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Prevention by Essential Oils of the Occurrence and Growth of Aspergillus flavus and Aflatoxin B1 Production in Food Systems: Review

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Yamina Ben Miri, Azem Belasli, Djamel Djenane and Agustín Ariño

Submitted: April 21st, 2019Reviewed: June 26th, 2019Published: July 31st, 2019

DOI: 10.5772/intechopen.88247

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Aspergillus flavus has been reported to be one of the most common fungal species in foods. Under conditions of high humidity and moderate temperature, this fungus may synthetize the mycotoxin Aflatoxin B1 (AFB1), which is reported to be hepatotoxic, teratogenic, mutagenic and immunosuppressive to human beings and livestock and it is classified as carcinogenic to humans (Group 1 by IARC). AFB1 affects cereals, oilseeds, nuts, spices, legumes, and dried fruits, while Aflatoxin M1 is a metabolite of AFB1 that can occur in milk and milk products. Current control is aimed at controlling fungal growth and AFB1 production in food by eco-friendly, biodegradable and safer alternatives, in contrast to synthetic chemicals that can be toxic to humans and cause adverse environmental effects. Recently, considerable attention has been directed towards natural compounds, such as essential oils (EOs) as a promising approach for controlling AFB1 production in food. The main reason for supporting the application of natural products is the consumer’s preference for natural methods to preserve foods. The aim of the present review is to summarize knowledge of EOs and AFB1 production from the literature.


  • Aspergillus flavus
  • aflatoxin B1 (AFB1)
  • essential oils
  • food system

1. Introduction

Molds are ubiquitous micro-organisms with a high capacity to colonize different types of substrates and to proliferate under extreme environmental conditions [1]. They alter various types of foods namely cereals, nuts, oil seeds, legumes, spices, vegetables, fruits, etc. and some species produce mycotoxins. Of all mycotoxins, Aflatoxin B1 (AFB1) produced primarily by Aspergillus flavusand A. parasiticusis the most toxic form (hepatotoxic, teratogenic, mutagenic and carcinogenic) for humans and animals [2, 3, 4, 5]. The health impact of this compound has justified the introduction of a consumer protection measure by the establishment of maximum levels in certain food categories. However, the existence of these standards also has significant economic repercussions restricting trade from certain areas where the contamination is frequent and strongly decreasing the economic value of some productions in case of contamination. These losses are estimated by FAO (Food and Agriculture Organization of The United Nations) at about 1 billion tons a year. Therefore, it seems imperative to develop ways of combating contamination of food with these toxic compounds and/or to limit their harmful effects.

Pesticides and fungicides have been widely used to prevent the development of fungal agents. However, because of their own toxicity, their use is subjected to certain restrictions. Biological control is also a possible option. Thus, antiaflatoxigenic bacterial and fungal strains were found effective in reducing the development of toxic strains of A. flavus. However, none of these strategies seems to be able to solve the problem of contamination of raw materials by aflatoxins, as evidenced by the numerous researches that show high levels of contamination, particularly in areas where the climate is favorable for the development of the toxigenic fungal species. At present, there is growing interest in identifying natural compounds able to limit the growth and/or the production of mycotoxins. Thus, the use of essential oils (EOs) of plants or spices could show their ability to limit food contamination. The aim of this review is to summarize the results from the literature on the effects of EOs against A. flavusgrowth and AFB1 production.


2. Aflatoxins

Aflatoxins are produced primarily by the common fungus Aspergillus flavusand the closely related species A. parasiticus, and they can be found in feedstuffs and foodstuffs throughout the world. These mycotoxins are a family of several molecules of which the most important are AFB1, B2, G1 and G2 ( Figure 1 ). The letters refer to the fluorescence blue (B) or green (G) under UV and the numbers (1 or 2) refer to their relative chromatographic mobility. They are molecules with a polycyclic structure belonging to the furanocoumarin class. There are also other aflatoxins; there are in total more than a dozen (M1, P1, Q 1, B2a, G2a, etc.). The most are products resulting from the metabolic metabolism of the four molecules produced by mold in food [6]. For example, after ingestion of contaminated feed, AFB1 is transformed into the liver of mammals by cytochrome P450 into several metabolites, mainly AFM1 excreted in milk, which is produced by hydroxylation of the tertiary carbon of the difuranocoumarin cycle. The hydroxyl group formed makes AFM1 more soluble in water and therefore rapidly excreted in mammalian milk, urine, bile and feces. The AFM1 owes its name to its presence in Milk [7]. Aflatoxins are stable molecules and very resistant to the various processes of food processing such as roasting, extrusion and cooking [8]. Indeed, the decomposition of aflatoxins takes place at very high temperatures which are difficult to comply with the manufacturing or processing processes of food. A. flavusand A. parasiticusare the main aflatoxin producers; A. flavusis responsible for the production of type B aflatoxins, while A. parasiticusproduces both type B and G [9]. Aflatoxins can contaminate cereals, oil seeds, nuts, spices, legumes, dried fruits, milk and milk products, posing a high risk to public health [10, 11, 12, 13]. Maize, peanuts and tree nuts (i.e. pistachios) are susceptible to aflatoxin contamination in the field, while other cereals, oilseeds and dried fruits are mostly contaminated at postharvest and during storage [14, 15, 16].

Figure 1.

Chemical structures of AFB1, B2, M1, G1 and G2.


3. Methods of aflatoxin decontamination

Foodstuffs should not be hazardous to consumer health; as consequence, elimination of mycotoxin from products is a challenge for the food industry. Concerns have been directed towards aflatoxins because of their global threat and toxicity. Most of the factors obtained from studies on aflatoxins can be applied to other mycotoxins. Although prevention is the most effective intervention, chemical, physical and biological methods have been investigated to eliminate aflatoxins or reduce them ( Figure 2 ). However, these techniques are not completely safe, are expensive and not well preferred by consumers.

Figure 2.

Some commonly used physical, chemical and biological methods of aflatoxin detoxification.


4. Essential oils: an alternative strategy for control against aflatoxin contamination

The frequency of contamination of world crops by aflatoxins shows that the strategies currently used are insufficient to guarantee the security of the foods and that it is necessary to develop others, as a complement or substitution of those already existing. In this context, strategies based on the use of compounds naturally recognized as not harmful to the environment and to health, seem interesting. Indeed, plants produce different secondary metabolites (terpenoids, phenolic compounds, etc.) for their protection against external agents (mechanical, biological or climatic). These compounds could possibly be used as a means of combating fungal contamination and/or mycotoxins [17].

4.1 Essential oils

4.1.1 Overview

EOs are a mixture of volatile compounds (secondary metabolites) isolated from plants mainly by hydro-distillation. They are mostly consisting of mono- and sesquiterpenes but may also contain non-terpenoid hydrocarbons, phenylpropanoids, esters, lactones, phthalides, nitrogen or sulfurized structures and isothiocyanates. They are lipophilic compounds which are distinguished by their aromatic properties, hence their use as flavorings or perfumes [18]. In addition, certain compounds are also used for their many biological activities: bactericide, fungicide and antioxidant [19].

4.1.2 Mechanism of cellular action of essential oils

The mode of action of EOs has not been completely understood yet [20, 21]. In general, EOs actions are described in three phases. Firstly, EOs spreading on the cell wall of fungi changes the membrane permeability resulting in the loss of cellular components. Secondly, an acidification inside the cell that blocks the production of cellular energy (ATP) due to ion loss, the collapse of proton pumps, the reduction of membrane potential, and destruction of genetic materials that leads to the death of fungus. Furthermore, some reports have indicated that EOs can also coagulate the cytoplasm and damage lipids, proteins, cell walls and membranes that can lead to the leakage of macromolecules and the lysis [22, 23, 24, 25, 26, 27].

Phenolic compounds are known to affect microbial cell permeability, allowing the loss of macromolecules from the interior. They could also interact with membrane proteins, causing a deformation in their structure and functionality [28].

4.1.3 Use of essential oils as antifungal and antiaflatoxigenic agents

In view of their different biological properties, EOs have been tested as alternative strategy for combating mycotoxins, especially aflatoxins [29, 30, 31, 32, 33, 34] ( Table 1 ). EOs are molecules of natural origin, biodegradable, and are therefore considered as a possible alternative to synthetic pesticides [35]. Their use as food additives or flavorings has recently been authorized in the USA [36]. As their active components are highly volatile, they are mainly used as fumigants for products after harvest. A number of commercially available EOs can be used in crops produced according to the specifications such as E-Rase™ (jojoba EO, Simmondsia californica), Sporan™ (rosemary EO, Rosmarinus officinalis), Promax™ (thyme EO, Thymus vulgaris) [37], Cinnamite™ and Valero™ (cinnamon EO, Cinnamomum verum) [19], Talent® (based on carvone, EO of cumin or dill) and eugenol-Tween® [38].

Plant scientific namePlant common nameApplied concentrations in culture mediumInhibition of A. flavusgrowthInhibition of AFB1 productionReference
Ageratum conyzoidesMentrasto0.10 μg/mL
0.04 μg/ mL
Pimpinella anisumAnise0.50 μg/g100.00%100.00%[31]
Ocimum sanctumHoly basil0.10 μg/ mL
0.20 μg/ mL
Ocimum sanctumHoly basil0.10 μL/ mL
0.40 μL/ mL
Piper betleBetel0.40 μL/ mL
0.60 μL/ mL
Callistemon lanceolatusCallistemon0.546 mg/ mL
0.819 mg/ mL
Cinnamomum jensenianumCinnamon4.00 μL/ mL
6.00 μL/ mL
Amomum subulatumCardamom0.25 mg/ mL
0.50 mg/ mL
Cicuta virosaWater hemlock1.00 μL/ mL
4.00 μL/ mL
Cymbopogon citratusLemongrass0.20 mg/ mL3.00%100.00%[32]
Coriandrum sativumCoriander0.75 μL/ mL66.50%25.00%[50]
Cuminum cyminumCumin0.40 μL/ mL
0.50 μL/ mL
Curcuma longaTurmeric0.50% (v/v)nd99.00%[59]
Foeniculum vulgareFennel0.75 μL/ mL54.40%23.00%[52]
Mentha spicataMint0.60 μL/ mL
0.90 μl/ mL
Cymbopogon martiniPalmarosa-Indian geranium0.30 μL/ mL
0.40 μL/ mL
Citrus sinensis
250.00 ppm
1000.00 ppm
Citrus maximaPomelo250.00 ppm
1000.00 ppm
Rosmarinus officinalisRosemary0.45% (v/v)0.00%100.00%[33]
Thymus vulgarisThyme0.30 μL/ mL
0.70 μL/ mL
Thymus daenensis
62.50 mg/L
500.00 mg/L
Satureja khozistanica
62.50 mg/L
500.00 mg/L
Satureja macrosiphoniaSater62.50 mg/L
500.00 mg/L
Lippia rugosaVerbenacea600.00 μg/mL
1000.00 μg/mL

Table 1.

Inhibition effect of some EOs on the growth of A. flavusand the production of AFB1.

The antifungal activity of EOs of T. vulgarisand camphor (Eucalyptus rostrataL.) was tested on A. flavus. They completely inhibited mycelial growth of the fungus at 1000 and 2000 ppm (mg/kg), and aflatoxin production at 500 and 1000 ppm, respectively [39].

The EO of Satureja hortensiswas assessed for antifungal activity against A. flavus in vitroon solid and liquid culture, and under storage conditions. The EO showed strong antifungal activity based on the inhibition zone and minimal inhibitory concentration (MIC) values on solid culture. The very low concentrations of EOs also reduced wet and dry mycelium weight of A. flavusin liquid culture [40]. The antifungal potential of EOs of leaves and seeds of Aframomum daniellii, Aframomum meleguetaand Aframomum latifoliumand those of husk of A. latifoliumwas evaluated against A. flavus. Results showed that the inhibition of tested EOs were between 28.06 and 100%, respectively for EOs of seeds of A. meleguetaand EO of the husk of A. latifoliumat 500 ppm. EO of leaves of A. meleguetaand husk of A. latifoliumexhibited the most effective inhibition [41]. EOs extracted from Mentha arvensis(0.5 mg/mL) caused total inhibition of A. flavusgrowth and of AFB1 production [42]. Cymbopogon martinii, Foeniculum vulgareand Trachyspermum ammiEOs were tested against A. flavus. The MIC was recorded at 1 μL/mL for T. ammiEO and 4 μL/mL for C. martiniiand F. vulgare. At these concentrations, the EOs completely inhibited the growth of A. flavus[43].

Ageratum conyzoidesEO inhibited A. flavusgrowth and reduced AFB1 production at 0.10 μg/mL. The ultra-structural changes in A. flavuscell under transmission electron microscopy (TEM) were observed on the endomembrane system, mainly the mitochondria. The plasma membrane cells lost its linear aspect. The fibrillar layers lost their building and failed to deposit on the cell wall. The mitochondria in treated cells suffered a disruption of the internal structure [1]. Ocimum sanctumEO was evaluated to inhibit A. flavusgrowth and AFB1 production. The MIC of O. sanctumagainst A. flavuswas found at 0.3 μL/mL while AFB1 production was recorded at 0.2 μL/mL [44]. The efficacy of boldo (Peumus boldusMol.), poleo (Lippia turbinatavar. integrifolia (Griseb.), clove (Syzygium aromaticumL.), anise (Pimpinella anisum), and thyme (T. vulgaris) EOs was tested against A. flavusand A. parasiticusgrowth and AFB1 at different water activity (aW) levels (0.98, 0.95, 0.93). Inhibition was estimated at 75, 83, and 100% at 0.98, 0.95, and 0.93 aW, respectively [45].

The effects of EOs of Ocimum gratissimumand Plectranthus glandulosusleaves on growth and AFB1 production by A. flavuswere assessed at five levels (200, 400, 600, 800 and 1000 mg/L). Growth of A. flavuswas completely inhibited by 800 mg/L of O. gratissimumEO and by 1000 mg/L of P. glandulosusEO. The AFB1 production was inhibited by 1000 mg/L of both EOs of O. gratissimumand P. glandulous[46]. Cinnamomum camphoraand Alpinia galangaEOs inhibited A. flavusat 1000 ppm and the AFB1 production at 500 ppm for A. galangaand 750 ppm for C. camphora. The combination of the two EOs was more effective than the individual ones. The mixture showed total inhibition of the mycelium growth at 750 ppm and AFB1 production starting from 250 ppm [47]. Lippia rugosaEO was effective against fungal growth and production of AFB1 from A. flavuswas totally inhibited at 1000 mg/L. The inhibition was attributed to the presence of geraniol [48].

Both A. flavusgrowth and AFB1 production were inhibited by EOs of Citrus maximaBurm, Citrus sinensis(L.) Osbeck, and their combination. DL-Limonene inhibited AFB1 productionat a concentration of 250 ppm that is lower than the individual EOs and the combination. It has been suggested that remaining constituents in the EO would mask the efficacy of DL-limonene and they may act in negatively. Furthermore, the authors declared that there was no synergism between the EO constituents when the two EOs were mixed at the same concentration, attaining aflatoxin inhibition at 500 ppm [49].

Similar types of results were also found in the case of Piper betlevar. magahi EO, where eugenol was more effective as inhibitor of fungal growth and aflatoxin production than the whole EO. It was suggested that the components of the EO acted synergistically in negative direction and diminished the activity of eugenol [3]. The effect of basil, fennel, coriander, caraway, peppermint and rosemary EOs on A. flavusgrowth and AFB1 production at 500, 750 and 1000 ppm was also studied. The complete inhibition of A. flavusgrowth was observed at 1000 ppm concentrations of basil, coriander, caraway and rosemary EOs. While, EOs of basil and coriander showed interesting inhibition of AFB1 at all concentrations [50].

Cicuta virosaL. EO inhibited the growth of A. flavusand AFB1 production at 4 μL/mL of EO. The AFB1 was reduced to about half compared to the control at 2 μL/mL [51]. Similar type of results was found with Cinnamomum jensenianumEO, which reduced AFB1 to about half compared to the control at 2 μL/mL. At this concentration of the EO, the plasma membrane of A. flavusbecame rough with continuous folding into the cytoplasm and festooned with small lomasomes. A decreased cytoplasmic matrix was also observed. They showed that some mitochondria suffered extensive disruption of the internal structure with a decrease in mitochondrial cristae. The cell ultrastructure damage was aggravated when the EO concentration was doubled. Major alterations were observed, including massive vacuolation of cytoplasm with vacuole fusion, appearance of numerous lomasomes with folding, and detachment of plasma membrane from the cell wall. The fibrillar layers gradually lost their integrity, becoming thinner, and eventually failing to deposit on the cell wall. The plasma membrane was also folded at many sites. The cytoplasmic matrix and some cytoplasmic organelles were absent. Moreover, the mitochondria suffered a severe disruption of the internal structure with complete lysis. The antifungal mode of action of EO was evaluated by quantification of the ergosterol production in cells. At concentration of 2 μL/mL, the ergosterol content in the plasma membrane of A. flavuswas significantly reduced by the different concentrations of EO. A dose dependent decrease in ergosterol production was observed when isolates were grown in the presence of the EO. Therefore, this EO exerts its effect directly on the plasma membrane without any obvious damage to the cell wall. This emphasizes that the antimicrobial components of the EOs cross the cell membrane, interact with the enzymes and proteins of the membrane, thus producing a flux of protons towards the cell exterior which induces disruption to the fungal cell organization and, ultimately, their death [34].

The EO of Anethum graveolenswas evaluated on A. flavus. Morphological changes in the cells of A. flavusand a reduction in the ergosterol quantity was caused by A. graveolensEO. An augmentation of mitochondrial membrane potential (MMP), and the suppression of the glucose-induced decrease in external pH were observed at concentration of 4 mL/mL. A decrease of the activities of ATPase and dehydrogenase in A. flavuscells were also observed. The authors attributed the dysfunctions of the mitochondria to the reactive oxygen species (ROS) accumulation in A. flavus. The addition of L-cysteine caused a reduction in cell viability, which indicates that ROS is an interesting mediator of the antifungal activity of A. graveolensEO [52].

The Callistemon lanceolatus(Sm.) Sweet EO inhibited AFB1 production at concentrations lower than its fungitoxic concentration [53]. As well, the EO of Lantana indicashowed in vitroantifungal and antiaflatoxigenic activities against A. flavus. The antifungal activity of the L. indicaEO, tested by disk diffusion test and by SMKY liquid culture, completely inhibited mycelia growth and AFB1 production at 1.5 and 0.75 μg/mL, respectively [54]. The antifungal and antiaflatoxigenic activities of Litsea cubebaEO were tested on A. flavus. The EO showed a high activity against three toxigenic isolates of A. flavus. Under the scanning electron microscopy (SEM), the EO showed alterations of the hyphae and conidiophores structures. The results exhibited that L. cubebaEO could inhibit fungal growth and AFB1 production [55]. Caesulia axillarisRoxb EO showed complete inhibition of the fungal growth at 1.0 μL/mL and AFB1 at 0.8 μL/mL. Thus, the EO showed antiaflatoxigenic effects at concentration lower than their fungitoxic concentrations indicating two different mode of action for inhibition of fungal growth and AFB1 production [56]. Jamrosa EO (Cymbopogon khasans) showed antifungal activity and inhibition of AFB1 production at 0.4 μL/mL. The authors indicated that inhibition of AFB1 production was secondary to inhibition of fungal growth [57]. The capacity of 14 EO components and their combinations to inhibit fungal growth and AFB1 production revealed that thymol, eugenol, menthol, and their combinations were more effective for inhibition of fungal growth and AFB1 was completely inhibited at 1.0 μL/mL. Geranyl acetate, linalool, β-asarone, 1, 8-cineol, and E-citral were moderately antifungal between 1.0 and 5.0 μL/mL [58].

The inhibition of AFB1 production by A. flavuswas observed at 1.0 and 42.7 μL/mL, respectively, for the samples treated with the EO of Curcuma longaL. and curcumin at a concentration of 0.5%. The authors suggested that the antiaflatoxigenic activity might be attributed to phenolic compounds that inhibit lipid peroxidation. Thus, the antioxidant activity of C. longacould be important for the inhibition of AFB1 production [59]. The Boswellia carteriiBirdw EO inhibited A. flavusgrowth and AFB1 production at 1.75 and 1.25 μL/mL, respectively. The EO caused reduction in ergosterol content of plasma membrane of A. flavus[60]. This observation showed that plasma membrane is an interesting site for the mechanism of EO supporting the findings of other authors [51]. The Cuminum cyminumL. EO was tested on A. flavusgrowth and AFB1 production. The EO inhibited the fungal growth and AFB1 production at 0.6 and 0.5 μL/mL, respectively. The EO totally reduced the ergosterol content at 0.6 μL/mL [31]. T. vulgarisL. EO was tested against A. flavusgrowth and AFB1 production. Total inhibition of fungal growth was observed at 250 μg/mL. The T. vulgarisEO reduced ergosterol production by A. flavus. The morphological structure of A. flavuswas analyzed by SEM, alterations in conidiophore characteristics were observed. Conidial head size varied between 71.3 and 20.5 μm at concentrations between 50 and 500 μg/mL. A decrease of cytoplasmic content and modifications of membrane integrity were observed. The results were proportional to ergosterol production, which decreased with each EO concentration. Such modifications induced by the EO might be related to the interference caused by its constituents in cell wall synthesis, which affects A. flavusgrowth and morphology. Complete inhibition of AFB1 production was recorded at 150 μg/mL. T. vulgarisEO exhibited antiaflatoxigenic activity, as AFB1 biosynthesis inhibition occurred at lower concentration (50 μg/mL) than that required for inhibition of ergosterol production (100 μg/mL) and for morphological alterations of hyphae, conidiophores and conidia (100 μg/mL) [61].

On the other hand, cinnamaldehyde was assessed on AFB1 production of A. flavus. The results demonstrated that with cinnamaldehyde treatment, ROS formation reduction was associated with AFB1 production inhibition, which indicate that AFB1 inhibition induced by cinnamaldehyde is related to ROS reduction. Lipid peroxidation is the consequence of ROS formation and has been shown to be involved in AFB1 biosynthesis [62].

Ben Miri et al. [74] reported that Citrus limonEO at 1.75 mg/mL and Citrus sinensisat 2 mg/mL could totally inhibit fungal growth as well as AFB1 production. Additionally, the EOs showed notable antioxidant activity and were non phytotoxic to wheat seeds.


5. In vivoassays of essential oils

Although in vitroassays of EOs is an important first step in determination of the strong activity of plants, in vivoconfirmation of activity is important because food models may interact with the bioactive compounds, decreasing their efficacy. Generally, to obtain the same effect in food items as those found in vitroexperiences, higher concentrations of EOs must be applied. Thyme, summer savory and clove EOs was tested in tomato paste and all inhibited the mycelia growth of A. flavus. The thyme and summer savory EOs, exhibited the strongest inhibition at concentrations of 350 and 500 ppm, respectively. Taste panel evaluations were carried out in a tomato ketchup base, and the percent of inhibition of each EO in tomato paste was lower than in culture medium. Panelists accepted the results of taste panel with concentration of 500 ppm of thyme EO [69]. Under storage conditions, lemon fruits were completely prevented of A. flavusby S. hortensisat concentrations of 25, 12.5 and 6.25 μL/mL [40].

The effect of hemlock (Cicuta virosaL. var. latisectaCelak) EO on inhibition of decay development in cherry tomatoes was assessed by exposing them to EO vapor at 200 μL/mL. Results showed that the C. virosavar. latisecta EO has potential to control food spoilage [51]. Mentha viridisEO can reduce A. flavusand aflatoxin production in stored corn. The authors showed that this of 300 μL of the EO in 100 g of corn is enough to control the fungal growth and the aflatoxin synthesis [70].

EOs of Origanum majoranaL., Coriandrum sativumL., Hedychium spicatumHam. ex Smith, Commiphora myrrha(Nees) Engl., and Cananga odorataHook.f. and Thomson, were tested in vivoat different concentration against A. flavusin chickpea seed. During the investigations in food system all EOs exhibited above 50% protection of chickpea seed from A. flavuscontamination [71]. The holy basil O. sanctumEO reduced the number of A. flavusup to 62.94, 67.87 and 74.01% when fumigated at concentrations of 0.3, 0.5 and 1.0 μL/mL, respectively, on Rauvolfia serpentinamedicinal plant during storage [44]. Boswellia carteriiBirdw EO showed protection of the fumigated black pepper fruits up to 65.38% from A. flavuscontamination after 6 months of storage [60]. The efficacy of the combined application of chitosan (CH) and Locust Bean Gum (LBG) in combination with bergamot and bitter orange EOs was evaluated to inhibit A. flavuson artificially infected dates. In fruit decay assays coatings based on CH incorporating Citrus,EOs were capable to reduce fungal decay between 52 and 62%. Furthermore, the complete absence of off-flavors and off-odors demonstrated the potential of CH coatings carrying bergamot and bitter orange EOs at sub-inhibitory concentrations to control postharvest growth of A. flavusin dates [72].


6. Limitations of the use of EOs in food systems

In spite of the great potential of EOs against fungal growth and mycotoxin production, their large scale utilization is limited because of volatile nature, organoleptic effect in food systems and susceptibility to oxidation under light, heat, oxygen and moisture. To develop stability, control the release and enhance the efficacy of EOs in food systems, it is necessary for the current research to develop some structural barriers to enclose these bioactive compounds. In this regards, encapsulation of EOs by different physical, physico-chemical and mechanical methods with the assistance of carrier matrices is a trending area of research.

Thus, although the use of EOs can be an interesting strategy, it faces several constraints:

Phytotoxicity:The alteration of the integrity of the cell membrane following exposure to EO (responsible for their anti-fungal effect) could also affect plants and induce phytotoxicity at slightly higher than those used to control fungi [19]. It should also be noted that the most effective EOs are generally the most phytotoxic [21].

Toxicity to mammals:exposure to EOs or their components may be toxic to mammals. For instance, EO with a high content of furanocoumarins may cause dermal irritation and burns during exposure to light due to photosensitization. The linalool, present in the EO of thyme and lavender is also toxic to human dermal cells [73].

Rapid volatilization:Compounds of EO are highly volatile and may also be oxidatively degraded following exposure to light or temperature rise. This loss of activity would therefore require their reintroduction continuously to maintain the protective effect [35].

Alteration of organoleptic qualities: EOs consists of substances aromatic and are often used in cosmetics industry for their pleasant scent. Their application to foods could change their organoleptic qualities altering the taste [54]. To mitigate this effect, strategies such as encapsulation of EOs have been designed to strengthen the prospective use of EOs in the food industry.

The present review has focused on the antifungal and antiaflatoxigenic activity of essential oils. Additionally, other plant extracts possess potential antifungal activities against A. flavusand AFB1 production, but they are generally similar to those observed with the EOs. However, it would seem interesting to further explore the potential of these extracts and their bioactive compounds as they may have several advantages over EOs, such as less sensorial impact on the food.


7. Conclusion

In view of the potential of EOs as inhibitory of A. flavusgrowth and AFB1 production and their efficacy in food system in controlling fungal contamination, the EOs may be recommended for the formulation of plant based preservatives for enhancement of shelf life and safety of foodstuffs during post-harvest processing because consumers are looking for food with natural characteristics.



Thanks to the Government of Aragón and FEDER 2014-2020 (Grant Grupo de Investigación A06_17R) and the Ministry of Higher Education and Scientific Research of Algeria (Project number: PRFU/D00L01UN150120180002) for financial support.


Conflict of interest

The authors declare that there are no conflicts of interest.


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Written By

Yamina Ben Miri, Azem Belasli, Djamel Djenane and Agustín Ariño

Submitted: April 21st, 2019Reviewed: June 26th, 2019Published: July 31st, 2019