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Review

Mycotoxin Contamination in Hazelnut: Current Status, Analytical Strategies, and Future Prospects

by
Maria Michela Salvatore
1,2,
Anna Andolfi
1,3,* and
Rosario Nicoletti
4,5
1
Department of Chemical Sciences, University of Naples Federico II, 80126 Naples, Italy
2
Institute for Sustainable Plant Protection, National Research Council, 80055 Portici, Italy
3
BAT Center—Interuniversity Center for Studies on Bioinspired Agro-Environmental Technology, University of Naples Federico II, 80055 Portici, Italy
4
Department of Agricultural Sciences, University of Naples Federico II, 80055 Portici, Italy
5
Council for Agricultural Research and Economics, Research Center for Olive, Fruit, and Citrus Crops, 81100 Caserta, Italy
*
Author to whom correspondence should be addressed.
Toxins 2023, 15(2), 99; https://doi.org/10.3390/toxins15020099
Submission received: 27 December 2022 / Revised: 17 January 2023 / Accepted: 18 January 2023 / Published: 19 January 2023
(This article belongs to the Special Issue Detection, Control and Contamination of Mycotoxins (Volume II))
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Abstract

:
Hazelnuts represent a potential source of mycotoxins that pose a public health issue due to their increasing consumption as food ingredients worldwide. Hazelnuts contamination by mycotoxins may derive from fungal infections occurring during fruit development, or in postharvest. The present review considers the available data on mycotoxins detected in hazelnuts, on fungal species reported as infecting hazelnut fruit, and general analytical approaches adopted for mycotoxin investigation. Prompted by the European safety regulation concerning hazelnuts, many analytical methods have focused on the determination of levels of aflatoxin B1 (AFB1) and total aflatoxins. An overview of the available data shows that a multiplicity of fungal species and further mycotoxins have been detected in hazelnuts, including anthraquinones, cyclodepsipeptides, ochratoxins, sterigmatocystins, trichothecenes, and more. Hence, the importance is highlighted in developing suitable methods for the concurrent detection of a broad spectrum of these mycotoxins. Moreover, control strategies to be employed before and after harvest in the aim of controlling the fungal contamination, and in reducing or inactivating mycotoxins in hazelnuts, are discussed.
Keywords:
fungal secondary metabolites; analytical techniques; detoxification; decontamination; Corylus avellanae
Key Contribution: Hazelnuts are one of the most commonly cultivated nuts worldwide, resulting in a large exposure of consumers to its potential contaminants. This review is focused on the available data concerning the occurrence, detection, and control strategies of mycotoxins in hazelnuts.

1. Introduction

Hazelnut is one of the most commonly cultivated nut crops worldwide, with Turkey (665,000 tons) and Italy (140,560 tons) representing the leading countries in the global production, with a market portion in constant growth [1]. In fact, hazelnut kernels are a key ingredient for bakery, confectionary, and chocolate products, due to their characteristic flavor and good nutritional properties [2]. The qualitative composition characterized by a special assortment of fats, proteins, carbohydrates, fiber, and vitamins qualifies the nutritional properties of hazelnuts, and accounts for their beneficial effects on health [3].
The abundance of nutrients in hazelnuts, such as lipids and carbohydrates, makes them susceptible to decay and to the development of pathogenic and saprophytic fungi that are of utmost concern for producing mycotoxins, which are known for their cytotoxic, mutagenic, neurotoxic, and carcinogenic effects in humans and animals [4]. Exposure to mycotoxins can happen by eating contaminated foods or from animals that are fed contaminated feed. These fungal secondary metabolites are produced in the field and/or during storage, when environmental conditions are favorable for fungal growth [5], and are very difficult to eliminate from the food chain, causing a loss of product, and economic damage [6].
In this context, mycotoxin control in hazelnuts is of greatest importance, and is a global challenge to safeguard consumers’ health. Nevertheless, to date, only aflatoxin B1 (AFB1) and total aflatoxins have been included in the European safety regulation concerning hazelnuts [7].
In this review, we compile the available data on mycotoxins detected in hazelnuts, and on fungal species reported as infecting hazelnut fruit. We intend to generate interest among researchers and stakeholders to investigate the multiplicity of mycotoxins, without focusing on a single or target group of mycotoxins (e.g., aflatoxins). Furthermore, we also discuss some aspects concerning control strategies to be employed before and after harvest, to reduce or to inactivate mycotoxins in hazelnuts.

2. Occurrence of Mycotoxins in Hazelnuts

Mycotoxins identified in hazelnuts have a great diversity in chemical structure belonging to different classes of natural products, including aflatoxins, amino acid derivatives, anthraquinones, benzodiazepines, cyclodepsipeptides, macrolides, ochratoxins, resorcylic acid lactones, sterigmatocystins, trichothecenes, and several miscellaneous compounds (Table 1). This structural heterogeneity reflects a huge variety of toxic effects, with an impact on health essentially depending on the consumed amount and their occurrence in varied assortments.
On a worldwide scale, aflatoxins represent the most important mycotoxins in food and animal feedstuffs, raising the greatest concern due to their frequent occurrence and severe effects on health [23,24]. Aflatoxin B1 (AFB1) is classified as a group 1 human carcinogen by the International Agency for Research on Cancer (IARC) [25]. The European Commission has laid down maximum levels for AFB1 and total aflatoxins (i.e., the sum of aflatoxins B1, B2, G1, and G2) in hazelnuts for direct human consumption and/or for use as an ingredient in foodstuffs, which are 5 µg/kg for AFB1 and 10 µg/kg for total aflatoxins [7]. From a chemical perspective, aflatoxins are highly substituted coumarins: AFB1 and AFB2 have a difuro-coumaro-cyclopentenone structure, while a five-membered lactone ring replaces the cyclopentenone in AFG1 and AFG2 (Figure 1).
Aspergillus spp. in the section Flavi are the most widespread aflatoxin producers [23]. The presence of these mycotoxins in hazelnuts has been investigated in many countries, such as Turkey [11,12,15,17,26], Italy [8], China [16], Iraq [10], Bosnia-Herzegovina [18], Germany [13], and Portugal [19]. Following the increasing global trade of food products, the European Commission has recently implemented border controls on aflatoxins in nuts, which have proven to be relevant for reducing the health risk for population [27]. As an example, a study by Imperato et al. [9] revealed a high rate of contamination for hazelnuts and foods containing hazelnuts, imported in Italy from Turkey. Demirhan et al. [28] investigated the mycotoxin contamination of nut-based products (e.g., hazelnut butter and chocolate), obtained from local markets in Ankara (Turkey), observing that most samples were contaminated by AFB1 and other mycotoxins.
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Figure 1. Chemical structures of aflatoxins (AFs) detected in hazelnuts.
Figure 1. Chemical structures of aflatoxins (AFs) detected in hazelnuts.
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Sterigmatocystin (STE) and its 3-O-methyl derivative (OMSTE) have been also identified in hazelnuts [12]. STE was isolated for the first time from cultures of Aspergillus versicolor, but subsequently, species from different fungal genera (e.g., Aschersonia, Botryotrichum, Fusarium) showed the ability to produce this secondary metabolite [29]. STEs consist of a xanthone nucleus bond to a bifuranic structure with a hydroxyl or a methoxy group (Figure 2). STE is biosynthesized through the acetate-malonate pathway, and can be converted to OMSTE, and then to aflatoxins. In fact, the oxidative cleavage of the aromatic ring with the loss of one carbon and recyclization generates both AFB1 and AFG2. As a biosynthetic precursors of aflatoxins, it is not unusual to find these mycotoxins in the same food samples [30,31]; this has also been documented in the case of hazelnut-based products [28]. Besides structural similarities, STE shares with AFB1 hepatotoxic and nephrotoxic effects, inducing IARC to classify them as a possible human carcinogen (group 2B) [32].
As can be inferred from the existing literature, ochratoxin A (OTA) seems to be greatly diffused in hazelnuts [10,12,22,33], and as a contaminant of hazelnut-based food [28]. Moreover, the presence in hazelnuts of the dechloro analog of OTA, namely ochratoxin B (OTB), has been also reported [12,16]. Ochratoxins are mostly known as secondary metabolites of several Aspergillus and Penicillium spp. [34]. Biosynthetically, these mycotoxins are pentaketides derived from the dihydrocoumarin family coupled to phenylalanine (Figure 3). OTA is regarded as the most toxic member of ochratoxins, having been shown to be nephrotoxic, hepatotoxic, teratogenic, and immunotoxic to several species of animals. It has also been proven to be carcinogenic in kidney and liver, and has been classified as a group 2B human carcinogen by the IARC and World Health Organization (WHO) [35].
Most of the published data on ochratoxins, other than OTA, describe OTB toxicity. In fact, OTB was investigated for its nephrotoxic, hepatotoxic and immunotoxic effects [34].
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Figure 3. Chemical structures of ochratoxins (OTs) detected in hazelnuts.
Figure 3. Chemical structures of ochratoxins (OTs) detected in hazelnuts.
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Commonly produced by Alternaria fungi, alternariol (AOH) and alternariol methyl ether (AME) were first identified in hazelnut samples by Varga et al. [12]. These mycotoxins belong to the group of resorcylic acid lactones which are characterized by the presence of a dibenzo-α-pyrone moiety (Figure 4). Even if no specific regulations in food and feed exist, AOH and AME are considered as emerging toxins because of the increasing evidence of their occurrence and toxicological properties [36]. To date, AOH has been reported to be cytotoxic, dermally toxic, and potentially carcinogenic. Moreover, various in vitro experiments and a few in vivo investigations were conducted to evaluate the genotoxicity of AOH [37].
The 14-membered macrolide zearalenone (ZEA), also known as F-2 toxin, and zearalenone-14-sulphate (ZEA14S), are mainly produced by fungi of the genus Fusarium [38]. ZEA has immunotoxic, hepatotoxic, and xenogenic effects, and its activity in living organisms depends on the immune status of the organism and on the reproductive system state, due to the strong estrogenic and anabolic effects which have been reported [39]. These mycotoxins share the chemical structure of a macrocyclic β-resorcylic acid lactone with curvularin (CVL), another mycotoxin isolated from contaminated hazelnuts [12] (Figure 5).
Apicidin (APC), alamethicin F30 (ALMF30), and tentoxin (TEN) are amino acid and peptide derivatives detected in hazelnuts [12,16]. APC and TEN are cyclic tetrapeptides, while ALMF30 is a 20-residue polypeptide belonging to the so-called peptaibiotics [40] (Figure 6).
The class of cyclodepsipeptides includes N-methylated cyclic hexadepsipeptides, consisting of three residues of hydroxy acids (i.e., 2-hydroxyisovaleric acids) alternating with three N-methyl-L-amino acids, generally valine, leucine, and isoleucine. Peptide bonds and intramolecular ester bonds link the subunits to form an 18-membered ring. During the last few years, three papers have reported on the occurrence of depsipeptides in hazelnuts [12,16,21], including seven enniatins (ENs) and beauvericin (BEA) (Table 1). The latter presents three 2-hydroxyisovaleryl residues alternated to three N-methyl-phenylalanyl groups [41] (Figure 7). Again, these products are mainly known from Fusaria [42].
Members of this class are considered as emerging mycotoxins because mixtures or individual compounds have been shown to possess substantial in vitro cytotoxicity against different cell lines [41,43].
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Figure 7. Chemical structures of cyclodepsipeptides detected in hazelnuts.
Figure 7. Chemical structures of cyclodepsipeptides detected in hazelnuts.
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Three anthraquinones were detected in Turkish hazelnut samples by Varga et al. [12], namely physcion (= parietin, PHY), macrosporin (MCP), and emodin (EMO) (Figure 8). Anthraquinones are a valuable class of natural and synthetic compounds with a broad pharmacological function, including anti-bacterial, antioxidant, anti-tumor, and other activities, which are produced by many fungal species [44,45]. A growing number of toxicological data highlight the potential toxicity of compounds belonging this class [46].
Several trichothecenes were identified from hazelnuts samples [12,19] and from hazelnut-based food [28]. Trichothecenes are a large family of sesquiterpenoids with the common core chemical structure consisting of a cyclohexene fused to a tetrahydropyran, which is bridged by a two-carbon chain forming a cyclopentyl moiety. A 12,13-epoxy ring completes this core (Figure 9). These fungal secondary metabolites are of major food safety concern because of the harmful effects that result from acute and chronic exposure [47,48]. They are produced by several fungi, including Fusarium, Trichothecium, Trichoderma, Myrothecium, and Stachybotrys, and they have an ample spectrum of toxicity for humans and animals [49].
Cyclopenin (CPN) is a benzodiazepine alkaloid deriving from the cyclization of the dipeptide of anthranilic acid and phenylalanine [50]. In the biosynthesis, CPN serves as precursor of cyclopenol (CPL), which explains the frequent co-occurrence of these toxic fungal metabolites. Both these benzodiazepine alkaloids were identified in commercial samples of hazelnuts by Spadaro et al. [20] (Figure 10).
Other mycotoxins detected in hazelnuts present heterogeneous structures (Figure 11). This is the case of patulin (PA), a polyketide lactone primarily produced by Penicillium, Aspergillus, and Byssochlamys spp., which is considered a serious health concern and an economic threat [51]. As the subject of a huge investigational activity, patulin content has also been determined in hazelnuts as function of fungal infections based on a relationship with aflatoxin and ergosterol concentrations in different categories of samples [11].
Mycophenolic acid (MPA) is a phenyl-terpenoid secondary metabolite produced by several species of Penicillium [52] showing antiviral, antibacterial, antitumoral, antifungal, and immunosuppressive activities [53]. It has been detected in hazelnuts in a couple of studies [12,20]; one of them [12] also reported the indole alkaloid roquefortine C, another mycotoxin essentially produced by the Penicillium species.
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Figure 11. Structures of compounds from the group “miscellaneous” detected in hazelnuts.
Figure 11. Structures of compounds from the group “miscellaneous” detected in hazelnuts.
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3. Analytical Methods for the Determination of Mycotoxins in Hazelnuts

A number of methods have been developed for the identification and accurate quantification of single or chemically related mycotoxins in food samples [54]. Table 2 summarizes the analytical strategies employed for the detection of mycotoxins in real hazelnut samples. Many analytical methods have focused on the qualitative and quantitative determination of AFB1 and total aflatoxins, also prompted by the fact that these are the only mycotoxins included in the European regulation for hazelnuts [8,55,56]. However, different classes of mycotoxins could be found to co-occur in hazelnuts, with possible synergistic effects [57]. This is quite understandable, considering that many fungal species, which are reported as producers of toxic secondary metabolites belonging to different classes of natural compounds, can be concurrently isolated from hazelnuts, as is examined in more detail in Section 4.
The possible co-occurrence of different mycotoxins highlights that more information is needed on other fungal contaminants in hazelnuts, and stresses the importance of developing multi-mycotoxin approaches instead of single analyte methods, to monitor a higher number of compounds.
The analysis of mycotoxins in hazelnuts is a challenging task, due to the complexity of the sample (i.e., high fat content) along with the low concentrations at which these contaminants are usually present. To cover the broad spectrum of mycotoxins, different analytical methods are often employed.
Firstly, sample preparation, determinations, and analytical performance criteria must be coherent in order to obtain comparable data. In fact, the use of validated analytical methods is essential to ensure that the results of surveys provide a reliable content assessment. Based on the guidelines in the EU Commission Decision [58], the analytic methods with similar validation parameters, such as the limit of detection (LOD), limit of quantification (LOQ), linearity (r2), range of matrix effects, recovery, and relative standard deviation, are used for estimating the mycotoxin contamination levels.
In general, conventional analytical methods, including TLC, LC-fluorescence, HPLC-UV, and ELISA are employed for the single or group target determination of mycotoxins, while LC-MS methods are preferred for multiclass analyses.
Some LC-MS/MS methods for the simultaneous determination of toxic fungal metabolites in hazelnuts have been optimized and validated [12,20,33,59,60,61]. These methods include a first step of sample treatment based on solid–liquid extraction with an organic solvent. Although LC-MS has multi-analyte capabilities, the choice of extraction solvents and sample preparation may not be suitable for certain mycotoxins due to the high chemical diversity (Table 1). It was demonstrated that for the extraction of multiple contaminants in different food and feed matrices, a mixture of acidified water with organic solvents, such as methanol, acetonitrile, and acetone, is the most suitable system [62]. In general, a second step involves a clean-up using combinations of MgSO4 and different sorbents such as florisil, carbon black, C18, or primary and secondary amines, to remove interfering substances. For example, the procedure employed by Škrbić et al. [33] is based on the simultaneous extraction of selected mycotoxins from hazelnuts and other nuts with a mixture of acetonitrile/water/acetic acid (79:20:1, v/v/v), and defatting the obtained extract with hexane in order to remove the lipids. However, it was proven that the common cleaning-up decreases the recovery of mycotoxins [63]; hence, alternative cleaning-up methods, such as dispersive liquid–liquid microextraction (DLLME), have been employed for the analysis of mycotoxins [63]. DLLME is a three phase system constituting the extraction solvent, the dispersive solvent, and the aqueous phase. A suitable mixture of an organic extraction solvent (usually with a density higher than water) and a disperser solvent (miscible with the extraction solvent and with water) is rapidly injected into the aqueous phase, resulting in the formation of a stable emulsion. Centrifugation allows for phase separation, and the organic phase containing the analytes is subsequently analyzed using the chosen techniques [63,64,65]. Arroyo-Manzanares et al. [60] developed a multiclass method based on DLLME for the determination of 14 mycotoxins in different nuts and seeds, including hazelnuts. Nevertheless, every clean-up step is cost/time consuming and limits the number of analytes, as some of the target substances might not be amenable to the chosen procedure. Varga et al. [12] developed an UHPLC-MS/MS method, including a single extraction step and direct injection of the diluted raw extract into the instrument without any sample clean-up. This method allowed for the determination of several mycotoxins in different nut samples, including hazelnuts (Table 2).
As can be deduced from the above discussion, the choice of an appropriate multi-target methods for the quantification and determination of mycotoxins is essential for researchers involved in the study of toxic fungal metabolites in hazelnuts.

4. Mycotoxins in Hazelnuts and Fungal Infections

Kernel contamination by mycotoxins may derive from fungal infections occurring during fruit development, or in postharvest. In the field, the symptoms of fruit rot are various, in that they may involve the whole fruit and be visible externally, or they may specifically affect the kernel and be hidden by the shell. A list of fungi known as disease agents of hazelnut fruits is provided in Table 3. However, most frequently, the observed damage cannot be referred to a specific agent; rather, it results from overlapping infections by multiple species. On the other hand, the infectious capacity by several species is variable in space and time, with reference to the point of entry and the phenological stage of fruit development. In this respect, the incidence of Diaporthe spp. was found to be higher at the full ripening stage than in early ripening, and higher in defective than in healthy kernels. A similar pattern also characterized Botryosphaeria; however, the incidence of Diaporthe was positively correlated with both hidden and visible defects, while Botryosphaeria was essentially found in nuts with hidden defects [66]. The simultaneous occurrence in this study of Diaporthe and Aspergillus emphasizes the need to assess the outcome of their interaction, in terms of both kernel damage and the effects on mycotoxin production and accumulation. Due to the major concern for the accumulation of aflatoxins, some investigations have been carried out with special reference to Aspergillus spp., essentially species in the section Flavi. Indeed, their incidence may be quite remarkable in some environmental contexts, and is reported to increase throughout the season until the harvesting time [67].
The above data refer to fungal infections occurring in the field. Indeed, the issue of the fungal infestation of hazelnuts during storage and commercialization is basically different in its assumptions, considering that any saprophytic microbe may be able to contaminate the nuts at this stage, and to unpredictably contribute to mycotoxin accumulation.
A multitude of studies/investigations have been carried out concerning the fungal contamination of hazelnuts from commerce, particularly in Western Asian countries. In an investigation carried out in Saudi Arabia, 12 genera and 23 species were isolated, including a varied assortment of Aspergillus and Penicillium spp., which by far represents the most frequent contaminants at the marketing stage [87]. Isolates of Aspergillus (including A. flavus), Penicillium, Rhizopus, Fusarium, Geotrichum, Syncephalastrum, and Cladosporium were recovered in a Turkish survey [88]. Three studies carried out in Iran disclosed a broad set of fungal contaminants, consisting of Alternaria, Aspergillus, Cladosporium, Drechslera, Fusarium, Mucor, Paecilomyces, Penicillium, Rhizopus, Scopulariopsis, and Trichothecium [89,90,91]. Aspergillus flavus, Aspergillus niger, Penicillium italicum, and other Penicillium and Cladosporium spp. resulted in an investigation carried out in Iraq [10]. In another study carried out in Egypt, a total of 37 species were identified, including Alternaria atra (=Ulocladium atrum), A. alternata, Chaetomium globosum, Cladosporium herbarum, Cladosporium cladosporioides, Cladosporium macrocarpum, Curvularia lunata (=Cochliobolus lunatus), Mucor circinelloides, Mucor hiemalis, Rhizomucor pusillus, Sarocladium (=Acremonium) strictum, Scopulariopsis brevicaulis, Talaromyces funiculosus, Talaromyces variabile, Trichocladium griseum (=Humicola grisea), and Trichothecium roseum, six species of Penicillium and 15 species of Aspergillus [14]. An investigation carried out in Lithuania reported the occurrence of A. niger, Aspergillus fumigatus, A. versicolor, Fusarium chlamydosporum (=F. sporotrichioides), Rhizopus stolonifer, Penicillium chrysogenum, and other Penicillium spp. [92].
A couple of studies reported on fungi occurring in roasted hazelnuts, indicating that contamination with these fungi may be independent of the conditions of the product at harvest, and that rather, it can start during processing and marketing. Particularly, the species T. roseum, Aspergillus glaucus, A. flavus, and A. niger, as well as other Aspergillus, Penicillium, Fusarium, Alternaria, Mucor, and Rhizopus spp. were recovered in a Spanish study [93], while Aspergillus spp., mostly belonging to the sections Flavi and Nigri, were found to be quite abundant in an investigation carried out in Algeria, representing as much as 66% of the total fungal contaminants; however, just about half of the members of the section Flavi were found to be aflatoxigenic, essentially producing AFB1 [94]. Finally, as has occurred for mycotoxin analysis [95], other studies have been published that present collective data concerning other kind of nuts too, hence not allowing for an inference of specific associations with hazelnuts [15,96].
Most frequently, Aspergillus spp. are prevalent in these studies. However, the mycotoxin pattern remarkably varies among the species in this genus, calling for more circumstantial studies to further analyze the real taxonomic assortments involved in hazelnut contamination. In a recent study carried out in Iran, Aspergillus isolates from hazelnuts were identified to belong to 13 species grouped in 5 sections and 9 series based on sequencing of calmodulin and β-tubulin genes. Particularly, these are species from the section Flavi, including A. caelatus (series Kitamyces), A. nomius (series Nomiarum), A. flavus, A. parasiticus, and A. arachidicola (series Flavi); from the section Nidulantes, including A. quadrilineatus (series Nidulantes), A. unguis (series Unguium), and A. spelunceus (series Speluncei); from the section Circumdati, including A. ochraceus and A. westerdijkiae (series Circumdati); A. pseudoglaucus from the section Aspergillus (series Rubri); and A. taichungensis from section Candidi (series Candidi) [97,98]. Some of these species might be agents of contamination with additional mycotoxins, such as A. pseudoglaucus, which is known to produce echinulins [99]. In the above-mentioned Egyptian study, as many as 15 species were identified based on morphology, including A. flavus, A. niger, A. ochraceus (=A. alutaceus), A. candidus, A. fumigatus, A. parasiticus, A. sydowii, A. tamari, A. terreus, A. versicolor, A. nidulans, A. amstelodami, A. chevalieri, A. rubrum, and A. rugulosus [14]. Moreover, this study also reported on the occurrence of a varied assortment of Penicillium spp., including P. chrysogenum, P. citrinum, P. corylophilum, P. cyclopium, P. janthinellum, and P. oxalicum, which represents the second most frequent genus.
Although limited and somehow approximate, the available data are indicative that these fungi are reported as possible producers of about one half of the compounds listed in Table 1, namely aflatoxins, anthraquinones, cyclopenins, curvularin, ochratoxins, sterigmatocystins, chaetoglobosins, kojic acid, mycophenolic acid, patulin, and viridicatin [100,101]. However, their biosynthetic capacities go well beyond this limited number, and it should be taken into consideration that any mycotoxin that is known as a product of the species of these genera can potentially contaminate the kernels and the derivatives used in the food industry.
As for the other genera, an outstanding position pertains to Diaporthe (= Phomopsis), considering the high number of species reported in association with hazelnuts, and the remarkable biosynthetic capacities that exteriorize in a long series of secondary metabolites that are so far reported from these fungi [102,103]. With reference to the mycotoxins listed in Table 1, production is to be mentioned of 3-nitropropionic acid by a pathogenic strain of D. gulyae on sunflower [104], alternariol and alternariol methyl ether by an endophytic strain of an unidentified species [105], and emodin by an endophytic strain of D. lithocarpi [106]. Moreover, the sterigmatocystin analogues secosterigmatocystin and dihydrosterigmatocystin have been extracted from an endophytic strain of D. amygdali [107]. However, more products of these fungi have been reported for their toxic effects, which should be considered as possible contaminants of hazelnuts; this is the case for phomoxanthone, pinselin, and other xanthones, as well as several benzofuranones, quinones, and alkaloids [103].

5. Control Strategies

Several pre- and post-harvest operations of hazelnuts and other food products can help with controlling the fungal contamination, and also significantly reduce the quantity of mycotoxins in them [108,109]. Chemical control is a successful strategy in crop protection for reducing mycotoxigenic fungi in the field, but it is associated with undesirable effects. The application of appropriate storage conditions (e.g., the use of hermetic containers, temperature and humidity control, and ventilation) is an essential post-harvest strategy to avoid fungal growth and mycotoxins accumulation [110,111]. Moreover, the additional processing of these commodities may be associated with secure and safe consumption.
Several decontamination strategies, including physical (e.g., cleaning, thermal inactivation, irradiation with UV or gamma rays, and cooling), chemical (e.g., treatments with hydrogen peroxide, acids or bases, or enzymes) or biological (e.g., atoxigenic microbes) tools, have been tested against fungi and their mycotoxins. However, these methods may cause undesirable effects on the sensory, nutritional and functional properties of foods [6].
A promising non-thermal alternative for reducing the fungal load is cold atmospheric plasma, which enables a microbial multi-target inactivation on food surfaces, covering an ample range of microorganisms, including bacteria and fungi [112,113]. Plasma is considered as the fourth state of matter obtained by energetic species formed from the collisions of energetic electrons with heavy particles (e.g., atoms, molecules, and ions). Cold plasma generated under atmospheric pressure produces antimicrobial effects at temperature below 40 °C. Dasan et al. focused on the effect of process parameters on the inactivation efficiency of cold atmospheric plasma on aflatoxigenic Aspergillus spp. spores in hazelnuts [114,115]. To achieve this goal, hazelnuts were artificially contaminated with A. flavus and A. parasiticus, then treated with dry air or cold plasma. On an experimental scale, these studies showed that cold atmospheric plasma is an efficient post-harvest sanitation system, affording a reasonable reduction in contamination by Aspergillus spp.
Cold atmospheric plasma has the potential for aflatoxin detoxification in food, also because it preserves the organoleptic properties. Siciliano et al. [116] used cold atmospheric plasma to detoxify hazelnuts from aflatoxins, investigating the effect of different gases (N2, 0.1% O2 and 1% O2, or 21% O2), power (400, 700, 1000, or 1150 W) and exposure time (1, 2, 4, or 12 min) to optimize the method. A reduction in the concentration of total aflatoxins and AFB1 in hazelnuts of over 70% was obtained. This result was also confirmed by Sen et al. [117], who observed that cold atmospheric pressure and low-pressure plasmas are more effective than gamma irradiation for the reduction in AFB1 and total aflatoxins in hazelnuts. Furthermore, sensory evaluation tests showed that hazelnuts maintain optimal attributes after these treatments.
Even if the mechanism of degradation or resistance of mycotoxins is not fully understood, it is thought that a primary role is played by the mycotoxin structure [113]. In fact, it has been observed that the sensitivities of AFB1 and AFG1 to cold atmospheric plasma are higher than AFB2 and AFG2. The reason was attributed to the possible destruction of the C8–C9 double bond (olefinic site) on the furan ring, which is responsible for the toxicities of AFB1 and AFG1; whereas this double bond is not present in AFB2 and AFG2 [116]. These treatments cause the opening of the terminal furan ring in the double bond, leading to the formation of organic acids, aldehydes, ketones, and other degradation products [118].

6. Conclusions

In the present review paper, the available data concerning the literature on mycotoxins detected in hazelnuts were examined. A high variety of mycotoxins with different chemical properties and toxicities have been detected in the hazelnut samples. These toxic fungal metabolites can be classified at least in 10 groups (i.e., aflatoxins, amino acid and peptide derivatives, anthraquinones, benzodiazepine alkaloids, cyclodepsipeptides, macrolides, ochratoxins, resorcylic acid lactones, sterigmatocystins, and trichothecenes).
Mycotoxins and fungal producers represent a great public health issue. Hence, further investigations should also be carried out to increase the available data concerning conditions that are conducive to the development of mycotoxigenic fungi in the field, particularly with reference to the possible effects deriving from interactions with other components of the hazelnut microbiome [119,120].
Evidence from investigations carried out by several laboratories and research groups worldwide supports concern for the contamination of hazelnuts by mycotoxins. Indeed, the increasing number of fungal secondary metabolites identified in kernels and that are known to possibly induce a range of toxic effects on human health, calls for a revision of the analytical procedures that are currently limited to aflatoxins, at least in the European Union.

Author Contributions

Conceptualization, R.N. and A.A.; writing—original draft preparation, M.M.S.; writing—review and editing, M.M.S., R.N. and A.A. All authors have read and agreed to the published version of the manuscript.

Funding

This study was carried out within the Agritech National Research Center, and received funding from the European Union Next-Generation EU (PIANO NAZIONALE DI RIPRESA E RESILIENZA (PNRR)—MISSIONE 4 COMPONENTE 2, INVESTIMENTO 1.4—D.D. 1032 17/06/2022, CN00000022). This manuscript reflects only the authors’ views and opinions; neither the European Union nor the European Commission can be considered responsible for them.

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

Not applicable.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Król, K.; Gantner, M. Morphological traits and chemical composition of hazelnut from different geographical. Agriculture 2020, 10, 375. [Google Scholar] [CrossRef]
  2. Squara, S.; Stilo, F.; Cialiè Rosso, M.; Liberto, E.; Spigolon, N.; Genova, G.; Castello, G.; Bicchi, C.; Cordero, C. Corylus avellana L. aroma blueprint: Potent odorants signatures in the volatilome of high quality hazelnuts. Front. Plant Sci. 2022, 13, 840028. [Google Scholar] [CrossRef] [PubMed]
  3. Alasalvar, C.; Fereidoon, S. Compositional characteristics and health effects of hazelnut (Corylus avellana L.): An overview. In Tree Nuts; CRC Press: Boca Raton, FL, USA, 2020; Volume 5, pp. 248–253. ISBN 9781119130536. [Google Scholar]
  4. Ukwuru, M.U.; Ohaegbu, C.G.; Muritala, A. A critical overview of mycotoxin contamination of foods and feeds. Curr. Res. Agric. Food Sci. 2021, 4, 77–98. [Google Scholar]
  5. Molyneux, R.J.; Mahoney, N.; Kim, J.H.; Campbell, B.C. Mycotoxins in edible tree nuts. Int. J. Food Microbiol. 2007, 119, 72–78. [Google Scholar] [CrossRef]
  6. Colović, R.; Puvača, N.; Cheli, F.; Avantaggiato, G.; Greco, D.; Ðuragić, O.; Kos, J.; Pinotti, L. Decontamination of mycotoxin-contaminated feedstuffs and compound feed. Toxins 2019, 11, 617. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  7. European Union. Commission Regulation (EC) No 165/2010 of 26 February 2010, amending Regulation (EC) No 1881/2006 setting maximum levels for certain contaminants in foodstuffs as regards aflatoxins. Off. J. Eur. Union. 2010, 50, 8–12. [Google Scholar]
  8. Bacaloni, A.; Cavaliere, C.; Cucci, F.; Foglia, P.; Samperi, R.; Laganà, A. Determination of aflatoxins in hazelnuts by various sample preparation methods and liquid chromatography-tandem mass spectrometry. J. Chromatogr. A 2008, 1179, 182–189. [Google Scholar] [CrossRef]
  9. Imperato, R.; Campone, L.; Piccinelli, A.L.; Veneziano, A.; Rastrelli, L. Survey of aflatoxins and ochratoxin a contamination in food products imported in Italy. Food Control 2011, 22, 1905–1910. [Google Scholar] [CrossRef]
  10. Abdulla, N.Q.F. Evaluation of fungal flora and mycotoxin in some important nut products in erbil local markets. Res. J. Environ. Earth Sci. 2013, 5, 330–336. [Google Scholar] [CrossRef]
  11. Ekinci, R.; Otaǧ, M.; Kadakal, Ç. Patulin & ergosterol: New quality parameters together with aflatoxins in hazelnuts. Food Chem. 2014, 150, 17–21. [Google Scholar]
  12. Varga, E.; Glauner, T.; Berthiller, F.; Krska, R.; Schuhmacher, R.; Sulyok, M. Development and validation of a (semi-)quantitative UHPLC-MS/MS method for the determination of 191 mycotoxins and other fungal metabolites in almonds, hazelnuts, peanuts and pistachios. Anal. Bioanal. Chem. 2013, 405, 5087–5104. [Google Scholar] [CrossRef] [Green Version]
  13. Reinhold, L.; Reinhardt, K. Mycotoxins in foods in Lower Saxony (Germany): Results of official control analyses performed in 2009. Mycotoxin Res. 2011, 27, 137–143. [Google Scholar] [CrossRef]
  14. Abdel-Hafez, A.I.I.; Saber, S.M. Mycoflora and mycotoxin of hazelnut (Corylus avellana L.) and walnut (Juglans regia L.) seeds in Egypt. Zentralbl. Mikrobiol. 1993, 148, 137–147. [Google Scholar] [CrossRef]
  15. Gürses, M. Mycoflora and aflatoxin content of hazelnuts, walnuts, peanuts, almonds and roasted chickpeas (LEBLEBI) sold in Turkey. Int. J. Food Prop. 2007, 9, 395–399. [Google Scholar] [CrossRef]
  16. Wang, Y.; Nie, J.; Yan, Z.; Li, Z.; Cheng, Y.; Chang, W. Occurrence and co-occurrence of mycotoxins in nuts and dried fruits from China. Food Control 2018, 88, 181–189. [Google Scholar] [CrossRef]
  17. Keskin, Z.S.; Gürsoy, N. Investigation of natural mycoflora and aflatoxin formation in hazelnuts and products. Cumhur. Sci. J. 2019, 40, 967–977. [Google Scholar]
  18. Zvizdic, S.; Hamzic, S.; Rodinis-Pejic, I.; Avdic-Kamberovic, F.; Bektas, S.; Sacic, E. Detection of mycotoxins in selected foods sample. Mater. Sociomed. 1988, 21, 47–76. [Google Scholar]
  19. Cunha, S.C.; Sá, S.V.M.; Fernandes, J.O. Multiple mycotoxin analysis in nut products: Occurrence and risk characterization. Food Chem. Toxicol. 2018, 114, 260–269. [Google Scholar] [CrossRef]
  20. Spadaro, D.; Meloni, G.R.; Siciliano, I.; Prencipe, S.; Gullino, M.L. HPLC-MS/MS method for the detection of selected toxic metabolites produced by Penicillium spp. in nuts. Toxins 2020, 12, 307. [Google Scholar] [CrossRef]
  21. Tolosa, J.; Font, G.; Mañes, J.; Ferrer, E. Nuts and dried fruits: Natural occurrence of emerging Fusarium mycotoxins. Food Control 2013, 33, 215–220. [Google Scholar] [CrossRef]
  22. Salem, N.M.; Ahmad, R. Mycotoxins in food from Jordan: Preliminary survey. Food Control 2010, 21, 1099–1103. [Google Scholar] [CrossRef]
  23. Nazhand, A.; Durazzo, A.; Lucarini, M.; Souto, E.B.; Santini, A. Characteristics, occurrence, detection and detoxification of aflatoxins in foods and feeds. Foods 2020, 9, 644. [Google Scholar] [CrossRef] [PubMed]
  24. Ismail, A.; Naeem, I.; Gong, Y.Y.; Routledge, M.N.; Akhtar, S.; Riaz, M.; Ramalho, L.N.Z.; de Oliveira, C.A.F.; Ismail, Z. Early life exposure to dietary aflatoxins, health impact and control perspectives: A review. Trends Food Sci. Technol. 2021, 112, 212–224. [Google Scholar] [CrossRef]
  25. IARC; IARC Working Group on the Evaluation of Carcinogenic Risks to Humans; International Agency for Research on Cancer; WHO. Some traditional herbal medicines, some mycotoxins, naphthalene and styrene. In Some Traditional Herbal Medicines, Some Mycotoxins, Naphthalene and Styrene; IARC: Lyon, France, 2002. [Google Scholar]
  26. Heperkan, D. The importance of mycotoxins and a brief history of mycotoxin studies in Turkey. ARI Bull. Istanbul Tech. Univ. 2015, 54, 18–27. [Google Scholar]
  27. Van de Perre, E.; Jacxsens, L.; Lachat, C.; El Tahan, F.; De Meulenaer, B. Impact of maximum levels in European legislation on exposure of mycotoxins in dried products: Case of aflatoxin B1 and ochratoxin A in nuts and dried fruits. Food Chem. Toxicol. 2015, 75, 112–117. [Google Scholar] [CrossRef]
  28. Demirhan, B.E.; Demirhan, B. Investigation of twelve significant mycotoxin contamination in nut-based products by the LC—MS/MS method. Metabolites 2022, 12, 120. [Google Scholar] [CrossRef]
  29. Díaz Nieto, C.H.; Granero, A.M.; Zon, M.A.; Fernández, H. Sterigmatocystin: A mycotoxin to be seriously considered. Food Chem. Toxicol. 2018, 118, 460–470. [Google Scholar] [CrossRef]
  30. Zhao, Y.; Wang, Q.; Huang, J.; Ma, L.; Chen, Z.; Wang, F. Aflatoxin B1 and sterigmatocystin in wheat and wheat products from supermarkets in China. Food Addit. Contam. Part B Surveill. 2018, 11, 9–14. [Google Scholar] [CrossRef]
  31. Zheng, R.; Xu, H.; Wang, W.; Zhan, R.; Chen, W. Simultaneous determination of aflatoxin B1, B2, G1, G2, ochratoxin A, and sterigmatocystin in traditional Chinese medicines by LC-MS-MS. Anal. Bioanal. Chem. 2014, 406, 3031–3039. [Google Scholar] [CrossRef]
  32. Zingales, V.; Fernández-Franzón, M.; Ruiz, M.J. Sterigmatocystin: Occurrence, toxicity and molecular mechanisms of action—A review. Food Chem. Toxicol. 2020, 146, 111802. [Google Scholar] [CrossRef]
  33. Škrbić, B.; Živančev, J.; Godula, M. Multimycotoxin analysis of crude extracts of nuts with ultra-high performance liquid chromatography/tandem mass spectrometry. J. Food Compos. Anal. 2014, 34, 171–177. [Google Scholar] [CrossRef]
  34. Heussner, A.H.; Bingle, L.E.H. Comparative ochratoxin toxicity: A review of the available data. Toxins 2015, 7, 4253–4282. [Google Scholar] [CrossRef] [Green Version]
  35. Tao, Y.; Xie, S.; Xu, F.; Liu, A.; Wang, Y.; Chen, D.; Pan, Y.; Huang, L.; Peng, D.; Wang, X.; et al. Ochratoxin A: Toxicity, oxidative stress and metabolism. Food Chem. Toxicol. 2018, 112, 320–331. [Google Scholar] [CrossRef]
  36. Solhaug, A.; Eriksen, G.S.; Holme, J.A. Mechanisms of action and toxicity of the mycotoxin alternariol: A review. Basic Clin. Pharmacol. Toxicol. 2016, 119, 533–539. [Google Scholar] [CrossRef]
  37. Miao, Y.; Wang, D.; Chen, Y.; Zhu, X.; Tang, X.; Zhang, J.; Zhang, L.; Chen, J. General toxicity and genotoxicity of alternariol: A novel 28-day multi-endpoint assessment in male Sprague–Dawley rats. Mycotoxin Res. 2022, 38, 231–241. [Google Scholar] [CrossRef]
  38. Rai, A.; Das, M.; Tripathi, A. Occurrence and toxicity of a fusarium mycotoxin, zearalenone. Crit. Rev. Food Sci. Nutr. 2020, 60, 2710–2729. [Google Scholar] [CrossRef]
  39. Ropejko, K.; Twaru, M. Zearalenone and its metabolites—General overview, occurrence, and toxicity. Toxins 2021, 13, 35. [Google Scholar] [CrossRef]
  40. Degenkolb, T.; Kirschbaum, J.; Brückner, H. New sequences, constituents, and producers of peptaibiotics: An updated review. Chem. Biodivers. 2007, 4, 1052–1067. [Google Scholar] [CrossRef]
  41. Caloni, F.; Fossati, P.; Anadón, A.; Bertero, A. Beauvericin: The beauty and the beast. Environ. Toxicol. Pharmacol. 2020, 75, 103349. [Google Scholar] [CrossRef]
  42. Liuzzi, V.C.; Mirabelli, V.; Cimmarusti, M.T.; Haidukowski, M.; Leslie, J.F.; Logrieco, A.F.; Caliandro, R.; Fanelli, F.; Mulè, G. Enniatin and beauvericin biosynthesis in Fusarium species: Production profiles and structural determinant prediction. Toxins 2017, 9, 45. [Google Scholar] [CrossRef] [Green Version]
  43. Ivanova, L.; Skjerve, E.; Eriksen, G.S.; Uhlig, S. Cytotoxicity of enniatins A, A1, B, B1, B2 and B3 from Fusarium avenaceum. Toxicon 2006, 47, 868–876. [Google Scholar] [CrossRef] [PubMed]
  44. Gessler, N.N.; Egorova, A.S.; Belozerskaya, T.A. Fungal anthraquinones. Appl. Biochem. Microbiol. 2013, 49, 85–99. [Google Scholar] [CrossRef]
  45. Mendili, M.; Khadhri, A.; Mediouni-Ben Jemâa, J.; Andolfi, A.; Tufano, I.; Aschi-Smiti, S.; DellaGreca, M. Anti-inflammatory potential of compounds isolated from tunisian lichens species. Chem. Biodivers. 2022, 19, e202200134. [Google Scholar] [CrossRef] [PubMed]
  46. Li, X.; Chu, S.; Yang, S.; Peng, Y.; Ren, S.; Wen, B.; Chen, N. Physcion and physcion 8-O-β-glucopyranoside: A review of their pharmacology, toxicities and pharmacokinetics. Chem. Biol. Interact. 2019, 310, 108722. [Google Scholar] [CrossRef]
  47. Arunachalam, C.; Doohan, F.M. Trichothecene toxicity in eukaryotes: Cellular and molecular mechanisms in plants and animals. Toxicol. Lett. 2013, 217, 149–158. [Google Scholar] [CrossRef]
  48. Gutiérrez, S.; McCormick, S.P.; Cardoza, R.E.; Lindo, L.; Alexander, N.J.; Proctor, R.H. Trichoderma trichothecenes: Beyond their toxic effect. In New and Future Developments in Microbial Biotechnology and Bioengineering; Elsevier: Amsterdam, The Netherlands, 2020; pp. 281–301. ISBN 978-0-12-819453-9. [Google Scholar]
  49. Sliwi, M.P. Trichothecenes in food and feed, relevance to human and animal health and methods of detection: A systematic review. Molecules 2021, 26, 454. [Google Scholar]
  50. Nover, L.; Luckner, M. On the biosynthesis of cyclopenin and cyclopenol, benzodiazepine alkaloids from Penicillium cyclopium westling. Eur. J. Biochem. 1969, 10, 268–273. [Google Scholar] [CrossRef]
  51. Mahato, D.K.; Kamle, M.; Sharma, B.; Pandhi, S.; Devi, S.; Dhawan, K.; Selvakumar, R.; Mishra, D.; Kumar, A.; Arora, S.; et al. Patulin in food: A mycotoxin concern for human health and its management strategies. Toxicon 2021, 198, 12–23. [Google Scholar] [CrossRef]
  52. Frisvad, J.C.; Smedsgaard, J.; Larsen, T.O.; Samson, R.A. Mycotoxins, drugs and other extrolites produced by species in Penicillium subgenus Penicillium. Stud. Mycol. 2004, 2004, 201–241. [Google Scholar]
  53. Bentley, R. Mycophenolic acid: A one hundred year odyssey from antibiotic to immunosuppressant. Chem. Rev. 2000, 100, 3801–3825. [Google Scholar] [CrossRef]
  54. Krska, R.; Schubert-Ullrich, P.; Molinelli, A.; Sulyok, M.; MacDonald, S.; Crews, C. Mycotoxin analysis: An update. Food Addit. Contam.—Part A Chem. Anal. Control. Expo. Risk Assess. 2008, 25, 152–163. [Google Scholar] [CrossRef]
  55. Şengül, Ü. Comparing determination methods of detection and quantification limits for aflatoxin analysis in hazelnut. J. Food Drug Anal. 2016, 24, 56–62. [Google Scholar] [CrossRef] [Green Version]
  56. Jeurissen, S.M.F.; Seyhan, F.; Kandhai, M.C.; Dekkers, S.; Booij, C.J.H.; Bos, P.M.J.; Van Der Fels-Klerx, H.J. An indicator based “traffic light” model to pro-actively assess the occurrence of mycotoxins in tree nuts. World Mycotoxin J. 2011, 4, 405–412. [Google Scholar] [CrossRef]
  57. Mahdjoubi, C.K.; Arroyo-manzanares, N.; Hamini-kadar, N. Multi-mycotoxin occurrence and exposure assessment approach in foodstuffs from Algeria. Toxins 2020, 12, 194. [Google Scholar] [CrossRef] [Green Version]
  58. EU European Union. Commission Regulation (EU), No.1058/2012 of 12 November 2012 amending Regulation (EC) No. 1881/2006 as regards maximum levels for aflatoxins in dried figs. Off. J. Eur. Union 2012, 313, 14–15. [Google Scholar]
  59. Malachová, A.; Sulyok, M.; Beltrán, E.; Berthiller, F.; Krska, R. Optimization and validation of a quantitative liquid chromatography-tandem mass spectrometric method covering 295 bacterial and fungal metabolites including all regulated mycotoxins in four model food matrices. J. Chromatogr. A 2014, 1362, 145–156. [Google Scholar] [CrossRef] [Green Version]
  60. Arroyo-Manzanares, N.; Huertas-Pérez, J.F.; Gámiz-Gracia, L.; García-Campaña, A.M. A new approach in sample treatment combined with UHPLC-MS/MS for the determination of multiclass mycotoxins in edible nuts and seeds. Talanta 2013, 115, 61–67. [Google Scholar] [CrossRef]
  61. Dreolin, N.; Stead, S.; Hird, S.; Jenkins, T. Determination of regulated and emerging mycotoxins in cereals, nuts, figs, and animal feeds using Pass-Through SPE and UPLC- MS/MS. Waters Corporation Application Note (720007377EN). Available online: https://www.waters.com (accessed on 12 December 2022).
  62. Lacina, O.; Zachariasova, M.; Urbanova, J.; Vaclavikova, M.; Cajka, T.; Hajslova, J. Critical assessment of extraction methods for the simultaneous determination of pesticide residues and mycotoxins in fruits, cereals, spices and oil seeds employing ultra-high performance liquid chromatography-tandem mass spectrometry. J. Chromatogr. A 2012, 1262, 8–18. [Google Scholar] [CrossRef]
  63. Arroyo-Manzanares, N.; García-Campaña, A.M.; Gámiz-Gracia, L. Multiclass mycotoxin analysis in Silybum marianum by ultra high performance liquid chromatography-tandem mass spectrometry using a procedure based on QuEChERS and dispersive liquid-liquid microextraction. J. Chromatogr. A 2013, 1282, 11–19. [Google Scholar] [CrossRef]
  64. Campone, L.; Piccinelli, A.L.; Celano, R.; Rastrelli, L. Application of dispersive liquid-liquid microextraction for the determination of aflatoxins B 1, B 2, G 1 and G 2 in cereal products. J. Chromatogr. A 2011, 1218, 7648–7654. [Google Scholar] [CrossRef]
  65. Mousavi, L.; Tamiji, Z.; Khoshayand, M.R. Applications and opportunities of experimental design for the dispersive liquid–liquid microextraction method—A review. Talanta 2018, 190, 335–356. [Google Scholar] [CrossRef] [PubMed]
  66. Arciuolo, R.; Chiusa, G.; Castello, G.; Camardo Leggieri, M.; Spigolon, N.; Battilani, P. Diaporthe spp. is confirmed as the main fungus associated with defective Turkish hazelnuts. Plant Health Prog. 2022, 25. [Google Scholar] [CrossRef]
  67. Ozay, G.; Seyhan, F.; Pembeci, C.; Saklar, S.; Yilmaz, A. Factors influencing fungal and aflatoxin levels in Turkish hazelnuts (Corylus avellana L.) during growth, harvest, drying and storage: A 3-year study. Food Addit. Contam. 2008, 25, 209–218. [Google Scholar] [CrossRef]
  68. Duran, P.; Barra, P.J.; de la Luz Mora, M.; Morina, F.; Viscardi, S.; Meriño-Gergichevich, C. First report of fungal complex causing grey necrosis of hazelnut in Chile. New Dis. Rep. 2020, 42, 7. [Google Scholar] [CrossRef]
  69. Belisario, A.; Maccaroni, M.; Coramusi, A.; Corazza, L.; Pryor, B.M.; Figuli, P. First report of Alternaria species groups involved in disease complexes of hazelnut and walnut fruit. Plant Dis. 2004, 88, 426. [Google Scholar] [CrossRef]
  70. Battilani, P.; Chiusa, G.; Arciuolo, R.; Somenzi, M.; Fontana, M.; Castello, G.; Spigolon, N. Diaporthe as the main cause of hazelnut defects in the Caucasus region. Phytopathol. Mediterr. 2018, 54, 241–252. [Google Scholar]
  71. Xu, Y.; Bianchini, A.; Hanna, M.A. Evaluation of mold and mycotoxin contaminations in hybrid hazelnuts grown in Nebraska. Food Process. Technol. 2011, 2, 119. [Google Scholar] [CrossRef] [Green Version]
  72. Arciuolo, R.; Santos, C.; Soares, C.; Castello, G.; Spigolon, N.; Chiusa, G.; Lima, N.; Battilani, P. Molecular characterization of Diaporthe species associated with hazelnut defects. Front. Plant Sci. 2020, 11, 611655. [Google Scholar] [CrossRef]
  73. Pscheidt, J.W.; Heckert, S.; Wiseman, M.; Jones, L. Fungi associated with and influence of moisture on development of kernel mold of hazelnut. Plant Dis. 2019, 103, 922–928. [Google Scholar] [CrossRef]
  74. Sezer, A.; Dolar, F. Hazelnut kernel defects and associated fungi in three provinces in Turkey. In Proceedings of the VII International Scientific Agriculture Symposium,” Agrosym 2016”, Jahorina, Bosnia and Herzegovina, 6–9 October 2016; pp. 1312–1318. [Google Scholar]
  75. Sezer, A.; Dolar, F.S. Colletotrichum acutatum, a new pathogen of hazelnut. J. Phytopathol. 2012, 160, 428–430. [Google Scholar] [CrossRef]
  76. Król, K.; Gantner, M.; Piotrowska, A. Morphological traits, kernel composition and sensory evaluation of hazelnut (Corylus avellana L.) cultivars grown in Poland. Agronomy 2019, 9, 703. [Google Scholar] [CrossRef] [Green Version]
  77. Sezer, A.; Dolar, F.S.; Ünal, F. First report of Colletotrichum fioriniae infection of hazelnut. Mycotaxon 2017, 132, 495–502. [Google Scholar] [CrossRef]
  78. Guerrero Contreras, J.; Galdames Gutierrez, R.; Ogass Contreras, K.; Pérez Fuentealba, S. First report of Diaporthe foeniculina causing black tip and necrotic spot on hazelnut kernel in Chile. Plant Dis. 2020, 104, 975. [Google Scholar] [CrossRef]
  79. Scarpari, M.; Vitale, S.; Di Giambattista, G.; Luongo, L.; De Gregorio, T.; Schreiber, G.; Petrucci, M.; Belisario, A.; Voglmayr, H. Didymella corylicola sp. nov., a new fungus associated with hazelnut fruit development in Italy. Mycol. Prog. 2020, 19, 317–328. [Google Scholar] [CrossRef] [Green Version]
  80. Bobev, S.G.; Angelov, L.T.; Van Poucke, K.; Maes, M. First report of kernel spot caused by Eremothecium coryli on hazelnut in Bulgaria. Plant Dis. 2018, 102, 243. [Google Scholar] [CrossRef]
  81. Halliwell, G. The breakdown of cellulose and its derivatives by enzymes from Myrothecium verrucaria. Biochem. J. 1962, 85, 67–72. [Google Scholar] [CrossRef] [Green Version]
  82. Bobev, S.G.; Angelov, L.T.; Van Poucke, K.; Maes, M. First report of hazelnut kernel rot caused by Eremothecium cymbalariae in Bulgaria. Plant Dis. 2018, 102, 818. [Google Scholar] [CrossRef]
  83. Santori, A.; Vitale, S.; Luongo, L.; Belisario, A. First report of Fusarium lateritium as the agent of nut gray necrosis on hazelnut in Italy. Plant Dis. 2010, 94, 484. [Google Scholar] [CrossRef]
  84. Turco, S.; Grottoli, A.; Drais, M.I.; De Spirito, C.; Faino, L.; Reverberi, M.; Cristofori, V.; Mazzaglia, A. Draft genome sequence of a new Fusarium isolate belonging to Fusarium tricinctum species complex collected from hazelnut in central italy. Front. Plant Sci. 2021, 12, 2835. [Google Scholar] [CrossRef]
  85. Sezer, A.; Dolar, F.S. Determination of Pestalotiopsis sp. causing disease on fruit clusters in hazelnut growing areas of Ordu, Giresun and Trabzon provinces in Turkey. J. Agric. For. 2015, 61, 183. [Google Scholar]
  86. Ebrahimi, K.S.; Ansari, M.; Hosseyni Moghaddam, M.S.; Ebrahimi, Z.; Salehi, Z.; Shahlaei, M.; Moradi, S. In silico investigation on the inhibitory effect of fungal secondary metabolites on RNA dependent RNA polymerase of SARS-CoV-II: A docking and molecular dynamic simulation study. Comput. Biol. Med. 2021, 135, 104613. [Google Scholar] [CrossRef] [PubMed]
  87. Abdel-gawad, K.M.; Zohri, A.A. Fungal flora and mycotoxins of six kinds of nut seeds for human consumption in Saudi Arabia. Mycopathologia 1993, 124, 55–64. [Google Scholar] [CrossRef] [PubMed]
  88. Simsek, O.; Arici, M.; Demir, C. Mycoflora of hazelnut (Corylus avellana L.) and aflatoxin content in hazelnut kernels artificially infected with Aspergillus parasiticus. Food/Nahrung 2002, 46, 194–196. [Google Scholar] [CrossRef] [PubMed]
  89. Khosravi, A.R.; Shokri, H.; Ziglarí, T. Evaluation of fungal flora in some important nut products (pistachio, peanut, hazelnut and almond) in Tehran, Iran. Pak. J. Nutr. 2007, 6, 460–462. [Google Scholar] [CrossRef] [Green Version]
  90. Saffari, E.; Madani, M.; Karbasizade, V.; Shakib, P. Detection of fungal and bacterial contamination of hazelnut and determination of aflatoxin B by HPLC method in Isfahan, Iran. Curr. Med. Mycol. 2021, 7, 1–5. [Google Scholar] [CrossRef]
  91. Mir Hosseini Moghaddam, S.A.; Taherzadeh, M. Isolated fungi from hazelnut, their damage and economic importance in Guilan province. Iran. J. For. Range Prot. Res. 2007, 5, 96–98. [Google Scholar]
  92. Krasauskas, A.; Paulauskienė, A.; Tarasevičienė, Ž. Micromycetes contaminating nuts used for food. Biologija 2015, 61, 109–115. [Google Scholar] [CrossRef] [Green Version]
  93. Jiménez, M.; Mateo, R.; Querol, A.; Huerta, T.; Hernández, E. Mycotoxins and mycotoxigenic moulds in nuts and sunflower seeds for human consumption. Mycopathologia 1991, 115, 121–127. [Google Scholar] [CrossRef]
  94. Amar, R.; Amina, M.; Salim, M.; Florence, M.; Nasserdine, S. Investigations on aflatoxigenic fungi and aflatoxins contamination in some nuts sampled in Algeria. Afr. J. Microbiol. Res. 2013, 7, 4974–4980. [Google Scholar] [CrossRef] [Green Version]
  95. Wang, Y.-j.; Nie, J.-y.; Yan, Z.; Li, Z.-x.; Cheng, Y.; Farooq, S. Multi-mycotoxin exposure and risk assessments for Chinese consumption of nuts and dried fruits. J. Integr. Agric. 2018, 17, 1676–1690. [Google Scholar] [CrossRef]
  96. Alhussaini, M.S.R. Mycobiota and mycotoxins of nuts and some dried fruits from Saudi Arabia. J. Am. Sci. 2012, 8, 525–534. [Google Scholar]
  97. Habibi, A.; Afzali, D. Aspergillus section Flavi from four agricultural products and association of mycotoxin and sclerotia production with isolation source. Curr. Microbiol. 2021, 78, 3674–3685. [Google Scholar] [CrossRef]
  98. Habibi, A. Aspergillus species in retail samples of pistachio, walnut and hazelnut in Kerman, Iran. Mycol. Iran. 2022, 8, 77–94. [Google Scholar]
  99. Greco, M.; Kemppainen, M.; Pose, G.; Pardo, A. Taxonomic characterization and secondary metabolite profiling of Aspergillus section Aspergillus contaminating feeds and feedstuffs. Toxins 2015, 7, 3512–3537. [Google Scholar] [CrossRef]
  100. Perrone, G.; Gallo, A. Aspergillus species and their associated mycotoxins. In Mycotoxigenic Fungi; Springer: Berlin/Heidelberg, Germany, 2017; pp. 33–49. ISBN 978-1-4939-6705-6. [Google Scholar]
  101. Perrone, G.; Susca, A. Penicillium species and their associated mycotoxins. In Mycotoxigenic Fungi; Springer: Berlin/Heidelberg, Germany, 2017; pp. 107–119. ISBN 978-1-4939-6705-6. [Google Scholar]
  102. Chepkirui, C.; Stadler, M. The genus Diaporthe: A rich source of diverse and bioactive metabolites. Mycol. Prog. 2017, 16, 477–494. [Google Scholar] [CrossRef]
  103. Xu, T.C.; Lu, Y.H.; Wang, J.F.; Song, Z.Q.; Hou, Y.G.; Liu, S.S.; Liu, C.S.; Wu, S.H. Bioactive secondary metabolites of the genus Diaporthe and anamorph Phomopsis from terrestrial and marine habitats and endophytes: 2010–2019. Microorganisms 2021, 9, 217. [Google Scholar] [CrossRef]
  104. Andolfi, A.; Boari, A.; Evidente, M.; Cimmino, A.; Vurro, M.; Ash, G.; Evidente, A. Gulypyrones A and B and phomentrioloxins B and C produced by Diaporthe gulyae, a potential mycoherbicide for saffron thistle (Carthamus lanatus). J. Nat. Prod. 2015, 78, 623–629. [Google Scholar] [CrossRef]
  105. Talontsi, F.M.; Islam, M.T.; Facey, P.; Douanla-Meli, C.; Von Tiedemann, A.; Laatsch, H. Depsidones and other constituents from Phomopsis sp. CAFT69 and its host plant Endodesmia calophylloides with potent inhibitory effect on motility of zoospores of grapevine pathogen Plasmopara viticola. Phytochem. Lett. 2012, 5, 657–664. [Google Scholar] [CrossRef]
  106. Riga, R.; Happyana, N.; Quentmeier, A.; Zammarelli, C.; Kayser, O.; Hakim, E.H. Secondary metabolites from Diaporthe lithocarpus isolated from Artocarpus heterophyllus. Nat. Prod. Res. 2021, 35, 2324–2328. [Google Scholar] [CrossRef]
  107. Hu, Q.; Yang, Y.; Yang, S.; Cao, H.; Chunyang, M.; Yang, H.; Gao, X.; Du, G. Xanthones from the fermentation products of the endophytic fungus of Phomopsis amygdali. Chem. Nat. Compd. 2015, 51, 456–459. [Google Scholar] [CrossRef]
  108. Peng, W.X.; Marchal, J.L.M.; van der Poel, A.F.B. Strategies to prevent and reduce mycotoxins for compound feed manufacturing. Anim. Feed Sci. Technol. 2018, 237, 129–153. [Google Scholar] [CrossRef]
  109. Wan, J.; Chen, B.; Rao, J. Occurrence and preventive strategies to control mycotoxins in cereal-based food. Compr. Rev. Food Sci. Food Saf. 2020, 19, 928–953. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  110. Valente, S.; Meloni, G.R.; Prencipe, S.; Spigolon, N.; Somenzi, M.; Fontana, M.; Gullino, M.L.; Spadaro, D. Effect of drying temperatures and exposure times on Aspergillus flavus growth and aflatoxin production on artificially inoculated hazelnuts. J. Food Prot. 2020, 83, 1241–1247. [Google Scholar] [CrossRef] [PubMed]
  111. Vrtodušić, R.; Ivić, D.; Jemrić, T.; Vuković, M. Hazelnut postharvest technology: A review. J. Cent. Eur. Agric. 2022, 23, 423–454. [Google Scholar] [CrossRef]
  112. Misra, N.N.; Yadav, B.; Roopesh, M.S.; Jo, C. Cold plasma for effective fungal and mycotoxin control in foods: Mechanisms, inactivation effects, and applications. Compr. Rev. Food Sci. Food Saf. 2019, 18, 106–120. [Google Scholar] [CrossRef] [Green Version]
  113. Yousefi, M.; Mohammadi, M.A.; Khajavi, M.Z.; Ehsani, A. Application of novel non-thermal physical technologies to degrade mycotoxins. J. Fungi 2021, 7, 395. [Google Scholar] [CrossRef]
  114. Dasan, B.G.; Boyaci, I.H.; Mutlu, M. Nonthermal plasma treatment of Aspergillus spp. spores on hazelnuts in an atmospheric pressure fluidized bed plasma system: Impact of process parameters and surveillance of the residual viability of spores. J. Food Eng. 2017, 196, 139–149. [Google Scholar] [CrossRef]
  115. Dasan, B.G.; Mutlu, M.; Boyaci, I.H. Decontamination of Aspergillus flavus and Aspergillus parasiticus spores on hazelnuts via atmospheric pressure fluidized bed plasma reactor. Int. J. Food Microbiol. 2016, 216, 50–59. [Google Scholar] [CrossRef]
  116. Siciliano, I.; Spadaro, D.; Prelle, A.; Vallauri, D.; Cavallero, M.C.; Garibaldi, A.; Gullino, M.L. Use of cold atmospheric plasma to detoxify hazelnuts from aflatoxins. Toxins 2016, 8, 125. [Google Scholar] [CrossRef]
  117. Sen, Y.; Onal-Ulusoy, B.; Mutlu, M. Detoxification of hazelnuts by different cold plasmas and gamma irradiation treatments. Innov. Food Sci. Emerg. Technol. 2019, 54, 252–259. [Google Scholar] [CrossRef]
  118. Jalili, M. A review on aflatoxins reduction in food. Iran. J. Health Saf. Environ. 2015, 3, 445–459. [Google Scholar]
  119. Kashanian, A.; Panjekeh, N.; Fakhtak, T. Investigating diversity and spatial distribution of endophytic fungi in hazelnut (Corylus avellana) in its different habitats of Iran. Biol. J. Microorg. 2021, 10, 53–69. [Google Scholar]
  120. Nicoletti, R.; Petriccione, M.; Curci, M.; Scortichini, M. Hazelnut-associated bacteria and their implications in crop management. Horticulturae 2022, 8, 1195. [Google Scholar] [CrossRef]
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Figure 2. Chemical structures of sterigmatocystins detected in hazelnuts.
Figure 2. Chemical structures of sterigmatocystins detected in hazelnuts.
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Figure 4. Chemical structures of resorcylic acid lactones detected in hazelnuts.
Figure 4. Chemical structures of resorcylic acid lactones detected in hazelnuts.
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Figure 5. Chemical structures of macrolides detected in hazelnuts.
Figure 5. Chemical structures of macrolides detected in hazelnuts.
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Figure 6. Chemical structures of amino acid and peptide derivatives detected in hazelnuts.
Figure 6. Chemical structures of amino acid and peptide derivatives detected in hazelnuts.
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Figure 8. Chemical structures of anthraquinones detected in hazelnuts.
Figure 8. Chemical structures of anthraquinones detected in hazelnuts.
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Figure 9. Chemical structures of trichothecenes detected in hazelnuts.
Figure 9. Chemical structures of trichothecenes detected in hazelnuts.
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Figure 10. Chemical structures of benzodiazepine alkaloids detected in hazelnuts.
Figure 10. Chemical structures of benzodiazepine alkaloids detected in hazelnuts.
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Table
Table 1. Mycotoxins detected in hazelnuts.
Table 1. Mycotoxins detected in hazelnuts.
MycotoxinFormulaNominal Mass (U)Reference
Aflatoxins
Aflatoxin B1 (AFB1)C17H12O6312[8,9,10,11,12,13,14,15,16,17,18]
Aflatoxin B2 (AFB2)C17H14O6314[8,9,10,11,12,13,14,16,17,18]
Aflatoxin G1 (AFG1)C17H12O7328[8,9,10,11,12,13,14,17,18]
Aflatoxin G2 (AFG2)C17H14O7330[9,10,11,12,13,14,17,18,19]
Amino acid derivatives
Alamethicin F30 (ALMF30)C92H150N22O251964[12]
Apicidin (APC)C34H49N5O6624[12]
Tentoxin (TEN)C22H30N4O4414[12,16]
Anthraquinones
Emodin (EMO)C15H10O5270[12]
Macrosporin (MCP)C16H12O5284[12]
Physcion (= parietin) (PHY)C16H12O5284[12]
Benzodiazepine alkaloids
Cyclopenin (CPN)C17H14N2O3294[20]
Cyclopenol (CPL)C17H14N2O4310[20]
Cyclodepsipeptides
Beauvericin (BEA)C45H57N3O9784[12,21]
Enniatin A (ENA)C36H63N3O9682[12,16,21]
Enniatin A1 (ENA1)C35H61N3O9668[12,16,21]
Enniatin B (ENB)C33H57N3O9640[12,16,21]
Enniatin B1 (ENB1)C34H59N3O9654[16,21]
Enniatin B2 (ENB2)C32H55N3O9626[12]
Enniatin B3 (ENB3)C31H53N3O9612[12]
Enniatin B4 (ENB4)C34H59N3O9654[12]
Macrolides
Curvularin (CVL)C16H20O5292[12]
Zearalenone (ZEA)C18H22O5318[12]
Zearalenone-14-sulphate (ZEA14S)C18H22O8S398[12]
Ochratoxins
Ochratoxin A (OTA)C20H18ClNO6404[10,12,22]
Ochratoxin B (OTB)C20H19NO6369[12,16]
Resorcylic acid lactones
Alternariol (AOH)C14H10O5258[12,16]
Alternariol methyl ether (AME)C15H12O5272[12,16]
Sterigmatocystins
3-O-Methylsterigmatocystin (OMST)C19H14O6338[12]
Sterigmatocystin (STE)C18H12O6324[12]
Trichothecenes
Deoxynivalenol (DON)C15H20O6296[19]
Fuserenone X (FUS X)C17H22O8354[19]
HT-2 toxin (HT-2)C22H32O8424[12]
Neosolaniol (NEO)C19H26O8382[19]
T-2 toxin (T-2)C24H34O9467[12]
Miscellaneous
Altertoxin I (ALI)C20H16O6352[12]
Chaetoglobosin A (CHA)C32H36N2O5529[20]
Equisetin (EQS)C22H31NO4373[12]
Kojic acid (KA)C6H6O4142[12]
Moniliformin (MON)C4H2O398[12]
Mycophenolic acid (MPA)C17H20O6320[12,20]
3-Nitropropionic acid (BNP)C3H5NO4119[12]
Patulin (PA)C7H6O4154[11]
Pestalotin (PE)C11H18O4214[12]
Roquefortine C (ROQC)C22H23N5O2389[20]
Viridicatin (VRD)C15H11NO2237[12]
Table
Table 2. Analytical strategies employed to determine mycotoxins in real hazelnut samples.
Table 2. Analytical strategies employed to determine mycotoxins in real hazelnut samples.
Type of SampleMycotoxinsSamplesSample PreparationDetectionLevels (µg kg−1)Ref.
HazelnutsAFB135Ultrasound extraction with ACN:H2O (8:2, v/v), cleaning up with a Carbograph-4 SPE cartridge eluted with CH2Cl2:MeOH:acetic acid (88:10:2, v/v/v)LC/ESI-MS/MS
Mobile phase:
(A) ACN:H2O (95:5, v/v);
(B) H2O		not detected (n.d.)–0.9[8]
AFB2n.d.–<LOQ
AFG1n.d.–0.1
Hazelnut pasteAFB15Extraction with MeOH:H2O (8:2, v/v) and n-hexane, cleaning up with immunoaffinity columns (IAC) eluted with MeOHHPLC-FLD
Mobile phase: ACN:MeOH:H2O (20:20:60, v/v/v)		0.45–3.61[9]
AFB2<LOQ–0.55
AFG1n.d.–1.84
AFG2<LOQ–0.30
Hazelnuts without shellAFB1320.20
AFG1031
Roasted hazelnutsAFB193.45
AFB21.16
AFG10.16
AFG21.82
HazelnutsTotal AFs-Extraction with 70% MeOH and filtrationCommercially available kit based on CD-ELISA10.3[10]
OTA1.5
Sound hazelnutsAFB15AFs determination:
extraction in MeOH:H2O (8:2, v/v), cleaning up with immunoaffinity assays.
PA determination:
extraction with ethyl acetate and filtration, subsequent extraction with 3% sodium carbonate solution, acidification of the organic phase		AFs determination:
HPLC-FLD
Mobile phase: H2O:ACN:MeOH (6:2:3, v/v/v).
PA determination:
HPLC-DAD:
Mobile phase:
H2O:ACN (1:9, v/v)		0.4–0.9[11]
Moldy hazelnutsAFB1510–246
AFB24.4–1.6
AFG1205–98.7
AFG21.3–4.0
PA65.8–25.6
Hidden moldy hazelnutsAFB1422–141
AFB20.8–2.0
AFG178.6–96.4
AFG20.5–2.1
PA67.6–16.6
HazelnutsAFB122Extraction with ACN:H2O:Acetic acid (79:20:1, v/v/v), dilution of the extract with ACN:H2O:acetic acid (79:20:1, v/v/v)UHPLC-MS/MS
Mobile phase:
(A) MeOH:H2O:Acetic acid (10:89:1, v/v/v)
(B) MeOH:H2O:Acetic acid (97:2:1, v/v/v)		7.4[12]
AFB25.5
AFG116
AFG25.5
ALMF30110
AOH78
AME59
ALI7.0
APC3.4
BEA2.4
CVL19
EMO5.5
ENA28
ENA1140
ENB37
ENB23.0
ENB30.06
ENB422
EQS110
HT-239
KA1100
MCP280
OMST1.7
MPA700
BNP440
OTA220
OTB6.9
PE3.1
PHY700
STE2.3
T-232
TEN5.4
VRD5.7
ZEA7.6
ZEA14S3.9
HazelnutsAFB142Extraction with MeOH:H2O, cleaning up with immunoaffinity columnsHPLC-FLD1.37[13]
Total AFs4.11
HazelnutsAFB120Soxhlet extraction with n-hexane, subsequent extraction with CHCl3, cleaning up with silica gel columnsTLC
Mobile phase: MeOH:CHCl3 (3:97, v/v)		25–175[14]
AFB225–175
AFG125–175
AFG225–175
HazelnutsAFB128Extraction with CH2Cl2, cleaning up with columns eluted with CHCl3:acetone (90:10, v/v)TLC
Mobile phase: diethyl ether		34.4 ppb[15]
Edible part of hazelnutsAFB120Extraction with acidified ACN, cleaning up with C18 sorbentUPLC-MS/MS
Mobile phase:
(A) ACN
(B) 0.5% formic acid in water with 10 mMol/L citric acid		-[16]
AFB2-
ENA1.00
ENA14.48
ENB1.58
ENB11.04
Total Afs< LOQ–2.10
Raw hazelnutsTotal AFs30Neogen Veratox®CD-ELISA2.11–10.03[17]
Roasted hazelnutsTotal AFs500.1–4.04
Inner membrane of hazelnutsTotal AFs500.7–38.2
HazelnutsAFs43Immunocompetition assayELISA-[18]
HazelnutsAFG27QuEChERS extraction with acidified ACN, d-SPE cleaning up with C18 and Z-Sep+HPLC-MS/MS
Mobile phase:
(A) H2O:MeOH:Acetic acid (94:5:1, v/v/v)
(B) H2O:MeOH:Acetic acid (97:2:1, v/v/v)		2.6[19]
DON56.01
FUS X45.09
NEO<LOQ
HazelnutsCHA13Sequential extractions with solvents of different polarityHPLC-MS/MS
Mobile phase:
(A) acidified H2O
(B) ACN.		7.6–29.2[20]
CPN1.32–1.37
CPL11.02–21.45
MPA2.7
ROQC<LOQ
Hazelnut fruitENA4Ultrasonic extraction with CAN, cleaning up with C18 columns. Ultrasonic extraction of the residues dissolved in ACN:MeOH (5:5, v/v)LC-MS/MS
Mobile phase
(gradient elution):
(A) MeOH
(B) ACN		0.263[21]
ENA10.007
ENB0.146
Hazelnut shellBEA0.03
ENA0.732
ENB0.076
ENB10.417
HazelnutsOTA1Extraction with MeOH:H2O (7:3, v/v)Commercially available kit based on ELISA-[22]
Table
Table 3. Fungal species reported as infecting hazelnut fruit.
Table 3. Fungal species reported as infecting hazelnut fruit.
SpeciesCountryReferences
Alternaria alternataChile[68]
Italy[69]
Alternaria arborescensItaly[69]
Alternaria sp.Georgia[70]
Nebraska (USA)[71]
Turkey[72]
Alternaria tenuissimaItaly[69]
Aspergillus sp.Oregon (USA)[73]
Georgia[70]
Turkey[66,72,74]
Botryosphaeria sp.Turkey[66,72]
Botrytis cinereaTurkey[75]
Botrytis sp.Georgia[70]
Turkey[72]
Chrysonilia sp.Nebraska (USA)[71]
Ciboria (Monilia) coryliPoland[76]
Cladosporium sp.Georgia[70]
Nebraska, Oregon (USA)[71,73]
Turkey[72,74]
Colletotrichum acutatumTurkey[75]
Colletotrichum fioriniaeTurkey[77]
Colletotrichum sp.Georgia[70]
Diaporthe arecaeTurkey[72]
Diaporthe eresGeorgia[70]
Turkey[72]
Diaporthe foeniculinaChile[78]
Diaporthe hongkongensisTurkey[72]
Diaporthe oculiTurkey[72]
Diaporthe pseudoculiTurkey[72]
Diaporthe rudisOregon (USA)[73]
Diaporthe sojaeTurkey[72]
Diaporthe sp.Chile[68]
Georgia[70]
Turkey[66,72]
Diaporthe unshiuensisTurkey[72]
Didymella corylicolaItaly[79]
Diplodia sp.Oregon (USA)[73]
Eremothecium coryliBulgaria[80]
Oregon (USA)[81]
Eremothecium cymbalariaeBulgaria[82]
Fusarium chlamydosporum (= F. sporotrichioides)Chile[68]
Fusarium culmorumOregon (USA)[73]
Fusarium lateritiumItaly[83]
Oregon (USA)[73]
Fusarium sp.Georgia[70]
Nebraska (USA)[71]
Turkey[66,72]
Fusarium tricinctumItaly[84]
Gnomoniopsis idaeicolaOregon (USA)[73]
Mucor sp.Turkey[72]
Neofusicoccum sp.Chile[68]
Paecilomyces sp.Nebraska (USA)[71]
Penicillium sp.Georgia[70]
Nebraska, Oregon (USA)[71,73]
Turkey[66,72,74]
Pestalotiopsis sp.Georgia[70]
Turkey[72,85]
Phoma sp.Georgia[70]
Ramularia sp.Oregon (USA)[73,86]
Rhizopus sp.Georgia[70]
Turkey[72]
Septoria sp.Georgia[70]
Sphaceloma sp.Georgia[70]
Trichoderma sp.Turkey[72]
Trichothecium roseumTurkey[74]
Trichothecium sp.Georgia[70]
Turkey[72]
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Salvatore, M.M.; Andolfi, A.; Nicoletti, R. Mycotoxin Contamination in Hazelnut: Current Status, Analytical Strategies, and Future Prospects. Toxins 2023, 15, 99. https://doi.org/10.3390/toxins15020099

AMA Style

Salvatore MM, Andolfi A, Nicoletti R. Mycotoxin Contamination in Hazelnut: Current Status, Analytical Strategies, and Future Prospects. Toxins. 2023; 15(2):99. https://doi.org/10.3390/toxins15020099

Chicago/Turabian Style

Salvatore, Maria Michela, Anna Andolfi, and Rosario Nicoletti. 2023. "Mycotoxin Contamination in Hazelnut: Current Status, Analytical Strategies, and Future Prospects" Toxins 15, no. 2: 99. https://doi.org/10.3390/toxins15020099

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