Figures
Abstract
Interactions between herbivorous insects and plants storing terpenoids are poorly understood. This study describes the ability of Chrysolina herbacea to use volatiles emitted by undamaged Mentha aquatica plants as attractants and the plant's response to herbivory, which involves the production of deterrent molecules. Emitted plant volatiles were analyzed by GC-MS. The insect's response to plant volatiles was tested by Y-tube olfactometer bioassays. Total RNA was extracted from control plants, mechanically damaged leaves, and leaves damaged by herbivores. The terpenoid quantitative gene expressions (qPCR) were then assayed. Upon herbivory, M. aquatica synthesizes and emits (+)-menthofuran, which acts as a deterrent to C. herbacea. Herbivory was found to up-regulate the expression of genes involved in terpenoid biosynthesis. The increased emission of (+)-menthofuran was correlated with the upregulation of (+)-menthofuran synthase.
Citation: Atsbaha Zebelo S, Bertea CM, Bossi S, Occhipinti A, Gnavi G, Maffei ME (2011) Chrysolina herbacea Modulates Terpenoid Biosynthesis of Mentha aquatica L. PLoS ONE 6(3): e17195. https://doi.org/10.1371/journal.pone.0017195
Editor: Miguel Blazquez, Instituto de Biología Molecular y Celular de Plantas, Spain
Received: October 18, 2010; Accepted: January 23, 2011; Published: March 9, 2011
Copyright: © 2011 Atsbaha Zebelo et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: Financial support came from the doctorate school of Pharmaceutical and Biomolecular Sciences of the University of Turin. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Introduction
To deter herbivores, plants have evolved a broad range of defense mechanisms that can be generalized into two categories: pre-formed constitutive defenses and inducible defenses [1]. Constitutive defenses include the physical and chemical barriers that exist before insects attack, whereas induced defenses includes direct and indirect defenses. Direct defenses are plant traits that by themselves affect the susceptibility of host plants to insect attacks. Indirect defenses, on the other hand, include plant traits that by themselves do not affect the susceptibility of host plants, but can serve as attractants to natural enemies of attacking insects [2]–[7]. Insects may respond to plants by choosing different feeding sites, by altering their consumption rates or by induction of physiological/detoxification enzymes [8].
Approximately 90% of herbivorous insects have narrow host ranges, feeding on plants within a single taxonomic family, and many species are confined to a single host species [9]. The variability in fitness on different host plant species favors behavioral genotypes that restrict feeding to the most suitable hosts; on the other hand, maintaining mechanisms that nullify the disparate defensive adaptations of many different plant species is too costly for generalist herbivores [10]. Thus, the key to understanding why certain herbivores remain specialized lies in the observation that specialization involves both behavioral and physiological adaptation [8], [11], [12].
The defense strategy in aromatic plants like Mentha aquatica is a direct defense, through the constitutive production of terpenoids in specialized tissues known as the glandular trichomes [2]. These plants may have chemical barriers to potential herbivore colonists, and they appear to be accessible to relatively few insect lineages, which may be pre-adapted to chemically similar or related host plants [13]. As some insects become adapted to these metabolites, interactions between the two groups of organisms occasionally lead to highly specific relationships, as in the case of M. aquatica and the herbivore Chrysolina herbacea.
M. aquatica, or watermint, is a perennial plant belonging to the Lamiaceae. It produces leaf glandular trichomes secreting volatile organic compounds (VOCs) of varying chemical composition [14], [15]. The presence of the oxygenated monoterpenes (+)-pulegone and (+)-menthofuran contributes to the plant's toxicity. Both viridiflorol from the essential oil and (S)-naringenin from an ethanolic extract have been isolated by bioassay-guided fractionation with binding to the GABA-benzodiazepine site. Furthermore, M. aquatica contains psychoactive compounds that display both monoamine oxidase-inhibitory activity and mitochondrial respiration uncoupling [16]–[19]. At least 24 species of insect herbivores have been observed feeding on M. aquatica [20], [21], and among these, C. herbacea, also known as the mint beetle, is quite diffuse in mint fields. The feeding behavior of this beetle has been described recently [22]. Both larvae and adult beetles attack the leaves. Leaf beetles like C. herbacea are also known for their ability to import structurally distinct allelochemicals (reviewed by [23]). The ability to produce deterrents to natural enemies from plant-derived compounds is typical of some Chrysolina species [24]–[26]. Because herbivore feeding alters the aromatic profile of essential oil-producing plants like M. aquatica, the issue is both ecologically and economically relevant [27]–[29].
In this work we describe the chemical interaction between M. aquatica and C. herbacea by evaluating the ability of the herbivore to locate and recognize plant chemical cues and the capacity of the host plant to respond to herbivory by emitting deterrent molecules. To this end, plant VOC emissions we analyzed before and after herbivore feeding, and the ability of the emitted molecules to attract or deter C. herbacea was tested by bioassay.
Results
C. herbacea responds to M. aquatica VOC emission
Successful co-adaptation between plants and insects requires that plants produce specific compounds in response to herbivory, and that insects respond adequately to molecules emitted by plants. To look for possible relationships between M. aquatica VOC emissions and herbivore responses, the behavior of C. herbacea was first evaluated in Y-tube olfactometry tests.
C. herbacea was found to be attracted to undamaged plants, with respect to pure air. When the choice was between infested plants, undamaged plants or air, the insect was found to be deterred by infested plants (Fig. 1). Furthermore, the insects were found to lay eggs on undamaged plants and they produced larvae capable of surviving successive instars up to the adult phase (see Supporting Fig. S3). Preliminary studies demonstrated that the qualitative response of M. aquatica to larvae feeding was not significantly different from that of adult insects. For this reason, the study focused on adult insects.
A χ2 test served to evaluate differences from a 50∶50 distribution over two olfactometer arms. Insects that did not reach the end of either olfactometer arm within 10 min (NC: no choice) are indicated by white bars. The asterisks indicate significant (P<0.05) differences.
M. aquatica reacts to C. herbacea herbivory by emitting specific deterrent molecules
The reason why C. herbacea was differentially attracted to undamaged and infested plants was examined. VOCs emitted by untreated M. aquatica were analyzed by SPME, which revealed the presence of two major compounds, (+)-pulegone and (+)-menthofuran (Fig. 2a), along with other minor terpenoids including the monoterpenes (−)-limonene, (−)-menthone and α-terpineol, and the sesquiterpene, (E)-β-caryophyllene (Fig. 2b). However, it is important to note that the major compounds were emitted at much higher levels (0.13–0.75 µg g−1 f. wt) than the minor compounds in the range of 3–35 ng g−1 f. wt. The feeding activity of C. herbacea significantly changed the quantitative VOC composition of M. aquatica VOC emissions by dramatically increasing the content of (+)-menthofuran and decreasing the content of (+)-pulegone (Fig. 2a). The levels of all minor compounds, with particular reference to myrcene, were also elevated significantly upon herbivory; with the sole exception of p-cymene, which declined significantly (Fig. 2b). Since herbivory leads to the rupture of glandular trichomes, which are the main storage tissues of terpenoids in the Lamiaceae [2], [30], whether mechanical injury alone was able to increase the VOC emissions in M. aquatica was evaluated. Surprisingly, leaves damaged mechanically by a pattern wheel and having the same extent of herbivore damage had lower emissions of both major and minor compounds in comparison to control plants, particularly in comparison to herbivore wounded leaves (Figs. 2a and 2b).
a, Content of the major components; b, content of the minor components. Bars indicate the standard error over the mean of at least three biological replicates. Asterisks indicate significant differences with respect to controls (P<0.05).
C. herbacea responds differentially to specific monoterpenes emitted by M. aquatica
Following assessment of the chemical composition of the major VOCs released by undamaged and infested M. aquatica, the responses of C. herbacea to the main monoterpenes (+)-menthofuran and (+)-pulegone were tested. C. herbacea was significantly attracted to (+)-pulegone when the choice was limited to pure air, infested plants or (+)-menthofuran, whereas the insect preferred undamaged plants when offered with (+)-pulegone. On the contrary, (+)-menthofuran was always found to repel the insects, no matter which choice test was performed (Fig. 3). To evaluate whether the synthetic mixture composed of both major and minor compounds identified from leaf volatiles affected C. herbacea behavior, insect preference was determined by performing choice tests with several comparisons. C. herbacea was significantly attracted to the synthetic mixture typical of uninfested plants when compared to both air and a synthetic mixture typical of infested plants (Fig. 3). When only minor compounds of synthetic mixtures were compared to either air or other mixtures, no significant difference could be found (Fig. 3).
A χ2 test served toevaluate differences from a 50∶50 distribution over two olfactometer arms. Insects that did not reach the end of either olfactometer arm within 10 min (NC: no choice) are indicated by white bars. Asterisks indicate significant differences (P<0.05).
Feeding of C. herbacea induces terpenoid gene expression in M. aquatica
Herbivory was found to affect the percentage of some monoterpenes emitted by M. aquatica. For this reason, gene expression involved in the biosynthetic pathway leading to the bioactive monoterpenes (+)-pulegone and (+)-menthofuran was evaluated. Previous studies have established the biochemical pathway that in mints that leads to the production of these two important monoterpenes (Fig. 4) [31]. We considered early genes such as Dxs and Ippi, which are involved in the formation and isomerization of the precursors isopentenyl diphosphate (IPP) and dimethylallyl diphosphate (DMAPP), respectively. Dxp showed no regulation by either herbivory or mechanical damage, whereas Ippi was down-regulated by mechanical damage and up-regulated by herbivory. Gpps, the gene coding for the enzyme that condenses one unit each of IPP and DMAPP into the monoterpene precursor geranyl pyrophosphate (GPP), was up-regulated almost 3-fold by herbivory and to a lesser extent by mechanical damage. Ls, coding for the enzyme conducting cyclisation of the universal precursor GPP to the parent olefin (−)-limonene, showed the same trend as Ippi, being up-regulated by herbivory and down-regulated by mechanical damage (Fig. 5). Several genes were always up-regulated by herbivory and showed no regulation after mechanical damage (Fig. 5). The genes included L3oh, which codes for the enzyme responsible for the NADPH- and O2-dependent hydroxylation of (−)-limonene to (−)-trans-isopiperitenol, Ipd, which codes the operationally soluble, NAD-dependent isopiperitenol dehydrogenase that catalyzes allylic oxidation to the α,β-unsaturated ketone (−)-isopiperitenone, Ipr, which codes the soluble enzyme (−)-isopiperitenone reductase that catalyzes the stereospecific, NADPH-dependent reduction of (−)-isopiperitenone to (+)-(1R,4R)-cis-isopulegone, and Mfs, which codes for menthofuran synthase, an enzyme responsible for the transformation of (+)-pulegone to (+)-menthofuran (Fig. 4). Isopulegone isomerase, which catalyzes double bond migration and causes the isopropenyl double bond of (+)-(1R,4R)-cis-isopulegone to yield (+)-pulegone, has not yet been isolated and was not assayed. Finally, Pr, which codes for pulegone reductase, the enzyme responsible for NADPH-dependent reduction of the conjugated double bond of the terpenone to yield (−)-menthone, was down-regulated by herbivory and showed no significant regulation upon mechanical damage (Figs. 4 and 5).
Dxs, 1-deoxy-D-xylulose-5-phosphate synthase; Gpps indicates geranyl diphosphate synthase; Ls indicates (−)-limonene synthase; L3oh indicates (−)-limonene-3-hydroxylase; Ipd indicates (−)-(3S,4R)-trans-isopiperitenol dehydrogenase; Ipr indicates (−)-isopiperitenone reductase; Mfs indicates (+)-menthofuran synthase; and Pr indicates (+)-pulegone reductase.
Bars indicate the standard error over the mean of at least three biological replicates. Asterisks indicate significant differences with respect to controls (P<0.05).
Discussion
Over the past two decades it has been documented that plants produce blends of volatile compounds in vegetative tissues in response to damage and herbivore attack [4], [6], [32]–[38], suggesting that these substances act in plant defense [39]. Several lines of evidence indicate that VOCs released from vegetative tissues act as direct repellents against herbivores [40] and that the release of VOCs can result from the bursting of pre-existing structures in which volatiles are stored, such as glandular trichomes [41]. Plant VOCs can also attract natural enemies of attacking herbivores, such as parasitic wasps, flies, predatory mites or birds that can protect the signaling plant from further damage [7], [32], [37], [42], [43]
The results of this work show that C. herbacea is perfectly adapted to the blend of terpenoids emitted by undamaged M. aquatica and it uses this blend as a cue to locate plants. The fact that the insect lays eggs on undamaged plants is further evidence of such adaptation. In the case of the lepidopteran Plutella xylostella, the insect does not normally lay eggs on Chrysanthemum morifolium, because of the repellence of the monoterpene volatiles emitted from undamaged plants [44].
In the attracting blend of terpenoids produced by M. aquatica, (+)-pulegone was found to be the major compound in undamaged leaves and a potent attractant to C. herbacea in olfactometer bioassays. Volatiles emitted from plants can stimulate the behavioral or antennal responses of herbivores [45].
As a response to herbivore feeding, M. aquatica activates genes for terpenoid biosynthesis, diverting most of the terpene production toward the synthesis of (+)-menthofuran, which was found to repel C. herbacea in bioassay tests. Over the past decade, evidence that vegetative volatile compounds function to directly repel herbivores has begun to accumulate [39], [46]. However, the minor compounds emitted by uninfested and infested leaves were not effective in attracting or deterring C. herbacea.
An open question is why M. aquatica produces a herbivore attractant. One possible explanation is that the emission of (+)-pulegone is exploited by plants because of the antimicrobial [47], [48], nematocidal [49], acaricidal [50], antifeedant [51] and mitochondrial respiration uncoupling [19] properties of this compound. Preliminary studies have identified a C. herbacea egg parasite and studies on its behavior are under way.
This work suggests that constitutive plant defense can be modulated by interactions with herbivorous insects. The latter can trigger plant terpenoid gene expression and synthesis in a way that simple mechanical damage cannot. Usually, mechanical damage to plant foliage elevates VOC release in case of artificial damage carried out by researchers [40]; however, mechanically damaged M. aquatica does not exhibit emissions as intense or with the same compositional pattern as after herbivory.
Most genes directly involved in the biosynthesis of p-menthane monoterpenes in mints are transcriptionally regulated in a coordinated fashion [52] and it seems likely that the expression of these genes is controlled by a common transcription factor [53]. Herbivory had no effect on the expression of M. aquatica Dxs, a gene involved in the early steps of terpenoid biosynthesis for the mevalonate-independent (MEP)-pathway gene, the product of which is considered to catalyze one of the rate-limiting steps of this pathway [54]. On the contrary, herbivory up-regulated almost all other genes involved in the pathway. Over-expression of Gpps, Ls and L3oh would be expected to increase production of both GPP and other key monoterpenes [53]. The synthesis of (−)-limonene, providing the first committed intermediate of the pathway, is a possible rate limiting step of monoterpene production in mints [31]. Thus, the over-expression of both Gpps and Ls justifies the increase in the precursor (−)-limonene and the end-products of the pathway (particularly (+)-menthofuran). The up-regulation of Mfs parallels the increase in (+)-menthofuran; the latter was found to be a competitive inhibitor of Pr [55]. In transgenic lines with increased expression of Mfs and more (+)-menthofuran in the essential oil, (+)-pulegone amounts were greater than in controls. This finding led to the hypothesis that the metabolic fate of (+)-pulegone is controlled by (+)-menthofuran-mediated transcriptional down-regulation of Pr levels [56]. In M. aquatica, herbivory down-regulated the expression of Pr and up-regulated Ipr; however, the amounts of (+)-pulegone were never significantly different from those in the controls. This might indicate the presence of other factors that may exert post-translational control over the enzyme activity of Mfs or the regulation of the isopulegone isomerase, which has not yet been isolated.
In general, following herbivore attack, plants release green leaf volatiles (GLV), six-carbon aldehydes, alcohols, and esters, that are considered typical wound signals [4], [32], [57]–[59]. By contrast, significant amounts of green-leaf volatiles were not emitted by M. aquatica during herbivory. This may be related the high amount of terpenoids produced in the glandular trichomes; by comparison plants that do not accumulate these compounds in secretory tissues (e.g., Arabidopsis or Lima bean) usually released smaller amounts of terpenoids [36], [60]. In some cases it has been suggested that oxidative damage of membranes is one of the primary factors inducing GLV emissions [58]. The function of VOCs in alleviating oxidative stresses has been shown to be related to the high reactivity of certain monoterpenes [40], suggesting that the release of VOCs upon herbivory in M. aquatica might have other functions in addition to deterrence.
The proportions of emitted monoterpenes (VOCs) may differ from those in the plant oil of glandular trichomes with regard to chemical composition [27], [61]. Nonetheless, molecular data support the hypothesis that terpenoid biosynthesis is modulated by C. herbacea herbivory.
In conclusion, C. herbacea attacks undamaged M. aquatica, but it avoids herbivore-infested M. aquatica. Upon herbivory, M. aquatica produces repellent compounds, thus reducing the damage from further insect attacks (Fig. 6, see also Supporting Fig. S4).
a, Undamaged plants emit (+)-pulegone, which acts as an attractant for C. herbacea. b, Feeding activity induces gene expression and increases content of the deterrent compound (+)-menthofuran, along with the emission of the attractant compound (+)-pulegone; as a result, fewer insects are attracted to the plants. c, Intense feeding induces a reduction in (+)-pulegone content and a dramatic increase in the repellent compound (+)-menthofuran; C. herbacea avoids over-fed plants and moves towards undamaged plants.
Materials and Methods
Plant material and growth conditions
Stolons of Mentha aquatica L. were collected from wild populations growing in Cambiano (Turin province, Italy, alt 240 m a.s.l.) and San Secondo di Pinerolo (Turin province, Italy, alt 413 m a.s.l.). Stolons were surface sterilized with 70% ethanol (Sigma-Aldrich, St. Louis, MO, USA) for 20 s and with sodium hypochlorite (1% v/v available chlorine) (Sigma-Aldrich) for 5 min. Stolons were then rinsed three times with sterile distilled water. Plants were grown in plastic pots with sterilized peat and vermiculite (V/V 4∶1) at 23°C and 60% humidity using daylight fluorescent tubes at 270 µE m−2 s−1 with a photophase of 16 h.
Insect collection and rearing
Adults of Chrysolina herbacea (Duftschmid 1825) (Coleoptera, Chrysomelidae, Chrysomelinae) were collected by hand picking from infested M. aquatica fields. After collection, beetles were reared at 22°C in ventilated glass chambers and fed to M. aquatica cuttings. The beetles were starved for 24 h. prior the experiments.
Collection of plant volatiles, gas chromatography and mass spectrometry
Experiments were conducted in 4 l glass desiccators by using non-flowering M. aquatica five-node cuttings, placed in 100 ml Erlenmeyer's flasks filled with 60 ml tap water and sealed with aluminium foil to prevent fall of insects into the water during experiments. Three cuttings per flask in a single desiccator where used. Plants were illuminated with fluorescent light bulbs generating about 50 µmol m−2 s−1 with a photophase of 16 h, the temperature inside desiccators was about 24°C and the relative humidity about 70%. Glass desiccators were connected to a GC-grade air generator (HPZA-3500-220, Parker Balston, Cleveland, OH, USA) through a cork plug with two openings allowing gases to go in and out. Air was pumped into the jars at a flow rate of 300 ml min−1. A clean Pasteur glass pipette was inserted in the outlet of the cork plug and VOCs were sampled with a Carboxen/Polydimethylsiloxane (CAR/PDMS) Supelco (Bellefonte, PA, USA) solid-phase micro-extraction (SPME) fibre (model 57334-U). Before use, SPME fibres were always conditioned at 250°C, according to manufacturer's instructions (see also Supporting Fig. S1 for more details).
Undamaged plants, leaves mechanically damaged with a pattern wheel and plants infested for 6 h were assayed for VOC emission. All experiments were standardized at 6 h, because the presence of eight herbivores for 6 h was found to cause about 30% of leaf damage.
SPME fibres, which were placed in various paths to adsorb VOCc for 6 h (see Supporting Figs. S1 and S2), were desorpted and VOCs were analyzed by gas-chromatography mass spectrometry (GC-MS 6890N-5973A, Agilent Technologies, Santa Clara, CA, US). The desorpted compounds were separated on a ZB-5MS Zebron (7HG-G010-11, Phenomenex, Torrance, CA, US) capillary column (stationary phase: polydimethylsiloxane - 5% diphenyl, 30 m length, 250 µm internal diameter, and 0.25 µm film thickness) with a temperature program of 60°C (kept for 5 min) followed by a temperature rise at a rate of 3°C min−1 to 270°C (kept for 5 min). Working conditions were: injector 250°C, transfer line to MSD 280°C, oven temperature: start 60°C, hold 5 min, programmed from 60°C to 270°C at 3°C min-1, hold 5 min; carrier gas was He under a constant flow of 1 ml min-1; in SPME desorption and subsequent analysis the fibre was exposed in the injection port during the entire GC run; the injector was maintained in splitless mode during the desorption phase; ionization energy: EI 70 eV; acquisition parameters: scanned m/z 50–250 amu. Separated compounds were identified by pure standard comparison, by comparison of their mass spectra and retention indexes (Kováts indexes) with those of reference substances and by comparison with the NIST mass spectral search software v2.0 using the libraries NIST 98 library and Adams [62] library. Different concentraitions of (+)-menthofuran, (+)-pulegone, myrcene, p-cymene, (−)-limonene, (−)-menthone, α-terpineol and (E)-β-caryophyllene were used to create a standard curve used as an external standard for SPME quantitative measurements. Reference compounds were mixed in relative proportions similar to those that were quantified in the plant samples.
Total RNA extraction and quantitative Real Time-PCR (qPCR)
After each experiment, leaves were collected and immediately frozen in liquid nitrogen. One hundred mg of frozen control, herbivore damaged, and mechanically damaged leaves were ground in liquid nitrogen with mortar and pestle. Total RNA was isolated using Qiagen RNeasy Plant RNA kit and RNase-Free DNase set (Qiagen, Hilden, Germany). Sample quality and quantity was checked by using the RNA 6000 Nano kit and the Agilent 2100 Bioanalyzer (Agilent Technologies) according to manufacturer's instructions. Quantification of RNA was also confirmed spectrophotometrically by using a NanoDrop ND-1000 (Thermo Fisher Scientific, Waltham, MA, US).
First strand cDNA synthesis was accomplished with 2 µg of total RNA and random primers using the High-Capacity cDNA Reverse Transcription Kit (Applied Biosystems, Foster City, CA, US), according to the manufacturer's recommendations. Primers for real-time PCR were designed on Mentha piperita available sequences using the Primer 3 software [63]. qPCR was done on an Mx3000P Real-Time PCR System (Stratagene, La Jolla, CA, US). The reaction was performed with 25 µl of mixture consisting of 12.5 µl of 2× Maxima™ SYBR Green qPCR Master Mix (Fermentas International, Inc, Burlington, ON, Canada), 0.5 µl of cDNA and 100 nM primers (Integrated DNA Technologies, Coralville, IA, US).
Relative RNA levels were calibrated and normalized with the level of two housekeeping genes: actin and 18S ribosomal mRNA.
PCR conditions were determined by comparing threshold values in dilution series of the RT product, followed by non-template control for each primer pair. Relative expression levels of genes were calculated by using the Pfaffl method [64]. A suitable melt curve analysis was always performed.
PCR conditions were the following: 18S: initial polymerase activation of 10 min at 95°C; and 40 cycles of 15 s at 95°C, 30 s at 58°C, and 30 s at 72°C; Actin: initial polymerase activation of 10 min at 95°C; and 40 cycles of 15 s at 95°C, 30 s at 57°C, and 30 s at 72°C; Dxs: initial polymerase activation of 10 min at 95°C; and 40 cycles of 15 s at 95°C, 30 s at 58°C, and 30 s at 72°C; Ippi: initial polymerase activation of 10 min at 95°C; and 40 cycles of 15 s at 95°C, 30 s at 57°C, and 30 s at 72°C; Gpps: initial polymerase activation of 10 min at 95°C; and 40 cycles of 15 s at 95°C, 30 s at 58°C, and 30 s at 72°C; Ls: initial polymerase activation of 10 min at 95°C; and 40 cycles of 15 s at 95°C, 30 s at 57°C, and 30 s at 72°C; L3oh: initial polymerase activation of 10 min at 95°C; and 40 cycles of 15 s at 95°C, 30 s at 57°C, and 30 s at 72°C; Ipd: initial polymerase activation of 10 min at 95°C; and 40 cycles of 15 s at 95°C, 30 s at 58°C, and 30 s at 72°C ; Ipr: initial polymerase activation of 10 min at 95°C; and 40 cycles of 15 s at 95°C, 30 s at 57°C, and 30 s at 72°C; Pr: initial polymerase activation of 10 min at 95°C; and 40 cycles of 15 s at 95°C, 30 s at 57°C, and 30 s at 72°C; Mfs: initial polymerase activation of 10 min at 95°C; and 40 cycles of 15 s at 95°C, 30 s at 58°C, and 30 s at 72°C.
Primers used for qPCR were the following: 18S, (NCBI GenBank accession no. NR_022795), forward primer 5′-ATGATAACTCGACGGATCGC-3′, reverse primer 5′-CTTGGATGTGGTAGCCGTTT -3′; actin, (NCBI GenBank accession no. AW255057), forward primer 5′-GCTCCAAGGGCTGTGTTCC-3′, reverse primer 5′- TCTTTCTGTCCCATGCCAAC-3′ [65]. Dxs, (NCBI GenBank accession no. AF019383), [66], forward primer 5′-CCACCAGGCTTACCCACACAA-3′, reverse primer 5′-GCCACCGCCATCCCTAAAC-3. Ippi, (NCBI GenBank accession no. AW255524), [65], forward primer 5′-CTCTTGGGGTGAGAAATGCT-3′ reverse primer 5′-CATCTGAGGGGGCTTTGTA-3. Gpps, (NCBI GenBank accession no. EU108696), [67], forward primer 5′-ATGATAAGCGGGCTGCATAG-3′ reverse primer 5′-CCGAAATTCCTCAGCTTCTG-3′. Ls, (NCBI GenBank accession no. AW255536), [65], forward primer 5′-CGGTGGTGGAGAAATACTGGGTTT-3′, reverse primer 5′-CCGTAATCAGAGCGTGACTTTGC-3′. L3oh, (NCBI GenBank accession no. AF124817), [68], forward primer 5′-CCCCATCACCACCAACTCCA-3′, reverse primer 5′-GCTCCGCCAGCACCCATAG-3′; Ipd, (NCBI GenBank accession no. AY641428), [69], forward primer 5′-GAGCTTCTATGGGCAGGTCA-3′, reverse primer 5′- GGCCACGAATGGTAAACACT-3′. Ipr, (NCBI GenBank accession no. AY300162), [70], forward primer 5′-AGCCAATGGAGAAATGATCG-3′, reverse primer 5′- GAGAGGAATGAGGGCTTGTG-3′. Pr, (NCBI GenBank accession no. AAQ75423), [70], forward primer 5′-ACAGCCTGAAGCAGCCTGAA-3′, reverse primer 5′-CGGCAGAACCATCTCAAGGA-3′. Mfs, (NCBI GenBank accession no. AF346833), [71], forward primer 5′-GCAGAACGAGGTGCGAGAAG -3′, reverse primer 5′-TGCGAAAGGTGGATGTAGGC-3′. The length of PCR products was from 98 to 200 bp.
Bioassays
Experiments were conducted in a glass Y-tube olfactometer connected to the glass jars. GC-grade air was pumped into the jars at a flow rate of 300 ml min−1. The Y-tube was housed in a blackened box with a diffused fluorescent lamp giving a constant light directly above the centre point of the Y-tube. Thirty C. herbacea were monitored for up to 7 min by recording “choice” or “no-choice” events. All glassware was carefully washed to remove any contaminating substances and air-dried at 120°C for 4 h to remove volatile compounds. Test temperature was maintained at about 24°C and 70% humidity. (+)-Menthofuran, (−)-pulegone, myrcene, p-cymene, (−)-limonene, (−)-menthone, α-terpineol and (E)-β-caryophyllene pure standards were purchased from Sigma-Aldrich and were used in chemical tests (see also Supporting Fig. S2). The concentration of pure standards in Y-tube tests was used at the same concentrations as found in leaf volatile emissions.
Statistical analysis
Initial and final choice data were analyzed using a Chi-squared test. Yates' correction was applied to adjust for the data with only one degree of freedom. Data were also statistically processed using a log-likelihood test (G-test) and by ANOVA by using the statistical program SPSS (version 16.0,SPSS Inc., Chicago, IL, USA). For genomic and chemical analyses, the overall data sets are expressed as mean values of at least three biological replicates each one repeated three times (technical replicates). Metric bars indicate SD. Significance of differences observed in data sets was tested by ANOVA using the SYSTAT 10 software.
Supporting Information
Figure S1.
Left panel, glass desiccators containing the plants are connected to the GC-grade air generator. The cork plug has two holes: one for allowing the GC-grade air to enter the jar and the other hosts a glass Pasteur pipette. In the right figure the arrow indicates the SPME fibre that adsorbs the VOCs exiting from the jar.
https://doi.org/10.1371/journal.pone.0017195.s001
(PDF)
Figure S2.
Left panel, a glass Y-tube olfactometer is connected to the jars where a flux of GC-grade air blows the VOCs produced by undamaged and infested leaves. Arrows indicate the presence of the SPME fibre which is located just before the olfactometer arms, into the air path. Right upper panel shows C. herbacea making a choice. The lower right panel shows the flow-meter used to standardize the air flow blowing from the jars and the timer used during the choice tests.
https://doi.org/10.1371/journal.pone.0017195.s002
(PDF)
Figure S3.
C. herbacea was found to lay eggs on undamaged M. aquatica plants. The left panel shows clutches of eggs laid on a young M. aquatica leaf. The right panel shows young C. herbacea larvae feeding on M. aquatica leaves.
https://doi.org/10.1371/journal.pone.0017195.s003
(PDF)
Figure S4.
M. aquatica plants observed in the wild. The upper left panel shows an undamaged M. aquatica in full bloom. The upper right panel shows male and female C. herbacea mating on partially damaged M. aquatica leaves. The two lower panels show the typical level of damage inferred by C. herbacea on wild M. aquatica leaves.
https://doi.org/10.1371/journal.pone.0017195.s004
(PDF)
Author Contributions
Conceived and designed the experiments: MEM SAZ. Performed the experiments: SAZ CMB SB AO GG. Analyzed the data: MEM SAZ GG. Contributed reagents/materials/analysis tools: MEM. Wrote the paper: MEM SAZ.
References
- 1. Chen MS (2008) Inducible direct plant defense against insect herbivores: A review. Insect Sci 15: 101–114.
- 2. Maffei M (2010) Sites of synthesis, biochemistry and functional role of plant volatiles. S Afr J Bot. In press, doi:10.1016/j.sajb.2010.03.003.
- 3. Dicke M, Loreto F (2010) Induced plant volatiles: from genes to climate change. Trends Plant Sci 15: 115–117.
- 4. Dicke M, Baldwin IT (2010) The evolutionary context for herbivore-induced plant volatiles: beyond the ‘cry for help’. Trends Plant Sci 15: 167–175.
- 5. Van Poecke RMP, Dicke M (2004) Indirect defence of plants against herbivores: Using Arabidopsis thaliana as a model plant. Plant Biol 6: 387–401.
- 6. Howe GA, Jander G (2008) Plant immunity to insect herbivores. Ann Rev Plant Biol 59: 41–66.
- 7. Kessler A, Baldwin IT (2001) Defensive function of herbivore-induced plant volatile emissions in nature. Science 291: 2141–2144.
- 8. Scriber JM (2002) Evolution of insect-plant relationships: chemical constraints, coadaptation, and concordance of insect/plant traits. Entomol Exper Appl 104: 217–235.
- 9.
Strong DR, Lawton JH, Southwood R (1984) Insects on plants. Cambridge: Harvard University Press.
- 10. Rausher MD (2001) Co-evolution and plant resistance to natural enemies. Nature 411: 857–864.
- 11. Cogni R, Futuyma DJ (2009) Local adaptation in a plant herbivore interaction depends on the spatial scale. Biol J Linn Soc 97: 494–502.
- 12. Smiseth PT, Wright J, Kolliker M (2008) Parent-offspring conflict and co-adaptation: behavioural ecology meets quantitative genetics. Proc Royal Soc B-Biol Sci 275: 1823–1830.
- 13. Farrell BD, Mitter C (1994) Adaptive radiation in insects and plants - Time and opportunity. Amer Zool 34: 57–69.
- 14. Malingré TM, Maarse H (1974) Composition of essential oil of Mentha aquatica. Phytochemistry 13: 1531–1535.
- 15. Jerkovic I, Mastelic J (2001) Composition of free and glycosidically bound volatiles of Mentha aquatica L. Croat Chem Acta 74: 431–439.
- 16. Jager AK, Almqvist JP, Vangsoe SAK, Stafford GI, Adsersen A, et al. (2007) Compounds from Mentha aquatica with affinity to the GABA-benzodiazepine receptor. S Afr J Bot 73: 518–521.
- 17. Olsen HT, Stafford GI, van Staden J, Christensen SB, Jager AK (2008) Isolation of the MAO-inhibitor naringenin from Mentha aquatica L. J Ethnopharmacol 117: 500–502.
- 18. van Staden J, Stafford GI, Almqvist JP, Vangsoe SAK, Olsen HT, et al. (2007) Psychotropic constituents of Mentha aquatica L. Planta Med 73: 339.
- 19. Mucciarelli M, Camusso W, Bertea CM, Bossi S, Maffei M (2001) Effect of (+)-pulegone and other oil components of Mentha x piperita on cucumber respiration. Phytochemistry 57: 91–98.
- 20. Warren PH (1993) Insect herbivory on water mint - You can't get there from here. Ecography 16: 11–15.
- 21.
Horwood AR (1919) British Wild Flowers - In Their Natural Haunts, The Gresham Publishing
Company.
- 22. Bienkowski AO (2009) Feeding Behavior of Leaf-Beetles (Coleoptera, Chrysomelidae). Zool Z 88: 1471–1480.
- 23. Burse A, Frick S, Discher S, Tolzin-Banasch K, Kirsch R, et al. (2009) Always being well prepared for defense: The production of deterrents by juvenile Chrysomelina beetles (Chrysomelidae). Phytochemistry 70: 1899–1909.
- 24. Pasteels JM, Duffey S, Rowellrahier M (1990) Toxins in Chrysomelid beetles - Possible evolutionary sequence from de novo synthesis to derivation from food-plant chemicals. J Chem Ecol 16: 211–222.
- 25. Laurent P, Braekman JC, Daloze D, Pasteels J (2003) Biosynthesis of defensive compounds from beetles and ants. Eur J Org Chem 2003: 2733–2743.
- 26. Laurent P, Braekman JC, Daloze S (2005) Insect chemical defense. Chem Pherom Oth Semiochem 240: 167–229.
- 27. Banchio E, Valladares G, Zygadlo J, Bogino PC, Rinaudi LV, et al. (2007) Changes in composition of essential oils and volatile emissions of Minthostachys mollis, induced by leaf punctures of Liriomyza huidobrensis. Biochem Syst Ecol 35: 68–74.
- 28. Banchio E, Zygadlo Y, Valladares GR (2005) Effects of mechanical wounding on essential oil composition and emission of volatiles from Minthostachys mollis. J Chem Ecol 31: 719–727.
- 29. Valladares GR, Zapata A, Zygadlo J, Banchio E (2002) Phytochemical induction by herbivores could affect quality of essential oils from aromatic plants. J Agric Food Chem 50: 4059–4061.
- 30. Maffei M, Chialva F, Sacco T (1989) Glandular trichomes and essential oil in developing peppermint leaves. I. Variation in peltate trichome number and terpene distribution within leaves. New Phytol 111: 707–716.
- 31. Croteau RB, Davis EM, Ringer KL, Wildung MR (2005) (−)-Menthol biosynthesis and molecular genetics. Naturwiss 92: 562–577.
- 32. Dudareva N, Negre F, Nagegowda DA, Orlova I (2006) Plant volatiles: Recent advances and future perspectives. Crit Rev Plant Sci 25: 417–440.
- 33. Heil M, Silva Bueno JC (2007) Within-plant signaling by volatiles leads to induction and priming of an indirect plant defense in nature. Proc Natl Acad Sci U S A 104: 5467–5472.
- 34. Baldwin IT, Halitschke R, Paschold A, von Dahl CC, Preston CA (2006) Volatile signaling in plant-plant interactions: “Talking trees” in the genomics era. Science 311: 812–815.
- 35. Maffei ME, Mithofer A, Boland W (2007) Before gene expression: early events in plant-insect interaction. Trends Plant Sci 12: 310–316.
- 36. Maffei ME, Mithofer A, Boland W (2007) Insects feeding on plants: Rapid signals and responses preceding the induction of phytochemical release. Phytochemistry 68: 2946–2959.
- 37.
Mithöfer A, Boland W, Maffei ME (2009) Chemical ecology of plant-insect interactions. In: Parker J, editor. Molecular Aspects of Plant Disease Resistance. Chirchester: Wiley-Blackwell. pp. 261–291.
- 38. Heil M (2008) Indirect defence via tritrophic interactions. New Phytol 178: 41–61.
- 39. Unsicker SB, Kunert G, Gershenzon J (2009) Protective perfumes: the role of vegetative volatiles in plant defense against herbivores. Curr Opin Plant Biol 12: 479–485.
- 40. Holopainen JK, Gershenzon J (2010) Multiple stress factors and the emission of plant VOCs. Trends Plant Sci 15: 176–184.
- 41. Paré PW, Tumlinson JH (1997) De novo biosynthesis of volatiles induced by insect herbivory in cotton plants. Plant Physiol 114: 1161–1167.
- 42. Turlings TCJ, Tumlinson JH, Lewis WJ (1990) Exploitation of herbivore-induced plant odors by host-seeking parasitic wasps. Science 250: 1251–1253.
- 43. Mäntylä E, Alessio GA, Blande JD, Heijari J, Holopainen JK, et al. (2008) From plants to birds: Higher avian predation rates in trees responding to insect herbivory. Plos One 3:
- 44. Wang H, Guo WF, Zhang PJ, Wu ZY, Liu SS (2008) Experience-induced habituation and preference towards non-host plant odors in ovipositing females of a moth. J Chem Ecol 34: 330–338.
- 45. Zhao YX, Kang L (2003) Olfactory responses of the leafminer Liriomyza sativae (Dipt., Agromyzidae) to the odours of host and non-host plants. J App Entomol-Z Angew Entomol 127: 80–84.
- 46. Scharf ME, Nguyen SN, Song C (2006) Evaluation of volatile low molecular weight insecticides using Drosophila melanogaster as a model. Pest Manag Sci 62: 655–663.
- 47. Mkaddem M, Bouajila J, Ennajar M, Lebrihi A, Mathieu F, et al. (2009) Chemical composition and antimicrobial and antioxidant activities of Mentha (longifolia L. and viridis) essential oils. J Food Sci 74: M358–M363.
- 48. Mora FD, Araque M, Rojas LB, Ramirez R, Silva B, et al. (2009) Chemical composition and in vitro antibacterial activity of the essential oil of Minthostachys mollis (Kunth) Griseb Vaught from the Venezuelan Andes. Nat Prod Comm 4: 997–1000.
- 49. Ntalli NG, Ferrari F, Giannakou I, Menkissoglu-Spiroudi U (2010) Phytochemistry and nematicidal activity of the essential oils from 8 Greek Lamiaceae aromatic plants and 13 terpene components. J Agric Food Chem 58: 7856–7863.
- 50. Ribeiro VL, Dos Santos JC, Bordignon SA, Apel MA, Henriques AT, et al. (2010) Acaricidal properties of the essential oil from Hesperozygis ringens (Lamiaceae) on the cattle tick Riphicephalus (Boophilus) microplus. Biores Technol 101: 2506–2509.
- 51. Dancewicz K, Gabrys B, Dams I, Wawrzenczyk C (2008) Enantiospecific effect of pulegone and pulegone-derived lactones on Myzus persicae (Sulz.) settling and feeding. J Chem Ecol 34: 530–538.
- 52. McConkey ME, Gershenzon J, Croteau RB (2000) Developmental regulation of monoterpene biosynthesis in the glandular trichomes of peppermint. Plant Physiol 122: 215–223.
- 53. Mahmoud SS, Croteau RB (2002) Strategies for transgenic manipulation of monoterpene biosynthesis in plants. Trends Plant Sci 7: 366–373.
- 54. Estevez JM, Cantero A, Reindl A, Reichler S, Leon P (2001) 1-deoxy-D-xylulose-5-phosphate synthase, a limiting enzyme for plastidic isoprenoid biosynthesis in plants. J Biol Chem 276: 22901–22909.
- 55. Rios-Estepa R, Turner GW, Lee JM, Croteau RB, Lange BM (2008) A systems biology approach identifies the biochemical mechanisms regulating monoterpenoid essential oil composition in peppermint. Proc Natl Acad Sci U S A 105: 2818–2823.
- 56. Mahmoud SS, Croteau RB (2003) Menthofuran regulates essential oil biosynthesis in peppermint by controlling a downstream monoterpene reductase. Proc Natl Acad Sci U S A 100: 14481–14486.
- 57. Frost Cj, Mescher MC, Dervinis C, Davis JM, Carlson JE, et al. (2008) Priming defense genes and metabolites in hybrid poplar by the green leaf volatile cis-3-hexenyl acetate. New Phytol 180: 722–734.
- 58. Arimura G, Matsui K, Takabayashi J (2009) Chemical and molecular ecology of herbivore-induced plant volatiles: proximate factors and their ultimate functions. Plant Cell Physiol 50: 911–923.
- 59. Matsui K (2006) Green leaf volatiles: hydroperoxide lyase pathway of oxylipin metabolism. Curr Opin Plant Biol 9: 274–280.
- 60. Aharoni A, Giri AP, Deuerlein S, Griepink F, de Kogel WJ, et al. (2003) Terpenoid metabolism in wild-type and transgenic Arabidopsis plants. Plant Cell 15: 2866–2884.
- 61. Gershenzon J, McConkey ME, Croteau RB (2000) Regulation of monoterpene accumulation in leaves of peppermint. Plant Physiol 122: 205–213.
- 62.
Adams RP (2001) Identification of essential oil component by gas
chromatography/quadrupole mass spectroscopy. Carol Stream, , IL: Allured Publishing Corporation.
- 63.
Rozen S, Skaletsky H (2000) Primer3 on the WWW for general users and for biologist
programmers. In: Krawetz S Misener S, editor. Bioinformatics Methods and Protocols. Totowa: Humana Press. pp. 365–386.
- 64. Luciano P, Bertea CM, Temporale G, Maffei ME (2007) DNA internal standard for the quantitative determination of hallucinogenic plants in plant mixtures. For Sci Internat: Genetics 1: 262–266.
- 65. Lange BM, Wildung MR, Stauber EJ, Sanchez C, Pouchnik D, et al. (2000) Probing essential oil biosynthesis and secretion by functional evaluation of expressed sequence tags from mint glandular trichomes. Proc Natl Acad Sci U S A 97: 2934–2939.
- 66. Lange BM, Wildung MR, Mccaskill D, Croteau R (1998) A family of transketolases that directs isoprenoid biosynthesis via a mevalonate-independent pathway. Proc Natl Acad Sci U S A 95: 2100–2104.
- 67. Burke CC, Wildung MR, Croteau R (1999) Geranyl diphosphate synthase: Cloning, expression, and characterization of this prenyltransferase as a heterodimer. Proc Natl Acad Sci U S A 96: 13062–13067.
- 68. Lupien S, Karp F, Wildung M, Croteau R (1999) Regiospecific cytochrome P450 limonene hydroxylases from mint (Mentha) species: cDNA isolation, characterization, and functional expression of (−)-4S-limonene-3-hydroxylase and (−)-4S-limonene-6-hydroxylase. Arch Biochem Biophys 368: 181–192.
- 69. Ringer KL, Davis EM, Croteau R (2005) Monoterpene metabolism. Cloning, expression, and characterization of (−)-isopiperitenol/(−)-carveol dehydrogenase of peppermint and spearmint. Plant Physiol 137: 863–872.
- 70. Ringer KL, McConkey ME, Davis EM, Rushing GW, Croteau R (2003) Monoterpene double-bond reductases of the (−)-menthol biosynthetic pathway: isolation and characterization of cDNAs encoding (−)-isopiperitenone reductase and (+)-pulegone reductase of peppermint. Arch Biochem Biophys 418: 80–92.
- 71. Bertea CM, Schalk M, Karp F, Maffei M, Croteau R (2001) Demonstration that menthofuran synthase of mint (Mentha) is a cytochrome P450 monooxygenase: Cloning, functional expression, and characterization of the responsible gene. Arch Biochem Biophys 390: 279–286.