EDP Sciences logo
Submit your paper
Search
Menu
Home All issues Volume 27 (2020) OCL, 27 (2020) 59 Full HTML
Issue
OCL
Volume 27, 2020
Innovative Cropping Systems / Systèmes innovants de culture
Article Number 59
Number of page(s) 15
DOI https://doi.org/10.1051/ocl/2020052
Published online 09 November 2020

© N. Ait-Kaci Ahmed et al., Hosted by EDP Sciences, 2020

Licence Creative CommonsThis is an Open Access article distributed under the terms of the Creative Commons Attribution License (https://creativecommons.org/licenses/by/4.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

1 Introduction

1.1 Oilseed crop production and protection

1.1.1 Factors that limit crop yield

Since 2015, soybean (Glycine max), rapeseed (Brassica napus subsp. napus) and sunflower (Helianthus annuus L.) have been the three main oilseed crops produced worldwide (FAOSTAT, 2020). In 2018, their worldwide production was ca. 345, 75 and 50 million t/annum, respectively (FAO, 2020). While the global area of these crops is expanding, unfavorable weather conditions threaten their production (FAO, 2018). Despite the moderate water requirements of sunflower, drought is the main environmental factor that limits its growth (Debaeke et al., 2017a), and high temperature can decrease its final production of seeds and oil (Harris et al., 1978). In most European countries that produce sunflower (Romania, Spain, France, Bulgaria, and Hungary), yield gaps of 1.1–2.4 t/ha have been reported, and climate change could be partly responsible for them (Debaeke et al., 2017a). Biotic stress also limits oilseed crop production worldwide. At least 30 sunflower diseases are known. The most damaging and widespread fungal diseases are downy mildew (Plasmopara halstedii), phoma black stem (Phoma macdonaldii), phomopsis stem canker (Phomopsis helianthi), white mold (Sclerotinia sclerotiorum) and Verticillium wilt (Verticillium dahliae) (Seassau, 2010; Vear, 2016; Debaeke et al., 2017b), most of which are soilborne pathogens (P. halstedii, S. sclerotiorum, V. dahliae). More recently, Cadophora malorum has been reported as a new soilborne fungus of sunflower (Martín-Sanz et al., 2018; Molinero-Ruiz, 2019). In the context of climate change, Macrophomina phaseolina could be favored by ground dryness and temperatures of 28–30 °C (Šárová et al., 2003). S. sclerotiorum and V. dahliae could tolerate unfavorable periods better (Wilhem, 1955; Debaeke et al., 2017a) via their long-term structures − sclerotia and microsclerotia (MS), respectively −, which remain viable in the soil for many years (Mol et al., 1995; Ćosić et al., 2012).

1.1.2 The challenge of managing soilborne fungi

Protecting crops from soilborne organisms is more challenging than protecting them from foliar pests (Matthiessen and Kirkegaard, 2006). Soilborne fungi such as V. dahliae and M. phaseolina can survive as MS up to 14 years (Wilhem, 1955) and 4 years (Watanabe, 1973), respectively. S. sclerotiorum produces sclerotia that may survive for 3 years (Ćosić et al., 2012). Soilborne pathogens can coexist in the soil (Raaijmakers et al., 2009), and their heterogeneous distribution makes monitoring them costly and usually ineffective (Matthiessen and Kirkegaard, 2006). For many oilseed diseases, genetic resistance is one of the most effective protection methods, but it breaks down frequently due to the appearance of new virulent strains, as observed for sunflower diseases (Vear, 2016; Debaeke et al., 2017b; Molinero-Ruiz, 2019). To reduce the pressure of soilborne pathogens, farmers used to fumigate vegetable and ornamental crops intensively with methyl bromide (Hoffmann and Malkomes, 1974; Duniway, 2002; Martin, 2003). However, methyl bromide was phased out under the Montreal Protocol in 2005 due to its depleting effects on the ozone layer (Laegdsmand et al., 2007; Gimsing and Kirkegaard, 2009). Other synthetic compounds were subsequently used to control soilborne pathogens, such as 1,3-dichloropropene (phased out in the European Union [EU] in 2007), chloropicrin (phased out in the EU in 2012) and methyl-isothiocyanate (MITC), the primary breakdown product of metam-sodium (Ibekwe, 2004). MITC has a broad biocidal activity but alters important soil functions such as nutrient cycling (Macalady et al., 1998). It is also highly volatile, with much of it transferred to the atmosphere after application (Dungan et al., 2003).

Like for genetic resistance, maintaining the efficacy of pesticides after repeated use is difficult (Matthiessen and Kirkegaard, 2006). Synthetic fumigants may become less toxic due to soilborne pathogens developing resistance (Goldman et al., 1994) and/or increased biodegradation of their chemicals (Warton et al., 2003). This latter misunderstood phenomenon comes from the ability of microorganisms, mainly bacteria, to catabolize xenobiotics in the soil after repeated exposures with a short interval between applications (Warton et al., 2003; Matthiessen and Kirkegaard, 2006). Microorganisms can accelerate the degradation, which decreases their persistence and effectiveness for soilborne pathogens (Warton et al., 2003; Di Primo et al., 2003). This phenomenon has been observed with metam sodium used for potato (Solanum tuberosum) Verticillium wilt (VW) (Di Primo et al., 2003). When a soil develops increased biodegradation, fumigation requires several years before it can recover an effective biocidal effect (Warton et al., 2003). In the meantime, the use of fumigants seems ineffective and wasteful (Matthiessen and Kirkegaard, 2006).

1.1.3 Alternatives for managing soilborne diseases

The breakdown of resistance and the current context of agroecological transition have decreased the use of broad-spectrum fumigants (Warmington and Clarkson, 2016) and increased interest in alternative methods of crop protection (Martin, 2003). Reliance on combined and natural mechanisms to protect crops has been encouraged by Integrated Pest Management (IPM), as described in the EU Framework Directive 2009/128/EC. IPM is implemented through eight principles, and the first one is based on preventing and/or suppressing harmful organisms using a variety of methods, such as crop rotations. IPM favors the use of sustainable biological methods (Barzman et al., 2015). Since isothiocyanates (ITCs) are biologically active compounds, and MITC is widely used as a fumigant, there is interest in transposing this biocidal activity of biological sources of ITCs to suppress soilborne pathogens and diseases (Brown and Morra, 1997; Matthiessen and Kirkegaard, 2006; Gimsing and Kirkegaard, 2006). This natural alternative to fumigation, called “biofumigation” (Kirkegaard et al., 1993), involves growing, chopping and incorporating crops that produce ITCs. Brassicaceae (crucifers) are widely used for this technique (see part 2).

The utility of biofumigation has been observed for protecting vegetable crops (Michel, 2014; Morris et al., 2020) and, to a lesser extent, wheat (Triticum aestivum, Kirkegaard et al., 2000) and beetroot (Beta vulgaris ssp. vulgaris, Motisi et al., 2009). Many studies of in vitro approaches have shown promising results of biofumigation for soilborne diseases. In the field, however, the effectiveness of biofumigation has varied more (Motisi et al., 2010; Morris et al., 2020). Nonetheless, mechanisms for suppressing pathogens effectively in the field are increasingly understood (Kirkegaard and Matthiessen, 2004; Matthiessen and Kirkegaard, 2006; Morris et al., 2020), and biofumigation appears to be an environmentally friendly defense strategy (Lazzeri et al., 2004) considered as a part of IPM (Gimsing and Kirkegaard, 2009; Kruger et al., 2013). Among oilseed crops, sunflower seems to be particularly suitable for protection using biofumigation. It is sown in spring, after a long fallow period when soils are usually left bare. A Brassicaceae cover crop introduced during this period would fit into the rotation easily, thus diversifying it. It would also improve:

To follow the fundamental agroecological principle of diversifying crop rotations (Altieri, 1999), this review does not discuss rapeseed protection using Brassicaceae cover crops and biofumigation. However, it does present studies that used Brassicaceae as a biofumigant crop. Biotic stresses are not still a major issue for soybean in France (Lamichhane et al., 2020) or in Europe. This is in part because soybean is currently grown on small areas and in diversified rotations (Lamichhane et al., 2020). The interest in biofumigation to protect soybean remains low and studies rare. Thus, this review excludes soybean protection using biofumigation, although some studies showed promising results. Fayzalla et al. (2009) showed that soybean root rot and soybean wilt, caused by Fusarium oxysporum, Rhizoctonia solani, M. phaseolina and Sclerotium rolfsii, could be reduces with mustard in field conditions.

With a focus on sunflower, the objectives of this review are to:

  • highlight the main factors that determine effective biofumigation;

  • review studies on laboratory or field experiments performed to evaluate suppressive effects of synthetic GSLs/ITCs or Brassicaceae incorporation on V. dahliae, S. sclerotiorum and M. phaseolina.

Since studies of sunflower protection using biofumigation are rare (to our knowledge), most studies concerned other plant hosts. Thus, after describing the biofumigation concept and process briefly, factors that drive ITC production are detailed to provide a set of mechanisms that results in effective biofumigation. Suppressive effects of glucosinolate (GSL) products on sunflower soilborne diseases are reviewed based on studies of a variety of host crops. Finally, non-GSL-related suppressive effects of biofumigation and the utility of including Fabaceae with Brassicaceae to protect sunflower against soilborne disease are also discussed.

2 The biofumigation process

2.1 Biofumigation concept and the use of Brassicaceae

Biofumigation is defined as the suppressive effect of GSL-containing species on soilborne pathogens through the liberation of volatile compounds, mainly ITCs, released after hydrolysis of GSLs by the enzyme myrosinase during tissue disruption and incorporation into the soil (Kirkegaard et al., 1993; Kirkegaard and Matthiessen, 2004). GSLs occur naturally in families of the order Capparales: Tovariaceae, Resedaceae, Cappareaceae, Moringaceae and mainly Brassicaceae (Fenwick et al., 1983; Brown and Morra, 1997; Van Dam et al., 2009). They are widely cultivated as vegetables (cabbage [B. oleracea var. capitata], radish [Raphanus raphanistrum subsp. sativus], and rocket [Eruca vesicaria ssp. sativa]), condiments (mustard [Brassica juncea]), forage (fodder radish [Raphanus sativus var. longipinnatus] and turnip rape [Brassica rapa subsp. rapa]), oilseed crops and cover crops during fallow periods. However, plants that contain GSLs can be used to control soilborne pathogens through biofumigation (Kirkegaard et al., 1993; Brown and Morra, 1997; Matthiessen and Kirkegaard, 2006) and are considered to be a biological alternative to conventional soil fumigation (Brown and Morra, 1997; Matthiessen and Kirkegaard, 2006; Laegdsmand et al., 2007; Clarkson et al., 2015). Bactericidal activity of ITCs has been reported (Brown and Morra, 1997; Smith and Kirkegaard, 2002; Bending and Lincoln, 2000), as have fungicidal (Angus et al., 1994; Manici et al., 2000; Smith and Kirkegaard, 2002), nematicidal (Lazzeri et al., 1993; Riga, 2011; Ntalli and Caboni, 2017), insecticidal (Borek et al., 1995a; Borek et al., 1998) and herbicidal activities (Haramoto and Gallandt, 2004). Biofumigation can reduce pest abundance and disease incidence (Morris et al., 2020), but its degree of pest suppression can vary significantly. Some studies concluded that biofumigation did not suppress soilborne pathogens (reviewed by Kirkegaard and Matthiessen, 2004; Motisi et al., 2010). After rape incorporation, Davis et al. (1996) observed no significant differences in V. dahliae population in the soil compared to that without residue incorporation, while the incidence of VW on potato was reduced significantly compared to that on potato grown after a fallow period. VW can be caused by an interaction between V. dahliae and nematodes like Pratylenchus penetrans (Martin et al., 1982; Rowe and Powelson 2002) or Pratylenchus neglectus (Scholte and s’Jacob, 1990) which may facilitate the penetration of V. dahliae in roots, but no information is available about the direct effect of residue incorporation on P. neglectus in this study. However, no significant correlation has been found between VW symptoms or yield and the nematode. Hartz et al. (2005) also reported that biofumigation (with mustard) did not significantly reduce V. dahliae population in the soil or VW on tomato (Solanum lycopersicum). A review of Motisi et al. (2010) noted an increase in disease intensity after biofumigation for some pathogens. Moreover, some studies may not be published because they unexpectedly observe no significant effects of biofumigation (Morris et al., 2020). This variability is due to the many biological and physical factors that influence the effectiveness of biofumigation (Motisi et al., 2010). Thus, knowledge about GSL and ITC production, and a systematic approach to field research through analytical studies are needed (Kirkegaard and Matthiessen, 2004).

2.2 The GSL-myrosinase system

GSLs are organic anions characterized by a common b-thioglucose, a sulfonated oxime moiety and a side-chain group (Fenwick et al., 1983). This side chain determines the type of GSL: aromatic, aliphatic or indolyl (Fenwick et al., 1983; Brown and Morra, 1997; Mithen, 2001). To date, 132 GSLs have been identified in Brassicaceae tissues (Couëdel et al., 2019). Native GSLs have little or no biocidal activity or toxicity (Manici et al., 1997). Species that contain GSL produce myrosinase, a group of similar-acting enzymes (Brown and Morra, 1997) that are also produced by some microorganisms in soils (Gimsing and Kirkegaard, 2009). In intact plant tissues, GSLs and myrosinase are physically separated (Gimsing and Kirkegaard, 2009). The isolation seems to be intercellular (Brown and Morra, 1997), with GSLs in the vacuoles and myrosinase in specialized myrosin cells (Höglund et al., 1992). Both compounds are distributed throughout Brassicaceae tissues (Wittstock and Gershenzon, 2002), and cells must be disrupted physically for them to contact each other (Brown and Morra, 1997). The result is rapid hydrolysis into biologically active products such as ITCs and other products of GSL degradation, such as nitriles, organic cyanides, oxazolidinethiones and ionic thiocyanates (Brown and Morra, 1997; Gardiner et al., 1999). Mature tissues have less myrosinase activity (Iversen and Baggerud, 1980).

2.3 GSL-hydrolysis products and non-GSL products

The biocidal effect of the products of GSL hydrolysis is function of the chemical composition of the GSL side chain, their concentration, environmental conditions and the exposure time of the target organism (Fenwick et al., 1983; Lazzeri et al., 1993; Laegdsmand et al., 2007; Gimsing and Kirkegaard, 2009). Each compound differs in its persistence in the soil, stability and toxicity (Borek et al., 1995b; Manici et al., 2000).

ITCs are produced rapidly after Brassicaceae tissues are disrupted (Morra and Kirkegaard, 2002). Their concentration in the soil peaks 30 min after incorporation and can be detected for up to 12 days (Gimsing and Kirkegaard, 2006). ITCs are highly volatile, and the shorter their side chain is, the more volatile they are (Brown and Morra, 1997). Due to their high volatility, their toxicity is assumed to spread around the point of chopping (Angus et al., 1994). Only aliphatic and aromatic GSLs produce ITCs (Matthiessen and Kirkegaard, 2006), and they are recognized as the most biologically active products of GSL hydrolysis, with broad-spectrum activity (Fenwick et al., 1983; Brown and Morra, 1997; Matthiessen and Kirkegaard, 2006). ITCs are toxic because of their irreversible interaction with proteins, mainly nucleophilic reagents (Brown and Morra, 1997; Borek et al., 1995a). The reaction damages the protein structure and functions of pest cells (Dufour et al., 2015).

Despite the lower toxicity of the other products of GSL hydrolysis, they may also help control soilborne organisms and work synergistically with ITCs (Brown and Morra, 1997). Other non-GSL secondary metabolites, such as sulfur-containing organic compounds (e.g. sulfoxides, amino acids such as methionine and cysteine, sulfonium compounds) may also have toxic effects on soil organisms (Bending and Lincoln, 1999).

3 Increasing biofumigation effectiveness for sunflower production

With more than 350 genera (Beilstein et al., 2006; Abideen et al., 2013) and 3200 species (Abideen et al., 2013), Brassicaceae present a wide scope for farmers to choose the most promising crops for effective biofumigation, based on their GSL concentrations and profiles, and biomass production (Sarwar et al., 1998). Farmers can act at multiple levels to improve the biofumigation potential (Borek et al., 1995b; Brown and Morra, 1997; Matthiessen and Kirkegaard, 2006; Gimsing and Kirkegaard, 2009):

  • choice of Brassicaceae species;

  • amount and profile of GSLs produced by the crop;

  • rate of GSL conversion into ITCs;

  • persistence of biocidal compounds in the soil.

3.1 The choice of the biofumigant Brassicaceae species

Morris et al. (2020) emphasized that species in the genus Eruca and Raphanus had the highest biofumigation effectiveness. However, most studies about biofumigation concern brown, white or Ethiopian mustard and rape (rapeseed and forage rape) (Sarwar et al., 1998; Kirkegaard and Matthiessen, 2004; Reau et al., 2005; Clarkson et al., 2015). Brown mustard has high concentrations of sinigrin GSL, which hydrolyzes into 2-propenyl-ITCs. Considered as a highly toxic ITC (Motisi, 2009), it may explain brown mustard’s promising results for crop protection (see part 4). The utility of choosing forage rape cultivars as a biofumigant crop was demonstrated by Gardiner et al. (1999), who studied products of hydrolysis after incorporation of cv. Dwarf Essex. Plants were incorporated using a rototiller at the bud-to-early-flowering stage. The most abundant product of hydrolysis measured in the soil was the 2-phenylethyl-ITC (2-PE-ITC), obtained from the aromatic 2-phenylethyl-GSL (2-PE-GSL), the main GSL in the roots of both cultivars. Smith and Kirkegaard (2002) demonstrated the toxicity of this ITC to pests. Moreover, Larkin et al. (2010) measured a lower VW incidence on potato after forage rape (cv. Dwarf Essex) incorporation as green manure compared to a continuous potato (non-rotation) control. However, farmers harvest rapeseed crops to produce oil, so destroying them at the flowering stage and/or incorporating them as a green manure seems unrealistic in the context of oilseed crop production. The advantage of rapeseed would rely more on an allelopathic effect during development, with continuous production of ITCs by its living roots (Rumberger and Marschner, 2003) or after harvest, during roots decomposition (Reau et al., 2005), both of which would provide a source of biocidal compounds (mainly ITCs) against soilborne fungi. Rumberger and Marschner (2003) demonstrated this phenomenon, observing that live roots of canola cv. Monty (low root GSL) and cv. Rainbow (high root GSL) released 2-PE-ITC continuously into the rhizosphere, which affected soil microbial communities (bacteria and eukaryotes) without accumulating in the soil. Despite the interest in rape for its allelopathic and, to a lesser extent, biofumigant effects, the trend since the 1960s has been to select and breed varieties with lower GSL concentrations. Thus, “double-low” varieties (i.e. low in erucic acid and GSLs) have been introduced (Boag et al., 1990). GSLs may be undesirable or even toxic to mammals (rats and roe deer) when GSL concentrations increase in rape tissues (Fenwick et al., 1983; Boag et al., 1990). It is possible, however, to breed canola with higher 2-PE-ITC concentration without affecting shoot or seed GSL concentrations (Potter et al., 2000). Since the GSL concentration necessary to have a toxic effect on soilborne pathogens remains unknown, low-GSL cultivars may still have biocidal effects (Couëdel et al., 2019). For example, Kirkegaard et al. (2000) found no significant difference in the decrease in inoculum survival of the fungus G. graminis var. tritici between canola with high (cv. Tamara and cv. Karoo) and low (cv. Oscar and cv. Monty) root GSL concentrations, even though the pairs of varieties produced different 2-PE-ITC concentrations. In a pot experiment, Michel et al. (2008) showed that the number of live MS of V. dahliae in soils after the low GSL canola (cv. Talent) were approximatively 60 MS/g of soil, compared to that in an unamended control (approximatively 90 MS/g of soil), but the differences were not significant. To our knowledge, no study has examined the potential of rapeseed to control soilborne diseases of sunflower in field (through biofumigation and/or allelopathic effects). Seassau et al. (2016) observed, in vitro, a significant reduction in the germination or the development of V. dahliae (strains from sunflower) exposed to rapeseed (cv. Mosa), selected for its low GSL concentration compared to the unamended control.

Although most studies have focused on Brassicaceae green manures for biofumigation, seed meals could be used as an alternative strategy (Mazzola et al., 2001) since they have more biological activity than green manures. GSLs are concentrated in the seeds and retained in the meal after crushing (Borek and Morra 2005). Thus, seed meals can be a source of GSLs (Brown and Morra, 1997; Morra and Borek, 2010) that stimulate soil microbial communities and suppress soilborne pathogens (Mazzola et al., 2017). This alternative, however, would be better suited for small areas of crops with high commercial value than large areas of sunflower because of the high cost of seed meals.

3.2 Increasing GSL concentrations and profiles

A positive relation exists between GSL concentrations in Brassicaceae tissues and their ability to suppress pests and diseases during biofumigation (Morris et al., 2020). The concentration and the profiles of GSLs (aliphatic, aromatic and indolyl) vary among Brassicaceae species (Kirkegaard and Sarwar, 1998; Bellostas et al., 2004; Bhandari et al., 2015) and between their shoots and roots (Kirkegaard and Sarwar, 1998; Van Dam et al., 2009; Bhandari et al., 2015). Roots usually have higher GSL concentrations than shoots, even though roots have lower biomass than shoots (Gimsing and Kirkegaard, 2006; Van Dam et al., 2009; Bhandari et al., 2015). This difference may be explained by a higher pathogen pressure belowground than aboveground (Van Dam et al., 2009; Bhandari et al., 2015). Biotic stress, such as herbivore damage and pathogen infection, increases GSL concentrations in Brassicaceae tissues (Van Dam et al., 2009). It is important that biotic stress does not decrease biomass production too much, however, because a positive relation exists between Brassicaceae biomass and its GSL concentrations (Kirkegaard and Sarwar, 1998). A large amount of biomass is thus required for effective biofumigation (Clarkson et al., 2015). Morris et al. (2020) predicted that less than 0.53 t dry matter of biomass/ha would result in ineffective biofumigation. Thus, it is important that cover crops be established well to maximize their biomass. While application of fertilizers (nitrogen and sulfur) increases GSL concentrations (Booth et al., 1991; Li et al., 2007), applying them to cover crops is neither recommended nor profitable.

The effectiveness of biofumigation also depends on the growth stage of the plant. During development of Brassicaceae, GSLs turn over or redistribute within its organs (Booth et al., 1991). GSL concentration peaks at the early flowering stage in the whole plant, then it starts to decrease in shoots and roots and increase in the seeds, whose GSL concentration peaks at maturity (Booth et al., 1991; Sarwar and Kirkegaard, 1998; Michel, 2008). Because seeds have much less biomass than shoots and roots, which decreases the amount of biomass available for biofumigation (Morris et al., 2020), the optimal timing for biofumigation is at the maximum value of biomass × GSL concentration (Matthiessen and Kirkegaard, 2006). The recommended stage at which to destroy crops is thus flowering (Michel, 2008), which also has the advantage of avoiding seed-set.

3.3 Improving the conversion of GSLs into ITCs

For effective biofumigation, maximizing the hydrolysis reaction that converts GSLs into ITCs is crucial to generate high ITC concentration in the soil (Borek et al., 1995b; Brown and Morra, 1997; Gimsing and Kirkegaard, 2009). Under laboratory conditions, Brassicaceae sometimes released only 19% of the total potential ITCs produced (Brown et al., 1991). This conversion efficiency reached 62.5–100% for Brassicaceae seed meals in sterile sand (Neubauer et al., 2015). In the field, the efficiency was estimated at 60% (Gimsing and Kirkegaard, 2006). The efficiency depends mainly on agronomic practices and soil and climate conditions. The stage of development of the Brassicaceae for biofumigation must be considered, due to the decrease in myrosinase activity in mature tissues (Iversen and Baggerud, 1980). Brassicaceae tissues must be chopped finely to maximize contact between myrosinase and GSLs (Matthiessen and Kirkegaard, 2006). Thus, chopping at high speed and using hammers instead of blades is recommended (Matthiessen et al., 2004; Michel, 2008). Dilution with large amounts of water is then crucial to ensure tissue maceration and soil moisture to hydrolyze GSLs into ITCs and other products (Matthiessen et al., 2004; Michel, 2008; Gimsing and Kirkegaard, 2009). ITC concentration increased by up to 7–10-fold when 42 mm of water was added to a soil after biofumigation (Matthiessen et al., 2004). However, Gimsing and Kirkegaard (2006) observed no difference after irrigating with 18 mm over 3 hours after biofumigation. Warmer temperatures also increase hydrolysis (Matthiessen and Kirkegaard, 2006; Michel, 2008; Gimsing and Kirkegaard, 2009). Matthiessen and Shackleton (2005) observed that the biological activity of 2-PE-ITC was significantly lower at 5 °C than at 10–20 °C. Consequently, farmers should carefully choose the day on which to perform biofumigation. Days with temperatures above 10 °C and with rain forecast to fall within a few days could improve the conversion of GSLs into ITCs, which would favor effective biofumigation. In the soil, a pH around neutral results in ITC production, while acid pH favors nitrile production (Brown and Morra, 1997).

3.4 Maximize persistence of ITCs in the soil

Un-hydrolyzed GSLs and the ITCs produced persist in soils from a few days to a few weeks (Brown and Morra, 1997), with the concentrations of GSL and ITC peaking 30 min after Brassicaceae incorporation (Gimsing and Kirkegaard, 2006) to 30 hours (Gardiner et al., 1999). Maximizing the persistence of ITCs is crucial to increase the duration of exposure of soilborne pathogens, which increases biofumigation effectiveness (Borek et al., 1995b; Brown and Morra, 1997).

The main pathway of ITC losses is volatility (Brown and Morra, 1997). To decrease these losses, solarization is used with vegetable crops to trap volatile ITCs (Morris et al., 2020). This technique consists of covering the soil with transparent polyethylene sheets (Katan, 1981), but it is impractical over larger areas, such as those of oilseed crops. Thus, rapid incorporation of the chopped Brassicaceae is highly recommended (Gimsing and Kirkegaard, 2006; Michel, 2008). Sorption on soil components is another pathway of ITC loss. For example, ITCs had lower toxicity in soils with high organic matter content (>1%) (Gimsing and Kirkegaard, 2009; Neubauer et al., 2014), which suggests that ITCs reacted with organic matter’s nucleophilic reagents. Soil pH and texture had little influence on ITC persistence in the soil (Brown and Morra, 1997), unlike heavy rainfall (70–90 mm), which could cause ITCs to leach, thus reducing their persistence (Laegdsmand et al., 2007).

Microbial degradation is a key factor that influences ITC losses in the soils (Brown and Morra, 1997). Using an autoclaved soil in biofumigation experiments increased the stability of ITCs (Rumberger and Marschner, 2003). Farmers have little influence on this factor, but soils that have never been fumigated may not experience increased biodegradation (Warton et al., 2003). Because fumigation is used less often with oilseed crops than with vegetable crops, mainly because of the high cost of protecting large areas, soils of oilseed crops may not experience this increased biodegradation.

4 Suppressive effects of GSL products on the soilborne diseases of sunflower targeted

Under optimal conditions that maximize GSL concentrations, their conversion into ITCs and persistence in the soil, the effectiveness of biofumigation will depend greatly on the target species, since pathogens vary greatly in their sensitivity to ITCs (Brown and Morra, 1997; Smith and Kirkegaard, 2002). To assess the sensitivity of sunflower pathogens to biofumigation, this review focuses on laboratory or field experiments performed to evaluate suppressive effects of synthetic GSLs/ITCs or Brassicaceae incorporation on V. dahliae, S. sclerotiorum and M. phaseolina (Tab. 1). Since studies of sunflower protection using biofumigation are rare (to our knowledge), most studies concerned other plant hosts of these pathogens, mainly vegetable.

Table 1

Summary of the suppressive effects of GSLs/ITCs or Brassicaceae against three soilborne fungi of sunflower: Verticillium dahliae, Sclerotinia slcerotiorum and Macrophomina phaseolina using synthetic GSLs-/-ITCs in vitro or in pot (a), Brassicaceae in vitro or in pot (b), Brassicaceae in greenhouse and in the field (c), and at the rotation scale (d).

Target pathogen/plant: fungus studied and plant from which it was isolated (when mentioned); methods: GSLs/ITCs used or destruction/incorporation mechanisms of the Brassicaceae; Brassica species (cv./var.): the Brassicaceae and the cultivar or variety (when mentioned) used for biofumigation; crop to protect: the host plant; GSL/ITC measured: compounds in the Brassicaceae; 2-PE-ITC: 2-phenylethyl-isothiocyanate; a.o.t: among other treatments; Br: Brassicaceae; M.p: Macrophomina phaseolina; MS: microsclerotia; NA: not available; NS: not significant; S.s: Sclerotinia sclerotiorum; UC: unamended/untreated control; V.d: Verticillium dahlia; VW: Verticillium wilt.

4.1 Experiment using synthetic ITCs/GSLs

In vitro studies of synthetic ITCs or synthetic GSL + myrosinase tested the sensitivity of pathogens and screened the most effective GSL profiles (Tab. 1, part a). Neubauer et al. (2014) tested five ITCs, all of which were lethal to V. dahliae MS. Aromatic ITCs (benzyl-ITC and phenylethyl-ITC obtained by Glucotropaeolin and Gluconasturtiin hydrolysis) were much more toxic than aliphatic ITCs. Among the same profiles of ITCs (aromatic or aliphatic), ITCs with lower molecular weight tended to be more effective than ITCs with higher molecular weight. To suppress S. sclerotiorum, aromatic ITCs were also more effective than aliphatic ITCs. Overall, benzyl-ITC was the most effective ITC against S. sclerotiorum mycelial development and sclerotia (Kurt et al., 2011), while methyl-ITC and allyl-ITC were among the most effective ITCs at reducing mycelial growth (Kurt et al., 2011; Ojaghian et al., 2012). For M. phaseolina, mycelial development was also reduced by allyl-ITC (Mazzola et al., 2017).

4.2 Experiments using Brassicaceae (in vitro or in pots)

To screen the potentially most effective varieties and/or species of Brassicaceae, and to assess effects of hydrolysis products of GSLs to manage soilborne fungi, experiments were performed using Brassicaceae biomass (e.g. crushed, ground, macerated) instead of synthetic compounds (Tab. 1, part b). To control V. dahliae, S. sclerotiorum and M. phaseolina, mustard varieties, especially Brassica juncea (brown/Indian mustard), were used mainly as a source of GSLs and ITCs in biofumigation studies. Mustard species often showed significant suppression of V. dahliae (Olivier et al., 1999; Neubauer et al., 2015; Seassau et al., 2016), S. sclerotiorum (Ojaghian et al., 2012; Rahimi et al., 2014; Warmington and Clarkson, 2016) and M. phaseolina (Mazzola et al., 2017). Some cultivars of turnip rape (Brassica rapa), forage radish (Raphanus sativus), Kohlrabi (Brassica oleracea cv. caulorapa) and B. napus were among the most effective species, but were more variable than B. juncea. In these studies, anti-fungal effects of ITCs and other products of GSL hydrolysis were assessed on mycelial growth and/or the long-term survival structures of the pathogens. Effectiveness of Brassicaceae varied among the forms of the pathogens. Seassau et al. (2016) showed that mycelial growth of V. dahliae isolated from sunflower was suppressed mainly by B. juncea, while MS germination was suppressed mainly by B. rapa. Since biofumigation occurs a few months before sunflower sowing, its suppressive effects would affect long-term survival structures of pathogens because of the low persistence of GSLs and ITCs.

4.3 Field approaches to biofumigation

In vitro and pot studies have shown promising biocidal effects on V. dahliae, S. sclerotiorum and M. phaseolina. In field conditions, however, results varied more among studies (Tab. 1, part c), due to the many factors that influence the effectiveness of biofumigation. The only study of sunflower crop protection reported a significant reduction in VW incidence and severity following three Brassicaceae cover crops and biofumigation compared to that with a bare soil (Galaup et al., pers. comm.). In both years of its field experiment, R. sativus was the Brassicaceae that reduced VW incidence the most, followed by B. rapa and B. juncea. The ability of biofumigation with a given species to reduce VW varied between years due to differences in the biomass incorporated into the soil each year. The largest reduction in VW was associated with the largest biomass produced. In strawberry (Fragaria × ananassa) field experiments, Michel et al. (2008) observed a significant reduction of MS in soils after biofumigation with B. juncea. Conversely, Hartz et al. (2005) considered B. juncea an ineffective biofumigant: it did not decrease the density of V. dahliae in the soil and had no effect on tomato productivity compared to a fallow control. Michel (2014) observed no significant effects of B. juncea on V. dahliae density in the soil, in the short-term, but a reduction of 80% was observed a few months after biofumigation. Because of the low persistence of ITCs, they could not have caused this suppressive effect. Instead, the reduction in MS may have been caused by stimulation of specific groups of microbial communities during mustard decomposition and organic matter addition, as supported by other studies (Mazzola et al., 2007; Ochiai et al., 2008; Mazzola et al., 2017). Thus, organic inputs could improve soil biological status by increasing both the diversity and size of populations of beneficial species through physico-chemical changes (Ochiai et al., 2008; Davis et al., 2010; Omirou et al., 2011).

5 Non-GSL-related suppressive effects on pathogens, and the multifunctionality of Brassicaceae

Pathogen suppression by green manure addition has been attributed to indirect effects of higher microbial competition rather than a direct effect on pathogen inoculum (Davis et al., 1996; Davis et al., 2010). This involvement of microbial communities was supported by long-term studies at the rotation scale when Brassicaceae and non-Brassicaceae species were incorporated (Tab. 1, part d). Davis et al. (2010) observed that cover crops reduced VW on potatoes more than fallow did. Sudangrass (Sorghum vulgare var. sudanense cv. Monarch) was a more effective cover crop than B. napus cv. Dwarf Essex and cv. Bridger. The authors also suggested that another beneficial effect of sudangrass was the potential control of root knot nematodes. Larkin et al. (2010) also observed a significant reduction in VW on potato after a canola cover crop and to a lesser extent after a rapeseed cover crop. Davis et al. (2010) and Larkin et al. (2010) concluded that, beside the direct toxic effects of products of GSL hydrolysis, VW may have been suppressed due to a change in microbial communities that increased microbial competition after cover crop incorporation. The reduction in VW may be explained by the increase in Fusarium equiseti in the soil observed by Davis et al. (2010), which suggests a potential antagonism between the two fungi.

Increasingly, biofumigation benefits are considered along with other green manure benefits, such as addition of organic matter to soils (Kirkegaard and Matthiessen, 2004). This non-GSL-related pathway of suppression may be involved in reducing pathogens and disease severity in the studies that used low-GSL cultivars observed by Kirkegaard et al. (2000) and Michel et al. (2008). The potential key role of microbial communities in suppressing pathogens emphasizes the need to assess potential disservices of products of GSL hydrolysis on these beneficial communities. To date, these disservices and their influence have been rarely studied, and the review of Couëdel et al. (2019) reported inconsistent impacts of Brassicaceae on non-target species. No effect of Brassicaceae incorporation was observed on nitrifying bacteria in field studies (Omirou et al., 2011). Conversely, Bending and Lincoln (2000) observed that application of ITCs disrupted microbial communities, reducing the growth of nitrifying bacteria in clay-loam soils. One mechanism to avoid these potential disservices could be cover crop mixtures (Couëdel et al., 2019), which would provide more nutrients, and thus increase microbial diversity and activity, while preserving GSL production. Couëdel et al. (2018c) showed that, compared to Brassicaceae sole crops, 50/50 bi-species mixtures of Brassicaceae and Fabaceae reduced GSL production/ha by an average of only 19%. Mixtures would maintain most of the potential of Brassicaceae to suppress pathogens and could mutualize other benefits provided by either Brassicaceae or Fabaceae. Couëdel et al. (2018a) showed that this mixture captured the same amount of nitrate as Brassicaceae alone and had a larger nitrogen-green manure effect. This mixture also provided the same sulphate-catch crop and sulfur-green manure effects as Brassicaceae sole crops (Couëdel et al., 2018b). This result could be due to increased biomass production and abiotic-resource-use efficiency (Jensen, 1996). Besides protecting against pathogens and nutrient enrichment, mixtures provide a bundle of ecosystem services. They reduce soil disturbance and erosion, maximize water-use efficiency, increase long-term carbon sequestration and support pollinators and other beneficial insects (Therond et al., 2017; Justes and Richard, 2017; Chapagain et al., 2020). Thus, mixtures of Brassicaceae and Fabaceae could increase sunflower productivity. Combining cover cropping of mixtures with biofumigation represents a holistic multi-pest protection approach that relies on several ecological mechanisms, which is in line with the principles of IPM. Besides diversifying rotations (which may provide break-crop effects), encouraged by IPM Principle 1 (P1), it is a major environmentally friendly protection method (Lazzeri et al., 2004). It may prevent reliance on the synthetic compounds used in fumigation (Clarkson et al., 2015), and thus fulfill the principles of giving preference to non-chemical methods (P4), selecting pesticides to avoid undesired impacts of broad-spectrum fumigants on non-target beneficial communities (P5) and reducing pesticide use (P6). Some of biofumigation’s ability to protect of sunflower would be due to the ITCs produced by Brassicaceae, and developing resistance to them is highly improbable because of the complex cluster of chemically different components involved (Ntalli and Caboni, 2017). Moreover, ITC toxicity varies among pests (Smith and Kirkegaard, 2002), which could allow for specific actions on targeted pests (P5). The potential increase in some antagonist fungi (e.g. Fusarium spp., as reported by Davis et al. (2010)) after incorporating cover crops represents another ecological mechanism to suppress soilborne pathogens (Médiène et al., 2011), which could be enhanced by including Fabaceae in mixtures, because it could diversifies the tissues incorporated (Couëdel et al., 2019).

Some principles of IPM, however, could be difficult to implement for soilborne fungi of sunflower. Monitoring microscopic and heterogeneous pathogens such as V. dahliae, as recommended by P2, would be too expensive. Thus, it is challenging to determine thresholds for intervention (P3). Nevertheless, biofumigation could still help farmers reach the underlying objectives of IPM: minimize use of broad-spectrum biocides, environmental contamination, disruption of beneficial communities and development of resistance (Matthiessen and Kirkegaard, 2006; Barzman et al., 2015).

6 Conclusion

Soilborne diseases threaten sunflower productivity. VW, sclerotinia head and stalk rots, and charcoal rot have been expanding worldwide in the past several years or could be in the future. They are challenging to manage because of their ability to survive in the soil and the lack of sustainable effective control methods. Thus, biofumigation could be an interesting agroecological alternative for protecting sunflower, especially as a part of IPM. This review showed that multiple factors must be considered for effective biofumigation. For sunflower production, a biofumigant crop can be grown during the fallow period just before sunflower. Ideally, the Brassicaceae should be chopped at early flowering, temperatures of ca. 10 °C minimum and just before a rainy period, since high temperatures and soil water content increase the hydrolysis of GSLs into ITCs. Brassicaceae should be incorporated quickly into the soil after pulverization to reduce volatile losses.

For effective suppression by biofumigation, Brassicaceae with high GSL concentrations are recommended. The types of GSLs/ITCs produced by Brassicaceae are also important to consider, since the biocidal effect of GSLs depend on the target pathogen. According to the ITCs tested and the Brassicaceae incorporated, long-term survival structures and mycelia of V. dahliae, S. sclerotiorum and M. phaseolina were susceptible most of the time.

While aromatic ITCs and mustards seem to be the most effective, an increasing number of studies emphasize non-GSL-related effects of Brassicaceae and non-Brassicaceae cover crops. Nutrient enrichment after incorporating cover crops has strong effects on microbial communities that may stimulate antagonist species of pathogens in the soil. These effects are supported by studies that show negative correlations between microbial activity/diversity and the incidence of symptoms. The potential key role of microbial communities in the suppressive effect of Brassicaceae incorporation could explain the positive results obtained with Brassicaceae with low GSL concentration, such as canola. This highlights the need to assess effects of Brassicaceae incorporation on beneficial communities precisely, since the results to date are scarce and inconsistent. Nonetheless, cover crop mixtures that include Fabaceae could be an interesting mechanism to avoid potential disservices to beneficial communities, while maintaining suppressive effects on target pathogens. Further research, including field experiments, are needed to confirm the benefits of these mixtures.

References

  • Abideen SNU, Nadeem F, Abideen SA. 2013. Genetic variability and correlation studies in Brassica napus L. genotypes. Int J Inn Appl St 2(4): 574–581. [Google Scholar]
  • Altieri MA. 1999. The ecological role of biodiversity in agroecosystems. Agric Ecosyst Environ 74: 19–31. [Google Scholar]
  • Angus JF, Gardner PA, Kirkegaard JA, Desmarchelier JM. 1994. Biofumigation: isothiocyanates released from brassica roots inhibit growth of the take-all fungus. Plant Soil 162: 107–112. [Google Scholar]
  • Barzman M, Bàrberi P, Birch ANE, et al. 2015. Eight principles of integrated pest management. Agron Sustain Dev 35: 1199–1215. [Google Scholar]
  • Beilstein MA, Al-Shehbaz IA, Kellogg EA. 2006. Brassicaceae phylogeny and trichome evolution. Am J Bot 93(4): 607–619. [PubMed] [Google Scholar]
  • Bellostas N, Sørensen JC, Sørensen H. 2004. Qualitative and quantitative evaluation of glucosinolates in cruciferous plants during their life cycles. Agroindustria 3(3): 5–10. [Google Scholar]
  • Bending GD, Lincoln SD. 1999. Characterisation of volatile sulphur-containing compounds produced during decomposition of Brassica juncea tissues in soil. Soil Biol Biochem 31(5): 695–703. [Google Scholar]
  • Bending GD, Lincoln SD. 2000. Inhibition of soil nitrifying bacteria communities and their activities by glucosinolate hydrolysis products. Soil Biol Biochem 32(8–9): 1261–1269. [Google Scholar]
  • Berbegal M, García-Jiménez J, Armengol J. 2008. Effect of cauliflower residue amendments and soil solarization on Verticillium wilt control in artichoke. Plant Dis 92(4): 595–600. [CrossRef] [PubMed] [Google Scholar]
  • Bhandari SR, Jo JS, Lee JG. 2015. Comparison of glucosinolate profiles in different tissues of nine Brassica crops. Molecules 20(9): 15827–15841. [CrossRef] [PubMed] [Google Scholar]
  • Boag B, Smith WM, Griffiths DW. 1990. Observations on the grazing of double low oilseed rape and other crops by roe deer. Appl Anim Behav Sci 28(3): 213–220. [Google Scholar]
  • Booth EJ, Walker KC, Griffiths DW. 1991. A time-course study of the effect of sulphur on glucosinolates in oilseed rape (Brassica napus) from the vegetative stage to maturity. J Sci Food Agric 56(4): 479–493. [Google Scholar]
  • Borek V, Elberson LR, McCaffrey JP, Morra MJ. 1995a. Toxicity of aliphatic and aromatic isothiocyanates to eggs of the black vine weevil (Coleoptera: Curculionidae). J Econ Entomol 88(5): 1192–1196. [Google Scholar]
  • Borek V, Morra MJ, Brown PD, McCaffrey JP. 1995b. Transformation of the glucosinolate-derived allelochemicals allyl isothiocyanate and allylnitrile in soil. J Agric Food Chem 43(7): 1935–1940. [Google Scholar]
  • Borek V, Elberson LR, McCaffrey JP, Morra MJ. 1998. Toxicity of isothiocyanates produced by glucosinolates in Brassicaceae species to black vine weevil eggs. J Agric Food Chem 46(12): 5318–5323. [Google Scholar]
  • Borek V, Morra MJ. 2005. Ionic thiocyanate (SCN-) production from 4-hydroxybenzyl glucosinolate contained in Sinapis alba seed meal. J Agric Food Chem 53(22): 8650–8654. [CrossRef] [PubMed] [Google Scholar]
  • Brown PD, Morra MJ, McCaffrey JP, Auld DL, Williams L. 1991. Allelochemicals produced during glucosinolate degradation in soil. J Chem Ecol 17(10): 2021–2034. [CrossRef] [PubMed] [Google Scholar]
  • Brown PD, Morra MJ. 1997. Control of soil-borne plant pests using glucosinolate containing plants. Adv Agron 61: 167–231. [CrossRef] [Google Scholar]
  • Chapagain T, Lee EA, Raizada MN. 2020. The potential of multi-species mixtures to diversify cover crop benefits. Sustainability 12(2058): 1–16. [Google Scholar]
  • Clarkson J, Michel V, Neilson R. 2015. Mini-paper-Biofumigation for the control of soil-borne diseases. Available from http://ec.europa.eu/eip/agriculture/sites/agri-eip/files/9_eip_sbd_mp_biofumigation_final_0.pdf. [Google Scholar]
  • Constantin J, Beaudoin N, Laurent F, Cohan JP, Duyme F, Mary B. 2011. Cumulative effects of catch crops on nitrogen uptake, leaching and net mineralization. Plant Soil 341: 137–154. [Google Scholar]
  • Ćosić J, Jurković D, Vrandečić K, Kaučić D. 2012. Survival of buried Sclerotinia sclerotiorum sclerotia in undisturbed soil. Helia 35(56): 73–78. [CrossRef] [Google Scholar]
  • Couëdel A, Alletto L, Tribouillois H, Justes E. 2018a. Cover crop crucifer-legume mixtures provide effective nitrate catch crop and nitrogen green manure ecosystem services. Agric Ecosyst Environ 254: 50–59. [Google Scholar]
  • Couëdel A, Alletto L, Justes E. 2018b. Crucifer-legume cover crop mixtures provide effective sulphate catch crop and sulphur green manure services. Plant Soil 426(1–2): 61–76. [Google Scholar]
  • Couëdel A, Alletto L, Kirkegaard J, Justes E. 2018c. Crucifer glucosinolate production in legume-crucifer cover crop mixtures. Eur J Agron 96: 22–33. [Google Scholar]
  • Couëdel A, Kirkegaard J, Alletto L, Justes E. 2019. Crucifer-legume cover crop mixtures for biocontrol: toward a new multi-service paradigm. Adv Agron 157: 55–139. [CrossRef] [Google Scholar]
  • Davis JR, Huisman OC, Westermann DT, et al. 1996. Effects of green manures on Verticillium wilt of potato. Phytopathology 86(5): 444–453. [Google Scholar]
  • Davis JR, Huisman OC, Everson DO, Nolte P, Sorensen LH, Schneider AT. 2010. Ecological relationships of Verticillium wilt suppression of potato by green manures. Am J Potato Res 87(4): 315–326. [CrossRef] [Google Scholar]
  • Debaeke P, Casadebaig P, Flenet F, Langlade N. 2017a. Sunflower crop and climate change: vulnerability, adaptation, and mitigation potential from case-studies in Europe. OCL 24(1): D102. [CrossRef] [EDP Sciences] [Google Scholar]
  • Debaeke P, Bedoussac L, Bonnet C, et al. 2017b. Sunflower crop: environmental-friendly and agroecological. OCL 24(3): D304. [CrossRef] [EDP Sciences] [Google Scholar]
  • Di Primo P, Gamliel A, Austerweil M, et al. 2003. Accelerated degradation of metam-sodium and dazomet in soil: characterization and consequences for pathogen control. Crop Prot 22(4): 635–646. [Google Scholar]
  • Dufour V, Stahl M, Baysse C. 2015. The antibacterial properties of isothiocyanates. Microbiology 161(2): 229–243. [CrossRef] [PubMed] [Google Scholar]
  • Dungan RS, Gan J, Yates SR. 2003. Accelerated degradation of methyl isothiocyanate in soil. Water Air Soil Poll 142(1–4): 299–310. [CrossRef] [Google Scholar]
  • Duniway JM. 2002. Status of chemical alternatives to methyl bromide for pre-plant fumigation of soil. Phytopathology 92(12): 1337–1343. [CrossRef] [PubMed] [Google Scholar]
  • Fan CM, Xiong GR, Qi P, Ji GH, He YQ. 2008. Potential biofumigation effects of Brassica oleracea var. caulorapa on growth of fungi. J Phytopathol 156(6): 321–325. [CrossRef] [Google Scholar]
  • FAOSTAT. 2020. Available from http://www.fao.org/faostat/fr (last consult 30/06/2020). [Google Scholar]
  • FAO. 2018. FAO food outlook July 2018. Available from http://www.fao.org/3/ca0239en/CA0239EN.pdf (last consult 30/06/2020). [Google Scholar]
  • FAO. 2020. FAO food outlook June 2020. Available from http://www.fao.org/3/ca9509en/ca9509en.pdf (last consult 30/06/2020). [Google Scholar]
  • Fayzalla EA, El-Barougy E, El-Rayes MM. 2009. Control of soil-borne pathogenic fungi of soybean by biofumigation with mustard seed meal. J Appl Sci 9(12): 2272–2279. [CrossRef] [Google Scholar]
  • Fenwick GR, Heaney RK, Mullin WJ, VanEtten CH. 1983. Glucosinolates and their breakdown products in food and food plants. CRC Crit Rev Food Sci Nutr 18(2): 123–201. [Google Scholar]
  • Gardiner JB, Morra MJ, Eberlein CV, Brown PD, Borek V. 1999. Allelochemicals released in soil following incorporation of rapeseed (Brassica napus) green manures. J Agric Food Chem 47(9): 3837–3842. [CrossRef] [PubMed] [Google Scholar]
  • Garibaldi A, Gilardi G, Clematis F, Gullino ML, Lazzeri L, Malaguti L. 2009. Effect of green Brassica manure and Brassica defatted seed meals in combination with grafting and soil solarization against Verticillium wilt of eggplant and Fusarium wilt of lettuce and basil. In: 7th International Symposium on Chemical and Non-Chemical Soil and Substrate Disinfestation, Leuven, Belgium, Sep. 13–18, 2009. Conference Proceedings, p. 295. [Google Scholar]
  • Gimsing AL, Kirkegaard JA. 2006. Glucosinolate and isothiocyanate concentration in soil following incorporation of Brassica biofumigants. Soil Biol Biochem 38(8): 2255–2264. [Google Scholar]
  • Gimsing AL, Kirkegaard JA. 2009. Glucosinolates and biofumigation: fate of glucosinolates and their hydrolysis products in soil. Phytochem Rev 8: 299–310. [Google Scholar]
  • Goldman GH, Hayes C, Harman GE. 1994. Molecular and cellular biology of biocontrol by Trichoderma spp. Trends Biotechnol 12(12): 478–482. [CrossRef] [PubMed] [Google Scholar]
  • Haramoto ER, Gallandt ER. 2004. Brassica cover cropping for weed management: a review. Renew Agric Food Syst 19(4): 187–198. [CrossRef] [Google Scholar]
  • Harris HC, McWilliams JR, Mason WK. 1978. Influence of temperature on oil content and composition of sunflower seed. Aust J Agric Res 29: 1203–1212. [Google Scholar]
  • Hartz TK, Johnstone PR, Miyao EM, Davis RM. 2005. Mustard cover crops are ineffective in suppressing soilborne disease or improving processing tomato yield. HortScience 40(7): 2016–2019. [Google Scholar]
  • Hoffmann GM, Malkomes HP. 1974. Bromide residues in vegetable crops after soil fumigation with methyl bromide. Agric Environ 1(3): 321–328. [CrossRef] [Google Scholar]
  • Höglund AS, Rödin J, Larsson E, Rask L. 1992. Distribution of napin and cruciferin in developing rape seed embryos. Plant Physiol 98(2): 509–515. [Google Scholar]
  • Ibekwe AM. 2004. Effects of fumigants on non-target organisms in soils. Adv Agron 83: 2–37. [Google Scholar]
  • Iversen TH, Baggerud C. 1980. Myrosinase activity in differentiated and undifferentiated plants of Brassicaceae. Z Pflanzenphysiol 97(5): 399–407. [CrossRef] [Google Scholar]
  • Jensen ES. 1996. Grain yield, symbiotic N 2 fixation and interspecific competition for inorganic N in pea-barley intercrops. Plant Soil 182(1): 25–38. [Google Scholar]
  • Justes E, Richard G. 2017. Contexte, concepts et définition des cultures intermédiaires multi-services. Innov Agron 62: 1–15. [Google Scholar]
  • Justes E, Beaudoin N, Bertuzzi P, et al. 2012. The use of cover crops to reduce nitrate leaching: effect on the water and nitrogen balance and other ecosystem services. Synopsis of the study report. France: INRA, 68 p. [Google Scholar]
  • Katan J. 1981. Solar heating (solarization) of soil for control of soilborne pests. Annu Rev Phytopathol 19(1): 211–236. [Google Scholar]
  • Kirkegaard JA, Gardner PA, Desmarchelier JM, Angus JF. 1993. Biofumigation: using Brassica species to control pests and diseases in horticulture and agriculture. In: 9th Australian Research Assembly on Brassicas, Wagga Wagga, Australia, Oct. 5–7, 1993. Conference Proceedings, p. 77. [Google Scholar]
  • Kirkegaard JA, Sarwar M. 1998. Biofumigation potential of brassicas, I. Variation in glucosinolate profiles of diverse field-grown brassicas. Plant Soil 201: 71–89. [Google Scholar]
  • Kirkegaard JA, Sarwar M, Wong PTW, Mead A, Howe G, Newell M. 2000. Field studies on the biofumigation of take-all by Brassica break crops. Aust J Agric Res 51: 445–456. [Google Scholar]
  • Kirkegaard JA, Matthiessen JN. 2004. Developing and refining the biofumigation concept. Agroindustria 3(3): 233–239. [Google Scholar]
  • Kruger DHM, Fourie JC, Malan AP. 2013. Cover crops with biofumigation properties for the suppression of plant-parasitic nematodes: a review. S Afr J Enol Vitic 34(2): 287–295. [Google Scholar]
  • Kurt Ş, Güneş U, Soylu EM. 2011. In vitro and in vivo antifungal activity of synthetic pure isothiocyanates against Sclerotinia sclerotiorum. Pest Manag Sci 67(7): 869–875. [CrossRef] [PubMed] [Google Scholar]
  • Laegdsmand M, Gimsing AL, Strobel BW, Sørensen JC, Jacobsen OH, Hansen HCB. 2007. Leaching of isothiocyanates through intact soil following simulated biofumigation. Plant Soil 291(1–2): 81–92. [Google Scholar]
  • Lamichhane JR, Constantin J, Schoving C, et al. 2020. Analysis of soybean germination, emergence, and prediction of a possible northward establishment of the crop under climate change. Eur J Agron 113: 125972. [Google Scholar]
  • Larkin RP, Griffin TS, Honeycutt CW. 2010. Rotation and cover crop effects on soilborne potato diseases, tuber yield, and soil microbial communities. Plant Dis 94(12): 1491–1502. [CrossRef] [PubMed] [Google Scholar]
  • Lazzeri L, Tacconi R, Palmieri S. 1993. In vitro activity of some glucosinolates and their reaction products toward a population of the nematode Heterodera schachtii. J Agric Food Chem 41(5): 825–829. [Google Scholar]
  • Lazzeri L, Curto G, Leoni O, Dallavalle E. 2004. Effects of glucosinolates and their enzymatic hydrolysis products via myrosinase on the root-knot nematode Meloidogyne incognita (Kofoid et White) Chitw. J Agric Food Chem 52(22): 6703–6707. [CrossRef] [PubMed] [Google Scholar]
  • Li S, Schonhof I, Krumbein A, Li L, Stützel H, Schreiner M. 2007. Glucosinolate concentration in turnip (Brassica rapa ssp. rapifera L.) roots as affected by nitrogen and sulfur supply. J Agric Food Chem 55(21): 8452–8457. [CrossRef] [PubMed] [Google Scholar]
  • Macalady JL, Fuller ME, Scow KM. 1998. Effects of metam sodium fumigation on soil microbial activity and community structure. J Environ Qual 27(1): 54–63. [Google Scholar]
  • Manici LM, Lazzeri L, Palmieri S. 1997. In vitro fungitoxic activity of some glucosinolates and their enzyme-derived products toward plant pathogenic fungi. J Agric Food Chem 45(7): 2768–2773. [Google Scholar]
  • Manici LM, Lazzeri L, Baruzzi G, Leoni O, Galletti S, Palmieri S. 2000. Suppressive activity of some glucosinolate enzyme degradation products on Pythium irregulare and Rhizoctonia solani in sterile soil. Pest Manag Sci 56(10): 921–926. [Google Scholar]
  • Martin MJ, Riedel RM, Rowe RC. 1982. Verticillium dahliae and Pratylenchus penetrans: interactions in the early dying complex of potato in Ohio. Phytopathology 72(6): 640–644. [Google Scholar]
  • Martin FN. 2003. Development of alternative strategies for management of soilborne pathogens currently controlled with methyl bromide. Annu Rev Phytopathol 41(1): 325–350. [CrossRef] [PubMed] [Google Scholar]
  • Martín-Sanz A, Rueda S, García-Carneros AB, Molinero-Ruiz L. 2018. Cadophora malorum, a new threat for sunflower production in Russia and Ukraine. In: International Symposium, Sunflower and Climate Change, Toulouse, France, Feb. 5–6, 2018. Conference Proceedings, p. 52. [Google Scholar]
  • Matthiessen JN, Warton B, Shackleton MA. 2004. The importance of plant maceration and water addition in achieving high Brassica-derived isothiocyanate levels in soil. Agroindustria 3(3): 277–281. [Google Scholar]
  • Matthiessen JN, Shackleton MA. 2005. Biofumigation: environmental impacts on the biological activity of diverse pure and plant-derived isothiocyanates. Pest Manag Sci 61(11): 1043–1051. [CrossRef] [PubMed] [Google Scholar]
  • Matthiessen JN, Kirkegaard J. 2006. Biofumigation and enhanced biodegradation: opportunity and challenge in soilborne pest and disease management. Crit Rev Plant Sci 25: 235–265. [CrossRef] [Google Scholar]
  • Mawar R, Lodha S. 2002. Brassica amendments and summer irrigation for the control of Macrophomina phaseolina and Fusarium oxysporum f. sp. cumini in hot arid region. Phytopathol Mediterr 41(1): 45–54. [Google Scholar]
  • Mazzola M, Granatstein DM, Elfving DC, Mullinix K. 2001. Suppression of specific apple root pathogens by Brassica napus seed meal amendment regardless of glucosinolate content. Phytopathology 91(7): 673–679. [CrossRef] [PubMed] [Google Scholar]
  • Mazzola M, Brown J, Izzo AD, Cohen MF. 2007. Mechanism of action and efficacy of seed meal-induced pathogen suppression differ in a Brassicaceae species and time-dependent manner. Phytopathology 97(4): 454–460. [CrossRef] [PubMed] [Google Scholar]
  • Mazzola M, Agostini A, Cohen MF. 2017. Incorporation of Brassica seed meal soil amendment and wheat cultivation for control of Macrophomina phaseolina in strawberry. Eur J Plant Pathol 149(1): 57–71. [Google Scholar]
  • Médiène S, Valantin-Morison M, Sarthou JP, et al. 2011. Agroecosystem management and biotic interactions: a review. Agron Sustain Dev 31(3): 491–514. [Google Scholar]
  • Michel VV. 2008. Biofumigation − principe et application. Rev Suisse Vitic Arboric Hortic 40(2): 95–99. [Google Scholar]
  • Michel VV, Dahal-Tscherrig S, Ahmed H, Dutheil A. 2008. Biofumigation to control Verticillium wilt of strawberry: potency and pitfalls. In: Workshop on Integrated Soft Fruit Production, East Malling, United Kingdom, Sep. 24–27, 2007. Conference Proceedings, p. 169. [Google Scholar]
  • Michel VV. 2014. Ten years of biofumigation research in Switzerland. Asp Appl Biol 126: 33–42. [Google Scholar]
  • Mithen R. 2001. Glucosinolates − biochemistry, genetics and biological activity. Plant Growth Regul 34(1): 91–103. [Google Scholar]
  • Mol L, Scholte K, Vos J. 1995. Effects of crop rotation and removal of crop debris on the soil population of two isolates of Verticillium dahliae. Plant Pathol 44(6): 1070–1074. [Google Scholar]
  • Molinero-Ruiz L. 2019. Recent advances on the characterization and control of sunflower soilborne pathogens under climate change conditions. OCL 26: 2. [CrossRef] [EDP Sciences] [Google Scholar]
  • Morra MJ, Kirkegaard JA. 2002. Isothiocyanate release from soil-incorporated Brassica tissues. Soil Biol Biochem 34(11): 1683–1690. [Google Scholar]
  • Morra MJ, Borek V. 2010. Glucosinolate preservation in stored Brassicaceae seed meals. J Stored Prod Res 46(2): 98–102. [Google Scholar]
  • Morris EK, Fletcher R, Veresoglou SD. 2020. Effective methods of biofumigation: a meta-analysis. Plant Soil 446(1): 379–392. [Google Scholar]
  • Motisi N. 2009. Réguler les maladies d’origine tellurique par une culture intermédiaire de Brassicacées : mécanismes d’action et conditions d’expression dans une rotation betterave-blé. Thèse de doctorant. Agrocampus Ouest, Université européenne de Bretagne. [Google Scholar]
  • Motisi N, Montfort F, Faloya V, Lucas P, Doré T. 2009. Growing Brassica juncea as a cover crop, then incorporating its residues provide complementary control of Rhizoctonia root rot of sugar beet. Field Crop Res 113: 238–245. [CrossRef] [Google Scholar]
  • Motisi N, Doré T, Lucas P, Montfort F. 2010. Dealing with the variability in biofumigation efficacy through an epidemiological framework. Soil Biol Biochem 42, 2044–2057. [Google Scholar]
  • Neubauer C, Heitmann B, Müller C. 2014. Biofumigation potential of Brassicaceae cultivars to Verticillium dahliae. Eur J Plant Pathol 140(2): 341–352. [Google Scholar]
  • Neubauer C, Hüntemann K, Heitmann B, Müller C. 2015. Suppression of Verticillium dahliae by glucosinolate-containing seed meal amendments. Eur J Plant Pathol 142(2): 239–249. [Google Scholar]
  • Ntalli N, Caboni P. 2017. A review of isothiocyanates biofumigation activity on plant parasitic nematodes. Phytochem Rev 16(5): 827–834. [Google Scholar]
  • Ochiai N, Powelson ML, Dick RP, Crowe FJ. 2007. Effects of green manure type and amendment rate on Verticillium wilt severity and yield of Russet Burbank potato. Plant Dis 91(4): 400–406. [CrossRef] [PubMed] [Google Scholar]
  • Ochiai N, Powelson ML, Crowe FJ, Dick RP. 2008. Green manure effects on soil quality in relation to suppression of Verticillium wilt of potatoes. Biol Fert Soils 44(8): 1013–1023. [CrossRef] [Google Scholar]
  • Ojaghian MR, Jiang H, Xie GL, Cui ZQ, Zhang J, Li B. 2012. In vitro biofumigation of Brassica tissues against potato stem rot caused by Sclerotinia sclerotiorum. Plant Pathol J 28(2): 185–190. [Google Scholar]
  • Olivier C, Vaughn SF, Mizubuti ES, Loria R. 1999. Variation in allyl isothiocyanate production within Brassica species and correlation with fungicidal activity. J Chem Ecol 25(12): 2687–2701. [Google Scholar]
  • Omirou M, Rousidou C, Bekris F, et al. 2011. The impact of biofumigation and chemical fumigation methods on the structure and function of the soil microbial community. Microb Ecol 61(1): 201–213. [Google Scholar]
  • Pinkerton JN, Ivors KL, Miller ML, Moore LW. 2000. Effect of soil solarization and cover crops on populations of selected soilborne plant pathogens in western Oregon. Plant Dis 84(9): 952–960. [CrossRef] [PubMed] [Google Scholar]
  • Potter MJ, Vanstone VA, Davies KA, Rathjen AJ. 2000. Breeding to increase the concentration of 2-phenylethyl glucosinolate in the roots of Brassica napus. J Chem Ecol 26(8): 1811–1820. [Google Scholar]
  • Raaijmakers JM, Paulitz TC, Steinberg C, Alabouvette C, Moënne-Loccoz Y. 2009. The rhizosphere: a playground and battlefield for soilborne pathogens and beneficial microorganisms. Plant Soil 321(1–2): 341–361. [Google Scholar]
  • Rahimi F, Rahmanpour S, Rezaee S, Larijani K. 2014. Effect of volatiles derived from Brassica plants on the growth of Sclerotinia sclerotiorum. Arch Phytopathol Pfl 47(1): 15–28. [CrossRef] [Google Scholar]
  • Reau R, Bodet JM, Bordes JP, et al. 2005. Effets allélopathiques des Brassicacées via leurs actions sur les agents pathogènes telluriques et les mycorhizes : analyse bibliographique. Parite 1. OCL 12(3): 261–271. [CrossRef] [EDP Sciences] [Google Scholar]
  • Riga E. 2011. The effects of Brassica green manures on plant parasitic and free living nematodes used in combination with reduced rates of synthetic nematicides. J Nematol 43(2): 119–121. [PubMed] [Google Scholar]
  • Rowe RC, Powelson ML. 2002. Potato early dying: management challenges in a changing production environment. Plant Dis 86(11): 1184–1193. [CrossRef] [PubMed] [Google Scholar]
  • Rumberger A, Marschner P. 2003. 2-phenylethylisothiocyanate concentration and microbial community composition in the rhizosphere of canola. Soil Biol Biochem 35(3): 445–452. [Google Scholar]
  • Šárová J, Kudlikova I, Zalud Z, Veverka K. 2003. Macrophomina phaseolina (Tassi) Goid moving north temperature adaptation or change in climate? J Plant Dis Prot 110: 444–448. [Google Scholar]
  • Sarwar M, Kirkegaard, JA. 1998. Biofumigation potential of brassicas: II. Effect of environment and ontogeny on glucosinolate production and implications for screening. Plant Soil 201(1): 91–101. [Google Scholar]
  • Scholte K, s’Jacob JJ. 1990. Effect of crop rotation, cultivar and nematicide on growth and yield of potato (Solanum tuberosum L.) in short rotations on a marine clay soil. Potato Res 33(2): 191–200. [Google Scholar]
  • Sarwar M, Kirkegaard JA, Wong PTW, Desmarchelier JM. 1998. Biofumigation potential of brassicas, III In vitro toxicity of isothiocyanates to soil-borne fungal pathogens. Plant Soil 201: 103–112. [Google Scholar]
  • Seassau C. 2010. Étiologie du syndrome de dessèchement précoce du tournesol : implication de Phoma macdonaldii et interaction avec la conduite de culture. Thèse de doctorat. INP Toulouse. [Google Scholar]
  • Seassau C, Desserre D, Desplanques J, Mestries E, Dechamp-Guillaume G, Alletto L. 2016. Control of Verticillium dahliae causing sunflower wilt using Brassica cover crops. In: 19th International Sunflower Conference, Edirne, Turkey, Jun. 1–3, 2016. Conference Proceedings, p. 718. [Google Scholar]
  • Sharma SK, Aggarwal RK, Lodha S. 1995. Population changes of Macrophomina phaseolina and Fusarium oxysporum f. sp. cumini in oil-cake and crop residue-amended sandy soils. Appl Soil Ecol 2(4): 281–284. [Google Scholar]
  • Smith BJ, Kirkegaard JA. 2002. In vitro inhibition of soil microorganisms by 2-phenylethyl isothiocyanate. Plant Pathol 51(5): 585–593. [Google Scholar]
  • Subbarao KV, Hubbard JC, Koike ST. 1999. Evaluation of broccoli residue incorporation into field soil for Verticillium wilt control in cauliflower. Plant Dis 83(2): 124–129. [CrossRef] [PubMed] [Google Scholar]
  • Subbarao KV, Kabir Z, Martin FN, Koike ST. 2007. Management of soilborne diseases in strawberry using vegetable rotations. Plant Dis 91(8): 964–972. [CrossRef] [PubMed] [Google Scholar]
  • Therond O, Tichit M, Tibi A, et al. 2017. Volet « écosystèmes agricoles » de l’évaluation française des écosystèmes et des services écosystémiques. Rapport d’étude. France: INRA, 966 p. [Google Scholar]
  • Thorup-Kristensen K, Magid J, Jensen LS. 2003. Catch crops and green manures as biological tools in nitrogen management in temperate zones. Adv Agron 79: 227–302. [CrossRef] [Google Scholar]
  • Van Dam NM, Tytgat TO, Kirkegaard JA. 2009. Root and shoot glucosinolates: a comparison of their diversity, function and interactions in natural and managed ecosystems. Phytochem Rev 8(1): 171–186. [Google Scholar]
  • Vear F. 2016. Changes in sunflower breeding over the last fifty years. OCL 23(2): D202. [CrossRef] [EDP Sciences] [Google Scholar]
  • Warmington R, Clarkson JP. 2016. Volatiles from biofumigant plants have a direct effect on carpogenic germination of sclerotia and mycelial growth of Sclerotinia sclerotiorum. Plant Soil 401(1–2): 213–229. [Google Scholar]
  • Warton B, Matthiessen JN, Shackleton MA. 2003. Cross-enhancement: enhanced biodegradation of isothiocyanates in soils previously treated with metham sodium. Soil Biol Biochem 35(8): 1123–1127. [Google Scholar]
  • Watanabe T. 1973. Survivability of Macrophomina phaseoli (Maubl.) Ashby in naturally-infested soils and longevity of the sclerotia formed in vitro. Jpn J Phytopathol 39(4): 333–337. [CrossRef] [Google Scholar]
  • Wilhem S. 1955. Longevity of the Verticillium wilt fungus in the laboratory and field. Phytopathology 45: 180–181. [Google Scholar]
  • Wittstock U, Gershenzon J. 2002. Constitutive plant toxins and their role in defense against herbivores and pathogens. Curr Opin Plant Biol 5(4): 300–307. [CrossRef] [PubMed] [Google Scholar]

Cite this article as: Ait-Kaci Ahmed N, Dechamp-Guillaume G, Seassau C. 2020. Biofumigation to protect oilseed crops: focus on management of soilborne fungi of sunflower. OCL 27: 59.

All Tables

Table 1

Summary of the suppressive effects of GSLs/ITCs or Brassicaceae against three soilborne fungi of sunflower: Verticillium dahliae, Sclerotinia slcerotiorum and Macrophomina phaseolina using synthetic GSLs-/-ITCs in vitro or in pot (a), Brassicaceae in vitro or in pot (b), Brassicaceae in greenhouse and in the field (c), and at the rotation scale (d).

Target pathogen/plant: fungus studied and plant from which it was isolated (when mentioned); methods: GSLs/ITCs used or destruction/incorporation mechanisms of the Brassicaceae; Brassica species (cv./var.): the Brassicaceae and the cultivar or variety (when mentioned) used for biofumigation; crop to protect: the host plant; GSL/ITC measured: compounds in the Brassicaceae; 2-PE-ITC: 2-phenylethyl-isothiocyanate; a.o.t: among other treatments; Br: Brassicaceae; M.p: Macrophomina phaseolina; MS: microsclerotia; NA: not available; NS: not significant; S.s: Sclerotinia sclerotiorum; UC: unamended/untreated control; V.d: Verticillium dahlia; VW: Verticillium wilt.

In the text

Current usage metrics show cumulative count of Article Views (full-text article views including HTML views, PDF and ePub downloads, according to the available data) and Abstracts Views on Vision4Press platform.

Data correspond to usage on the plateform after 2015. The current usage metrics is available 48-96 hours after online publication and is updated daily on week days.

Initial download of the metrics may take a while.