Ochoa and Casas [47], sophorolipids took the role of carbon source and were synthesized by yeast Candida bombicola to form sophorose disaccharide [47].
Furthermore, antimicrobial properties can be observed in different mixtures of sophorolipids to impede the growth of microorganisms such as bacteria and fungi. Based on Ito et al. [48], the lactonic form of sophorolipid produced by S. bombicola has antimicrobial properties such as microbial growth inhibition, as in Candida albicans [48]. The antimicrobial activity of sophorolipids mainly targets the destruction of the cellular membrane and interferes with the structure of microorganisms, resulting in growth inhibition of pathogenic microbes not limited to bacteria only, but also yeasts and fungi [49].
Surface-active properties of sophorolipids depend on the measure of surface tension and critical micelle concentration (CMC) of the compound [26]. The properties of surface and interfacial tension of sophorolipids are based on their configuration and structures with different degrees of acetylation. Sophorolipids have been reported to lower the surface tension of water while dissolving in aqueous solution [13]. Additionally, a low CMC value indicates that low concentration of sophorolipids is used to decrease the surface and interfacial tension at the interface [13]. Hence, sophorolipids possess good emulsifying and solubilizing properties, making them a good candidate in manufacturing cleaning agents, wetting agents, and stabilizers [13]. Acidic forms of sophorolipids commonly show better performance of foaming and solubility properties while the lactonic forms of sophorolipids generally possess a higher level of surface activity than the acidic form [13].
In addition, biological and physicochemical properties can be affected due to different forms and structures of sophorolipids. For instance, esterified sophorolipids such as sophorolipid-hexyl ester exhibited superior emulsifying properties on the oil–water system compared to the non-ionic surfactants such as Triton X-100 [50]. According to Ma et al. [51], surface and functional activities of both forms of sophorolipids, lactonic and acidic, could be influenced by the length of the carbon chain as well as the degree of saturation and acetylation of the compounds [51]. The emulsifying capacity and surface activity of sophorolipids will increase when the length of the carbon chain in the structure is increased [52]. Lactonic sophorolipids have been reported to show higher CMC values than acidic sophorolipids [51]. Moreover, another study showed that natural sophorolipids containing a lactic-acid ratio of 72:28 exhibited the lowest surface tension and CMC value compared to the other sophorolipids tested due to the increased hydrophobicity of lactonic compounds [53]. Additionally, lactonic sophorolipid appeared to have higher cytotoxic effects relative to the sophorolipid without lactonic properties [51].

3. Recent Progress in the Applications of Sophorolipids (Food and Health)

3.1. Food

Sophorolipids are used in many food applications including food preservation, agricultural practices, and bioconversion from food waste. They can be applied as a form of strategy for food waste management for sustainable production of sophorolipids. Olanya et al. proposed that pathogen control by sophorolipids is important to provide health benefits for consumers [54]. In recent years, foodborne pathogens continue to rise and thus result in significant food contamination and food safety risks to consumers throughout the world [55]. The most common types of pathogens that present in food causing foodborne illness include Salmonella enterica serovars, Escherichia coli O157:H7, and Listeria monocytogenes [56]. Therefore, control of foodborne pathogens is of immediate concern in the population to provide food and health safety for consumers. Biobased antimicrobial compounds such as sophorolipids have been reported to show beneficial effects for pathogen control due to their properties of having a low toxicity and being highly biodegradable [57]. These properties demonstrated by sophorolipids can help in enhancing postharvest processes to produce fresh and safe fruits and vegetables for consumers [57]. Additionally, the combined usage of sophorolipids with sanitizer was shown to give synergistic antimicrobial effects on E. coli O157:H7. However, limited data were documented for the application of pathogen control by combining sophorolipids with antimicrobial sanitizer [54]. Sophorolipids were also reported to exhibit good performance in growth inhibition of foodborne fungi such as F. oxysporum through membrane destabilization of fungal pathogens [58,59,60]. Such sophorolipids could be produced by S. bombicola [58], Metschnikowia churdharensis [59], and Rhodotorula babjevae YS3 [60].
Sophorolipids have been introduced as a useful material in manufacturing food packaging films and are widely known to display antimicrobial activity directly against the pathogenic microorganisms found in food [61]. According to Silveira et al. [61], antimicrobial packaging films were made by using polylactic acid (PLA) and sophorolipids, which were used as film plasticizer via a casting process in order to control foodborne pathogens [61]. Results showed that good dispersion of the compounds is achieved and forms a smooth appearance of the films, hence the films produced are beneficial in food packaging because a good appearance of the package is the main concern for consumers [61]. Additionally, the addition of sophorolipids into PLA films make them more water-soluble due to the hydrophilic sugar moiety of sophorolipids [62,63]. Higher water solubility of the films contributes to a better release of the antimicrobial components in the food itself, providing antimicrobial effects against the poultry pathogens such as Staphylococcus aureusSalmonella spp., and Listeria monocytogenes [64].
Further research reported on the different structures and composition of sophorolipids for the antimicrobial efficiency against foodborne pathogen Escherichia coli O157:H7 [65]. As stated by Zhang et al. [65], lactonic sophorolipids from S. bombicola showed a significant decline in E. coli population growth compared to the corresponding acidic sophorolipids. Moreover, the introduction of ethanol into sophorolipids was studied and was shown to provide increased antimicrobial effects to the sophorolipids for growth inhibition of pathogens by interrupting the membrane integrity of the cells [65,66]. Zhang et al. [67] observed that lactonic sophorolipids derived from oleic, palmitic, and stearic acids were more effective than acidic forms against Listeria spp. (Gram-positive bacteria) and Salmonella spp. (Gram-negative bacteria), in which Listeria spp. showed a higher sensitivity towards sophorolipids [67]. Production of sophorolipids from marine yeast Rhodotorula rubra has been observed to show antibacterial activities against foodborne pathogens E. coli and S. aureus with the utilization of Macrocystis pyrifera extract as a nutrient source [68]. Similar antibacterial potentials were demonstrated by Chen et al. when they combined nisin with sophorolipids to form antimicrobial food preservatives [69]. Based on Gaur et al. [70], sophorolipids from Candida albicans and Candida glabrata have been shown to be effective antibacterial biomolecules against both Gram-positive and Gram-negative bacterial pathogens through the formation of reactive oxygen species (ROS) [70].
The emulsifying capacity of sophorolipids has been evaluated against different vegetable oils and results showed that sophorolipids from Candida species have high emulsifying activity, developing great promise for their use in the food industry [70]. Sophorolipids were reported to be excellent emulsifying agents for various oil phases such as lemon oil [71] and oregano oil [72] to enhance the stability and texture of food products [73]. Silveira et al. [74] utilized poultry isolates of Clostridium perfringens and Campylobacter jejuni cultures to evaluate the antibacterial activity of sophorolipids from S. bombicola [74]. In this study, the combination of sophorolipids with lactic acid showed the additive effects of antibacterial properties against the pathogens mentioned [74]. Years later, lactonic sophorolipids and lactic acid were studied again for their synergism against L. monocytogenes and S. aureus, which are different types of poultry pathogens compared to the previous study [75]. This combination was effective for growth inhibition of the pathogens due to their known antibacterial properties [75]. Sophorolipids were reported to have inhibitory effects on plant pathogens such as Pythium ultimum [76] and Moesziomyces sp. [77], making them suitable antimicrobial agents against plant pathogens in the agriculture industry. Additionally, sophorolipids from Wickerhamiella domercqiae were tested against fungal and oomycete pathogens such as Fusarium oxysporum and P. ultimum and showed that they inhibited mycelial growth and spore germination of pathogens [78]. A study performed by Vaughn et al. [78] reported that sophorolipids were found to be applied as postemergence herbicides for enhanced plant cuticle permeability [79].
Bioconversion of food waste into sophorolipids has been reported to show potential in a broad range of applications. Inedible Jatropha oil can be used as fermentation feedstock in the production of sophorolipids by S. bombicola [80]. The synthesized sophorolipids have excellent surfactant properties and can reduce tension of distilled water with a low critical micelle concentration (CMC) value [81]. Joshi-Navare et al. [81] demonstrated that oil-derived sophorolipids displayed better emulsification activity and stability as compared with those standard chemical surfactants based on the evaluation of environmental parameters such as pH, temperature, and water hardness [81]. Waste glycerol can be used as fermentation feedstock to produce sophorolipids by various yeast species such as Candida floricola [82]. From the study, it was reported that yeast strain C. floricola with the use of waste glycerol as a carbon source can produce only the acidic form of sophorolipids but not lactonic sophorolipids [82]. This is because the absence of the lactone esterase enzyme for esterification of the compound will result in the production of sophorolipids without lactone forms by the strain of C. floricola. Hence, waste glycerol serves as a cost-effective feedstock for sophorolipid production which suggests its potential use in various aspects [82]. Another study presented by Wang et al. [83] showed that waste streams can also be utilized as feedstock to produce sophorolipids from S. bombicola via fed-batch fermentation with a volumetric productivity of 3.7 g/L/h [83].
Sunflower acid oil, which is a by-product from vegetable oil refineries, was evaluated as fermentation feedstock to produce both acidic and lactonic sophorolipids from S. bombicola [5]. Sophorolipids formed were shown to have good surface activity, wetting and foaming capacity, as well as superior emulsifying activities [5]. Residual sunflower oil cake obtained from the oil industry through the process of winterizing was proven successful in the production of sophorolipids via solid-state fermentation by S. bombicola [84]. Good emulsifying properties and displacement activities were observed from the sophorolipids formed by waste from the oil processing industry [84]. Successful industrial production of sophorolipids can be obtained from the bioconversion of food waste through the process of enzymatic hydrolysis [85] and conversion of waste frying oils using dual lipophilic substrates [86]. Kim et al. [39] further investigated the production of sophorolipids by valorization of waste cooking oils through the process of fed-batch fermentation of yeast S. bombicola [39]. Later, sophorolipids formed by the bioconversion of waste cooking oils were further explored for bioplastics production by synthesizing methyl hydroxy branched fatty acids (MHBFAs) as co-monomers [39]. Today, bioplastics have been of interest to the public as they are recognized as lower toxicity products and are better for the environment compared to traditional plastics [87]. 

3.2. Health

Sophorolipids derived from hydrolyzed horse oil have been proven to show excellent anti-wrinkle effects as well as to improve skin elasticity and firmness [88]. Additionally, sophorolipids have shown antibacterial effects against Pseudomonas aeruginosaStaphylococcus aureus, and Escherichia coli as well as displayed antifungal activity against Candida albicans and Aspergillus niger, in which all five of these microbes are recognized as the most relevant microorganisms found in cosmetic formulations [88]. Based on Zerhusen et al. [89], the formation of long chain non-ionic sophorolipids was reported to lower the surface tension between phases and to exhibit potent emulsifying activities in oil-water mixtures [89]. The produced sophorolipids had good emulsifying behavior as they stabilized the emulsion and prevented water and oil phases from separating, making them superior in manufacturing of pharmaceutical creams, ointments and lotions [89]. A few studies highlighted the use of sophorolipids as natural antimicrobial agents for applications in skincare pharmaceutical formulations due to their non-toxic nature and good skin compatibility [90,91,92]. The authors in that study observed antimicrobial efficiency on Propionibacterium acnes by sophorolipids embedded in different composite films such as plant-based composites pectin and alginate [90] and poly(3-hydroxybutyric acid-co-3-hydroxyvaleric acid) (PHB/HV) composites [91]. Solaiman et al. [92] demonstrated that long carbon chains of acidic sophorolipids (22 carbon chains) had the strongest antibacterial effects on the tested bacteria Cutibacterium acne compared to the others including the lactonic form of sophorolipids consisting of 18 carbon chains only [92]. These results suggest that 22:0 sophorolipids are better suited biosurfactants as they possess antimicrobial properties for various applications [92].
Sophorolipids, which often form themselves into a vesicle-like structure through self-assembling, are known to be effective in skin delivery of molecules for application in cosmetic and pharmaceutical industries. Based on Ishii et al. [93], acidic sophorolipids play a role in increasing skin permeation and achieving higher amounts of bovine lactoferrin penetration across the skin barrier [93]. This study highlighted the use of sophorolipids as a suitable carrier for transdermal delivery because they do not affect the original property of lactoferrin but to improve the skin absorption of lactoferrin [93,94]. Furthermore, formation of biodegradable transferosomal hydrogels for cosmetic applications has been investigated by Naik et al. via the combined use of lignans and sophorolipids [94]. Sophorolipid-based transfersomes were proven to enhance skin permeation for transdermal delivery of active components across the skin barrier due to their amphiphilic properties [94]. Imura et al. [95] also examined the transdermal permeation and absorption of mogrosides V by incorporating triterpene glycoside into the vesicles of acidic sophorolipids to display various pharmacological activities of mogrosides V [95].
Sophorolipids were shown to be effective for growth inhibition of bacterial pathogens when combined with antibiotics such as kanamycin or cefotaxime [28] as well as natural compounds such as sericin and calcium alginate [96]. These results suggested the potential use of sophorolipids as an active ingredient in antimicrobial formulations for wound healing applications, without any evidence of side effects on skin tissue [28]. This combination demonstrated a rapid rate of wound healing and contraction, thus shorter time is used for the wound healing process compared to the traditional formulation [96]. The healing potential of sophorolipids was demonstrated using HT-29 cell lines and results showed that sophorolipids could increase cell proliferation and migration, which is beneficial in the application of intestinal healing [97]. Sophorolipids are widely studied in industrial and pharmaceutical industries due to their possession of unique properties, being antiviral, antibacterial, antimicrobial, and antibiofilm. The potential use of sophorolipids as antimicrobial formulating agents has been of great interest in recent years due to their attractive properties such as low toxicities and better biodegradability. Their ability to show numerous biological activities makes them suitable and efficacious alternatives for synthetic surfactants in the pharmaceutical sectors [98,99].
According to Díaz De Rienzo et al. [57], sophorolipids from C. bombicola were shown to have antibacterial properties against both Gram-positive and Gram-negative microorganisms by inducing plasma membrane damage of the microbes [58]. Cell membrane disruption occurs when sophorolipids can alter the morphology and structure of the bacteria resulting in increased membrane permeability and disturbance of membrane integrity [100]. This ensures sophorolipids penetrate cell membranes and release intracellular materials, causing ruptures in cell membranes and growth inhibition of the bacteria [101]. In general, it might be somewhat difficult for sophorolipids to penetrate the cell membrane of Gram-negative bacteria due to the presence of lipopolysaccharide surrounding the outer cell membrane [102]. However, this study showed that sophorolipids inhibit the growth of both Gram-positive and Gram-negative bacteria at the same MIC of 5% v/v [100]. Other similar studies also demonstrated antibacterial activity of sophorolipids produced from Candida species such as C. bombicola and C. tropicalis RA1 against Gram-positive bacteria [75,103,104]. Meanwhile, Archana et al. [104] also reported on the antibacterial efficiency and the growth inhibition of Gram-negative bacteria such as E. coli and P. aeruginosa [104]. Oil-derived sophorolipids, which are natural products, could be used to replace synthetic surfactant detergent formulations as they were reported to display antibacterial activity against S. aureus [81]. Abhyankar et al. [105] also studied the antibacterial activity exhibited by myristic acid derived sophorolipid against both Gram-positive and Gram-negative organisms [105].
On top of that, the antibiofilm and antiadhesive potential of sophorolipids were observed against Gram-positive bacteria [100]. Such action is achieved through alteration in surface properties of the bacterial cells and antiadhesive activities exhibited by sophorolipids [100,106]. Valotteau et al. [107] reported the ability of sophorolipids to disrupt biofilm formation and reduce bacterial adhesion of pathogen strains such as S. aureus and E. coli [107]. The action of sophorolipids on the inhibition of biofilm formation and reduced microbial adhesion from different surfaces could suggest their promising use in various industries including the biomedical and pharmaceutical sectors [107]. Moreover, sophorolipids had been proven to display antibiofilm properties and prevent cell attachment of S. aureus, suggesting them to be coating materials in medical-grade silicon devices for application in the pharmaceutical industry [108,109].
Nguyen et al. [110] also proved the antibiofilm activity of sophorolipids combined with sodium dodecyl sulfate (SDS), which is an anionic surfactant, against Pseudomonas aeruginosa PAO1 [110]. However, they found that sophorolipids do not show any antibacterial action on PAO1 but only disperse biofilm formation of the bacterial strain [110]. Vasudevan and Prabhune [111] evaluated that curcumin-sophorolipid nanoparticles exhibited good antibiofilm activities by quorum quenching against P. aeruginosa [111]. Sophorolipids were reported to have antifungal action against C. albicans by interrupting their growth and the formation of biofilm of the fungal strain [7,112,113]. Such actions were also achieved through increased cell permeability and generation of reactive oxygen species (ROS), resulting in fungal necrosis and apoptosis due to high oxidative stress [7]. Furthermore, sophorolipids were found to prevent fungal infections such as tinea pedis and dermatophytosis because of their evident antifungal activities against Trichophyton mentagrophytes [114,115].
Dengle-Pulate et al. [116] also examined sophorolipids synthesized from medium-chain lauryl alcohol for their antibacterial effects on various pathogenic microorganisms and revealed that lauryl alcohol derived sophorolipids (SLLA) exhibited higher antibacterial activities than lauryl alcohol alone [116]. Antimicrobial action against oral pathogens such as Streptococcus oralis [117] and Lactobacillus acidophilus [118] have been reported through inhibition of biofilm formation of oral cariogenic bacteria. Solaiman et al. [119] studied the antimicrobial activity of sophorolipids against a mixed culture of Gram-positive and Gram-negative bacteria and revealed that sophorolipids were effective against a wide range of microorganisms found in hides, which will be useful for further application in the leather industry [119].
Joshi-Navare and Prabhune [120] further proved that sophorolipids have potent antimicrobial activity against bacterium E. coli and S. aureus in combination with antibiotics [120]. However, growth inhibition of bacteria was not completely performed by sophorolipids alone [120]. In this study, sophorolipids combined with tetracycline inhibited growth of S. aureus while the antibacterial action against E. coli was observed through the combination of sophorolipids with cefaclor [120]. Combinatorial antibacterial effects of antibiotics and sophorolipids have been shown to exhibit adjuvant activities against bacterial pathogens as well as to overcome the issue of bacterial antibiotic resistance [28,120]. In addition, incorporation of acidic sophorolipids into amphotericin B was reported to show antifungal and antibiofilm effects against C. albicans in the treatment of fungal infections. This study indicated that sophorolipids can be used to develop fungicidal agents with amphotericin B by preventing gene expression and growth of fungal pathogens [113].
Baccile et al. [121] reported that acidic sophorolipids from C. bombicola have been used to develop functionalized iron oxide nanoparticles due to great colloidal stability of the compound [121]. A similar study also showed that sophorolipid was found to be a good stabilizer in forming zinc oxide nanoparticles (ZON) to show inhibitory effects on the tested microorganisms including Salmonella enterica and C. albicans [122]. They reported that antimicrobial activities were exhibited by diacetate acidic sophorolipids from Cryptococcus sp. against both bacterial and fungal pathogens [122]. Owing to the antimicrobial trait of sophorolipids and their additive effects with zinc oxide, they can be explored in the production of functionalized nanoparticles for the control of pathogenic microbes [122]. Another study showed that long-chain quaternary ammonium sophorolipids possess antimicrobial activities towards both Gram-positive and Gram-negative bacteria, in which a higher MIC of sophorolipids is used for growth inhibition of Gram-negative E. coli [123]. The anticancer effects of sophorolipids with different structures were reported by a few researchers, in which C18:1 DLSL was shown to have the highest activity compared to diacetylated lactonic sophorolipid with a C18 saturated fatty acid (C18:0 DLSL) against human esophageal cancer cells [124], breast cancer cells [17], human cervical cancer cells [125], and colorectal cancer cells [126]. These results indicated that increasing the degree of unsaturation of the compound will result in lower efficiency on apoptosis of cancer cells.
Sophorolipids combined with cetyl alcohol (SLCA) were shown to have anticancer activity against human cervical cancer cells by inducing apoptosis through a rise in intracellular calcium ions leading to the depolarization of mitochondrial membrane potential [127]. Anticancer action against colon cancer cell lines by sophorolipid-based nanocapsules was demonstrated by Haggag et al. in both in vivo and in vitro experiments [128]. Lactonic sophorolipids were shown to be effective in growth inhibition of liver hepatocellular carcinoma cells [129] and inducing angiogenesis [130]. Sophorolipids have been shown to target the cancerous cells without affecting the normal cells, thus reducing unwanted side effects that are normally associated with the current therapeutic regimens [127].


  1. Shekhar, S.; Sundaramanickam, A.; Balasubramanian, T. Biosurfactant Producing Microbes and their Potential Applications: A Review. Crit. Rev. Environ. Sci. Technol. 201545, 1522–1554. [Google Scholar] [CrossRef]
  2. Vijayakumar, S.; Saravanan, V. Biosurfactants-types, sources and applications. Res. J. Microbiol. 201510, 181–192. [Google Scholar]
  3. Thakur, P.; Saini, N.K.; Thakur, V.K.; Gupta, V.K.; Saini, R.V.; Saini, A.K. Rhamnolipid the Glycolipid Biosurfactant: Emerging trends and promising strategies in the field of biotechnology and biomedicine. Microb. Cell Factories 202120, 1. [Google Scholar] [CrossRef]
  4. Borsanyiova, M.; Patil, A.; Mukherji, R.; Prabhune, A.; Bopegamage, S. Biological activity of sophorolipids and their possible use as antiviral agents. Folia Microbiol. 201561, 85–89. [Google Scholar] [CrossRef]
  5. Jadhav, J.V.; Pratap, A.P.; Kale, S.B. Evaluation of sunflower oil refinery waste as feedstock for production of sophorolipid. Process Biochem. 201978, 15–24. [Google Scholar] [CrossRef]
  6. Mondal, M.; Halder, G.; Oinam, G.; Indrama, T.; Tiwari, O.N. Bioremediation of organic and inorganic pollutants using microalgae. In New and Future Developments in Microbial Biotechnology and Bioengineering. In New and Future Developments in Microbial Biotechnology and Bioengineering; Elsevier: Amsterdam, The Netherlands, 2019; pp. 223–225. [Google Scholar]
  7. Haque, F.; Verma, N.K.; Alfatah, M.; Bijlani, S.; Bhattacharyya, M.S. Sophorolipid exhibits antifungal activity by ROS mediated endoplasmic reticulum stress and mitochondrial dysfunction pathways in Candida albicansRSC Adv. 20199, 41639–41648. [Google Scholar] [CrossRef]
  8. Oliveira, M.R.; Magri, A.; Baldo, C.; CAmiliou-Neto, D.; Minucelli, T.; Celligoi, M.A.P.C. Review: Sophorolipids A Promising Biosurfactant and it’s Applications. Int. J. Adv. Biotechnol. Res. 20156, 161–174. [Google Scholar]
  9. Akubude, V.C.; Sule, S.; Chinweuba, D.C.; Okafor, V.C. Application of biosurfactant in food industry. In Green Sustainable Process for Chemical and Environmental Engineering and Science; Elsevier: Amsterdam, The Netherlands, 2021; pp. 109–125. [Google Scholar]
  10. Celligoi, M.A.P.C.; Silveira, V.A.I.; Hipólito, A.; Caretta, T.O.; Baldo, C. Sophorolipids: A review on production and perspectives of application in agriculture. Span. J. Agric. Res. 202018, e03R01. [Google Scholar] [CrossRef]
  11. Gorin, P.A.J.; Spencer, J.F.T.; Tulloch, A.P. Hydroxy Fatty Acid Glycosides of Sophorose from Torulopsis MagnoliaeCan. J. Chem. 196139, 846–855. [Google Scholar] [CrossRef]
  12. Tulloch, A.P.; Spencer, J.F.T.; Deinema, M.H. A new hydroxy fatty acid sophoroside from Candida bogoriensisCan. J. Chem. 196846, 345–348. [Google Scholar] [CrossRef]
  13. Van Bogaert, I.N.A.; Saerens, K.; De Muynck, C.; Develter, D.; Soetaert, W.; Vandamme, E.J. Microbial production and application of sophorolipids. Appl. Microbiol. Biotechnol. 200776, 23–34. [Google Scholar] [CrossRef] [PubMed]
  14. Spencer, J.F.T.; Gorin, P.A.J.; Tulloch, A.P. Torulopsis bombicola sp. n. Antonie Van Leeuwenhoek 197036, 129–133. [Google Scholar] [CrossRef] [PubMed]
  15. Rosa, C.A.; Lachance, M.A. The yeast genus Starmerella gen. nov. and Starmerella bombicola sp. nov., the teleomorph of Candida bombicola (Spencer, Gorin & Tullock) Meyer & Yarrow. Int. J. Syst. Bacteriol. 199848 Pt 4, 1413–1417. [Google Scholar]
  16. Chen, J.; Song, X.; Zhang, H.; Qu, Y.B.; Miao, J.Y. Production, structure elucidation and anticancer properties of sophorolipid from Wickerhamiella domercqiaeEnzym. Microb. Technol. 200639, 501–506. [Google Scholar] [CrossRef]
  17. Ribeiro, I.A.C.; Faustino, C.M.C.; Guerreiro, P.S.; Frade, R.F.M.; Bronze, M.R.; Castro, M.F.; Ribeiro, M.H.L. Development of novel sophorolipids with improved cytotoxic activity toward MDA-MB-231 breast cancer cells. J. Mol. Recognit. 201528, 155–165. [Google Scholar] [CrossRef]
  18. Sałek, K.; Euston, S.R. Sustainable microbial biosurfactants and bioemulsifiers for commercial exploitation. Process Biochem. 201985, 143–155. [Google Scholar] [CrossRef]
  19. Davila, A.M.; Marchal, R.; Vandecasteele, J.P. Sophorose lipid fermentation with differentiated substrate supply for growth and production phases. Appl. Microbiol. Biotechnol. 199747, 496–501. [Google Scholar] [CrossRef]
  20. Gao, R.; Falkeborg, M.; Xu, X.; Guo, Z. Production of sophorolipids with enhanced volumetric productivity by means of high cell density fermentation. Appl. Microbiol. Biotechnol. 201397, 1103–1111. [Google Scholar] [CrossRef]
  21. Kachholz, T.; Schlingmann, M. Possible food and agriculture application of microbial surfactants: An assessment. In Biosurfactants and Biotechnology; Kosaric, N., Ed.; Dekker: New York, NY, USA, 1987; pp. 183–210. [Google Scholar]
  22. Marilyn, D.G.; Sofie, L.D.M.; Sophie, L.K.W.R.; Wim, S. Starmerella bombicola, an industrially relevant, yet fundamentally underexplored yeast. FEMS Yeast Res. 201818, 72. [Google Scholar]
  23. Lachance, M.A.; Wijayanayaka, T.M.; Bundus, J.D.; Wijayanayaka, D.N. Ribosomal DNA sequence polymorphism and the delineation of two ascosporic yeast species: Metschnikowia agaves and Starmerella bombicolaFEMS Yeast Res. 201111, 324–333. [Google Scholar] [CrossRef]
  24. Solaiman, D.K.Y.; Liu, Y.; Moreau, R.A.; Zerkowski, J.A. Cloning, characterization, and heterologous expression of a novel glucosyltransferase gene from sophorolipid-producing Candida bombicolaGene 2014540, 46–53. [Google Scholar] [CrossRef] [PubMed]
  25. Cletus, P.K.; Neil, P.J.P.; Karen, J.R.; Tsung-Min, K. Production of sophorolipid biosurfactants by multiple species of the Starmerella (Candidabombicola yeast clade. FEMS Microbiol. Lett. 2010311, 140–146. [Google Scholar]
  26. Ekaterina, K.; Tatiana, K. Physicochemical Properties of Yeast Extracellular Glycolipids. In Extracellular Glycolipids of Yeasts; Academic Press: Cambridge, MA, USA, 2014; pp. 29–34. [Google Scholar]
  27. Shu, Q.; Lou, H.; Wei, T.; Liu, X.; Chen, Q. Contributions of glycolipid biosurfactants and glycolipid-modified materials to antimicrobial strategy: A review. Pharmaceutics 202113, 227. [Google Scholar] [CrossRef] [PubMed]
  28. Lydon, H.L.; Baccile, N.; Callaghan, B.; Marchant, R.; Mitchell, C.A.; Banat, I.M. Adjuvant Antibiotic Activity of Acidic Sophorolipids with Potential for Facilitating Wound Healing. Antimicrob. Agents Chemother. 201761, e02547-16. [Google Scholar] [CrossRef]
  29. Ciesielska, K.; Van Bogaert, I.N.; Chevineau, S.; Li, B.; Groeneboer, S.; Soetaert, W.; Van de Peer, Y.; Devreese, B. Exoproteome analysis of Starmerella bombicola results in the discovery of an esterase required for lactonization of sophorolipids. J. Proteom. 201498, 159–174. [Google Scholar] [CrossRef]
  30. Shah, V.; Doncel, G.F.; Seyoum, T.; Eaton, K.M.; Zalenskaya, I.; Hagver, R.; Azim, A.; Gross, R. Sophorolipids, microbial glycolipids with anti-human immunodeficiency virus and sperm-immobilizing activities. Antimicrob. Agents Chemother. 200549, 4093–4100. [Google Scholar] [CrossRef]
  31. de Jesús Cortés-Sánchez, A.; Hernández-Sánchez, H.; Jaramillo-Flores, M.E. Biological activity of glycolipids produced by microorganisms: New trends and possible therapeutic alternatives. Microbiol. Res. 2013168, 22–32. [Google Scholar] [CrossRef]
  32. Morita, T.; Fukuoka, T.; Imura, T.; Kitamoto, D. Glycolipid Biosurfactants. In Reference Module in Chemistry, Molecular Sciences and Chemical Engineering (Issue Cmc); Elsevier Inc.: Amsterdam, The Netherlands, 2016. [Google Scholar]
  33. Dierickx, S.; Castelein, M.; Remmery, J.; De Clercq, V.; Lodens, S.; Baccile, N.; De Maeseneire, S.L.; Roelants, S.L.K.W.; Soetaert, W.K. From bumblebee to bioeconomy: Recent developments and perspectives for sophorolipid biosynthesis. Biotechnol. Adv. 202154, 107788. [Google Scholar] [CrossRef]
  34. Van Bogaert, I.N.A.; Buyst, D.; Martins, J.C.; Roelants, S.L.K.W.; Soetaert, W.K. Synthesis of bolaform biosurfactants by an engineered Starmerella bombicola yeast. Biotechnol. Bioeng. 2016113, 2644–2651. [Google Scholar] [CrossRef]
  35. Aleandri, S.; Casnati, A.; Fantuzzi, L.; Mancini, G.; Rispoli, G.; Sansone, F. Incorporation of a calixarene-based glucose functionalised bolaamphiphile into lipid bilayers for multivalent lectin recognition. Org. Biomol. Chem. 201311, 4811–4817. [Google Scholar] [CrossRef]
  36. Sohrabi, B.; Khani, V.; Moosavi-Movahedi, A.A.; Moradi, P. Investigation of DNA-cationic bolaform surfactants interaction with different spacer length. Colloids Surf. B Biointerfaces 2013110, 29–35. [Google Scholar] [CrossRef] [PubMed]
  37. Roelants, S.L.K.W.; Ciesielska, K.; De Maeseneire, S.L.; Moens, H.; Everaert, B.; Verweire, S.; Denon, Q.; Vanlerberghe, B.; Van Bogaert, I.N.A.; Van der Meeren, P.; et al. Towards the industrialization of new biosurfactants: Biotechnological opportunities for the lactone esterase gene from Starmerella bombicolaBiotechnol. Bioeng. 2016113, 550–559. [Google Scholar] [CrossRef] [PubMed]
  38. Jones, D.F.; Howe, R. Microbiological oxidation of long-chain aliphatic compounds. I. Alkanes and alk-1-enes. J. Chem. Soc. Perkin Trans. 196822, 2801–2808. [Google Scholar] [CrossRef] [PubMed]
  39. Kim, J.H.; Oh, Y.R.; Hwang, J.; Kang, J.; Kim, H.; Jang, Y.A.; Lee, S.S.; Hwang, S.Y.; Park, J.; Eom, G.T. Valorization of waste-cooking oil into sophorolipids and application of their methyl hydroxyl branched fatty acid derivatives to produce engineering bioplastics. Waste Manag. 2021124, 195–202. [Google Scholar] [CrossRef]
  40. Saerens, K.M.J.; Saey, L.; Soetaert, W. One-step production of unacetylated sophorolipids by an acetyltransferase negative Candida bombicolaBiotechnol. Bioeng. 2011108, 2923–2931. [Google Scholar] [CrossRef]
  41. Geys, R.; Soetaert, W.; Van Bogaert, I. Biotechnological opportunities in biosurfactant production. Curr. Opin. Biotechnol. 201430, 66–72. [Google Scholar] [CrossRef]
  42. Lodens, S.; Roelants, S.L.K.W.; Luyten, G.; Geys, R.; Coussement, P.; de Maeseneire, S.L.; Soetaert, W. Unraveling the regulation of sophorolipid biosynthesis in Starmerella bombicolaFEMS Yeast Res. 202020, foaa021. [Google Scholar] [CrossRef]
  43. Van Bogaert, I.N.A.; Holvoet, K.; Roelants, S.L.K.W.; Li, B.; Lin, Y.; Peer, Y. Van De, Soetaert, W. The biosynthetic gene cluster for sophorolipids: A biotechnological interesting biosurfactant produced by Starmerella bombicolaMol. Microbiol. 201388, 501–509. [Google Scholar] [CrossRef]
  44. Ciesielska, K.; Li, B.; Groeneboer, S.; Van Bogaert, I.; Lin, Y.C.; Soetaert, W.; Van De Peer, Y.; Devreese, B. SILAC-based proteome analysis of Starmerella bombicola sophorolipid production. J. Proteome Res. 201312, 4376–4392. [Google Scholar] [CrossRef]
  45. Rosa, C.A.; Lachance, M.A.; Silva, J.O.C.; Teixeira, A.C.P.; Marini, M.M.; Antonini, Y.; Martins, R.P. Yeast communities associated with stingless bees. FEMS Yeast Res. 20034, 271–275. [Google Scholar] [CrossRef]
  46. Hommel, R.K.; Weber, L.; Weiss, A.; Himmelreich, U.; Rilke, O.; Kleber, H.P. Production of sophorose lipid by Candida (Torulopsisapicola grown on glucose. J. Biotechnol. 199433, 147–155. [Google Scholar] [CrossRef]
  47. Garcia-Ochoa, F.; Casas, J.A. Process for the Production of Sophorose by Candida bombicola. 1996. Available online: (accessed on 18 March 2022).
  48. Ito, S.; Kinta, M.; Inoue, S. Growth of yeasts on n-alkanes: Inhibition by a lactonic sophorolipid produced by Torulopsis bombicolaAgric. Biol. Chem. 198044, 2221–2223. [Google Scholar] [CrossRef]
  49. Aparecida, C.; Queiroz, U.; Akemi, V.; Silveira, I.; Pedrine, M.A.; Celligoi, C. Antimicrobial applications of sophorolipid from Candida bombicola: A promising alternative to conventional drugs. J. Appl. Biol. Biotechnol. 20186, 87–90. [Google Scholar]
  50. Koh, A.; Wong, A.; Quinteros, A.; Desplat, C.; Gross, R. Influence of Sophorolipid Structure on Interfacial Properties of Aqueous-Arabian Light Crude and Related Constituent Emulsions. J. Am. Oil Chem. Soc. 201794, 107–119. [Google Scholar] [CrossRef]
  51. Ma, X.; Li, H.; Song, X. Surface and biological activity of sophorolipid molecules produced by Wickerhamiella domercqiae var. sophorolipid CGMCC 1576. J. Colloid Interface Sci. 2012376, 165–172. [Google Scholar] [CrossRef]
  52. Zhang, T.; Marchant, R.E. Novel Polysaccharide Surfactants: The Effect of Hydrophobic and Hydrophilic Chain Length on Surface Active Properties. J. Colloid Interface Sci. 1996177, 419–426. [Google Scholar] [CrossRef]
  53. Hirata, Y.; Ryu, M.; Igarashi, K.; Nagatsuka, A.; Furuta, T.; Kanaya, S.; Sugiura, M. Natural synergism of acid and lactone type mixed sophorolipids in interfacial activities and cytotoxicities. J. Oleo Sci. 200958, 565–572. [Google Scholar] [CrossRef]
  54. Olanya, O.M.; Ukuku, D.O.; Solaiman, D.K.Y.; Ashby, R.D.; Niemira, B.A.; Mukhopadhyay, S. Reduction in Listeria monocytogenesSalmonella enterica and Escherichia coli O157:H7 in vitro and on tomato by sophorolipid and sanitiser as affected by temperature and storage time. Int. J. Food Sci. Technol. 201753, 1303–1315. [Google Scholar] [CrossRef]
  55. Nyachuba, D.G. Foodborne illness: Is it on the rise? Nutr. Rev. 201068, 257–269. [Google Scholar] [CrossRef]
  56. Phillips, C.A. Bacterial biofilms in food processing environments: A review of recent developments in chemical and biological control. Int. J. Food Sci. Technol. 201651, 1731–1743. [Google Scholar] [CrossRef]
  57. De Rienzo, M.A.D.; Banat, I.M.; Dolman, B.; Winterburn, J.; Martin, P.J. Sophorolipid biosurfactants: Possible uses as antibacterial and antibiofilm agent. New Biotechnol. 201532, 720–726. [Google Scholar] [CrossRef]
  58. Hipólito, A.; da Silva, R.A.A.; de Oliveira Caretta, T.; Silveira, V.A.I.; Amador, I.R.; Panagio, L.A.; Borsato, D.; Celligoi, M.A.P.C. Evaluation of the antifungal activity of sophorolipids from Starmerella bombicola against food spoilage fungi. Biocatal. Agric. Biotechnol. 202029, 101797. [Google Scholar] [CrossRef]
  59. Kumari, A.; Kumari, S.; Prasad, G.S.; Pinnaka, A.K. Production of Sophorolipid Biosurfactant by Insect Derived Novel Yeast Metschnikowia churdharensis f.a., sp. nov., and Its Antifungal Activity Against Plant and Human Pathogens. Front. Microbiol. 202112, 678668. [Google Scholar] [CrossRef]
  60. Sen, S.; Borah, S.N.; Bora, A.; Deka, S. Production, characterization, and antifungal activity of a biosurfactant produced by Rhodotorula babjevae YS3. Microb. Cell Factories 201716, 95. [Google Scholar] [CrossRef]
  61. Silveira, V.A.I.; Marim, B.M.; Hipólito, A.; Gonçalves, M.C.; Mali, S.; Kobayashi, R.K.T.; Celligoi, M.A.P.C. Characterization and antimicrobial properties of bioactive packaging films based on polylactic acid-sophorolipid for the control of foodborne pathogens. Food Packag. Shelf Life 202026, 100591. [Google Scholar] [CrossRef]
  62. Merci, A.; Marim, R.G.; Urbano, A.; Mali, S. Films based on cassava starch reinforced with soybean hulls or microcrystalline cellulose from soybean hulls. Food Packag. Shelf Life 201920, 100321. [Google Scholar] [CrossRef]
  63. Ziemba, A.M.; Lane, K.P.; Balouch, B.; D’Amato, A.R.; Totsingan, F.; Gross, R.A.; Gilbert, R.J. Lactonic Sophorolipid Increases Surface Wettability of Poly-L-lactic Acid Electrospun Fibers. ACS Appl. Bio Mater. 20192, 3153–3158. [Google Scholar] [CrossRef]
  64. Turalija, M.; Bischof, S.; Budimir, A.; Gaan, S. Antimicrobial PLA films from environment friendly additives. Compos. Part B Eng. 2016102, 94–99. [Google Scholar] [CrossRef]
  65. Zhang, X.; Ashby, R.D.; Solaiman, D.K.Y.; Liu, Y.; Fan, X. Antimicrobial activity and inactivation mechanism of lactonic and free acid sophorolipids against Escherichia coli O157:H7. Biocatal. Agric. Biotechnol. 201711, 176–182. [Google Scholar] [CrossRef]
  66. Zhang, X.; Fan, X.; Solaiman, D.K.Y.; Ashby, R.D.; Liu, Z.; Mukhopadhyay, S.; Yan, R. Inactivation of Escherichia coli O157:H7 in vitro and on the surface of spinach leaves by biobased antimicrobial surfactants. Food Control 201660, 158–165. [Google Scholar] [CrossRef]
  67. Zhang, X.; Ashby, R.; Solaiman, D.K.Y.; Uknalis, J.; Fan, X. Inactivation of Salmonella spp. and Listeria spp. by palmitic, stearic, and oleic acid sophorolipids and thiamine dilauryl sulfate. Front. Microbiol. 20167, 2076. [Google Scholar] [CrossRef] [PubMed]
  68. Leyton, A.; Araya, M.; Tala, F.; Flores, L.; Lienqueo, M.E.; Shene, C. Macrocystis pyrifera extract residual as nutrient source for the production of sophorolipids compounds by marine yeast Rhodotorula rubraMolecules 202126, 2355. [Google Scholar] [CrossRef]
  69. Chen, J.; Zhifei, L.U.; An, Z.; Ji, P.; Liu, X. Antibacterial Activities of Sophorolipids and Nisin and Their Combination against Foodborne Pathogen Staphylococcus aureusEur. J. Lipid Sci. Technol. 2020122, 1900333. [Google Scholar] [CrossRef]
  70. Gaur, V.K.; Regar, R.K.; Dhiman, N.; Gautam, K.; Srivastava, J.K.; Patnaik, S.; Kamthan, M.; Manickam, N. Biosynthesis and characterization of sophorolipid biosurfactant by Candida spp.: Application as food emulsifier and antibacterial agent. Bioresour. Technol. 2019285, 121314. [Google Scholar] [CrossRef]
  71. Koh, A.; Gross, R. A versatile family of sophorolipid esters: Engineering surfactant structure for stabilization of lemon oil-water interfaces. Colloids Surf. A Physicochem. Eng. Asp. 2016507, 152–163. [Google Scholar] [CrossRef]
  72. Wang, X.; Lin, R.J.; Gross, R.A. Sophorolipid Butyl Ester: An Antimicrobial Stabilizer of Essential Oil-Based Emulsions and Interactions with Chitosan and γ-Poly(glutamic acid). ACS Appl. Bio Mater. 20203, 5136–5147. [Google Scholar] [CrossRef] [PubMed]
  73. Xue, C.L.; Solaiman, D.K.Y.; Ashby, R.D.; Zerkowski, J.; Lee, J.H.; Hong, S.T.; Yang, D.; Shin, J.A.; Ji, C.M.; Lee, K.T. Study of structured lipid-based oil-in-water emulsion prepared with sophorolipid and its oxidative stability. JAOCS J. Am. Oil Chem. Soc. 201390, 123–132. [Google Scholar] [CrossRef]
  74. Silveira, V.A.I.; Nishio, E.K.; Freitas, C.A.U.Q.; Amador, I.R.; Kobayashi, R.K.T.; Caretta, T.; Macedo, F.; Celligoi, M.A.P.C. Production and antimicrobial activity of sophorolipid against Clostridium perfringens and Campylobacter jejuni and their additive interaction with lactic acid. Biocatal. Agric. Biotechnol. 201921, 101287. [Google Scholar] [CrossRef]
  75. Silveira, V.A.I.; Kobayashi, R.K.T.; de Oliveira Junior, A.G.; Mantovani, M.S.; Nakazato, G.; Celligoi, M.A.P.C. Antimicrobial effects of sophorolipid in combination with lactic acid against poultry-relevant isolates. Braz. J. Microbiol. 202152, 1769–1778. [Google Scholar] [CrossRef]
  76. de O Caretta, T.; I Silveira, V.A.; Andrade, G.; Macedo, F.; PC Celligoi, M.A. Antimicrobial activity of sophorolipids produced by Starmerella bombicola against phytopathogens from cherry tomato. J. Sci. Food Agric. 2021102, 1245–1254. [Google Scholar] [CrossRef]
  77. Tang, Y.; Ma, Q.; Du, Y.; Ren, L.; Van Zyl, L.J.; Long, X. Efficient purification of sophorolipids via chemical modifications coupled with extractions and their potential applications as antibacterial agents. Sep. Purif. Technol. 2020245, 116897. [Google Scholar] [CrossRef]
  78. Chen, J.; Liu, X.; Fu, S.; An, Z.; Feng, Y.; Wang, R.; Ji, P. Effects of sophorolipids on fungal and oomycete pathogens in relation to pH solubility. J. Appl. Microbiol. 2020128, 1754–1763. [Google Scholar] [CrossRef] [PubMed]
  79. Vaughn, S.F.; Behle, R.W.; Skory, C.D.; Kurtzman, C.P.; Price, N.P.J. Utilization of sophorolipids as biosurfactants for postemergence herbicides. Crop Prot. 201459, 29–34. [Google Scholar] [CrossRef]
  80. Imura, T.; Kawamura, D.; Morita, T.; Sato, S.; Fukuoka, T.; Yamagata, Y.; Takahashi, M.; Wada, K.; Kitamoto, D. Production of sophorolipids from non-edible jatropha oil by Stamerella bombicola NBRC 10243 and evaluation of their interfacial properties. J. Oleo Sci. 201362, 857–864. [Google Scholar] [CrossRef]
  81. Joshi-Navare, K.; Khanvilkar, P.; Prabhune, A. Jatropha Oil Derived Sophorolipids: Production and Characterization as Laundry Detergent Additive. Biochem. Res. Int. 20132013, 169797. [Google Scholar] [CrossRef]
  82. Konishi, M.; Morita, T.; Fukuoka, T.; Imura, T.; Uemura, S.; Iwabuchi, H.; Kitamoto, D. Selective production of acid-form sophorolipids from glycerol by Candida floricolaJ. Oleo Sci. 201766, 1365–1373. [Google Scholar] [CrossRef]
  83. Wang, H.; Roelants, S.L.K.W.; To, M.H.; Patria, R.D.; Kaur, G.; Lau, N.S.; Lau, C.Y.; Van Bogaert, I.N.A.; Soetaert, W.; Lin, C.S.K. Starmerella bombicola: Recent advances on sophorolipid production and prospects of waste stream utilization. J. Chem. Technol. Biotechnol. 201994, 999–1007. [Google Scholar] [CrossRef]
  84. Jiménez-Peñalver, P.; Koh, A.; Gross, R.; Gea, T.; Font, X. Biosurfactants from Waste: Structures and Interfacial Properties of Sophorolipids Produced from a Residual Oil Cake. J. Surfactants Deterg. 201923, 481–486. [Google Scholar] [CrossRef]
  85. Kaur, G.; Wang, H.; To, M.H.; Roelants, S.L.K.W.; Soetaert, W.; Lin, C.S.K. Efficient sophorolipids production using food waste. J. Clean. Prod. 2019232, 1–11. [Google Scholar] [CrossRef]
  86. Hirata, Y.; Igarashi, K.; Ueda, A.; Quan, G.L. Enhanced sophorolipid production and effective conversion of waste frying oil using dual lipophilic substrates. Biosci. Biotechnol. Biochem. 202185, 1763–1771. [Google Scholar] [CrossRef]
  87. Haider, T.P.; Völker, C.; Kramm, J.; Landfester, K.; Wurm, F.R. Plastics of the Future? The Impact of Biodegradable Polymers on the Environment and on Society. Angew. Chem.-Int. Ed. 201958, 50–62. [Google Scholar] [CrossRef] [PubMed]
  88. Maeng, Y.; Kim, K.T.; Zhou, X.; Jin, L.; Kim, K.S.; Kim, Y.H.; Lee, S.; Park, J.H.; Chen, X.; Kong, M.; et al. A novel microbial technique for producing high-quality sophorolipids from horse oil suitable for cosmetic applications. Microb. Biotechnol. 201811, 917–929. [Google Scholar] [CrossRef] [PubMed]
  89. Zerhusen, C.; Bollmann, T.; Gödderz, A.; Fleischer, P.; Glüsen, B.; Schörken, U. Microbial Synthesis of Nonionic Long-Chain Sophorolipid Emulsifiers Obtained from Fatty Alcohol and Mixed Lipid Feeding. Eur. J. Lipid Sci. Technol. 2020122, 1900110. [Google Scholar] [CrossRef]
  90. Ashby, R.D.; Zerkowski, J.A.; Solaiman, D.K.Y.; Liu, L.S. Biopolymer scaffolds for use in delivering antimicrobial sophorolipids to the acne-causing bacterium Propionibacterium acnesNew Biotechnol. 201128, 24–30. [Google Scholar] [CrossRef]
  91. Solaiman, D.K.Y.; Ashby, R.D.; Crocker, N.V. High-titer production and strong antimicrobial activity of sophorolipids from Rhodotorula bogoriensisBiotechnol. Prog. 201531, 867–874. [Google Scholar] [CrossRef]
  92. Solaiman, D.K.Y.; Ashby, R.D.; Nuñez, A.; Crocker, N. Low-Temperature Crystallization for Separating Monoacetylated Long-Chain Sophorolipids: Characterization of Their Surface-Active and Antimicrobial Properties. J. Surfactants Deterg. 202023, 553–563. [Google Scholar] [CrossRef]
  93. Ishii, N.; Kobayashi, T.; Matsumiya, K.; Ryu, M.; Hirata, Y.; Matsumura, Y.; Suzuki, Y.A. Transdermal administration of lactoferrin with sophorolipid. Biochem. Cell Biol. 201290, 504–512. [Google Scholar] [CrossRef]
  94. Naik, N.J.; Abhyankar, I.; Darne, P.; Prabhune, A.; Madhusudhan, B. Sustained Transdermal Release of Lignans Facilitated by Sophorolipid based Transferosomal Hydrogel for Cosmetic Application. Int. J. Curr. Microbiol. Appl. Sci. 20198, 1783–1791. [Google Scholar] [CrossRef]
  95. Imura, T.; Morita, T.; Fukuoka, T.; Ryu, M.; Igarashi, K.; Hirata, Y.; Kitamoto, D. Spontaneous vesicle formation from sodium salt of acidic sophorolipid and its application as a skin penetration enhancer. J. Oleo Sci. 201463, 141–147. [Google Scholar] [CrossRef]
  96. Snehal, V.M.; Santosh, S.K.; Navnath, K.; Sachin, A.; Asmita, P. Formulation and Evaluation of Wound Healing Activity of Sophorolipid-Sericin Gel in Wistar Rats. Pharmacogn. Mag. 201915, 123–127. [Google Scholar]
  97. Kwak, M.J.; Park, M.Y.; Kim, J.; Lee, H.; Whang, K.Y. Curative effects of sophorolipid on physical wounds: In vitro and in vivo studies. Vet. Med. Sci. 20217, 1400–1408. [Google Scholar] [CrossRef]
  98. Diaz-Rodriguez, P.; Chen, H.; Erndt-Marino, J.D.; Liu, F.; Totsingan, F.; Gross, R.A.; Hahn, M.S. Impact of Select Sophorolipid Derivatives on Macrophage Polarization and Viability. ACS Appl. Bio Mater. 20192, 601–612. [Google Scholar] [CrossRef]
  99. Valotteau, C.; Banat, I.M.; Mitchell, C.A.; Lydon, H.; Marchant, R.; Babonneau, F.; Pradier, C.M.; Baccile, N.; Humblot, V. Antibacterial properties of sophorolipid-modified gold surfaces against Gram positive and Gram negative pathogens. Colloids Surf. B Biointerfaces 2017157, 325–334. [Google Scholar] [CrossRef]
  100. Liza, K.A.; Manefield, M. The role of lipids in activated sludge floc formation. AIMS Environ. Sci. 20152, 122–133. [Google Scholar] [CrossRef]
  101. Sana, S.; Datta, S.; Biswas, D.; Sengupta, D. Assessment of synergistic antibacterial activity of combined biosurfactants revealed by bacterial cell envelop damage. Biochim. Biophys. Acta-Biomembr. 20181860, 579–585. [Google Scholar] [CrossRef]
  102. Kim, K.; Yoo, D.; Kim, Y.; Lee, B.; Shin, D.; Kim, E.K. Characteristics of sophorolipid as an antimicrobial agent. J. Microbiol. Biotechnol. 200212, 235–241. [Google Scholar]
  103. Ankulkar, R.; Chavan, M. Characterisation and Application Studies of Sophorolipid Biosurfactant by Candida tropicalis RA1. J. Pure Appl. Microbiol. 201913, 1653–1665. [Google Scholar] [CrossRef]
  104. Archana, K.; Sathi Reddy, K.; Parameshwar, J.; Bee, H. Isolation and characterization of sophorolipid producing yeast from fruit waste for application as antibacterial agent. Environ. Sustain. 20192, 107–115. [Google Scholar] [CrossRef]
  105. Abhyankar, I.; Sevi, G.; Prabhune, A.A.; Nisal, A.; Bayatigeri, S. Myristic Acid Derived Sophorolipid: Efficient Synthesis and Enhanced Antibacterial Activity. ACS Omega 20216, 1273–1279. [Google Scholar] [CrossRef]
  106. Sambanthamoorthy, K.; Feng, X.; Patel, R.; Patel, S.; Paranavitana, C. Antimicrobial and antibiofilm potential of biosurfactants isolated from lactobacilli against multi-drug-resistant pathogens. BMC Microbiol. 201414, 197. [Google Scholar] [CrossRef]
  107. Valotteau, C.; Baccile, N.; Humblot, V.; Roelants, S.; Soetaert, W.; Stevens, C.V.; Dufrêne, Y.F. Nanoscale antiadhesion properties of sophorolipid-coated surfaces against pathogenic bacteria. Nanoscale Horiz. 20194, 975–982. [Google Scholar] [CrossRef]
  108. Ceresa, C.; Fracchia, L.; Williams, M.; Banat, I.M.; Díaz De Rienzo, M.A. The effect of sophorolipids against microbial biofilms on medical-grade silicone. J. Biotechnol. 2020309, 34–43. [Google Scholar] [CrossRef] [PubMed]
  109. Pontes, C.; Alves, M.; Santos, C.; Ribeiro, M.H.; Gonçalves, L.; Bettencourt, A.F.; Ribeiro, I.A.C. Can Sophorolipids prevent biofilm formation on silicone catheter tubes? Int. J. Pharm. 2016513, 697–708. [Google Scholar] [CrossRef]
  110. Nguyen, B.V.G.; Nagakubo, T.; Toyofuku, M.; Nomura, N.; Utada, A.S. Synergy between Sophorolipid Biosurfactant and SDS Increases the Efficiency of P. aeruginosa Biofilm Disruption. Langmuir 202036, 6411–6420. [Google Scholar] [CrossRef] [PubMed]
  111. Vasudevan, S.; Prabhune, A.A. Photophysical studies on curcumin-sophorolipid nanostructures: Applications in quorum quenching and imaging. R. Soc. Open Sci. 20185, 170865. [Google Scholar] [CrossRef] [PubMed]
  112. Haque, F.; Alfatah, M.; Ganesan, K.; Bhattacharyya, M.S. Inhibitory Effect of Sophorolipid on Candida albicans Biofilm Formation and Hyphal Growth. Sci. Rep. 20166, 23575. [Google Scholar] [CrossRef]
  113. Haque, F.; Sajid, M.; Cameotra, S.S.; Battacharyya, M.S. Anti-biofilm activity of a sophorolipid-amphotericin B niosomal formulation against Candida albicansBiofouling 201733, 768–779. [Google Scholar] [CrossRef]
  114. Sanada, H.; Nakagami, G.; Takehara, K.; Goto, T.; Ishii, N.; Yoshida, S.; Ryu, M.; Tsunemi, Y. Antifungal effect of non-woven textiles containing polyhexamethylene biguanide with sophorolipid: A potential method for tinea pedis prevention. Healthcare 20142, 183–191. [Google Scholar] [CrossRef]
  115. Sen, S.; Borah, S.N.; Kandimalla, R.; Bora, A.; Deka, S. Sophorolipid Biosurfactant Can Control Cutaneous Dermatophytosis Caused by Trichophyton mentagrophytes. Front. Microbiol. 202011, 329. [Google Scholar] [CrossRef]
  116. Dengle-Pulate, V.; Chandorkar, P.; Bhagwat, S.; Prabhune, A.A. Antimicrobial and SEM studies of sophorolipids synthesized using lauryl alcohol. J. Surfactants Deterg. 201417, 543–552. [Google Scholar] [CrossRef]
  117. Elshikh, M.; Moya-Ramírez, I.; Moens, H.; Roelants, S.; Soetaert, W.; Marchant, R.; Banat, I.M. Rhamnolipids and lactonic sophorolipids: Natural antimicrobial surfactants for oral hygiene. J. Appl. Microbiol. 2017123, 1111–1123. [Google Scholar] [CrossRef]
  118. Solaiman, D.K.Y.; Ashby, R.D.; Uknalis, J. Characterization of growth inhibition of oral bacteria by sophorolipid using a microplate-format assay. J. Microbiol. Methods 2017136, 21–29. [Google Scholar] [CrossRef] [PubMed]
  119. Solaiman, D.K.Y.; Ashby, R.D.; Birbir, M.; Caglayan, P. Antibacterial activity of sophorolipids produced by Candida bombicola on Gram-positive and Gram-negative bacteria isolated from salted hides. J. Am. Leather Chem. Assoc. 2016111, 358–363. [Google Scholar]
  120. Joshi-Navare, K.; Prabhune, A. A biosurfactant-sophorolipid acts in synergy with antibiotics to enhance their efficiency. BioMed Res. Int. 20132013, 512495. [Google Scholar] [CrossRef] [PubMed]
  121. Baccile, N.; Noiville, R.; Stievano, L.; Bogaert, I. Van. Sophorolipids-functionalized iron oxide nanoparticles. Phys. Chem. Chem. Phys. 201215, 1606–1620. [Google Scholar] [CrossRef] [PubMed]
  122. Basak, G.; Das, D.; Das, N. Dual role of acidic diacetate sophorolipid as biostabilizer for ZnO nanoparticle synthesis and biofunctionalizing agent against Salmonella enterica and Candida albicansJ. Microbiol. Biotechnol. 201424, 87–96. [Google Scholar] [CrossRef] [PubMed]
  123. Delbeke, E.I.P.; Movsisyan, M.; Van Geem, K.M.; Stevens, C.V. Chemical and enzymatic modification of sophorolipids. Green Chem. 201518, 76–104. [Google Scholar] [CrossRef]
  124. Shao, L.; Song, X.; Ma, X.; Li, H.; Qu, Y. Bioactivities of sophorolipid with different structures against human esophageal cancer cells. J. Surg. Res. 2012173, 286–291. [Google Scholar] [CrossRef]
  125. Li, H.; Guo, W.; Ma, X.J.; Li, J.S. In Vitro and in Vivo Anticancer Activity of Sophorolipids to Human Cervical Cancer. Appl. Biochem. Biotechnol. 2017181, 1372–1387. [Google Scholar] [CrossRef]
  126. Callaghan, B.; Lydon, H.; Roelants, S.L.K.W.; Van Bogaert, I.N.A.; Marchant, R.; Banat, I.M.; Mitchell, C.A. Lactonic sophorolipids increase tumor burden in Apcmin+/− mice. PLoS ONE 201611, e0156845. [Google Scholar]
  127. Nawale, L.; Dubey, P.; Chaudhari, B.; Sarkar, D.; Prabhune, A. Anti-proliferative effect of novel primary cetyl alcohol derived Sophorolipids against human cervical cancer cells HeLa. PLoS ONE 201712, e0174241. [Google Scholar] [CrossRef] [PubMed]
  128. Haggag, Y.; Elshikh, M.; El-Tanani, M.; Bannat, I.M.; McCarron, P.; Tambuwala, M.M. Nanoencapsulation of sophorolipids in PEGylated poly(lactide-co-glycolide) as a novel approach to target colon carcinoma in the murine model. Drug Deliv. Transl. Res. 202010, 1353–1366. [Google Scholar] [CrossRef] [PubMed]
  129. Wang, X.; Xu, N.; Li, Q.; Chen, S.; Cheng, H.; Yang, M.; Jiang, T.; Chu, J.; Ma, X.; Yin, D. Lactonic sophorolipid–induced apoptosis in human HepG2 cells through the Caspase-3 pathway. Appl. Microbiol. Biotechnol. 2021105, 2033–2042. [Google Scholar] [CrossRef] [PubMed]
  130. Kithur Mohamed, S.; Asif, M.; Nazari, M.V.; Baharetha, H.M.; Mahmood, S.; Yatim, A.; Abdul Majid, A.S.; Abdul Majid, A. Antiangiogenic activity of sophorolipids extracted from refined bleached deodorized palm olein. Indian J. Pharmacol. 201951, 45–54. [Google Scholar]
Contributors MDPI registered users' name will be linked to their SciProfiles pages. To register with us, please refer to : , , ,
View Times: 719
Revisions: 2 times (View History)
Update Date: 27 Sep 2022