The Scientific World Journal

Volume 2013 (2013), Article ID 313482, 6 pages

http://dx.doi.org/10.1155/2013/313482

Research Article

Effects of Chloroform Extract of Dryopteris crassirhizoma on the Ultramicroscopic Structures of Meloidogyne incognita

Ji-quan Liu,1,2 Shu-lian Xie,¹ Jia Feng,¹ and Jin Cai¹

¹School of Life Science, Shanxi University, Taiyuan 030006, China

²Department of Traditional Chinese Medicine, Shanxi College of Traditional Chinese Medicine, Taiyuan 030024, China

Received 28 August 2013; Accepted 23 September 2013

Academic Editors: Y. Moriyasu, N. Suganuma, and S. D. Yeh

Copyright © 2013 Ji-quan Liu et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Abstract.

In our early experiments, the chloroform extract of D. crassirhizoma was demonstrated to contain the highest concentrations of total phloroglucinols among several extract fractions and possessed the most effective nematicidal activity. This study aimed to ascertain the ultrastructural changes in M. incognita after treatment with a D. crassirhizoma chloroform extract at 1 mg·mL⁻¹ for 24 h. It was found that the extract exhibited significant destructive effects on the worm’s ultrastructure and caused distinctive damage to body surfaces and internal structures. These results will contribute to a deeper understanding of the nematicidal mechanism of D. crassirhizoma, as well as in the design of efficient bionematicides.

1. Introduction

Root-knot nematodes (Meloidogyne spp.) constitute a major group of plant-parasitic nematodes affecting crop production and substantially reducing food quality [1]. Meloidogyne incognita (Kofoid and White) Chitwood is one of the most common and important plant-parasitic nematodes in tropical and subtropical regions worldwide [2]. It has been estimated that global losses from this root-knot nematode amount to $78 billion [3]. The management of nematodes is more difficult than that of other pests because nematodes mostly inhabit the soil and usually attack underground parts of plants [4]. Although chemical nematicides are effective, easy to apply, and show rapid effects, they have begun to be withdrawn from the market in some developed countries owing to concerns about public health and environmental safety [5].

Therefore, there is a strong demand to develop more sustainable and environmentally friendly methods for nematode control. One such alternative is seen in the use of plants containing useful secondary plant metabolites. Nematicidal activity has been reported in several hundred plants, including members of the families Asteraceae, Brassicaceae, Leguminosae, Meliaceae, and Liliaceae [6]. Rhizomes from the ferns of Dryopteris spp. have been used as antibacterial, vermifuges, and anthelmintics in tapeworm infections [7, 8]. The vermifuge activity of Dryopteris spp. has been related to the presence of phloroglucinol derivatives in their extracts [9]. Characteristic phloroglucinol derivatives, such as aspidin and flavaspidic acid, have been reported as major constituents of the genus Dryopteris, and they have been found to possess antioxidant, antibacterial, and antitumor promoting activities [7, 8, 10].

In our previous studies, the nematicidal potential of Dryopteris crassirhizoma against root-knot nematode Meloidogyne incognita was demonstrated in in vitro and pot experiments. This nematicidal activity has been related to the presence of phloroglucinol derivatives in petroleum ether, chloroform, ethyl acetate, n-butyl alcohol, and water extract fractions from D. crassirhizoma on the basis of phloroglucinol analyses and LC₅₀ determinations [11]. Compared with other extracts, the chloroform extract from D. crassirhizoma contains the highest concentration of total phloroglucinols and displayed the most effective nematicidal activity.

The aim of this present work was to evaluate the nematicidal mechanisms of the chloroform extract of D. crassirhizoma against the root-knot nematode M. incognita through ultrastructural observations by scanning and transmission electron microscopies.

2. Materials and Methods

2.1. Plant Material

Rhizomes of Dryopteris crassirhizoma were collected from Jiayin County, Yichun City, Heilongjiang Province, China, dried at 50°C, and mechanically pulverized to a particle size of 1 mm. Then, about 10 g of plant material was extracted in 100 mL of 70% aqueous ethanol at 25°C for 3 d and the extracts stirred once every 8 h. After extraction, the solvent was evaporated in a rotary vacuum evaporator, and the residue then dissolved with water (50°C) and sequentially extracted with petroleum ether and chloroform to yield three fractions. The chloroform fraction was evaporated as above, weighed, dissolved in aqueous acetone (5% by vol), and kept as a 2 mg·mL⁻¹ stock chloroform extract solution.

2.2. Nematode Collection

Meloidogyne incognita specimens were collected from naturally infested tomato fields in Qinxu County, Taiyuan City, Shanxi Province, China, and cultured on tomato plants (Solanum lycopersicum “Hengli”) grown under greenhouse conditions. Egg masses were collected from heavily galled tomato roots and placed in sterile distilled water at 25°C to stimulate juvenile hatching, and the hatched second-stage juveniles were collected. Adult nematodes were collected from the plants by the Baermann method [12].

2.3. Nematode Treatment

Collected second-stage juveniles and adult nematodes were incubated at 25°C in chloroform extract solution at 1 mg·mL⁻¹ or 5% aqueous acetone as a control [13]. After 24 h, the nematodes were washed four times in fresh distilled water and used for ultrastructural observation by scanning and transmission electron microscopies.

2.4. Scanning Electron Microscopy Observation

Nematodes were fixed in 2% glutaraldehyde buffered with 0.1 M sodium cacodylate (pH 7.2) at 4°C for 4 h. Samples were postfixed for 2 h in 1% OsO₄ in the same buffer and then dehydrated through a graded ethanol series (10%, 20%, 30%, 40%, 50%, 60%, 70%, 80%, 90%, and 100%) at 15 min per step. For scanning electron microscopy, samples were critical point dried with CO₂, coated with gold-palladium, and observed in a JSM-35 scanning electron microscope at an electron accelerating voltage of 25 kV (JEOL, Ltd., Tokyo, Japan).

2.5. Transmission Electron Microscopy Observation

The fixing and postfixing of nematodes were the same as for scanning electron microscopy. Samples for transmission electron microscopy were agar-embedded before dehydration and finally embedded in Araldite 618 resin (Huntsman International, LLC, Salt Lake City, UT, USA). Nematodes were cut with PowerTome XL ultrathin slicing machine (RMC, Boeckeler Instruments, Inc., Tucson, AZ, USA). Thin sections were stained with uranyl acetate, followed by lead citrate, and observed in a JEM-1011 transmission electron microscope at an electron accelerating voltage of 80 kV (JEOL, Ltd.).

3. Results

3.1. Effects of Chloroform Extract of Dryopteris crassirhizoma on Body Surfaces of an Adult Nematode

On a normal or control nematode, the entire body was covered with cuticular tissue and many annuli visible in regular transverse rows (Figure 1(a)). Section enlargements of body surfaces showed the presence of a deeper ring groove occurring every three to five shallow ring grooves (Figure 1(c)) and further enlargement revealed the body surface natural texture to be similar to human skin (Figure 1(e)). In contrast, the body surfaces of a nematode exhibited distinctive and significant damage after treatment with a 24 h in vitro exposure to chloroform extract of D. crassirhizoma at 1 mg·mL⁻¹. After treatment, the typical annuli disappeared, yielding a velvety appearance (Figures 1(b) and 1(d)), and further section enlargement showed that the body surface was composed of many small particles (Figure 1(f)).

(a) Whole body of a control nematode, showing normal body surface and annuli

(b) Whole body of a nematode after 24 h incubation in chloroform extract, showing annuli disappearance

(c) Section enlargement of a control nematode. Ring groove is evident

(d) Section enlargement of a nematode treated with chloroform extract. Body surface is smooth

(e) Further section enlargement of a control nematode, showing natural body surface texture

(f) Further section enlargement of a nematode treated with chloroform extract, showing the granular body surface

Figure 1: Scanning electron micrographs of Meloidogyne incognita (adult).

3.2. Effects of Chloroform Extract of Dryopteris crassirhizoma on Body Surfaces of a Second-Stage Juvenile

Figure 2(a) illustrates the observation that the body surfaces of a control juvenile was in good condition and undamaged. In contrast, the appearance of a juvenile treated as described above showed distorted damage, such that the body surface was sloughed off as a flocculent and internal tissue exposed (Figure 2(b)).

(a) Section of a control nematode, showing normal body surface structure

(b) Section of a nematode treated with chloroform extract, showing body surface disruption

Figure 2: Scanning electron micrographs of M. incognita (juvenile).

3.3. Effects of Chloroform Extract of Dryopteris crassirhizoma on Cuticle and Hypoderm of an Adult Nematode

The cuticular architecture comprised two main layers, the external cortical cuticle and basal cuticle layers. The cortical cuticle layer appeared similar to a compact fence structure, which was tightly bounded by the basal cuticle layer (Figure 3(a)). After treatment with chloroform extract, as described above, the normally compact cortical cuticle layer was separated from the basal cuticle layer, broken into flakes, and sloughed off, exposing the basal cuticle layer (Figure 3(b)).

(a) Transverse section of a control nematode, showing the organization of the cortical and basal cuticle layers

(b) The sloughing of the external cortical layer treated with chloroform extract

(c) Section magnification of a control nematode, showing the tightly organized structure of the hypoderm

(d) A change of the hypoderm treated extract treatment in comparison with control

Figure 3: Transmission electron micrographs of cuticle and hypoderm of adult M. incognita.

Underlying the basal cuticle was the hypodermal tissue, which, for the most part in a healthy worm, consisted of a single large syncytium, in which the internal architectures were clear, compact, and well organized (Figure 3(c)). After treatment with chloroform extract, as described above, this layer's clear and organized architecture was severely disrupted and appeared blurred, with many gaps formed between the internal tissues (Figure 3(d)).

3.4. Effects of Chloroform Extract of Dryopteris crassirhizoma on the Muscle Layer and Nerve Fibers of an Adult Nematode

Internal to the hypodermis was the muscular layer, consisting of many large muscular cells, which under healthy conditions showed clear and integrated external contours and clearly visible internal ultrastructures (Figure 4(a)). After treatment with the chloroform extract, as described above, the integrity of muscular cells was compromised, and the structure of the protoplasts severely damaged (Figure 4(b)).

(a) Section magnification of a control nematode, showing the detailed fine structure of a muscle cell (m)

(b) Changes in the muscle cell (m) with extract treatment, compared with control

(c) Section magnification of a control nematode, showing tightly organized fibers (f)

(d) Section magnification showing broken fibers (f) treated with chloroform extract

Figure 4: Transmission electron micrographs of muscle and fibers of adult M. incognita.

The nerve fibers of a control nematode were not only arranged in an orderly and compact fashion but also appeared very elastic (Figure 4(c)). When treated by chloroform extract, as described above, the nerve fibers were fragmented into many pieces and lacked integrity (Figure 4(d)).

4. Discussion

Phloroglucinol derivatives have been reported to have a wide range of biological activities, including antioxidant, antibacterial, and antitumor activities [10]. In addition, it has been reported that phloroglucinol compounds from Dryopteris species are used as vermifuges in tapeworm infections [7, 8]. Some phloroglucinol derivatives show schistosomicidal effects in vitro against Schistosoma mansoni adult worms, producing integumental alterations [14], as well as inhibiting oxidative phosphorylation in rat heart mitochondria and inhibiting the native Mg²⁺-dependent ATPase and ATP–Pi exchange in mitochondria [15, 16]. Phloroglucinol derivatives are typical secondary metabolites widely present in ferns like Dryopteris, and those from D. crassirhizoma show strong toxicity against Ascaris lumbricoides, Leishmania donovani, Taenia solium, and T. saginata, mainly negatively affecting the digestive system and causing central nervous system disorders with tremors and convulsions that can lead to death [17, 18]. In addition, D. crassirhizoma is a traditional Chinese medicine commonly used in China and is safe for human and environment when it was applied as a nematicide in nature [17].

The body wall of the nematode M. incognita consists of cuticle, hypoderm, and muscle layers. The cuticle lies outermost in the nematode, as a multilayered extracellular structure that completely surrounds the animal, except for small openings into the pharynx, anus, excretory pore, and vulva [12]. The cuticle forms the barrier between the animal and its environment and, in addition to being a protective layer, constitutes an exoskeleton that is important in maintaining and defining the animal's normal shape [19]. For nematodes, the normal cuticle contributes in preventing most harmful chemicals from permeating to internal tissues and producing toxic effects.

In the present study, the chemical component in this solution of D. crassirhizoma chloroform extract was found to cause structural alterations of M. incognita’s cuticle, separating the cortical cuticle layer from the organism's body surface, which finally gives rise to integumental permeability changes. Harmful chemicals could thus easily permeate into the internal tissues and damage the normal structure and function of hypodermic and muscular tissues.

Nematode movement relies on the somatic musculature that runs longitudinally along the body wall. Neuromuscular synapses occur in the ventral and dorsal cords and employ an excitatory neurotransmitter, acetylcholine, to modulate muscle activity [20]. Acetylcholine is an impulse transmitting substance that bridges the gap of cholinergic synapses. The biological role of acetylcholinesterase in regulating nerve impulse transmissions across cholinergic synapses is by rapid acetylcholine hydrolysis [21, 22]. When this enzyme is inhibited, acetylcholine accumulates at the postsynaptic membrane, leading to continuous stimulation and paralysis of the organism [23]. Myrtus communis also contains phloroglucinol-type compounds [24–26] and its chloroform fraction exhibits high inhibition of acetylcholinesterase activity [27].

Here, treatment of a nematode with the chloroform extract resulted in nerve fiber breakage, but it remains unclear that this was caused by extract inhibition of acetylcholinesterase activity, resulting in acetylcholine accumulation and ultimately to continuous stimulation and fiber breakage. More research is required to elucidate the nematicidal mechanisms of this chloroform extract of D. crassirhizoma on the root-knot nematode M. incognita.

5. Conclusions

The ultrastructural observations of M. incognita by scanning and transmission electron microscopies suggested that the chloroform extract of D. crassirhizoma had significant destructive effects on the worm’s ultrastructure. It indicated that D. crassirhizoma might be an efficient bionematicide.

Acknowledgment

The authors thank Dr. Sabin Colton (University of Iowa) for his critical reviews of the paper and editorial assistance with the English.

References

Z. Khan, S. D. Park, S. Y. Shin, S. G. Bae, I. K. Yeon, and Y. J. Seo, “Management of Meloidogyne incognita on tomato by root-dip treatment in culture filtrate of the blue-green alga, Microcoleus vaginatus,” Bioresource Technology, vol. 96, no. 12, pp. 1338–1341, 2005.

J. N. Sasser, J. D. Eisenback, C. C. Carter, and A. C. Triantaphyllou, “The international Meloidogyne project, its goals and accomplishments,” Annual Review of Phytopathology, vol. 21, pp. 279–288, 1983.

Z. X. Chen, S. Y. Chen, and D. W. Dickson, Nematology Advance and Perspectives, vol. 2, CAB International Press, Wallingford, UK, 2004.

G. R. Stirling, Biological Control of Plant Parasitic Nematode: Progress, Problems and Prospects, pp. 76–80, CAB International Press, Wallington, UK, 1991.

S. M. Schneider, E. N. Rosskopf, J. G. Leesch, D. O. Chellemi, C. T. Bull, and M. Mazzola, “Research on alternatives to methyl bromide: pre-plant and post-harvest,” Pest Management Science, vol. 59, no. 6-7, pp. 814–826, 2003.

D. J. Chitwood, “Phytochemical based strategies for nematode control,” Annual Review of Phytopathology, vol. 40, pp. 221–249, 2002.

S. M. Lee, M. K. Na, R. B. An, B. S. Min, and H. K. Lee, “Antioxidant activity of two phloroglucinol derivatives from Dryopteris crassirhizoma,” Biological and Pharmaceutical Bulletin, vol. 26, no. 9, pp. 1354–1356, 2003.

M. Na, J. Jang, B. S. Min et al., “Fatty acid synthase inhibitory activity of acylphloroglucinols isolated from Dryopteris crassirhizoma,” Bioorganic and Medicinal Chemistry Letters, vol. 16, no. 18, pp. 4738–4742, 2006.

C. Socolsky, S. A. Borkosky, Y. Asakawa, and A. Bardo, “Molluscicidal phloroglucinols from the fern Elaphoglossum piloselloides,” Journal of Natural Products, vol. 72, no. 4, pp. 787–790, 2009.

G. J. Kapadia, H. Tokuda, T. Konoshima, M. Takasaki, J. Takayasu, and H. Nishino, “Anti-tumor promoting activity of Dryopteris phlorophenone derivatives,” Cancer Letters, vol. 105, no. 2, pp. 161–165, 1996.

J. Q. Liu, S. L. Xie, J. Feng, and J. Cai, “Protective effect of Dryopteris crassirhizoma extracts in the control of the root-knot nematode Meloidogyne incognita,” Journal of Plant Disease and Protection, vol. 120, no. 1, pp. 34–40, 2013.

Z. X. Feng, Plant Nematology, pp. 51–75, Agriculture Press, Beijing, China, 2000.

Q. F. Weng, G. H. Zhong, W. X. Wang, J. J. Luo, and M. Y. Hu, “Effectiveness of plant extracts for the control of Meloidogyne incognita,” Journal of South China Agricultural University, vol. 27, no. 6, pp. 55–60, 2006.

L. G. Magalhães, G. J. Kapadia, L. R. da Silva Tonuci et al., “In vitro schistosomicidal effects of some phloroglucinol derivatives from Dryopteris species against Schistosoma mansoni adult worms,” Parasitology Research, vol. 106, no. 2, pp. 395–401, 2010.

A. Pakarinen and L. Runeberg, “Comparison of the effects of phlorobutyrophenone derivatives on heart and liver mitochondria,” Biochemical Pharmacology, vol. 16, no. 8, pp. 1547–1553, 1967.

H. Y. Tsujimoto, B. D. McSwain, and D. I. Arnon, “Differential effects of desaspidin on photosynthetic phosphorylation,” Plant Physiology, vol. 41, no. 8, pp. 1376–1380, 1966.

X. M. Gao, Chinese Materia Medica, pp. 62–68, Medicine Science Press, Beijing, China, 2nd edition, 2009.

The Committee of National Pharmacopoeia, The Pharmacopoeia of the People’s Republic of China, pp. 310–312, Medicine Science Press, Beijing, China, 1st edition, 2010.

I. L. Johnstone, “The cuticle of the nematode Caenorhabditis elegans: a complex collagen structure,” BioEssays, vol. 16, no. 3, pp. 171–178, 1994.

C. H. Opperman and S. Chang, “Nematode acetylcholinesterases: molecular forms and their potential role in nematode behavior,” Parasitology Today, vol. 8, no. 12, pp. 406–411, 1992.

M. Schumacher, S. Camp, Y. Maulet, et al., “Primary structure of Torpedo californica acetylcholinesterase deduced from its cDNA sequence,” Nature, vol. 319, no. 6052, pp. 407–409, 1986.

B. D. Siegfried and J. G. Scott, “Properties and inhibition of acetylcholinesterase in resistant and susceptible German cockroaches (Blattella germanica L.),” Pesticide Biochemistry and Physiology, vol. 38, no. 2, pp. 122–129, 1990.

D. Nordmeyer and D. W. Dickson, “Biological activity and acetylcholinesterase inhibition by nonfumigant nematicides and their degradation products on Meloidogyne incognita,” Revue de Nématologie, vol. 13, pp. 229–232, 1990.

G. Appendino, F. Bianchi, A. Minassi, O. Sterner, M. Ballero, and S. Gibbons, “Oligomeric acylphloroglucinols from myrtle (Myrtus communis),” Journal of Natural Products, vol. 65, no. 3, pp. 334–338, 2002.

Y. Kashman, A. Rotstein, and A. Liftshitz, “The structure determination of two new acylphloroglucinols from Myrtus communis L.,” Tetrahedron, vol. 30, no. 8, pp. 991–997, 1974.

A. Rotstein, A. Lifshitz, and Y. Kashman, “Isolation and antibacterial activity of acylphloroglucinols from Myrtus communis,” Antimicrobial agents and chemotherapy, vol. 6, no. 5, pp. 539–542, 1974.

S. Begum, M. Ali, H. Gul et al., “In vitro enzyme inhibition activities of Myrtus communis L.,” African Journal of Pharmacy and Pharmacology, vol. 6, no. 14, pp. 1083–1087, 2012.