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Article

Potential Application of Lactic Acid Bacteria to Reduce Aflatoxin B1 and Fumonisin B1 Occurrence on Corn Kernels and Corn Ears

by
Tiago de Melo Nazareth
1,2,*,†,
Carlos Luz
1,†,
Raquel Torrijos
1,
Juan Manuel Quiles
1,
Fernando Bittencourt Luciano
2,
Jordi Mañes
1 and
Giuseppe Meca
1,*
1
Laboratory of Food Chemistry and Toxicology, Faculty of Pharmacy, University of Valencia, Av. Vicent Andrés Estellés s/n, 46100 Burjassot, Spain
2
School of Life Sciences, Pontifícia Universidade Católica do Paraná, st. Imaculada Conceição 1155, Curitiba 80215-901, PR, Brazil
*
Authors to whom correspondence should be addressed.
†
Authors have contributed equally to the study and should be considered co-first authors.
Toxins 2020, 12(1), 21; https://doi.org/10.3390/toxins12010021
Submission received: 29 November 2019 / Revised: 27 December 2019 / Accepted: 28 December 2019 / Published: 31 December 2019
(This article belongs to the Special Issue Aflatoxins: Food Sources, Occurrence and Toxicological Effects)
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Abstract

:
Fungal spoilage is an important issue for the food industry, leading to food sensory defects, food waste, economic losses and public health concern through the production of mycotoxins. Concomitantly, the search for safer natural products has gained importance since consumers began to look for less processed and chemically treated foods. In this context, the aim of this study was to evaluate the antifungal and antimycotoxigenic effect of seven strains of Lactobacillus plantarum. Lactic acid bacteria (LAB) were grown on Man Rogosa Sharpe (MRS) broth at 37 °C in anaerobic conditions. After that, the cell-free supernatant (CFS) were recovered to determine its antifungal activity by halo diffusion agar test. In addition, minimum inhibitory concentration (MIC) and minimum fungicidal concentration (MFC) was determined for each L. plantarum CFS by 96-well microplates method. Additionally, CFS was used as a natural biocontrol agent on corn kernels and corn ears contaminated with Aspergillus flavus and Fusarium verticillioides, respectively. The L. plantarum CECT 749 CFS showed the highest antifungal effect against all essayed strains. Moreover, the employment of this CFS in food reduced the mycotoxin production at a percentage ranging from 73.7 to 99.7%. These results suggest that the L. plantarum CECT 749 CFS could be promising for the biocontrol of corn.
Keywords:
Lactobacillus plantarum; aflatoxin B1; fumonisin B1; biopreservation
Key Contribution: In vitro analyses showed that Fusarium spp. was more susceptible to L. plantarum spp. CFS treatment than Aspergillus spp. In situ, the CFS treatment did not completely avoid the fungal growth but in both cases, on corn kernel and corn ears, the content of mycotoxin was significantly reduced.

1. Introduction

Filamentous fungi contaminate several types of food such as cereals, fruits and vegetables, dried fruits, feed products, dried spices, dried cured meats, and bread, among others [1,2,3,4,5,6,7,8,9].
Aspergillus and Fusarium are the major fungal genera associated with corn contamination [10]. Indeed, many Aspergillus and Fusarium species are considered common contaminants of food and feed due to their ability to colonize and grow in a wide range of environmental conditions. Furthermore, these species are also known to produce mycotoxins.
Mycotoxins are secondary metabolites produced by the mycelial structure of filamentous fungi that have no biochemical significance in fungal growth but have the potential to elicit undesirable effects on human and animal health, following consumption of contaminated food or feedstuffs [11,12,13]. Therefore, mycotoxin contaminated crops result in illness and economic losses once these grains cannot be ingested or marketed.
Several factors can influence the presence of mycotoxin in foods and feed such as fungal strain specificity, fungal strain variation, and toxin stability [14,15,16]. However, its occurrence is closely related to environmental conditions favorable to fungal growth, in particular, a hot and humid climate, i.e., mycotoxins are most frequent in tropical areas but they can also be found in a temperate climate [17,18]. Besides that, the mycotoxin contamination may also occur at various stages of the food production chain, e.g., in the storage, in the field, during harvest, processing, and distribution [19]. Currently, the worldwide contamination of food and feedstuffs with mycotoxins is a significant problem. Based on the recent data on food grains, the prevalence of mycotoxins could be as high as 60–80%, depending on the mycotoxin of concern, the analytical method used, and the equipment detection limit [20,21].
Aflatoxins are toxic compounds produced mainly by A. flavus and A. parasiticus. Among them, aflatoxin B1 (AFB1) is the most relevant for a health concern, which has been classified as Group 1 by the International Agency for Research on Cancer (IARC) owing to its carcinogenic effect (IARC, 2012). This mycotoxin is closely associated, in long-term exposure, to the hepatocellular carcinoma in humans, modulation of the immune system and malnutrition [22].
Fumonisins are a heterogeneous group of toxins synthesized by Fusarium species [23]. Fumonisins of group B have been widely studied due to their prevalence and toxicological effects. In particular, fumonisin B1 (FB1) is related to chronic effects in human health, e.g., hepatocarcinoma, nephrotoxicity, suppression of the immune system and defects in the neural-tubes [24]. In addition, this mycotoxin has been classified by the IARC as a group 2B (possible carcinogen for humans) [25].
The growing consumer interest in nutritional aspects and food quality has contributed to the increased consumption of organically produced foods [26,27]. However, naturally produced and highly nutritious foods such as corn and its byproducts are also prone to fungal spoilage and mycotoxin production.
Biopreservation is a natural tool to extend shelf life and to increase the safety of foods by applying microorganisms or their antimicrobial active metabolites [28]. Recently, authors have described the use of lactic acid bacteria (LAB) to avoid the fungal growth and prolong the shelf life of food as an alternative to synthetic biocides. However, there are no reports on the use of LAB to prevent fungal growth in corn kernels and corn ears.
Previously, it was believed that the organic acids produced by the LAB were the main antifungal agents because of the lowering of the pH. However, authors have shown that the antifungal activity of these compounds alone was too low to fully explain the antifungal activity observed [29,30]. Thus, other metabolites have been studied as the source of antifungal activity such as proteinaceous compounds, fatty acids, phenolic acid, hydrogen peroxide, and bacteriocins [31,32,33,34].
It seems that the LAB possess a large potential for biopreservation due to the production of antimicrobial compounds. Moreover, it is important to emphasize that most LAB are generally recognized as safe and QPS (qualified presumption of safety), which promote them as very favorable candidates for integration as natural preservatives in food and feedstuffs [35,36]. Indeed, they are already used as starter cultures in the food industry, in dairy and dry-fermented meat products [37].
Taking into account the growing interest in the use of natural antimicrobial compounds as an alternative to synthetic chemical control and the potential of LAB, the objective of this study was to evaluate the employment of Lactobacillus plantarum cell-free supernatant as a biocontrol agent in order to reduce the growth of A. flavus ISPA 8111 (AFB1 producer) and F. verticillioides CECT 2982 (FB1 producer) as well as mycotoxin production on corn kernels and corn ears.

2. Results and Discussion

2.1. In Vitro Antifungal Activity of L. plantarum spp.

The qualitative antifungal effect of cell-free supernatant (CFS) obtained by L. plantarum spp. fermentation was determined by halo inhibition test on the solid medium of potato dextrose agar (PDA). The analyses of results demonstrated that all evaluated strains of L. plantarum fermented MRS, and their CFS possessed antifungal effect (Table 1). Regarding the L. plantarum CECT 749, its CFS showed the highest halo inhibition zone against the strain of F. graminearum ITEM 126, F. cerealis CECT 20489, F. verticillioides CECT 2152, F. verticillioides CECT 2982, and A. flavus ITEM 8111 in comparison to others. Moreover, the strains of F. verticillioides showed higher sensitivity towards L. plantarum CECT 749 CFS related to other fungi.
In general, the quantitative results evidenced that the Fusarium strains were more sensitive to CFS than Aspergillus strains. Moreover, agreeing to qualitative results, all CFS showed antifungal effect, presenting minimum inhibitory concentration (MIC) values ranging from 4 to 125 g/L. Specifically, the L. plantarum CECT 748 and L. plantarum CECT 749 CFS evidenced the highest antifungal activity against Fusarium and Aspergillus strains (Table 2). Furthermore, these CFS were the only ones that demonstrated fungicidal doses against Aspergillus strains, more precisely, the minimum fungicidal concentration (MFC) values were 125 and 62 g of CFS/L, respectively.
Analyzing the results, it is important to emphasize that the L. plantarum CECT 749 CFS was more efficient than others, showing the lowest concentration of MIC and MFC against all evaluated strains. Therefore, based on results, this CFS was employed in the biocontrol assays in order to avoid the growth of A. flavus ITEM 8111 on corn kernels and F. verticillioides CECT 2982 on corn ears.

2.2. Phenolic Acids Produced by L. plantarum spp.

In this study, nine phenolic acids were identified in MRS broth fermented by L. plantarum (Figure 1). These compounds were determined according to the retention time peak and molecular mass spectra obtained from the injected standard solution in LC-ESI-qTOF-MS and reported information in the literature. The phenolic acids produced by strains of L. plantarum are summarized in Table 3 along with their molecular formula and mass spectrum. Between the samples with the highest antifungal effect, the L. plantarum CECT 749 produced DL-3-phenyllactic acid, salicylic acid, and vanillin, whereas the same compounds were generated by L. plantarum CECT 748, in addition to chlorogenic acid, sinapic acid, and 1,2-dihydroxybenzene, and with the exception of vanillin.
Previous studies also identified phenolic acids produced by LAB in MRS broth. Rodrígues et al. noticed the presence of 1,2-dihydroxybenzene and other hydroxybenzoic acids such as vanillic acid, syringic acid, and gallic acid generated after hydrolyzation and methylation of hydroxybenzoic acid by enzymes of L. plantarum [38]. Brosnan et al. also identified phenolic acids for all the strains evaluated, more specifically, vanillic acid, 2-hydroxyisocapric acid, azelaic acid, decanoic acid, propanoic acid, 3-hydroxydecanoic acid, benzoic acid, hydrocinnamic acid, DL-p-hydroxyphenyllactic acid, phenyllactic acid, DL-β-hydroxylauric acid, 4-hydroxybenzoic acid, 3-4-hydroxy-3-methoxyphenyl, and 1,2-dihydroxybenzene [39]. Indeed, it is known that L. plantarum synthesizes phenolic acids by decarboxylation and/or reduction [40]. These compounds can act as chaotropic stressors, causing a disorder and cellular stress with the consequent lysis of the plasma membrane [41].
Some phenolic acids—above described—were earlier studied as antifungal compounds. Among them, the 1,2-dihydroxybenzene—often known as pyrocatechol or catechol—is commonly found in its bound form in foods as part of complex structures such as lignins and hydrolyzable tannins. In addition, this phenolic acid was previously described as an antifungal compound [38,42].
Silva et al. assessed the correlations between phenolic compounds and their ability to avoiding aflatoxin production on soybeans. They demonstrated that phenolic compounds such as vanillin were able to contribute to a defense mechanism against fungal spoilage and AFB1 production depending on the level of contamination [43]. In addition, Romero-Cortes et al. evaluated the antifungal activity of vanillin against Alternaria alternata isolated from sorghum and barley. The vanillin showed a fungicidal effect in a dose-dependent manner; moreover, doses lower than 750 mg/L of vanillin reduced the fungal growth, increasing the lag phase from 50 to 112 h [44].
Saladino et al. evaluated the antifungal activity of LAB strains against A. parasiticus. The authors described that the fermentation of bread dough with LAB reduced the fungal growth as well as the content of aflatoxins. They also attributed the effectiveness of LAB by phenolic compounds and bioactive peptides presented in the media and the lowering of pH [28]. Our results pointed out that the L. plantarum CECT 220, CECT 221 and CECT 748 showed the highest capacity to produce phenolic compounds. And, the other strains of L. plantarum produced at least two phenolic compounds. In addition, it is important to highlight that the phenolic acids identified in this study were in agreement with those that have been detected by other authors.
Despite the fact that the phenolic acids found in the CFS have previously been reported as antifungal compounds, the antifungal and antimycotoxigenic effects evidenced in our study could be attributed to the bio-complex obtained by L. plantarum MRS fermentation. This bio-complex could contain other metabolites such as proteins, peptides, and organic acids that are widely known as antifungal compounds but have not been identified in our study [28,33,45]. In other words, it seems that the presence of phenolic acids in the CFS only contributed to enhancing the antifungal activity of the bio-complex.

2.3. L. plantarum CECT 749 CFS Characteristics and Composition

L. plantarum CECT 749 was incubated on MRS Broth for 72 h at 37 °C. After that, the bacteria cells were separated from the liquid fraction by centrifugation and, the CFS was recovered as described in Section 4.3. The methodology and composition of L. plantarum CECT 749 CFS are plotted in Table 4. The organic acids and the final pH of the solution play an important role in mycelial growth [46]. Gerez et al. evaluated the antifungal activity of lactic acid, acetic acid, phenyllactic acid, and propionic acid against Aspergillus niger, Fusarium graminearum, and Penicillium spp. under pH 3.5 and 6.0. These authors reported that the lowest concentration of organic acid -necessary to produce a 50% inhibition of conidia germination after 48 h of incubation was significantly reduced in pH 3.5. For instance, the MIC of lactic acid at pH 3.5 ranged from 2.5 to 180 mM whereas in pH 6.0 the MIC ranged from 50 to 300 mM [46]. Our results corroborate with those since the pH of 3.3 ± 0.3, as well as the high content of lactic acid (15 g/L) could also contribute to the antifungal activity of the CFS.

2.4. Biopreservation and Shelf-Life Improvement by L. plantarum CECT 749 CFS

In addition to evaluating the qualitative and quantitative antifungal activity of CFS, the ability to enhance shelf life was investigated on corn kernels and corn ears. The shelf life was determined by the first sign of visual fungal growth in the matrices.
The fungal growth of the control group under similar storage conditions was noticed on corn kernels after seven days, whereas on corn ears the shelf life was determined on the fifth day onwards. Compared to control, the spray of L. plantarum CECT 749 CFS delayed the growth of both A. flavus and F. verticillioides CECT 2982 in eight and two days, respectively (Table 5). In addition, it is noteworthy that the samples of corn kernels and corn ears were treated, dried, and contaminated with final moisture content (MC) of 18 and 20%, respectively. Thus, the lower reduction in shelf life noticed on corn ears could be explained by the higher MC.
These results suggested that the CFS may be used as a biocontrol to reduce F. verticillioides growth on corn ears and A. flavus growth on corn kernels during storage, even under inappropriate MC condition.
Corn is a rich substrate for aflatoxin production and earlier reports demonstrated the effective use of antifungal properties of bioactive compounds produced by LAB for inhibiting AFB1 in various crops [51]. In our study, the L. plantarum CECT 749 CFS reduced the fungal growth, hence, the AFB1 production by 100% at day 5. In addition, applying the CFS spray on the surface of corn before contamination reduced the AFB1 production by 99.7 and 97.5% at days 25 and 40, respectively (Figure 2). According to visual FG analyses, the L. plantarum CECT 749 CFS did not avoid the AFB1 production, but this preventive treatment inhibited its production by 10 days.
The data related to FB1 production are plotted in Figure 2. The results showed that L. plantarum CECT 749 CFS possess antimycotoxigenic activity against F. verticillioides CECT 2982, reducing the FB1 production by 90.6% at day 7. However, it was realized that the antimycotoxigenic effect provoked by treatment decreased over time, reaching to 73.7% of reduction after 15 days of storage. The mycotoxin reduction, evidenced in this study, could be explained perhaps because the treatment with CFS delayed the fungal growth, hence, the fungi need more time to achieve the secondary metabolism.
Authors have noticed that LAB have the potential to either bind and mitigate mycotoxin or, to some extent, inhibit the fungal growth [52,53,54,55]. Although the LAB antimycotoxigenic mechanisms of action have not yet been explained, analyzing our data, it seems that they may be closely linked to the antifungal effects evidenced in this work. Damayanti et al. isolated twenty-eight LAB from cassava and bean fermentation. The LAB with the highest activities was L. plantarum G7 [56]. Its CFS extract showed inhibition of mycelial growth between 39–63.1%. Consequently, the aflatoxin content was reduced. In addition, Russo et al. investigated the antifungal capacity of eighty-eight L. plantarum strains [57]. They concluded that the employment of LAB increased shelf life. Although they had investigated the antifungal activity of CFS against toxigenic fungi, the mycotoxin content was not evaluated in the food samples.
Overall, the treatment did not completely avoid AFB1 and FB1 production, however, in both corn kernels and corn ears, the final concentration of mycotoxin was significantly reduced after fumigation of L. plantarum CECT 749 CFS compared to the control group. For instance, after incubation time, the final AFB1 and FB1 concentration in the treatment group was 6.9 and 20.1 ng/g, whereas the concentration of AFB1 and FB1 in the control group reached values of 278.4 and 75.4 ng/g, respectively.
On the one hand, despite the large reduction of AFB1 provoked by CFS application, the levels of AFB1 were higher than those set by the European Union (5 ng/g). On the other hand, the levels of AFB1 and FB1 were lower than those established by the FDA (20 ng/g of AFB1 and 2000 ng/g of FB1) to non-processed corn for human consumption [58,59,60].
The present results suggested that metabolism products of LAB, due to their potential to reduce the growth of the mycotoxigenic fungi and the biosynthesis of the mycotoxins, could be promising for the biocontrol of grains such as corn.
Corn grains are constantly stored for a long time before commercialization, further studies could be performed, increasing samples analysis time and setting the MC at a percentage slightly over 14% since this percentage is adequate for grain storage [61]. In addition, we expect to isolate the antifungal compounds produced by the L. plantarum CECT 749 and evaluate the purified fraction activity as well as to compare them to the whole CFS extract. In addition, it might be worthwhile to increase the experiment from a laboratory scale to an industrial scale in order to produce more compounds and to evaluate their constancy of production.

3. Conclusions

In the past, LAB have shown potential as antifungal agents to avoid fungal spoilage and the related mycotoxin production in foods such as dairy and fermented products. In this study, in vitro analyses have shown that Fusarium strains were more susceptibility to CFS treatment than Aspergillus spp. In terms of fungal growth and mycotoxin production in both corn kernel and corn ears, the CFS treatment did not completely inhibit either the fungal growth or mycotoxin production. Probably, high levels of antifungal compounds associated with lower MC might be required to completely avoid the growth of A. flavus and F. verticillioides on corn kernels and corn ears. In contrast, even when the mycotoxin production occurred, the content of FB1 and AFB1 was significantly reduced. Therefore, these results provide new insights for the biotechnological employment of L. plantarum CECT 749 CFS for biopreservation of corn kernels and corn ears.

4. Materials and Methods

4.1. Chemicals

AFB1 and FB1 standard solutions (purity > 99%) were purchased from Sigma-Aldrich (St. Louis, MO, USA). The phenolic compounds gallic acid, sinapic acid, chlorogenic acid, caffeic acid, syringic acid, vanillin, vanillic acid, hydroxybenzoic acid, hydroxylcinnamic acid, p-coumaric acid, benzoic acid, DL-3-phenyllactic acid, 1,2-dihydroxybenzene, 3,4-dihydroxyhydrocinnamic, and DL-p-hydroxyphenyllatic acid were provided from Sigma-Aldrich (St. Louis, MO, USA). Phenyllactic acid was obtained from BaChem (Weil am Rhein, Germany). Ferulic acid was purchased from MP Biomedicals (Santa Ana, CA, USA) and protocatechuic acid from HWI pharma services (Ruelzheim, Germany). Acetonitrile (ACN) (99%), methanol (99%), ethyl acetate (EA) (99%) and formic acid (FA) (99%) used for liquid chromatography were of HPLC-grade and obtained from VWR Chemicals (Radnor, PA, USA). Magnesium sulfate (MgSO4), ammonium formate and sodium chloride (NaCl) were obtained from Sigma-Aldrich (St. Louis, MO, USA). SepraTM C18-E (50 μm, 65 Å) was purchased from Phenomenex (Madrid, Spain). Microbiological media such as potato dextrose broth (PDB), potato dextrose agar (PDA), Man Rogosa Sharpe (MRS) broth and MRS Agar were obtained from Liofilchem Bacteriology Products (Roseto degli Abruzzi, Italy). Deionized water (<18 MΩ cm resistivity) was obtained from a Milli-Q purification system (Millipore, Bedford, MA, USA).

4.2. Microorganisms and Culture Conditions

Fungal strains A. parasiticus CECT 2681, A. niger CECT 2088, F. verticillioides CECT 20926, F. verticillioides CECT 2152, F. verticillioides CECT 2982, F. cerealis CECT 20488, F. cerealis CECT 20489, F. mesoamericanum CECT 20490, and F. poae CECT 20,165 were obtained from the Spanish Type Culture Collection CECT (Valencia, Spain). F. graminearum ITEM 126, F. graminearum ITEM 6415 and A. flavus ITEM 8111 were obtained from the microbial culture collection of the Institute of Sciences of Food Production, ISPA (Bari, Italy). These microorganisms were maintained in sterile glycerol (30%) at −80 °C prior to analysis. The fungal strains were cultivated on PDB, transferring 1 mL of the glycerinated solution to 9 mL of PDB medium. The contaminated PDB was incubated for 72 h at 25 °C, and then, aliquots were plated on PDA Petri dishes in order to obtain spores. These spores were used to contaminate the corn samples.
LAB strains Lactobacillus plantarum CECT 220, L. plantarum CECT 221, L. plantarum CECT 223, L. plantarum CECT 224, L. plantarum CECT 748, L. plantarum CECT 749 and L. plantarum CECT 750 were obtained from the Spanish Type Culture Collection CECT (Valencia, Spain). The LAB were kept in frozen glycerol (3%) stocks at −80 °C until analysis. Prior to fermentation assays, 1 mL of LAB glycerinated was homogenized with 9 mL of MRS Broth culture medium and incubated under anaerobic conditions for 48 h at 37 °C.

4.3. LAB Growth and Preparation of Cell-Free Cupernatant

LAB were incubated on MRS Broth for 12 h at 37 °C in order to reach the exponential growth phase. Then, 10 mL of incubated MRS Broth at a concentration of 107 CFU/mL were placed in other Falcon tubes containing 40 mL of sterile MRS Broth. Subsequently, the tubes were incubated under anaerobic conditions for 72 h at 37 °C to allow for MRS fermentation. After that, LAB cells were separated from the fermented solution by centrifugation at 4000× g for 10 min. Lastly, cell-free supernatants (CFS) were recovered and freeze at −80 °C for 24 h before drying with a lyophilizer FreeZone 2.5 L Labconco (Kansas, MO, USA). The lyophilized CFS was stored at −18 °C prior to antifungal analyses.

4.4. Qualitative Antifungal Activity in Solid Medium

The antifungal effect of lyophilized CFS was evaluated towards strains of Aspergillus and Fusarium genera.
First, Petri dishes containing PDA were contaminated with harvested fungal conidia previously cultivated on PDA plates, as described by Section 4.2. The conidia were scraped from agar and dispersed on another PDA plate, using sterile cotton swabs. Briefly, 10 mm diameter wells were made using sterile pipette tips, whereas each well was filled with 50 µL of lyophilized CFS which was previously resuspended in sterile water at the concentration of 250 g/L. A sterile water solution containing lyophilized MRS Broth was used as negative control. After that, the PDA plates were incubated for 72 h at 25 °C to allow the fungal growth and diffusion of the CFS through agar. Finally, the antifungal effect was determined by measuring the inhibition zone around the well. The treatments which showed an inhibition zone larger than 7 mm between the well and fungal growth were considered positive for antifungal activity [62].

4.5. Quantitative Antifungal Activity in 96-Well Microplates

The quantitative assay was performed as described by the guidelines in CLSI document M38-A2 with slight modifications [63]. First, 100 μL of PDB containing lyophilized CFS at concentrations from 0.48 to 500 g/L was added to 96-well sterile microplates. Then, 100 μL of PDB containing 5 × 103 conidia of toxigenic fungi were added to each well. The positive control consisted of contaminated PDB medium with lyophilized non-fermented CFS (250 g/L) and the negative control was prepared with a non-contaminated PDB medium without any treatment. Posteriorly, the microplates were incubated at 25 °C for 3 days.
The MIC was defined as the lowest concentration of the fermented CFS that did not show any visible growth. Four replicates of each treatment were carried out. After that, 10 μL of the concentration corresponding to the MIC and higher concentrations evaluated were recultivated on PDA plates for the determination of the MFC. Plates were incubated at 25 °C for 72 h and the MFC was determined as the concentration that avoided any visible fungal growth.

4.6. Extraction and Identification of Phenolic Acids by LC-ESI-qTOF-MS

The CFS extracts were cleared by QuEChERS methodology prior to chromatographic analysis as described by Brosnan et al. [64]. Thus, ten milliliters of fermented CFS were extracted with 10 mL ethyl acetate 1% formic acid, 4 g of MgSO4, 1 g of NaCl and then vortexed for 1 min. The extract was centrifuged at 4000× g for 10 min, and the supernatant was recovered in a Falcon tube containing 150 mg of C18 and 900 mg MgSO4. The extraction was realized twice and the supernatant was evaporated under nitrogen flow. Afterward, the dried supernatant was resuspended in 1 mL of H2O: ACN (90:10) prior to chromatographic analysis.
The LC system used for the chromatographic determination was an Agilent 1200 (California, USA) equipped with a vacuum degasser, autosampler, and binary pump. The stationary phase was a Phenomenex column (Gemini C18 50 × 2 mm, 100 Å and particle size of 3 μm). Mobile phases consisted of water as solvent A, ACN as solvent B both acidified (0.1% formic acid) and the gradient elution was established as follows: 0 min, 5% B; 30 min 95% B; 35 min, 5% B. The column was equilibrated for 3 min prior to analyses. The flow rate used was 0.3 mL/min and the sample volume injected was 20 μL.
Mass spectrometry analysis was carried out using a Q-TOF-MS (6540 Agilent Ultra High Definition Accurate Mass) equipped with an Agilent Dual Jet Stream electrospray ionization (Dual AJS ESI) with interface in negative ionization mode at the following conditions: drying gas flow (N2), 8.0 L/min; nebulizer pressure at 30 psig; gas drying temperature at 350 °C; capillary voltage at 3.5 kV; fragmentor voltage and scan range were 175 V and m/z 20–380, respectively. Targeted MS/MS experiments were carried out using collision energy of 10, 20 and 40 eV. Integration and data elaboration were realized using Masshunter Qualitative Analysis Software B.08.00 [65].

4.7. Biopreservation of Corn Kernels and Corn Ears

To evaluate the antifungal and antimycotoxigenic activity of the CFS by L. plantarum CECT 749, the study was carried out using corn kernels contaminated with A. flavus ISPA 8111 (AFB1 producer) and corn ears contaminated with F. verticillioides CECT 2982 (FB1 producer). These strains were selected according to the fungal sensitivity to fermented CFS—demonstrated by qualitative and quantitative assays (Section 4.4 and Section 4.5); the main steps of food production chain in which the fungal contamination occurs; and the mycotoxin production—previously determined in corn and corn ears.
The biopreservation test was performed in laboratory scale silos as described by Nazareth et al. with modifications [60].
Samples of corn kernels (50 g) were divided into two groups: a group was sprayed with 10 mL of lyophilized CFS in order to obtain a final concentration of 12.5 mg of CFS/g of corn, and a control group was sprayed with 10 mL of sterile water (Figure 3). Next, the corn kernels were dried in an incubator (Memmert D06061 Modell 500; Memmert GmbH + Co. KG, Schwabach, Germany) at 50 °C for 30 min. Then, both groups were inoculated with suspensions containing 1 mL of A. flavus ISPA 8111 at 103 conidia/g. Lastly, the sampling was performed on days 0, 7, 15, 40 to determine the AFB1 production.
Similarly, 200 g of corn ears were treated with 6 mL of CFS equivalent to a concentration of 1.6 mg of lyophilized CFS/g of corn ears. In this case, corn ears were contaminated with 1 mL of F. verticillioides CECT 2982 suspension at a concentration of 103 conidia/g. Further, the FB1 production was determined on days 0, 7 and 15. Moreover, visual fungal growth was monitored daily in both studies. In addition, samples were placed in the incubator at 105 °C for 24 h and the initial MC was measured by gravimetric methodology [66].

4.8. Determination of Mycotoxins by LC-MS/MS Spectrometry

AFB1 and FB1 mycotoxins were extracted using the method described and validated by Quiles et al. [67]. Corn kernels were ground with an Oester Classic grinder (Madrid, Spain) in order to reduce particle size. Corn ears were frozen at −80 °C and lyophilized before grinding. The samples were weighed in 5 g, placed in a Falcon tube with 25 mL of MeOH, and homogenized for 3 min using an Ultra Ika T18 basic ultraturrax (Staufen, Germany). Following this, the extract was centrifuged at 4000× g for 15 min at 4 °C, and the supernatant was evaporated to dryness with Büchi Rotavapor R-200 (Postfach, Switzerland). Finally, the dried extracts were resuspended in 2 mL of methanol and filtered in 0.22 µm before LC-MS/MS analysis.
The liquid-chromatography system consisted of an LC-20AD pump coupled to a 3200QTRAP mass spectrometer (Applied Biosystems, Foster City, CA, USA) using an ESI interface in positive ion mode. The mycotoxins were separated on a Gemini NX C18 column 150 × 2 mm × 3 µm Phenomenex (Palo Alto, CA, USA). The mobile phases were the solvent A (5 mM ammonium formate and 0.1% formic acid in water) and solvent B (5 mM ammonium formate and 0.1% formic acid in methanol) at a flow rate of 0.25 mL/min. The elution was carried out using a linear gradient from 0 to 14 min. The injection volume set was 20 µL, the nebulizer, the auxiliary and the auxiliary gas were set at 55, 50, and 15 psi respectively. The capillary temperature and the ion spray voltage were 550 °C and 5500 V, respectively. The ions transitions used for the mycotoxins identification and quantification were: m/z 313.1, 241.3, and 284.9 for AFB1, m/z 352.4 and 334.4 for FB1.

4.9. Statistical Analysis

The software Prism version 3.0 (GraphPad, La Jolla, CA, USA) for Windows was used for the statistical analysis of data. The experiments were realized in triplicates and the difference between control and treated group was analyzed by Student’s t-test. The level of significance was considered as p ≤ 0.05.

Author Contributions

Conceptualization, The authors (T.d.M.N. and C.L.) consider that the first two authors should be considered as joint first authors. F.B.L., J.M., and G.M. conceived and proposed the idea; T.d.M.N. and C.L. performed the experiment and analyzed the data; T.d.M.N., C.L., and R.T. wrote the first draft of the manuscript; T.d.M.N., J.M.Q. and R.T. reviewed and edited the manuscript; T.d.M.N., C.L., R.T., and J.M.Q. contributed to the writing of the final version; F.B.L., J.M., and G.M. read and approved the paper final version. All authors have read and agreed to the published version of the manuscript.

Funding

The research was funded by the European Project (H2020-Research and Innovation Action) MycoKey “Integrated and innovative key actions for mycotoxin management in the food and feed chain”, grant number GA 678781”; the Spanish Ministry of Economy and Competitiveness, grant number AGL2016-77610R; the project Prometeo of Generalitat Valenciana, grant number 2018/126; the Ph.D. program of the Spanish Ministry of Science, Innovation and Universities, grant number FPU17/06104; and the Brazilian National Council for Scientific and Technological Development CNPq, grant number 400896/2014-1.

Acknowledgments

The authors would like to thank the scholarship support from the Ph.D. program of the University of Valencia (Atracció de Talent); the Spanish Ministry of Science, Innovation and Universities; and the Brazilian National Council for Scientific and Technological Development (CNPq).

Conflicts of Interest

The authors declare no conflicts of interest.

References

  1. Alshannaq, A.; Yu, J.H. Occurrence, toxicity and analysis of major mycotoxins in food. Int. J. Environ. Res. Public Health 2017, 14, 632. [Google Scholar] [CrossRef] [Green Version]
  2. Fleurat-Lessard, F. Integrated management of the risks of stored grain spoilage by seedborne fungi and contamination by storage mould mycotoxins—An update. J. Stored Prod. Res. 2017, 71, 22–40. [Google Scholar] [CrossRef]
  3. Gonçalves, B.L.; Coppa, C.F.S.C.; de Neeff, D.V.; Corassin, C.H.; Oliveira, C.A.F. Mycotoxins in fruits and fruit-based products: Occurrence and methods for decontamination. Toxin Rev. 2019, 38, 263–272. [Google Scholar] [CrossRef]
  4. Mditshwa, A.; Magwaza, L.S.; Tesfay, S.Z.; Mbili, N. Postharvest quality and composition of organically and conventionally produced fruits: A review. Sci. Hortic. 2017, 216, 148–159. [Google Scholar] [CrossRef]
  5. Azaiez, I.; Font, G.; Mañes, J.; Fernández-Franzón, M. Survey of mycotoxins in dates and dried fruits from Tunisian and Spanish markets. Food Control 2015, 51, 340–346. [Google Scholar] [CrossRef]
  6. Pereira, C.S.; Cunha, S.C.; Fernandes, J.O. Prevalent mycotoxins in animal feed: Occurrence and analytical methods. Toxins 2019, 11, 290. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  7. Pizzolato Montanha, F.; Anater, A.; Burchard, J.F.; Luciano, F.B.; Meca, G.; Manyes, L.; Pimpão, C.T. Mycotoxins in dry-cured meats: A review. Food Chem. Toxicol. 2018, 111, 494–502. [Google Scholar] [CrossRef] [PubMed]
  8. Filtenborg, O.; Frisvad, J.C.; Thrane, U. Moulds in food spoilage. Int. J. Food Microbiol. 1996, 33, 85–102. [Google Scholar] [CrossRef]
  9. Torrijos, R.; Nazareth, T.M.; Pérez, J.; Mañes, J.; Meca, G. Development of a bioactive sauce based on oriental mustard flour with antifungal properties for PITA bread shelf life improvement. Molecules 2019, 24, 1019. [Google Scholar] [CrossRef] [Green Version]
  10. Giorni, P.; Bertuzzi, T.; Battilani, P. Impact of fungi co-occurrence on mycotoxin contamination in maize during the growing season. Front. Microbiol. 2019, 10, 1265. [Google Scholar] [CrossRef]
  11. Marin, S.; Ramos, A.J.; Cano-Sancho, G.; Sanchis, V. Mycotoxins: Occurrence, toxicology and exposure assessment. Food Chem. Toxicol. 2013, 60, 218–237. [Google Scholar] [CrossRef]
  12. Alonso, V.A.; Pereyra, C.M.; Keller, L.A.M.; Dalcero, A.M.; Rosa, C.A.R.; Chiacchiera, S.M.; Cavaglieri, L.R. Fungi and mycotoxins in silage: An overview. J. Appl. Microbiol. 2013, 115, 637–643. [Google Scholar] [CrossRef]
  13. Reddy, K.R.N.; Salleh, B.; Saad, B.; Abbas, H.K.; Abel, C.A.; Shier, W.T. An overview of mycotoxin contamination in foods and its implications for human health. Toxin Rev. 2010, 29, 3–26. [Google Scholar] [CrossRef]
  14. Zain, M.E. Impact of mycotoxins on humans and animals. J. Saudi Chem. Soc. 2011, 15, 129–144. [Google Scholar] [CrossRef] [Green Version]
  15. Degraeve, S.; Madege, R.R.; Audenaert, K.; Kamala, A.; Ortiz, J.; Kimanya, M.; Tiisekwa, B.; De Meulenaer, B.; Haesaert, G. Impact of local pre-harvest management practices in maize on the occurrence of Fusarium species and associated mycotoxins in two agro-ecosystems in Tanzania. Food Control 2015, 59, 225–233. [Google Scholar] [CrossRef]
  16. Jackson, L.S.; Katta, S.K.; Fingerhut, D.D.; De Vries, J.W.; Bullerman, L.B. Effects of Baking and Frying on the Fumonisin B1 Content of Corn-Based Foods. J. Agric. Food Chem. 1997, 45, 4800–4805. [Google Scholar] [CrossRef]
  17. Magan, N.; Medina, A. Integrating gene expression, ecology and mycotoxin production by Fusarium and Aspergillus species in relation to interacting environmental factors. World Mycotoxin J. 2016, 9, 673–684. [Google Scholar] [CrossRef] [Green Version]
  18. Paterson, R.R.M.; Lima, N. Thermophilic fungi to dominate aflatoxigenic/mycotoxigenic fungi on food under global warming. Int. J. Environ. Res. Public Health 2017, 14, 199. [Google Scholar] [CrossRef] [Green Version]
  19. Kabak, B.; Dobson, A.D.W.; Var, I. Strategies to prevent mycotoxin contamination of food and animal feed: A review. Crit. Rev. Food Sci. Nutr. 2006, 46, 593–619. [Google Scholar] [CrossRef]
  20. Lee, H.J.; Ryu, D. Worldwide Occurrence of Mycotoxins in Cereals and Cereal-Derived Food Products: Public Health Perspectives of Their Co-occurrence. J. Agric. Food Chem. 2017, 65, 7034–7051. [Google Scholar] [CrossRef]
  21. Eskola, M.; Kos, G.; Elliott, C.T.; Hajšlová, J.; Mayar, S.; Krska, R. Worldwide contamination of food-crops with mycotoxins: Validity of the widely cited ‘FAO estimate’ of 25%. Crit. Rev. Food Sci. Nutr. 2019, 1–17. [Google Scholar] [CrossRef] [PubMed]
  22. Thanushree, M.P.; Sailendri, D.; Yoha, K.S.; Moses, J.A.; Anandharamakrishnan, C. Mycotoxin contamination in food: An exposition on spices. Trends Food Sci. Technol. 2019, 93, 69–80. [Google Scholar] [CrossRef]
  23. Stockmann-Juvala, H.; Savolainen, K. A review of the toxic effects and mechanisms of action of fumonisin B 1. Hum. Exp. Toxicol. 2008, 27, 799–809. [Google Scholar] [CrossRef] [PubMed]
  24. Kamle, M.; Mahato, D.K.; Devi, S.; Lee, K.E.; Kang, S.G.; Kumar, P. Human Health and their Management Strategies. Toxins 2019, 11, 328. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  25. International Agency for Research on Cancer. IARC Monographs on the Evaluation of Carcinogenic Risks to Humans. Available online: https://monographs.iarc.fr/wp-content/uploads/2018/06/mono82.pdf (accessed on 31 December 2019).
  26. Stanojević-Nikolić, S.; Dimić, G.; Mojović, L.; Pejin, J.; Djukić-Vuković, A.; Kocić-Tanackov, S. Antimicrobial Activity of Lactic Acid Against Pathogen and Spoilage Microorganisms. J. Food Process. Preserv. 2016, 40, 990–998. [Google Scholar] [CrossRef]
  27. Tajkarimi, M.M.; Ibrahim, S.A.; Cliver, D.O. Antimicrobial herb and spice compounds in food. Food Control 2010, 21, 1199–1218. [Google Scholar] [CrossRef]
  28. Saladino, F.; Luz, C.; Manyes, L.; Fernández-Franzón, M.; Meca, G. In vitro antifungal activity of lactic acid bacteria against mycotoxigenic fungi and their application in loaf bread shelf life improvement. Food Control 2016, 67, 273–277. [Google Scholar] [CrossRef]
  29. Niku-Paavola, M.L.; Laitila, A.; Mattila-Sandholm, T.; Haikara, A. New types of antimicrobial compounds produced by Lactobacillus plantarum. J. Appl. Microbiol. 1999, 86, 29–35. [Google Scholar] [CrossRef]
  30. Ndagano, D.; Lamoureux, T.; Dortu, C.; Vandermoten, S.; Thonart, P. Antifungal Activity of 2 Lactic Acid Bacteria of the Weissella Genus Isolated from Food. J. Food Sci. 2011, 76, M305–M311. [Google Scholar] [CrossRef]
  31. Broberg, A.; Jacobsson, K.; Ström, K.; Schnürer, J. Metabolite profiles of lactic acid bacteria in grass silage. Appl. Environ. Microbiol. 2007, 73, 5547–5552. [Google Scholar] [CrossRef] [Green Version]
  32. Schnürer, J.; Magnusson, J. Antifungal lactic acid bacteria as biopreservatives. Trends Food Sci. Technol. 2005, 16, 70–78. [Google Scholar] [CrossRef]
  33. Corrêa, J.A.F.; Evangelista, A.G.; de Melo Nazareth, T.; Luciano, F.B. Fundamentals on the molecular mechanism of action of antimicrobial peptides. Materialia 2019, 8, 100494. [Google Scholar] [CrossRef]
  34. Sadiq, F.A.; Yan, B.; Tian, F.; Zhao, J.; Zhang, H.; Chen, W. Lactic Acid Bacteria as Antifungal and Anti-Mycotoxigenic Agents: A Comprehensive Review. Compr. Rev. Food Sci. Food Saf. 2019, 18, 1403–1436. [Google Scholar] [CrossRef] [Green Version]
  35. Ghanbari, M.; Jami, M.; Domig, K.J.; Kneifel, W. Seafood biopreservation by lactic acid bacteria—A review. LWT Food Sci. Technol. 2013, 54, 315–324. [Google Scholar] [CrossRef]
  36. Sanders, M.E.; Akkermans, L.M.A.; Haller, D.; Hammerman, C.; Heimbach, J.; Hörmannsperger, G.; Huys, G.; Levy, D.D.; Lutgendorff, F.; Mack, D.; et al. Safety assessment of probiotics for human use. Gut Microbes 2010, 1, 1–22. [Google Scholar] [CrossRef] [PubMed]
  37. Leroy, F.; De Vuyst, L. Lactic acid bacteria as functional starter cultures for the food fermentation industry. Trends Food Sci. Technol. 2004, 15, 67–78. [Google Scholar] [CrossRef]
  38. Rodríguez, H.; Landete, J.M.; de las Rivas, B.; Muñoz, R. Metabolism of food phenolic acids by Lactobacillus plantarum CECT 748T. Food Chem. 2008, 107, 1393–1398. [Google Scholar] [CrossRef] [Green Version]
  39. Brosnan, B.; Coffey, A.; Arendt, E.K.; Furey, A. Rapid identification, by use of the LTQ Orbitrap hybrid FT mass spectrometer, of antifungal compounds produced by lactic acid bacteria. Anal. Bioanal. Chem. 2012, 403, 2983–2995. [Google Scholar] [CrossRef]
  40. Sánchez-Maldonado, A.F.; Schieber, A.; Gänzle, M.G. Structure-function relationships of the antibacterial activity of phenolic acids and their metabolism by lactic acid bacteria. J. Appl. Microbiol. 2011, 111, 1176–1184. [Google Scholar] [CrossRef]
  41. Cray, J.A.; Stevenson, A.; Ball, P.; Bankar, S.B.; Eleutherio, E.C.A.; Ezeji, T.C.; Singhal, R.S.; Thevelein, J.M.; Timson, D.J.; Hallsworth, J.E. Chaotropicity: A key factor in product tolerance of biofuel-producing microorganisms. Curr. Opin. Biotechnol. 2015, 33, 228–259. [Google Scholar] [CrossRef]
  42. Le Lay, C.; Coton, E.; Le Blay, G.; Chobert, J.M.; Haertlé, T.; Choiset, Y.; Van Long, N.N.; Meslet-Cladière, L.; Mounier, J. Identification and quantification of antifungal compounds produced by lactic acid bacteria and propionibacteria. Int. J. Food Microbiol. 2016, 239, 79–85. [Google Scholar] [CrossRef] [PubMed]
  43. Silva, B.; Souza, M.M.; Badiale-Furlong, E. Antioxidant and antifungal activity of phenolic compounds and their relation with aflatoxin B1 occurrence in soybeans (Glycine max L.). J. Sci. Food Agric. 2019. [Google Scholar] [CrossRef] [PubMed]
  44. Romero-Cortes, T.; Pérez España, V.H.; López Pérez, P.A.; Rodríguez-Jimenes, G.D.C.; Robles-Olvera, V.J.; Aparicio Burgos, J.E.; Cuervo-Parra, J.A. Antifungal activity of vanilla juice and vanillin against Alternaria alternate. CyTA J. Food 2019, 17, 375–383. [Google Scholar] [CrossRef] [Green Version]
  45. Luz, C.; Izzo, L.; Ritieni, A.; Mañes, J.; Meca, G. Antifungal and antimycotoxigenic activity of hydrolyzed goat whey on Penicillium spp: An application as biopreservation agent in pita bread. LWT 2020, 118, 108717. [Google Scholar] [CrossRef]
  46. Gerez, C.L.; Torino, M.I.; Rollán, G.; Font de Valdez, G. Prevention of bread mould spoilage by using lactic acid bacteria with antifungal properties. Food Control 2009, 20, 144–148. [Google Scholar] [CrossRef]
  47. Willits, C.O. Methods for Determination of Moisture-Oven Drying. Anal. Chem. 1951, 23, 1058–1062. [Google Scholar] [CrossRef]
  48. Reiners, W.A.; Reiners, N.M. Comparison of Oxygen-Bomb Combustion with Standard Ignition Techniques for Determining Total Ash. Ecology 1972, 53, 132–136. [Google Scholar] [CrossRef]
  49. Miloski, K.; Wallace, K.; Fenger, A.; Schneider, E.; Bendinskas, K. Comparison of Biochemical and Chemical Digestion and Detection Methods for Carbohydrates. Am. J. Undergrad. Res. 2008, 7, 7–18. [Google Scholar] [CrossRef]
  50. Nuryana, I.; Andriani, A.; Lisdiyanti, P. Analysis of organic acids produced by lactic acid bacteria. IOP Conf. Ser. Earth Environ. Sci. 2019, 251, 012054. [Google Scholar] [CrossRef]
  51. Reddy, K.R.N.; Reddy, C.S.; Muralidharan, K. Potential of botanicals and biocontrol agents on growth and aflatoxin production by Aspergillus flavus infecting rice grains. Food Control 2009, 20, 173–178. [Google Scholar] [CrossRef]
  52. Ahlberg, S.H.; Joutsjoki, V.; Korhonen, H.J. Potential of lactic acid bacteria in aflatoxin risk mitigation. Int. J. Food Microbiol. 2015, 207, 87–102. [Google Scholar] [CrossRef] [PubMed]
  53. Haskard, C.A.; El-Nezami, H.S.; Kankaanpää, P.E.; Salminen, S.; Ahokas, J.T. Surface Binding of Aflatoxin B 1 by Lactic Acid Bacteria. Appl. Environ. Microbiol. 2001, 67, 3086–3091. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  54. Niderkorn, V.; Boudra, H.; Morgavi, D.P. Binding of Fusarium mycotoxins by fermentative bacteria in vitro. J. Appl. Microbiol. 2006, 101, 849–856. [Google Scholar] [CrossRef] [PubMed]
  55. Juodeikiene, G.; Bartkiene, E.; Cernauskas, D.; Cizeikiene, D.; Zadeike, D.; Lele, V.; Bartkevics, V. Antifungal activity of lactic acid bacteria and their application for Fusarium mycotoxin reduction in malting wheat grains. LWT Food Sci. Technol. 2018, 89, 307–314. [Google Scholar] [CrossRef]
  56. Damayanti, E.; Indriati, R.; Sembiring, L.; Julendra, H. Antifungal Activities of Lactic Acid Bacteria against Aspergillus flavus, A. parasiticus and enicillium citrinum as Mycotoxin Producing Fungi. In Proceedings of the 16th AAAP Animal Science Congress, Yogyakarta, Indonesia, 10–14 November 2014; Volume 3, pp. 1742–1745. [Google Scholar]
  57. Russo, P.; Arena, M.P.; Fiocco, D.; Capozzi, V.; Drider, D.; Spano, G. Lactobacillus plantarum with broad antifungal activity: A promising approach to increase safety and shelf-life of cereal-based products. Int. J. Food Microbiol. 2017, 247, 48–54. [Google Scholar] [CrossRef]
  58. European Commission. Commission Regulation (EC) No 401/2006 laying down the methods of sampling and analysis for the official control of the levels of mycotoxins in foodstuffs. Off. J. Eur Union 2006, 70, 12–34. [Google Scholar]
  59. Dohlman, E. Mycotoxin Hazards and Regulations. Available online: https://www.ers.usda.gov/webdocs/publications/41603/15640_aer828h_1_.pdf?v=42055 (accessed on 31 December 2019).
  60. Nazareth, T.M.; Corrêa, J.A.F.; Pinto, A.C.S.M.; Palma, J.B.; Meca, G.; Bordin, K.; Luciano, F.B. Evaluation of gaseous allyl isothiocyanate against the growth of mycotoxigenic fungi and mycotoxin production in corn stored for 6 months. J. Sci. Food Agric. 2018, 98, 5235–5241. [Google Scholar] [CrossRef]
  61. Suleiman, R.A.; Rosentrater, K.A.; Bern, C.J. Effects of Deterioration Parameters on Storage of Maize: A Review. J. Nat. Sci. Res. 2013, 3, 147–165. [Google Scholar]
  62. Varsha, K.K.; Priya, S.; Devendra, L.; Nampoothiri, K.M. Control of spoilage fungi by protective lactic acid bacteria displaying probiotic properties. Appl. Biochem. Biotechnol. 2014, 172, 3402–3413. [Google Scholar] [CrossRef]
  63. Clinical and Laboratory Standards Institute. Reference Method for Broth Dilution Antifungal Susceptibility Testing of fi Lamentous Fungi; Approved Standard CLSI Document M38-A2; Clinical and Laboratory Standards Institute, WayneCLS: Wayne, PA, USA, 2008. [Google Scholar]
  64. Brosnan, B.; Coffey, A.; Arendt, E.K.; Furey, A. The QuEChERS approach in a novel application for the identification of antifungal compounds produced by lactic acid bacteria cultures. Talanta 2014, 129, 364–373. [Google Scholar] [CrossRef]
  65. Denardi-Souza, T.; Luz, C.; Mañes, J.; Badiale-Furlong, E.; Meca, G. Antifungal effect of phenolic extract of fermented rice bran with Rhizopus oryzae and its potential use in loaf bread shelf life extension. J. Sci. Food Agric. 2018, 98, 5011–5018. [Google Scholar] [CrossRef] [PubMed]
  66. Nazareth, T.D.M.; Quiles, J.M.; Torrijos, R.; Luciano, F.B.; Mañes, J.; Meca, G. Antifungal and antimycotoxigenic activity of allyl isothiocyanate on barley under different storage conditions. LWT 2019, 112, 108237. [Google Scholar] [CrossRef]
  67. Quiles, J.M.; Nazareth, T.d.M.; Luz, C.; Luciano, F.B.; Mañes, J.; Meca, G. Development of an antifungal and antimycotoxigenic device containing allyl isothiocyanate for silo fumigation. Toxins 2019, 11, 137. [Google Scholar] [CrossRef] [PubMed] [Green Version]
Toxins 12 00021 g001 550
Figure 1. Chemical structures and molecular weight of the phenolic acids identified in the L. plantarum cell-free supernatant (CFS): (a) gallic acid; (b) protocatechuic; (c) chlorogenic acid; (d) vanillin; (e) p-coumaric acid; (f) salicylic acid; (g) sinapic acid; (h) phenyllactic acid; (i) 1,2-dihydroxybenzene; MW, molecular weight in g/mol.
Figure 1. Chemical structures and molecular weight of the phenolic acids identified in the L. plantarum cell-free supernatant (CFS): (a) gallic acid; (b) protocatechuic; (c) chlorogenic acid; (d) vanillin; (e) p-coumaric acid; (f) salicylic acid; (g) sinapic acid; (h) phenyllactic acid; (i) 1,2-dihydroxybenzene; MW, molecular weight in g/mol.
Toxins 12 00021 g001
Toxins 12 00021 g002 550
Figure 2. Effect of L. plantarum CECT 749 CFS on mycotoxin production: (a) AFB1 content (ng/g) in corn kernels contaminated with A. flavus ITEM 8111 at different storage times (0, 10, 25 and 40 days). Control samples (dark grey) and treated samples (clear grey); (b) FB1 content (ng/g) in corn ears contaminated with Fusarium verticillioides CECT 2982 at different storage times (0, 7 and 15 days). Control samples (dark grey) and treated samples (clear grey). (*) Represents a significant difference among the treatments (p ≤ 0.05). The experiment was carried out twice with analyses in triplicate (n = 6).
Figure 2. Effect of L. plantarum CECT 749 CFS on mycotoxin production: (a) AFB1 content (ng/g) in corn kernels contaminated with A. flavus ITEM 8111 at different storage times (0, 10, 25 and 40 days). Control samples (dark grey) and treated samples (clear grey); (b) FB1 content (ng/g) in corn ears contaminated with Fusarium verticillioides CECT 2982 at different storage times (0, 7 and 15 days). Control samples (dark grey) and treated samples (clear grey). (*) Represents a significant difference among the treatments (p ≤ 0.05). The experiment was carried out twice with analyses in triplicate (n = 6).
Toxins 12 00021 g002
Toxins 12 00021 g003 550
Figure 3. Biopreservation test of corn ears and corn kernels in a lab system. The samples were treated with Lactobacillus plantarum CECT 749 cell-free supernatant. After drying, corn kernels were contaminated with Aspergillus flavus ISPA 8111 and corn ears were contaminated with Fusarium verticillioides CECT 2982.
Figure 3. Biopreservation test of corn ears and corn kernels in a lab system. The samples were treated with Lactobacillus plantarum CECT 749 cell-free supernatant. After drying, corn kernels were contaminated with Aspergillus flavus ISPA 8111 and corn ears were contaminated with Fusarium verticillioides CECT 2982.
Toxins 12 00021 g003
Table
Table 1. Antifungal activity evaluated in potato dextrose agar (PDA) solid medium and treated with Lactobacillus plantarum cell-free supernatant (CFS) at 250 g/L against toxigenic fungi of Aspergillus and Fusarium genera. The antifungal activity was expressed as follows: (+) means 8 mm of inhibition zone between the well and fungal growth, (+ +) means 8–10 mm of inhibition zone between the well and fungal growth, (+ + +) means > 10 mm of inhibition zone between the well and fungal growth.
Table 1. Antifungal activity evaluated in potato dextrose agar (PDA) solid medium and treated with Lactobacillus plantarum cell-free supernatant (CFS) at 250 g/L against toxigenic fungi of Aspergillus and Fusarium genera. The antifungal activity was expressed as follows: (+) means 8 mm of inhibition zone between the well and fungal growth, (+ +) means 8–10 mm of inhibition zone between the well and fungal growth, (+ + +) means > 10 mm of inhibition zone between the well and fungal growth.
Fungal StrainL. plantarum
CECT 220CECT 221CECT 223CECT 224CECT 748CECT 749CECT 750
F. graminearum
ITEM 126		++++++ + ++
F. graminearum
ITEM 6415		+++++++
F. cerealis
CECT 20488		+++++++
F. cerealis
CECT 20489		+++ +++++
F. verticillioides
CECT 20926		+++++ ++ + ++
F. verticillioides
CECT 2152		+ +++ +++ ++ + ++ +
F. verticillioides
CECT 2982		+ ++ ++ +++ ++ + ++
F. mesoamericanum
CECT 20490		+++++++
F. poae
CECT 20165		+++++++
A. flavus
ITEM 8111		++++++ ++
A. parasiticus
CECT 2681		−−−−++−
A. niger
CECT 2088		−+−−+++
Table
Table 2. Minimum inhibitory concentration (MIC) and minimum fungicidal concentration (MFC) expressed in g/L of Lactobacillus plantarum cell-free supernatants (CFS) against Aspergillus and Fusarium strains.
Table 2. Minimum inhibitory concentration (MIC) and minimum fungicidal concentration (MFC) expressed in g/L of Lactobacillus plantarum cell-free supernatants (CFS) against Aspergillus and Fusarium strains.
Fungal StrainL. plantarum
CECT 220CECT 221CECT 223CECT 224CECT 748CECT 749CECT 750
MICMFCMICMFCMICMFCMICMFCMICMFCMICMFCMICMFC
F. graminearum
ITEM 126		8881681681688816816
F. graminearum
ITEM 6415		816813813813416416416
F. cerealis
CECT 20488		81683181681688816816
F. cerealis
CECT 20489		81616161631416416416431
F. verticillioides
CECT 20926		16311631163116318168311631
F. verticillioides
CECT 2152		431431431431431431431
F. verticillioides
CECT 2982		1631163116311631163116311631
F. mesoamericanum
CECT 20490		816831816816816816816
F. poae
CECT 20165		1631816816816816816816
A. flavus
ITEM 8111		250nd 1250nd 1250nd 1250nd 112525062125250nd 1
A. Parasiticus
CECT 2681		nd 1nd 1nd 1nd 1nd 1nd 1nd 1nd 1250nd 1125250250nd 1
A. niger
CECT 2088		nd 1nd 1250nd 1nd 1nd 1nd 1nd 1250nd 1250nd 1250nd 1
1 nd = non-detected.
Table
Table 3. Phenolic compounds quantified in the cell-free supernatant (CFS) of Lactobacillus plantarum strains by LC-ESI-qTOF-MS.
Table 3. Phenolic compounds quantified in the cell-free supernatant (CFS) of Lactobacillus plantarum strains by LC-ESI-qTOF-MS.
CompoundMolecular FormulaL. plantarum
CECT
220		CECT
221		CECT
223		CECT
224		CECT
748		CECT
749		CECT
750
Gallic acidC7H6O50.7 ± 0.2nd 1nd 1nd 1nd 1nd 1nd 1
ProtocatechuicC7H6O4nd 1nd 10.4 ± 0.1nd 1nd 1nd 1nd 1
Chlorogenic acidC16H18O90.6 ± 0.1nd 1nd 1nd 10.5 ± 0.1nd 1nd 1
VanillinC8H8O3nd 10.3 ± 0.1nd 1nd 1nd 10.5 ± 0.2nd 1
p-coumaric acidC9H8O3nd 10.3 ± 0.1nd 10.6 ± 0.1nd 1nd 1nd 1
Salicylic acidC7H6O30.4 ± 0.10.3 ± 0.10.5 ± 0.20.3 ± 0.10.6 ± 0.20.5 ± 0.10.6 ± 0.1
Sinapic acidC11H12O50.7 ± 0.1nd 1nd 1nd 11.0 ± 0.2nd 10.4 ± 0.1
Phenyllactic acidC9H10O31.0 ± 0.21.1 ± 0.10.9 ± 0.11.4 ± 0.23.9 ± 0.15.3 ± 0.32.8 ± 0.2
1,2-DihydroxybenzeneC6H6O2nd 10.5 ± 0.1nd 10.6 ± 0.21.1 ± 0.2nd 10.9 ± 0.2
1 nd = non-detected. Mean ± standard deviation (n = 6).
Table
Table 4. Characteristics and composition of cell-free supernatant (CFS) produced by L. plantarum CECT 749.
Table 4. Characteristics and composition of cell-free supernatant (CFS) produced by L. plantarum CECT 749.
ParametersL. plantarum CECT 749 CFS (%)MRS
(%)
Moisture [47]94.5 ± 2.1094.3 ± 2.40
Proteins [46]0.3 ± 0.072.5 ± 0.30
Ash [48]0.2 ± 0.060.2 ± 0.01
Carbohydrates [49]3.2 ± 0.312.7 ± 0.5
pH3.3 ± 0.216.2 ± 0.22
Lactic acid [50]1.5 ± 0.50nd 1
1 nd = non-detected. Mean ± standard deviation (n = 6).
Table
Table 5. Fungal growth monitored in corn kernels contaminated with Aspergillus flavus ITEM 8111 and corn ears contaminated with Fusarium verticillioides CECT 2982 during the storage period. Fungal growth is expressed as (+) and absence of fungal growth as (−).
Table 5. Fungal growth monitored in corn kernels contaminated with Aspergillus flavus ITEM 8111 and corn ears contaminated with Fusarium verticillioides CECT 2982 during the storage period. Fungal growth is expressed as (+) and absence of fungal growth as (−).
SamplesA. flavus ITEM 8111F. verticillioides CECT 2982
Days
07154005715
Control−+++−+++
CFS−−++−−++

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Nazareth, T.d.M.; Luz, C.; Torrijos, R.; Quiles, J.M.; Luciano, F.B.; Mañes, J.; Meca, G. Potential Application of Lactic Acid Bacteria to Reduce Aflatoxin B1 and Fumonisin B1 Occurrence on Corn Kernels and Corn Ears. Toxins 2020, 12, 21. https://doi.org/10.3390/toxins12010021

AMA Style

Nazareth TdM, Luz C, Torrijos R, Quiles JM, Luciano FB, Mañes J, Meca G. Potential Application of Lactic Acid Bacteria to Reduce Aflatoxin B1 and Fumonisin B1 Occurrence on Corn Kernels and Corn Ears. Toxins. 2020; 12(1):21. https://doi.org/10.3390/toxins12010021

Chicago/Turabian Style

Nazareth, Tiago de Melo, Carlos Luz, Raquel Torrijos, Juan Manuel Quiles, Fernando Bittencourt Luciano, Jordi Mañes, and Giuseppe Meca. 2020. "Potential Application of Lactic Acid Bacteria to Reduce Aflatoxin B1 and Fumonisin B1 Occurrence on Corn Kernels and Corn Ears" Toxins 12, no. 1: 21. https://doi.org/10.3390/toxins12010021

APA Style

Nazareth, T. d. M., Luz, C., Torrijos, R., Quiles, J. M., Luciano, F. B., Mañes, J., & Meca, G. (2020). Potential Application of Lactic Acid Bacteria to Reduce Aflatoxin B1 and Fumonisin B1 Occurrence on Corn Kernels and Corn Ears. Toxins, 12(1), 21. https://doi.org/10.3390/toxins12010021

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