Abstract
We studied mycotoxigenic fungi contaminating stored wheat grain, measured the toxins they secreted, and assessed their harmfulness. We focused on one common genus Alternaria, and chose 19 isolates representing A. compacta to study how different strains differed in their mycotoxin secretion and toxicity. Toxicity was assessed in a bioassay with a model bacteria Bacillus subtilis. All 19 A. compacta strains secreted toxins. Both the mycotoxin pattern and the fungal toxicity differed between the A. compacta stains. It seemed that some other toxins than alternariols or altenue acted as the main virulence factors of A. compacta against B. subtilis. We suggest that the most commonly studied mycotoxins do not necessarily indicate the toxicity of the fungi. The high variation in the amounts and toxins that different Alternaria species and strains secrete pose a challenge to the food supply chain.
Keywords: Alternaria, Mycotoxins, Wheat grains, B. subtilis
1. Introduction
Food mycotoxins are of great public health concern, especially in many countries in Asia and Africa. One cosmopolitan saprophytic fungal pathogenic species that infects crops is Alternaria. Most Alternaria species seem to be mycotoxigenic; more than 75% of Alternaria species, isolated in Argentina, secreted secondary metabolites that are potential mycotoxins (Andersen et al., 2015). Geographical regions seem to have different fungal species composition and, despite great efforts, the taxa of Alternaria has not yet been well organized (Simmons, 2007, Wenderoth et al., 2017). Moreover, the same Alternaria species may secrete different toxins depending on the region (Garganese et al., 2016, Lee et al., 2015). Therefore, more monitoring data from different regions are still needed.
The variety of mycotoxins secreted by fungi is great (Fox and Howlett, 2008, Sanzani et al., 2016). More than 70 compounds have been identified to be secreted by Alternaria sp.; the most commonly studied are alternariol (AOH), alternariol monomethyl ether (AME), altenuene (ALT), tenuazonic acid (TeA) and tentoxin (TEN) (Alexander et al., 2011, Barkai-Golan and Paster, 2011). Recent research has considerably increased knowledge on Alternaria secreted toxin concentrations in food, as well as on the actual toxicity of the compounds (Deshidi et al., 2017, Lee et al., 2015, López et al., 2016b, López et al., 2016a, Meena et al., 2017, Patriarca et al., 2014). However, the studies have focused on the most common toxins one at the time. The toxicity of the metabolite cocktail, which the fungi secrete, has received less attention and the methods to study the overall harmfulness of different species have not been well developed. The toxicity of the metabolite cocktail needs a multi-mycotoxin approach to be understood.
Our first aim was to increase regional knowledge about fungal species contaminating stored wheat grain; we identified species in Saudi Arabia. The second aim was to assess the harmfulness of wheat grain associated Alternaria spp. using a multi-mycotoxin approach. Specifically, we studied how the toxicity varied among different A. compacta strains and whether the actual toxicity can be assessed by measuring the most common toxins. We measured three toxins (ALT, AOH and AME) that the different A. compacta isolates secreted. We assessed the harmfulness of the fungal strains using a bioassay. In the bioassay, the toxicity was assessed as the capability of the fungi to inhibit a model bacteria B. subtilis. We assumed that the more the isolate inhibits the growth of B. subtilis, the more it secretes toxins and the higher its toxicity is in general and thus, the higher its potential to be harmful to humans. We collected 100 samples of stored wheat grains from Saudi Arabia, and (a) identified the mycobiota, (b) measured three mycotoxins that the A. compacta isolates secreted, and (c) assessed the toxicity of the isolates.
2. Materials and methods
Wheat grains were randomly collected from hundred (1 0 0) different grain storages in Riyadh city between May and July 2015. Samples were collected in sterilized polystyrene bottles and stored at 4 °C.
Dilution-plate method was used for isolation the fungal strains from wheat (Youssef et al., 2008). An aliquot of 20 g of grain was weighed (three replicates) into sterile conical flask and sterilized distilled water was added to reach the final volume of 100 ml. After making several dilutions, 1 ml of each dilution were transferred on Dichloran–Rose Bengal Chloramphenicol Agar (DRBC) and Dichloran–chloramphenicol–malt extract agar (DCMA) (HiMedia, India) dishes. The suspension was evenly distributed by moving the dishes and incubated at 25 ± 2 °C for 5–7 days. The fungal endophytic colonies growth was monitored daily. Fungi growing out of the seeds were isolated, purified and identified preliminary according to their morphological characteristics (Abe et al., 2015). The total colony forming units (CFU) were counted. CFU per grain dry weight wheat and the colonization frequency (CF (%); proportion of grain samples colonized by the species) were calculated. Isolates identified as A. alternata were chosen for further toxicity studies and their identification was complemented by DNA sequencing.
2.1. DNA extraction, amplification and sequencing
The mycelium was obtained after the spores were first incubated in potato dextrose (PD) broth, thereafter, the DNA was extracted as described by Ameen et al. (2018).
The ITS region of the ribosomal DNA was amplified by PCR with the primers ITS1-F (5′-TCCGTAGGTGAACCTGCGG-3′) and ITS4 (5′-TCCTCCGCTTATTGATATGC-3′) (Gashgari et al., 2016, White et al., 1990). PCR mixture contained 2 ml of DNA with 0.5 mM of each primer, 150 mM of dNTP, 1U of Taq DNA polymerase (Roche company), (Gherbawy, 2005), and PCR reaction buffer at a final volume of 50 µl. The DNA was amplified in a thermal cycler with the cycles: initial denaturation of 10 min at 94 °C, 30 cycles of 30 sec at 94 °C, 30 sec at 58 °C, 30 sec at 72 °C, and a final extension of 10 min at 72 °C.
The more detailed identification of the isolates was based on the separation of RAPD-PCR fragments according to Gherbawy, 2005, Choi et al., 2008. PCR were carried out with five random primers OPA03 (5′-AGT CAG CCA C-3′), OPA04 (5′-AAT CGG GCT G-3′), OPA10 (5′-GTG ATC GCA G-3′), V6 (5′-TGC AGC GTG G-3′) and M13 (5′-GAG GGT GGC GGT TCT-3′). The DNA was amplified in a reaction mixture with the final volume of 50 μl by mixing 2 μl of DNA with 0.5 μM of each primer, 150 μM of dNTP, 6 U of Taq DNA polymerase, and PCR reaction buffer. The thermal cycles were: initial denaturation of 3 min at 94 °C, 35 cycles of 1 min. at 94 °C, 1 min. at 50 °C, 1 min. at 72 °C, and a final extension of 10 min. at 72 °C.
Aliquots of PCR products were checked in electrophoresis using 1% agarose gel, ethidium bromide, and visualized by UV trans-illumination. The PCR products were purified by ExoSAPIT (USB Corporation, Amersham Place, UK, under license from GE Healthcare) based on manufacturer’s instructions. The purified products were sequenced using an automated DNA sequencer (ABI Prism 3700 automated DNA analyzer) using the BigDye Deoxy Terminator cycle-sequencing kit (Applied Biosystems, Darmstadt, Germany). Sequences were submitted to GenBank on the NCBI website (http://www.ncbi.nlm.nih.gov). Sequences were compared with the GenBank database using the BLAST software on the NCBI website (http://www.ncbi.nlm.nih.gov/BLAST/).
DNA sequences were aligned with Clustal X 1.81 (Thompson et al., 1997). TREECON (de Peer and De Wachter, 1994) was used to construct neighbor-joining tree using Jukes–Cantor model.
RAPD patterns (absence or presence of RAPD-bands) were analyzed as described by Halmschlager et al. (1995). Dendograms were constructed by the Unweighted paired group method of arithmetic average (UPGMA) based on Jaccard’s similarity coefficient by using Phoretex 1D Software (version 5.2).
2.2. Bioassay
We selected 19 A. compacta strains, which had been identified using RAPD, for the toxicity studies. The potential of the isolates to inhibit the growth of Bacillus subtilis was measured as three replicates with a dual culture technique (Oldenburg et al., 1996). The filtrate of the fungal spores was prepared as described in Ameen et al. (2018) Half of the filtrates had been boiled for 15 min and half not boiled.
B. subtilis was provided by the Armed forces hospital, Riyadh city. B. subtilis was first grown in Tryptone Glucose Yeast Extract (TGY) broth (HiMedia Laboratories) at 37 °C for 24 h. An aliquot of 1 ml of the bacterial broth was transferred to 100 ml of TGY agar. The inoculated medium was poured on petri dishes (10 ml for each) and left to solidify. At the center of each dish, the agar was punched by a sterilized corks borer to make a hole. A aliquot of 1 ml of sterilized water (control) or filtrate containing fungal spores was added to the holes by a sterilized pipette. Finally, all plates were incubated at 37 °C for 28 h and the radius of the inhibition zone was measured as mm.
2.3. Mycotoxins
The toxins secreted by the isolates were measured in polished rice media (Li et al., 2001). Polished rice (12.5 g) was weighed to flasks (250 ml) that were inoculated by one pure fungus from the plates and incubated at 25 °C for 21 days. Toxins were extracted by adding 30 ml methanol and shaking the mixture until homogenous. The suspension was filtrated through Whatman filter paper No. 1. The filter was purified by filtering 60 ml of ammonium sulfate (20%). The toxins were isolated with chloroform. High purity chloroform (10 ml) was added, the mixture was shaken and the layer of chloroform was evaporated. The isolation procedure was repeated three times. The dry film was dissolved in 4 ml of methanol and AOH, ALT and AME were analyzed with HPLC combined with UV-detection at 258 nm as previously described (Li et al., 2001). Pure mycotoxins (Wako pure chemicals industries, Ltd) were used as the standards.
The results were expressed as means and standard deviations (SD). Pearson correlation analysis and principal component analysis (PCA) using the correlation matrix were performed for the mycotoxin concentrations and inhibition zones.
3. Results
A total of 50 species and one class belonging to 18 genera were morphologically identified in 100 wheat grain samples (Table 1). The genera were Alternaria (9 species), Cladosporium (9 species and one class), Drechslera (5 species), Ulocladium (5 species), Aspergillus (4 species), Stemphylium (3 species), Scytalidium (2 species), Torula (2 species) and one species of Acremonium, Embellisial, Phoma, Penicillium, Mycovellosiella, Fusarium; Staphylotricum, Stachybotrys and Xylohypha and an unidentified Mycelium sterilium.
Table 1.
Total colony forming units (CFU) on DRBC and DCMA media and colonization frequency (CF) of fungi isolated from wheat grain.
| Fungi | Total count CFU (g dw/grain) |
CF % |
||
|---|---|---|---|---|
| DRBC | DCMA | DRBC | DCMA | |
| Acremonium strictum | 2 | – | 1 | – |
| Alternaria | 325 | 5.2 | 56 | 47 |
| A. alternata | 270 265 267 |
25.2 | 49 | 43 |
| A. brassicicola | 75.3 | – | 1 | – |
| A. dennisii | – | 5.4 | – | 1 |
| A. infectoria | 5.13 | 25.11 | 4 | 3 |
| A. longipes | 5.2 | 25.6 | 1 | 2 |
| A. phragmospora | 5.4 | – | 2 | – |
| A. radicina | 75.21 | 25.7 | 4 | 3 |
| A. infectoria | 5.3 | – | 1 | – |
| A. triticina | 5.5 | – | 2 | – |
| Aspergillus | 5.7 | 75.11 | 9 | 13 |
| A. flavus | 75.5 | 75.4 | 8 | 8 |
| A. niger | 75.1 | 7 | 4 | 8 |
| A. terreus | – | – | – | – |
| A. ustus | – | – | – | – |
| Cladosporium | 170 | 75.14 | 64 | 60 |
| C. cladosporiodes | 75.9 | 5.5 | 3 | 2 |
| C. cucumerinum | 75.5 | 32 | 15 | 11 |
| C. elatum | 25.8 | 75.4 | 4 | 3 |
| C. herbarum | 5.81 | 79 | 39 | 39 |
| C. phyllachorae | – | – | – | – |
| C. psoraleae | 25.2 | 5.2 | 1 | 1 |
| C. sphaerospermum | 5.5 | 4 | 1 | 1 |
| C. trichoides var. chlamydosporum | 5.4 | 5 | 2 | 2 |
| C. uredinicola | 75.1 | – | 1 | – |
| C. spongiosum | 75.8 | 14 | 3 | 6 |
| Drechslera | 7.14 | 75.12 | 57 | 53 |
| D. austrliensis | 25.6 | 25.6 | 26 | 24 |
| D. halodes | 75.5 | 42 | 21 | 20 |
| D. indica | 5.1 | 75.4 | 1 | 2 |
| D. papendorfii | 5.1 | – | 1 | – |
| D. specifire | 25.3 | 75.24 | 15 | 15 |
| Embellisial chlamydospora | – | 25.2 | – | 1 |
| Fusarium oxysporum | 50.3 | 5.2 | 91 | 87 |
| Mycelium strelium | 89 | 5.7 | 30 | 26 |
| Mycovellosiella perfoliata | 5.1 | 25.7 | 4 | 3 |
| Penicillium digitatum | 5.6 | 75.4 | 10 | 9 |
| Phoma pomorum | 75.5 | – | 1 | – |
| Scytalidium | 12 | 5.17 | 6 | 7 |
| S. lignicola | – | 5.1 | – | 1 |
| S. thermophilum | 12 | 25.16 | 6 | 6 |
| Stachybotrys atra | – | – | – | – |
| Staphylotricum coccusporum | 3 | – | 1 | – |
| Stemphylium | 5.75 | 5.74 | 27 | 33 |
| S. herbarum | 38 | 25.4 | 20 | 21 |
| S. lycopersici | 25.5 | 25.6 | 2 | 1 |
| S. vescarium | 25.14 | 28 | 6 | 11 |
| Torula | – | 4 | – | 2 |
| T. herbarum | – | 75.1 | – | 1 |
| T. herbarum f. quaternella | – | 25.2 | – | 1 |
| Ulocladium | 5.2 | 75.17 | 75 | 81 |
| U. atrum | 5.97 | 106 | 50 | 55 |
| U. chartarum | 5.7 | 68 | 30 | 32 |
| U. chlamydospora | 2 | – | 1 | – |
| U. odemansii | 1 | 75.2 | 1 | 1 |
| U. tuberculatum | 5.2 | – | 1 | – |
| Xylohypha pinicola | – | 5.6 | – | 1 |
A. compacta were the dominant Alternaria sp. with a total count of 270 CFU (g dw/grain) and 49% colonization frequency (Table 1). The next dominant Alternaria spp. were A. radicina and A. brassicicola (75 CFU). A. infectoria, A. triticina, A. phragmospora, A. state of Pleospora infectoria and A. longipes had relatively low CFU.
The phylogenetic tree revealed that all isolates morphologically identified as A. alternata belonged to one group of A. compacta No. EU1285291, (Fig. 1). The kinship tree for the A. compacta isolates divided the strains first into two groups (Fig. 2). In the first group (lowest in Fig. 2), the isolates (Aa2, Aa4 and Aa17) had 65% similarity. The second group contained all remaining 16 isolates and was further divided into 6 subgroups.
Fig. 1.
Phylogenetic tree of ITS rDNA sequences of the fungi isolated from wheat grain and the selected reference sequences from public databases. Sequences obtained in the present study and their GenBank accession numbers are circled with red. The tree was constructed by the neighbor-joining algorithm using the maximum composite likelihood model. Bootstrap percentages from 1000 replicates are shown.
Fig. 2.
Kinship tree of the 19 Alternaria compacta isolates growing from wheat grains. Sequences were obtained using five random primers.
All 19 A. compacta isolates inhibited the growth of B. subtilis before boiling the spores (Table 2). The inhibition zone varied between 16.2 and 20.0 mm before boiling. Boiling destroyed the inhibition potential of one isolate. All other 18 isolates retained their inhibition potential and about the same inhibition zones were measured after boiling (18.0–20.6 mm).
Table 2.
Inhibition (zone, mm, the mean of three replicates, SD = 1.0–1.4 for each) of fungal isolates against Bacillus subtilis. Fungal spores derived from wheat grain were studied as such (No Boiling) and after boiling (Boiling).
| Isolate | No Boiling | Boiling |
|---|---|---|
| Aa1 | 18.3 | 19.3 |
| Aa2 | 18 | 18.1 |
| Aa3 | 18.7 | 19.1 |
| Aa4 | 19.7 | 20 |
| Aa5 | 17.5 | 18.5 |
| Aa6 | 18.1 | 18.2 |
| Aa7 | 17.7 | 17.7 |
| Aa8 | 18 | 18.1 |
| Aa9 | 18.3 | 19.3 |
| Aa10 | 19 | 19 |
| Aa11 | 18.4 | 19.3 |
| Aa12 | 20 | 20.6 |
| Aa13 | 19.2 | 20.0 |
| Aa14 | 16.2 | 16.9 |
| Aa15 | 17.8 | 18 |
| Aa16 | 18.6 | 18.9 |
| Aa17 | 17.5 | 18.3 |
| Aa18 | 18.5 | 19.2 |
| Aa19 | 16.6 | – |
All A. compacta except one (Aa 1) isolates secreted mycotoxins ALT, AOH or AME, and 13 isolates secreted two or three of the toxins. The toxin patterns differed remarkably between the isolates, as indicated by PCA (Fig. 3), where the axis 1 (PC1) and axis 2 (PC2) explained 38% and 15% of the variation, respectively. The PCA sample score ordination indicated that three isolates, namely Aa 17, Aa 18 and Aa19 (left low corner in the ordination), differed from all other isolates. The variable loadings (vectors) indicate that the three isolates had relatively high ALT and low AME concentrations and relatively low inhibition zones against B. subtilis. However, the actual measured differences between the inhibition zones were small (Table 2). The PCA indicated a negative relation between the inhibition zones and toxin (ALT and AOH) concentrations because their vectors go to the opposite directions. Pearson correlation analysis, however, did not show any relation between the inhibition zones and toxin concentrations (r < 0.25 for each toxin).
Fig. 3.
Sample (19 A. compacta isolates) score ordination and the variable loadings (vectors) of principal component analysis using alternariol (AOH), alternariol monomethyl ether (AME), altenuene (ALT) and inhibition against B. subtilis (mean ± SD, n = 3). PC1 and PC2 explained 38% and 15% of the variation, respectively.
The highest concentration of ALT was 0.0119 µg/l (Aa18) followed by 0.0103 µg/l (Aa17). The highest concentration of the AOH was 0.581 µg/l (Aa14) followed by 0.578 µg/l (Aa9). Three isolates (Aa5, Aa7 and Aa 6) secreted relatively high amounts of AME (1.59, 1.21, and 0.939 µg/l respectively) (Table 3). None of the toxins correlated with the inhibition zone.
Table 3.
Concentrations of altenue (ALT), alternariol (AOH) and alternariol monomethyl ether (AME) the fungi isolated from wheat grain secreted in vitro.
| Isolate | Concentration of toxins µg/l |
||
|---|---|---|---|
| ALT | AOH | AME | |
| Aa 1 | 0 | 0 | 0 |
| Aa 2 | 0 | 0.18 ± 0.01 | 0 |
| Aa 3 | 0.001 ± 0.0004 | 0.4 ± 0.03 | 0.8 ± 0.3 |
| Aa 4 | 0.01 ± 0.009 | 0 | 0 |
| Aa 5 | 0.002 ± 0.0002 | 0.44 ± 0.03 | 1.57 ± 0.04 |
| Aa 6 | 0.5 ± 0.04 | 0.17 ± 0.01 | 0.78 ± 0.026 |
| Aa 7 | 0.24 ± 0.02 | 0.54 ± 0.03 | 1.2 ± 0.18 |
| Aa 8 | 0.13 ± 0.03 | 0.14 ± 0.04 | 0.34 ± 0.04 |
| Aa 9 | 0.22 ± 0.03 | 0.08 ± 0.01 | 0.02 ± 0.01 |
| Aa 10 | 0.45 ± 0.04 | 0.07 ± 0.014 | 0.162 ± 0.03 |
| Aa 11 | 0.33 ± 0.02 | 0.23 ± 0.032 | 0.34 ± 0.03 |
| Aa 12 | 0.04 ± 0.03 | 0.68 ± 0.036 | 0.008 ± 0.0001 |
| Aa 13 | 0 | 0.72 ± 0.03 | 0.64 ± 0.035 |
| Aa 14 | 0 | 0.03 ± 0.02 | 0.88 ± 0.025 |
| Aa 15 | 0.80 ± 0.02 | 0.59 ± 0.025 | 0.57 ± 0.02 |
| Aa 16 | 0 | 0.84 ± 0.04 | 0 |
| Aa 17 | 0.33 ± 0.04 | 0 | 0 |
| Aa 18 | 0.91 ± 0.025 | 0.29 ± 0.04 | 0 |
| Aa 19 | 0.58 ± 0.03 | 0 | 0 |
4. Discussion
The genus Alternaria is well known for its ability to secrete a wide range of toxins, which can be either specific for the host or common for several hosts. Our isolations from wheat grain showed that the toxin production varied within one species, A. compacta. It seems that the toxin production of the strains was regulated by the environmental factors of the host, i.e. the storing conditions of wheat. Optimum environmental conditions are known to differ between different Alternaria species, and the conditions are known to affect to their mycotoxin production as well (Lee et al., 2015).
Previous studies suggest that strains may differ in their mycotoxin secretion (Medina et al., 2017, Meena et al., 2017, Oviedo et al., 2010, Patriarca et al., 2014). This is supported by our data. Different A. compacta strains isolated from wheat had different patterns of toxins secreted; three strains seemed to differ remarkably from the rest of the 16 strains, as indicated by the PCA ordination, where these three species are situated in the left lower corner. The mycotoxin loadings in the PCA indicate that the three strains secreted a combination of relatively high ALT and low AME concentration compared to the other strains. The three strains were not phylogenetically the nearest strains of A. compacta, instead they were divided over the kinship tree.
The pathogenicity of fungi depends not only on the mycotoxins secreted but the susceptibility of the organisms to the mycotoxins. Studies on the toxicity to any organisms are limited in general and in most studies, pure toxins have been tested one at the time. Alternaria species are known to have antimicrobial virulence factors (Cota et al., 2008, da Cruz Cabral et al., 2017, Lou et al., 2013, Nemecek et al., 2012). Recently, AOH was found to have antibacterial activity against Gram-positive bacteria Staphylococcus aureus (Deshidi et al., 2017). All our A. compacta strains inhibited the growth of a common Gram-positive model bacteria Bacillus subtilis. We suggest that A. compacta has high virulence and therefore, the species may be harmful to humans.
As stated above, wheat originating fungi A. compacta secreted toxins that inhibited B. subtilis. However, the three toxins, ALT, AOH or AME, seemed not to be especially toxic to B. subtilis, because the PCA analysis indicated rather the opposite. Therefore, it seems that the fungi A. compacta secreted some other toxins that inhibited the B. subtilis growth in our experiment. We suggest that some other toxins or compounds, such as enzymes, acted as the main virulence factors. We support the suggestion of López et al. (2016b) that multi-mycotoxin approach is needed to be able to assess the harmfulness of Alternaria contamination. The measuring should be extended to include other toxins, such as TEN and TeA (López et al., 2016b). The latter has been shown to induce more pathogenicity symptoms to tomato than AOH and AME (Meena et al., 2016). Because of the great variety of toxins secreted, techniques to measure the overall harmfulness of the mycotoxigenic fungal species should be further developed as well.
Most mycotoxins are chemically and thermally stable and thus impossible to be destroyed by pasteurization or boiling (Alshannaq and Yu, 2017). We observed the heat resistance of fungal spores in 18 out of 19 isolates. Only one of the isolates lost its ability to inhibit B. subtilis growth after the spores were boiled. Resistance of the fungi against heat poses a difficult challenge to food security.
We observed that different Alternaria species were the most common and abundant species contaminating stored wheat grain in Saudi Arabia, Riyadh. A. compacta was the most common Alternaria species, contrary to results elsewhere. A. tenuissima was the most common species isolated from Argentinean wheat (Patriarca et al., 2007). A. alternata and A. infectoria have been reported as the predominant species in cereals in several studies worldwide (Lee et al., 2015).
In conclusion, all A. compacta strains that contaminated stored wheat grain secreted harmful toxins. Moreover, the fungal spores and thus, their toxicity were not possible to be destroyed by boiling. Different A. compacta stains had different mycotoxin cocktails of which toxicity differed. We interpret that some other toxins than the most commonly studied AOH, AOL or AME acted as the main virulence factors. We suggest that the mycotoxins most commonly studied do not necessarily indicate the harmfulness of the fungi. The high variation in the amounts and toxins that the different Alternaria species and strains secrete pose a challenge to the food supply chain in many regions of the world.
Acknowledgments
Acknowledgements
The authors extend their appreciation to the Deanship of Scientific Research at King Saud University for funding this work through research group No. (RGP-1438-029).
Competing interest
The authors declare that they have no competing interests.
Footnotes
Peer review under responsibility of King Saud University.
References
- Abe C.A.L., Faria C.B., de Castro F.F., de Souza S.R., dos Santos F.C., da Silva C.N., Tessmann D.J., Barbosa-Tessmann I.P. Fungi isolated from maize (Zea mays L.) grains and production of associated enzyme activities. Int. J. Mol. Sci. 2015;16:15328–15346. doi: 10.3390/ijms160715328. [DOI] [PMC free article] [PubMed] [Google Scholar]
- Alexander J., Benford D., Boobis A., Ceccatelli S., Cottrill B., Cravedi J., Di Domenico A., Doerge D., Dogliotti E., Edler L. Scientific opinion on the risks for animal and public health related to the presence of Alternaria toxins in feed and food. EFSA J. 2011;9:2407–2504. [Google Scholar]
- Alshannaq A., Yu J.-H. Occurrence, toxicity, and analysis of major mycotoxins in food. Int. J. Environ. Res. Public Health. 2017;14:632. doi: 10.3390/ijerph14060632. [DOI] [PMC free article] [PubMed] [Google Scholar]
- Ameen F., Hakmi H., Gashgari R., Al-Homaidan A.A., Al-Sabri A. Fungal contamination of non-renewable groundwater in the Arabian Peninsula: assessing the harmfulness to humans. Geomicrobiol. J. 2018 [Google Scholar]
- Andersen B., Nielsen K.F., Pinto V.F., Patriarca A. Characterization of Alternaria strains from Argentinean blueberry, tomato, walnut and wheat. Int. J. Food Microbiol. 2015;196:1–10. doi: 10.1016/j.ijfoodmicro.2014.11.029. [DOI] [PubMed] [Google Scholar]
- Barkai-Golan R., Paster N. Academic Press; 2011. Mycotoxins in Fruits and Vegetables. [Google Scholar]
- Choi S.-K., Park Y.-S., Choi D.-K., Chang H.-I. Effects of astaxanthin on the production of NO and the expression of COX-2 and iNOS in LPS-stimulated BV2 microglial cells. J. Microbiol. Biotechnol. 2008;18:1990–1996. [PubMed] [Google Scholar]
- Cota B.B., Rosa L.H., Caligiorne R.B., Rabello A.L.T., Almeida Alves T.M., Rosa C.A., Zani C.L. Altenusin, a biphenyl isolated from the endophytic fungus Alternaria sp., inhibits trypanothione reductase from Trypanosoma cruzi. FEMS Microbiol. Lett. 2008;285:177–182. doi: 10.1111/j.1574-6968.2008.01221.x. [DOI] [PubMed] [Google Scholar]
- da Cruz Cabral L., Rodriguero M., Stenglein S., Nielsen K.F., Patriarca A. Characterization of small-spored Alternaria from Argentinean crops through a polyphasic approach. Int. J. Food Microbiol. 2017;257:206–215. doi: 10.1016/j.ijfoodmicro.2017.06.026. [DOI] [PubMed] [Google Scholar]
- de Peer Y., De Wachter R. TREECON for Windows: a software package for the construction and drawing of evolutionary trees for the Microsoft Windows environment. Bioinformatics. 1994;10:569–570. doi: 10.1093/bioinformatics/10.5.569. [DOI] [PubMed] [Google Scholar]
- Deshidi R., Devari S., Kushwaha M., Gupta A.P., Sharma R., Chib R., Khan I.A., Jaglan S., Shah B.A. Isolation and quantification of alternariols from endophytic fungus, Alternaria alternata: LC-ESI-MS/MS analysis. ChemistrySelect. 2017;2:364–368. [Google Scholar]
- Fox E.M., Howlett B.J. Secondary metabolism: regulation and role in fungal biology. Curr. Opin. Microbiol. 2008;11:481–487. doi: 10.1016/j.mib.2008.10.007. [DOI] [PubMed] [Google Scholar]
- Garganese F., Schena L., Siciliano I., Prigigallo M.I., Spadaro D., De Grassi A., Ippolito A., Sanzani S.M. Characterization of citrus-associated Alternaria species in mediterranean areas. PLoS One. 2016;11:e0163255. doi: 10.1371/journal.pone.0163255. [DOI] [PMC free article] [PubMed] [Google Scholar]
- Gashgari R., Gherbawy Y., Ameen F., Alsharari S. Molecular characterization and analysis of antimicrobial activity of endophytic fungi from medicinal plants in Saudi Arabia. Jundishapur J. Microbiol. 2016;9 doi: 10.5812/jjm.26157. [DOI] [PMC free article] [PubMed] [Google Scholar]
- Gherbawy Y.A.M.H. Genetic variation among isolates of Alternaria spp. from select Egyptian crops. Arch. Phytopathol. Plant Prot. 2005;38:77–89. [Google Scholar]
- Halmschlager E., Messner R., Kowalski T., Prillinger H. Differentiation of Ophiostoma piceae and Ophiostoma quercus by morphology and RAPD analysis. Syst. Appl. Microbiol. 1995;17:554–562. [Google Scholar]
- Lee H.B., Patriarca A., Magan N. Alternaria in food: ecophysiology, mycotoxin production and toxicology. Mycobiology. 2015;43:93–106. doi: 10.5941/MYCO.2015.43.2.93. [DOI] [PMC free article] [PubMed] [Google Scholar]
- Li F.-Q., Yoshizawa T., Kawamura O., Luo X.-Y., Li Y.-W. Aflatoxins and fumonisins in corn from the high-incidence area for human hepatocellular carcinoma in Guangxi, China. J. Agric. Food Chem. 2001;49:4122–4126. doi: 10.1021/jf010143k. [DOI] [PubMed] [Google Scholar]
- López P., Venema D., de Rijk T., de Kok A., Scholten J.M., Mol H.G.J., de Nijs M. Occurrence of Alternaria toxins in food products in The Netherlands. Food Control. 2016;60:196–204. [Google Scholar]
- López P., Venema D., Mol H., Spanjer M., de Stoppelaar J., Pfeiffer E., de Nijs M. Alternaria toxins and conjugates in selected foods in the Netherlands. Food Control. 2016;69:153–159. [Google Scholar]
- Lou J., Fu L., Peng Y., Zhou L. Metabolites from Alternaria fungi and their bioactivities. Molecules. 2013;18:5891–5935. doi: 10.3390/molecules18055891. [DOI] [PMC free article] [PubMed] [Google Scholar]
- Medina A., Akbar A., Baazeem A., Rodriguez A., Magan N. Climate change, food security and mycotoxins: do we know enough? Fungal Biol. Rev. 2017;31:143–154. [Google Scholar]
- Meena M., Swapnil P., Upadhyay R.S. Isolation, characterization and toxicological potential of Alternaria-mycotoxins (TeA, AOH and AME) in different Alternaria species from various regions of India. Sci. Rep. 2017;7:8777. doi: 10.1038/s41598-017-09138-9. [DOI] [PMC free article] [PubMed] [Google Scholar]
- Meena M., Zehra A., Dubey M.K., Aamir M., Gupta V.K., Upadhyay R.S. Comparative evaluation of biochemical changes in tomato (Lycopersicon esculentum Mill.) infected by Alternaria alternata and its toxic metabolites (TeA, AOH, and AME) Front. Plant Sci. 2016;7:1408. doi: 10.3389/fpls.2016.01408. [DOI] [PMC free article] [PubMed] [Google Scholar]
- Nemecek G., Cudaj J., Podlech J. Revision of the structure and total synthesis of altenuisol. Eur. J. Org. Chem. 2012;2012:3863–3870. [Google Scholar]
- Oldenburg K.R., Vo K.T., Ruhland B., Schatz P.J., Yuan Z. A dual culture assay for detection of antimicrobial activity. J. Biomol. Screen. 1996;1:123–130. [Google Scholar]
- Oviedo M.S., Ramirez M.L., Barros G.G., Chulze S.N. Impact of water activity and temperature on growth and alternariol and alternariol monomethyl ether production of Alternaria alternata isolated from soybean. J. Food Prot. 2010;73:336–343. doi: 10.4315/0362-028x-73.2.336. [DOI] [PubMed] [Google Scholar]
- Patriarca A., Azcarate M.P., Terminiello L., Pinto V.F. Mycotoxin production by Alternaria strains isolated from Argentinean wheat. Int. J. Food Microbiol. 2007;119:219–222. doi: 10.1016/j.ijfoodmicro.2007.07.055. [DOI] [PubMed] [Google Scholar]
- Patriarca A., Medina A., Pinto V.F., Magan N. Temperature and water stress impacts on growth and production of altertoxin-II by strains of Alternaria tenuissima from Argentinean wheat. World Mycotoxin J. 2014;7:329–334. [Google Scholar]
- Sanzani S.M., Reverberi M., Geisen R. Mycotoxins in harvested fruits and vegetables: Insights in producing fungi, biological role, conducive conditions, and tools to manage postharvest contamination. Postharvest Biol. Technol. 2016;122:95–105. [Google Scholar]
- Simmons E.G. CBS Fungal Biodiversity Centre; Utrecht: 2007. Alternaria, An Identification Manual; p. 775. [Google Scholar]
- Thompson J.D., Gibson T.J., Plewniak F., Jeanmougin F., Higgins D.G. The CLUSTAL_X windows interface: flexible strategies for multiple sequence alignment aided by quality analysis tools. Nucleic Acids Res. 1997;25:4876–4882. doi: 10.1093/nar/25.24.4876. [DOI] [PMC free article] [PubMed] [Google Scholar]
- Wenderoth M., Pinecker C., Voß B., Fischer R. Establishment of CRISPR/Cas9 in Alternaria alternata. Fungal Genet. Biol. 2017;101:55–60. doi: 10.1016/j.fgb.2017.03.001. [DOI] [PubMed] [Google Scholar]
- White T.J., Bruns T., Lee S., Taylor J.W. Amplification and direct sequencing of fungal ribosomal RNA genes for phylogenetics. PCR Protoc. Guid. Methods Appl. 1990;18:315–322. [Google Scholar]
- Youssef M.S., El-Maghraby O.M.O., Ibrahim Y.M. Mycobiota and mycotoxins of Egyptian peanut (Arachis hypogeae L.) seeds. Int J Bot. 2008;4:349–360. [Google Scholar]