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Datasheet

Sitophilus zeamais (greater grain weevil)

Summary

  • Last modified
  • 11 October 2017
  • Datasheet Type(s)
  • Invasive Species
  • Pest
  • Preferred Scientific Name
  • Sitophilus zeamais
  • Preferred Common Name
  • greater grain weevil
  • Taxonomic Tree
  • Domain: Eukaryota
  •   Kingdom: Metazoa
  •     Phylum: Arthropoda
  •       Subphylum: Uniramia
  •         Class: Insecta

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Pictures

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PictureTitleCaptionCopyright
S. zeamais adult is usually blacker than S. oryzae, with fine microsculpture and is more shiny. Scutellum with lateral elevations further apart than their longitudinal length which is about half as long as the scutellum.
TitleAdult
CaptionS. zeamais adult is usually blacker than S. oryzae, with fine microsculpture and is more shiny. Scutellum with lateral elevations further apart than their longitudinal length which is about half as long as the scutellum.
Copyright©Georg Goergen/IITA Insect Museum, Cotonou, Benin
S. zeamais adult is usually blacker than S. oryzae, with fine microsculpture and is more shiny. Scutellum with lateral elevations further apart than their longitudinal length which is about half as long as the scutellum.
AdultS. zeamais adult is usually blacker than S. oryzae, with fine microsculpture and is more shiny. Scutellum with lateral elevations further apart than their longitudinal length which is about half as long as the scutellum. ©Georg Goergen/IITA Insect Museum, Cotonou, Benin
Adult beetle of S. zeamais.
TitleAdult
CaptionAdult beetle of S. zeamais.
CopyrightUSDA-ARS
Adult beetle of S. zeamais.
AdultAdult beetle of S. zeamais.USDA-ARS

Identity

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Preferred Scientific Name

  • Sitophilus zeamais Motschulsky

Preferred Common Name

  • greater grain weevil

Other Scientific Names

  • Calandra chilensis (Philippi & Philippi)
  • Calandra oryzae
  • Calandra oryzae platensis
  • Calandra platensis (Zacher)
  • Calandra quadrimacula (Walker)
  • Calandra zeamais Motschulsky
  • Calandra zemais (Motschulsky)
  • Calendra zeamais Motschulsky
  • Sitophilus oryzae platensis
  • Sitophilus oryzae zeamaiz Motschulsky

International Common Names

  • English: billbug, northern corn; maize weevil; weevil, greater rice; weevil, maize
  • Spanish: gorgojo del grano; gorgojo del maiz; gorgojo del maíz almacenado; picudo del maíz
  • French: calandre du mais
  • Portuguese: gorgulho do milho

Local Common Names

  • Germany: Kaefer, La-Plata-Mais-; Kaefer, Mais-
  • Iran: susske sorrat
  • Japan: kokuzo
  • Norway: maissnutebille
  • Turkey: misir biti

EPPO code

  • CALAZM (Sitophilus zeamais)

Taxonomic Tree

Top of page
  • Domain: Eukaryota
  •     Kingdom: Metazoa
  •         Phylum: Arthropoda
  •             Subphylum: Uniramia
  •                 Class: Insecta
  •                     Order: Coleoptera
  •                         Family: Dryophthoridae
  •                             Genus: Sitophilus
  •                                 Species: Sitophilus zeamais

Notes on Taxonomy and Nomenclature

Top of page The taxonomy of the Sitophilus group has been confused until recently, so that the value of much of the earlier literature on these insects has been reduced, because of the difficulty of knowing the species to which it refers.

First described by Linnaeus in 1798 as Curculio oryza, the first named species of the group was later revised by De Clairville and Scheltenburg in 1798 as Calandra oryzae, which uses the commonest generic synonym for Sitophilus. Many workers subsequently recognized that two distinct forms of the species existed, which were described as the 'large' and 'small' forms. In 1855, Motschulsky recognized the large form as a distinct species, which he named Sitophilus zeamais. Unfortunately, few workers recognized this revision and the name Calandra oryzae continued to be applied to all insects in this complex. Takahashi in 1928 and 1931 complicated matters by raising the small form to specific status as Calandra sasakii. This confused situation continued until 1959, when Floyd and Newsom (1959) revised the complex; this was followed by a further revision by Kuschel (1961). In these revisions it was shown that Linnaeus originally described the smaller species and that Motschulsky's description of the larger species was valid. Both species were therefore placed in the genus Sitophilus with the specific names proposed by Linnaeus and Motschulsky.

Unfortunately, the size difference between S. oryzae and S. zeamais is not consistent, so it is not possible to be sure that references to the large and small forms of Calandra oryzae refer to S. zeamais and S. oryzae, respectively. Therefore the only true and unconfused synonym of S. oryzae is Calandra sasakii; in pre-1960s literature, Calandra oryzae 'small' and 'large' forms could refer to either S. zeamais or S. oryzae, and it is also possible that some references to 'S. oryzae' in the 1960s and early 1970s literature actually relate to S. zeamais misidentified by use of old keys. The genus Sitophilus and its species may be identified using the keys of Gorham (1987) or Haines (1991).

Description

Top of page Eggs, Larvae and Pupae

These developmental stages are all found within tunnels and chambers bored in the grain and are thus not normally seen. The larvae are apodous.

Adults

Usually blacker than S. oryzae, with fine microsculpture and is more shiny. Scutellum with lateral elevations further apart than their longitudinal length which is about half as long as the scutellum.

Males with median lobe of aedeagus with two longitudinal grooves dorsally, except in the apical quarter, and is thus sinuous in cross section.

Females with lateral lobes of the Y-shaped sclerite pointed and their separation is greater than for S. oryzae.

S. oryzae and S. zeamais are almost indistinguishable from each other externally; identification is by examination of the genitalia. Both have the characteristic rostrum and elbowed antennae of the family Curculionidae. The antennae have eight segments and are often carried in an extended position when the insect is walking. Both species usually have four pale reddish-brown or orange-brown oval markings on the elytra, but these are often indistinct. (See also S. oryzae.)

Both species can be separated from S. granarius by the presence of wings beneath the elytra (absent in S. granarius) and by having circular, rather than oval, punctures on the prothorax. Molecular characters also separate S. oryzae and S. zeamais and confirm reproductive isolation (Hidayat et al., 1996).

Distribution

Top of page S. zeamais and S. oryzae are found in all warm and tropical parts of the world, but S. oryzae may also be found in temperate climates.

The detailed map plotted on the basis of actual country records gives a falsely restricted distribution. These pests are carried all over the world in grain shipments and can establish themselves wherever there is food and where grain moisture and temperature are favourable. In various locations, one species may be more common than the other. A global survey of resistance to pesticides (Champ and Dyte, 1976) contains detailed location lists for both species.

Distribution Table

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The distribution in this summary table is based on all the information available. When several references are cited, they may give conflicting information on the status. Further details may be available for individual references in the Distribution Table Details section which can be selected by going to Generate Report.

Continent/Country/RegionDistributionLast ReportedOriginFirst ReportedInvasiveReferenceNotes

Asia

AfghanistanPresentChamp and Dyte, 1976
BahrainPresentChamp and Dyte, 1976
BangladeshPresentTyler et al., 1983: Bhuiyah et al.; Tyler et al., 1988
ChinaPresentChamp and Dyte, 1976
IndiaPresentChamp and Dyte, 1976
-MaharashtraPresentChamp and Dyte, 1976
-SikkimPresentNatural History Museum London UK
-Uttar PradeshPresentChamp and Dyte, 1976
IndonesiaPresentChamp and Dyte, 1976
IranPresentChamp and Dyte, 1976
IraqPresentChamp and Dyte, 1976
IsraelPresentChamp and Dyte, 1976
JapanPresentChamp and Dyte, 1976
Korea, Republic ofPresentChamp and Dyte, 1976
KuwaitPresentChamp and Dyte, 1976
LaosPresentAPPPC, 1987
MalaysiaPresentChamp and Dyte, 1976
-SabahPresentNatural History Museum London UK
MyanmarPresentChamp and Dyte, 1976
NepalPresentChamp and Dyte, 1976
PakistanPresentChamp and Dyte, 1976
PhilippinesPresentChamp and Dyte, 1976
Saudi ArabiaPresentChamp and Dyte, 1976
SingaporeWidespreadChamp and Dyte, 1976; AVA, 2001
Sri LankaPresentGanesalingam, 1977
SyriaPresentChamp and Dyte, 1976
TaiwanPresentChamp and Dyte, 1976
ThailandPresentChamp and Dyte, 1976
TurkeyPresentChamp and Dyte, 1976
UzbekistanPresentAsanov, 1970
VietnamPresentStusak et al., 1986
YemenPresentChamp and Dyte, 1976

Africa

AlgeriaPresentChamp and Dyte, 1976
AngolaPresentPacavira et al., 2006
BeninPresentChamp and Dyte, 1976
BotswanaPresentMpuchane et al., 2000
CameroonPresentAyuk-Takem et al., 1982
Cape VerdePresentNatural History Museum London UK
Central African RepublicPresentChamp and Dyte, 1976
CongoPresentDelobel, 1992
Côte d'IvoirePresentClement et al., 1988
EgyptPresentChamp and Dyte, 1976
EthiopiaPresentChamp and Dyte, 1976
GambiaPresentChamp and Dyte, 1976
GhanaPresentMould, 1973
KenyaPresentChamp and Dyte, 1976
LesothoPresentThind and Muggleton, 1981
LiberiaPresentVirmani, 1980
LibyaPresentChamp and Dyte, 1976
MalawiPresentChamp and Dyte, 1976
MoroccoPresentChamp and Dyte, 1976
MozambiquePresentChamp and Dyte, 1976
NigeriaPresentChamp and Dyte, 1976
RwandaPresentWeaver et al., 1991
SenegalPresentChamp and Dyte, 1976
SomaliaPresentChamp and Dyte, 1976
South AfricaPresentChamp and Dyte, 1976
Spain
-Canary IslandsPresentNatural History Museum London UK
SudanPresentSeifelnasr, 1991
SwazilandPresentChamp and Dyte, 1976
TanzaniaPresentChamp and Dyte, 1976
TogoPresentDeuse and Pointel, 1975; Pantenius, 1988
TunisiaPresentYana, 1969
UgandaPresentEvans, 1985
ZambiaPresentChamp and Dyte, 1976
ZimbabwePresentChamp and Dyte, 1976

North America

MexicoPresentChamp and Dyte, 1976
USA
-ArkansasPresentChamp and Dyte, 1976
-CaliforniaPresentChamp and Dyte, 1976
-GeorgiaPresentBrown and Lee, 2002
-KansasPresentChamp and Dyte, 1976
-LouisianaPresentChamp and Dyte, 1976
-TexasPresentChamp and Dyte, 1976
-VirginiaPresentChamp and Dyte, 1976
-WisconsinPresentNansen et al., 2004

Central America and Caribbean

Antigua and BarbudaPresentChamp and Dyte, 1976
BelizePresentFortier et al., 1982
CubaPresentAviles and Guibert, 1986
El SalvadorPresentChamp and Dyte, 1976
GuatemalaPresentChamp and Dyte, 1976
HondurasPresentHoppe, 1986
JamaicaPresentChamp and Dyte, 1976
NicaraguaPresentChamp and Dyte, 1976
Trinidad and TobagoPresentChamp and Dyte, 1976

South America

ArgentinaPresentChamp and Dyte, 1976
BoliviaPresentSquire, 1972
Brazil
-AmazonasPresentChamp and Dyte, 1976
-GoiasPresentChamp and Dyte, 1976
-Minas GeraisPresentOliveira et al., 2007
-PiauiPresentFontes et al., 2003
-Rio de JaneiroPresentChamp and Dyte, 1976
-Rio Grande do SulPresentChamp and Dyte, 1976
-RoraimaPresentMarsaro et al., 2007
-Santa CatarinaPresentSantos and Wamser, 2006
-Sao PauloPresentChamp and Dyte, 1976
ChilePresentTrivelli et al., 1975
-Easter IslandPresentOlalquiaga, 1980
ColombiaPresentChamp and Dyte, 1976
French GuianaPresentChamp and Dyte, 1976
GuyanaPresentChamp and Dyte, 1976
ParaguayPresentNatural History Museum London UK
PeruPresentChamp and Dyte, 1976
UruguayPresentChamp and Dyte, 1976
VenezuelaPresentRevetti, 1972

Europe

AustriaPresentBerger and Hetfleis, 1985
BelgiumPresentLetellier et al., 1994
BulgariaPresentChamp and Dyte, 1976
CroatiaPresentHamel, 2007
CyprusPresentChamp and Dyte, 1976
GermanyPresentBahr and Prinz, 1977
GreecePresentChamp and Dyte, 1976
HungaryPresentSzeoke, 1989
ItalyPresentGelosi and Arcozzi, 1983
MacedoniaPresentPurrini, 1976
PolandPresentChamp and Dyte, 1976
PortugalPresentChamp and Dyte, 1976
RomaniaPresentChamp and Dyte, 1976
Russian FederationPresentChamp and Dyte, 1976
SpainPresentChamp and Dyte, 1976
SwitzerlandPresentBuchi, 1993
UKPresentChamp and Dyte, 1976
Yugoslavia (former)PresentChamp and Dyte, 1976

Oceania

Australia
-New South WalesPresentChamp and Dyte, 1976
-QueenslandPresentChamp and Dyte, 1976
-South AustraliaPresentChamp and Dyte, 1976
-TasmaniaPresentChamp and Dyte, 1976
-VictoriaPresentChamp and Dyte, 1976
-Western AustraliaPresentChamp and Dyte, 1976
FijiPresentPartridge, 1973
New CaledoniaPresentBrun and Attia, 1983
Papua New GuineaPresentChamp and Dyte, 1976
Solomon IslandsPresentNatural History Museum London UK
TongaPresentAPPPC, 1987

Hosts/Species Affected

Top of page Both S. oryzae and S. zeamais are able to develop on a wide range of cereals and also on processed cereal products such as pasta. However, food preferences of the two species are variable; it is clear that S. zeamais is predominantly found associated with maize grain, whereas S. oryzae is associated with wheat.

In the case of rice, detailed surveys in Indonesia have shown that S. zeamais is dominant on milled rice, whereas S. oryzae is more common on paddy (rough rice). Laboratory studies have shown that this is a result of their different rates of increase on these two forms of rice (Hussain et al., 1985). It is not yet known whether these relationships with the form of rice hold true throughout the tropics, but imports of milled rice into the UK from many countries are much more frequently infested by S. zeamais than by S. oryzae.

Both species are able to breed on dried cassava and have been reported as frequent pests of this commodity. A few strains of S. oryzae have been found which can develop on grain legumes (Coombs et al., 1977): peas, lentils and green or black gram are the pulses most often attacked by these strains.

Host Plants and Other Plants Affected

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Plant nameFamilyContext
Colocasia esculenta (taro)AraceaeUnknown
Glycine max (soyabean)FabaceaeUnknown
Manihot esculenta (cassava)EuphorbiaceaeMain
Oryza sativa (rice)PoaceaeMain
Phaseolus vulgaris (common bean)FabaceaeUnknown
Sorghum bicolor (sorghum)PoaceaeMain
stored products (dried stored products)Main
Triticum (wheat)PoaceaeMain
Triticum aestivum (wheat)PoaceaeUnknown
Vigna angularis (adzuki bean)FabaceaeUnknown
Vigna unguiculata (cowpea)FabaceaeUnknown
Zea mays (maize)PoaceaeMain

Growth Stages

Top of page Post-harvest

Symptoms

Top of page The eggs, larvae and pupae are not normally seen because they develop inside intact grains. Adult emergence holes with irregular edges are apparent some weeks after the initial attack. Adults can be found wandering over the surface of grain.

List of Symptoms/Signs

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Seeds

  • internal feeding

Biology and Ecology

Top of page The earlier confusion over the identity of S. zeamais and S. oryzae, and the fact that most of the major basic studies were made before the confusion was resolved, means we cannot be sure to which of the species many of the observations refer. The development of the two species is clearly very similar, but there are probably a number of differences in the effects of environmental factors. Thus, the information given below may be taken as generally applicable to both species, but it should be remembered that there may be specific differences in details.

The biology of S. zeamais and S. oryzae has been reviewed in detail by Longstaff (1981). The adults are long-lived (several months to one year). Eggs are laid throughout most of the adult life, although 50% may be laid in the first 4-5 weeks; each female may lay up to 150 eggs. The eggs are laid individually in small cavities chewed into cereal grains by the female; each cavity is sealed, thus protecting the egg, by a waxy secretion (usually referred to as an 'egg-plug') produced by the female. The incubation period of the egg is about 6 days at 25°C (Howe, 1952). Eggs are laid at temperatures between 15 and 35°C (with an optimum around 25°C) and at grain moisture contents over 10%; however, rates of oviposition are very low below 20°C or above 32°C, and below about 12% moisture content (Birch, 1944).

Upon hatching, the larva begins to feed inside the grain, excavating a tunnel as it develops. There are four larval instars: in English wheat at 25°C and 70% RH, pupation occurs after about 25 days, although development periods are extremely protracted at low temperatures (e.g. 98 days at 18°C and 70% RH). Pupation takes place within the grain; the newly developed adult chews its way out, leaving a large, characteristic emergence hole. Total development periods range from about 35 days under optimal conditions to over 110 days in unfavourable conditions (Birch, 1944; Howe, 1952). The actual length of the life cycle also depends upon the type and quality of grain being infested: for example, in different varieties of maize, mean development periods of S. zeamais at 27°C and 70% RH have been shown to vary from 31 to 37 days. The development of S. zeamais on different wheats (Triticum spelta, T. dicoccum and T. monococcum spikelets and kernels) has also been studied (Suss et al., 1999). A demographic population simulation model of S. zeamais in grain stores in West Africa has been devised (Meikle et al., 1999).

Although both species are capable of flight, S. zeamais has a greater ability and tendency to fly (Giles, 1969). Where grain is stored on small farms, S. zeamais is thus more likely than S. oryzae to fly to the ripening crop in the field and establish an infestation in the grain before harvest.

Natural enemies

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Natural enemyTypeLife stagesSpecificityReferencesBiological control inBiological control on
Acaropsellina docta Predator Larvae/Pupae
Anisopteromalus calandrae Parasite Larvae/Pupae
Beauveria bassiana Pathogen
Cerocephala dinoderi Parasite Larvae
Cerocephala oryzae Parasite Larvae/Pupae
Cerocephala spp. Parasite Larvae
Lariophagus distinguendus Parasite Larvae/Pupae
Mus musculus Predator
Pteromalus cerealellae Parasite
Theocolax elegans Parasite Larvae/Pupae
Tillus notatus Predator

Notes on Natural Enemies

Top of page Both S. zeamais and S. oryzae are commonly parasitized by pteromalids (and occasionally other Hymenoptera). Common pteromalid parasites found in the Tropics include Anisopteromalus calandrae, Lariophagus distinguendus and Theocolax elegans.

Impact

Top of page S. oryzae and S. zeamais are very important pests of cereals. In maize or sorghum, attack may start in the mature crop when the moisture content of the grain has fallen to 18-20%. Subsequent infestations in store result from the transfer of infested grain into store or from the pest flying into storage facilities, probably attracted by the odour of the stored grain.

In stored maize, heavy infestations of these pests may cause weight losses of as much as 30-40%, although losses are commonly 4-5%. S. zeamais has been found to be amongst the most important pests of maize in a number of studies; in South Carolina, USA, (Arbogast and Throne, 1997), in Kentucky (Sedlacek et al., 1998) and in steel silos in Taiwan (Peng, 1998), and in central Italy (Trematerra et al., 1999). Insect pests infesting stored pearl millet and their damage potential, were assessed in northeastern Nigeria by Lale and Yusuf (2000). S. zeamais caused ca. 0.6% damage. Damage was greater in grains stored in the underground pit storage system than in grains stored in a rumbu, clay pot or polypropylene sack.

S. zeamais has been detected in seeds during quarantine processing of germplasm imported into India (Babu, 1997), in pigeonpeas imported from Indonesia and sorghum from the USA.

Infestations in rice are damaging, but loss estimates from real, as opposed to laboratory situations, are lacking.

Detection and Inspection

Top of page Flight traps will collect S. zeamais, but seldom S. oryzae (which rarely flies). In milled rice stores, bag traps baited with brown rice have captured both species (Hodges et al., 1986). Disturbance of the grain causes adult Sitophilus spp. to migrate upwards and become visible on the surface.

A male-produced aggregation pheromone which attracts both sexes occurs in Sitophilus spp. Sitophilure, 5-hydroxy-4-methyl-3-heptanone, was reported to be the aggregation pheromone common for S. oryzae and S. zeamais, and Levinson et al. (1990) confirmed the activity of 4S,5R sitophinone and 2S,3R-sitophilate for Sitophilus spp. Some interspecific cross attraction between three Sitophilus species has been demonstrated to occur; more so between S. oryzae and S. zeamais than between S. granarius and either of the other species.

The responses of S. zeamais to pheromone and synthetic maize volatiles as lures in crevice or flight traps have been studied in Kenya (Hodges et al., 1998). Three trap types (probe, cone and sticky) were used to monitor S. zeamais populations infesting shelled maize housed in galvanized steel storage bins. The results of this study were similar to those reported by Weston and Barney (1998); a combination of sticky traps in the grain bin headspace and probe traps positioned just below the grain surface was most efficient for monitoring the presence of pest and beneficial insect species in grain storage. Likhayo and Hodges (2000) reported the field monitoring of S. zeamais and S. oryzae using refuge and flight traps baited with synthetic pheromone and cracked wheat. The combination of pheromone and cracked wheat had an additive effect on trap catch.

Similarities to Other Species/Conditions

Top of page S. oryzae and S. zeamais can be separated from S. granarius by the presence of wings beneath the elytra (absent in S. granarius) and by having circular, rather than oval, punctures on the prothorax.

Prevention and Control

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Cultural Control and Sanitary Methods

Good store hygiene plays an important role in limiting infestation by S. oryzae and S. zeamais. The removal of infested residues from last season's harvest is essential. The use of resistant maize varieties has also shown some potential in slowing the build-up of insect densities in stores. Phenolic compounds have been associated with grain resistance to S. zeamais.

A combination of controlled ambient aeration in the autumn and chilled aeration during summer storage has significant potential as a non-chemical preventative pest management technique (Maier et al., 1996). Aeration dramatically reduces the numbers of weevils compared with population levels in non-aerated maize (Arthur, 1998). Thorpe (1997) modelled ecosystems in ventilated conical-bottomed farm grain silos.

Host-Plant Resistance

Zea mays genotypes resistant to S. zeamais have been evaluated by Boica et al. (1997) and in the field in Benin (Meikle et al., 1998). Genetic variability for resistance to S. zeamais in domestic US maize germplasm has been identified by Li et al. (1998). In Brazil, tests were carried out with maize cultivars to evaluate the attractiveness and oviposition preference of S. zeamais (Toscano et al., 1999).

The mechanism of resistance in maize to S. zeamais was investigated in relation to secondary chemistry and other biochemical and physical characteristics of maize genotypes. Phenolic acid content was correlated strongly with hardness of the grain (Arnason et al., 1997). Huang et al. (1998) assessed alpha-Pinene for antifeedant and growth inhibitory effects against S. zeamais adults.

Chemical Control

Grain may be protected by the admixture of insecticide. Sitophilus spp. have a low susceptibility to synthetic pyrethroids but are readily killed by organophosphorous compounds such as fenitrothion and pirimiphos-methyl. Grain stocks may be fumigated with phosphine to eliminate existing infestation, but these treatments provide no protection against re-infestation. Sitophilus spp., particularly in the pupal stage, have a lower natural susceptibility to the fumigant phosphine and to carbon dioxide used in controlled-atmosphere storage than do other species tested and thus inadequate treatments are particularly likely to result in some survival.

Guedes and Heyde (1996) estimated the toxicity of deltamethrin to a number of resistant and susceptible populations of S. zeamais in traditional maize stores in Togo. In another study, a treatment with pirimiphos-methyl and deltamethrin was most effective in traditional granaries after pirimiphos-methyl, deltamethrin and permethrin were applied in various combinations (Richter et al., 1997, 1998). Srinivasacharayulu and Yadav (1997) evaluated the toxicity of deltamethrin, fluvalinate, chlorpyrifos-methyl, etrimfos and malathion against S. zeamais, and topical application bioassays of malathion, pirimiphos-methyl, deltamethrin and permethrin were undertaken with 11 field strains of S. zeamais, collected from nine states in Mexico (Perez-Mendoza, 1999).

A number of studies have investigated the efficacy of phosphine fumigation: Goto et al. (1996) reported its effects at concentrations of 0.5, 1 or 2 g/m³ on pupae at 15°C. The effects of phosphine on the development of S. zeamais was investigated by Zhang (1997). Field strains of S. zeamais from the Philippines were evaluated for resistance to phosphine by Gibe et al. (1997). Peng et al. (1999) and Peng (2000) studied vertical penetration and distribution of phosphine in corn and sorghum stored in steel silos and compared the distribution of phosphine in bins when aluminium phosphide was placed on the stack surface and on the floor.

Controlled Atmospheres

Guedes et al. (1996) reported that 20% carbon dioxide controlled S. zeamais in 5 days. Treatment with 15% carbon dioxide and 5% oxygen controlled the insects in 10 days. Santos et al. (1997) describes use of carbon dioxide-controlled atmosphere in Brazil for the control of S. zeamais on maize and wheat. Carbon dioxide at concentrations of 50% and 60% killed all life stages of the weevil after 10 days of exposure. In another study with fumigation periods of 15 and 20 days, the concentrations of 40%, 50% and 60% eliminated all stages of the insects (Santos et al., 1998). According to Casella et al. (1998), effective control of Sitophilus was achieved with a synthetic atmosphere and 0.5 or 0.75 g/m³ of phosphine, for an exposure period of 120 hours.

Natural carbon dioxide production in stored maize is affected by moisture content, the amount of broken corn and foreign materials and infestation by S. zeamais (Sone, 1999). Respiration by fungi including Aspergillus spp. appears to have a greater influence on carbon dioxide production in stores than the presence of insects. Under sealed storage conditions in maize, insects and fungi both deplete the oxygen supply, creating an unfavourable atmosphere for their own survival (Damcevski et al., 1998; Moreno-Martinez et al., 2000).

Contessi (1999) assessed the effectiveness of controlled atmospheres using generators of inert gases, such as carbonic anhydride and nitrogen, for the disinfestation of wheat stored in vertical silos and horizontal stores.

Irradiation

Irradiation of S. zeamais by microwave and gamma radiation has been studied. Insect mortality studies were carried out with a high-power microwave source operating at a frequency of 10.6 GHz at power levels of 9-20 kW to irradiate samples of Triticum aestivum infested with S. zeamais (Halverson et al., 1996). Applying high-power microwaves demonstrated that selective heating of insects and their resulting mortality is a non-linear function of frequency and increases at frequencies above 2.45 GHz in the vicinity of increasing relaxation processes associated with free water (Plarre et al., 1997). Tests were conducted at 12, 15, 17.9 and 55 GHz. The results indicated that 15 GHz produced greater mortality among adults than 12 and 17.9 GHz. However, 55 GHz produced the greatest mortality for the three developmental stages studied.

A sterilizing dose of gamma radiation from Cobalt-60 was determined for adults of S. zeamais on rice, maize and wheat grains (Franco et al., 1997) at 24-26°C and 65-75% RH with a dose rate of 3.00 kGy/h. The dose was found to be 60 Gy for S. zeamais.

Temperature Control

Low-temperature storage of rice is extensively practised to control insect pests in Japan. Nakakita et al. (1997) reported that both hatching and metamorphosis of S. zeamais were completely inhibited at 10°C; a small number of adult S. zeamais emerged at 15°C.

Dry heat treatment has been found to be an effective control against all developmental stages of S. zeamais (Mohammed-Dawd and Morallo-Rejesus, 2000). All eggs and adult weevils were killed following exposure to 60°C for 2 hours, or 70-80°C for 1 hour. All larvae were killed when seeds were exposed to 70-80°C for 1 hour.

Biological Control

The bionomics of the pteromalid parasitoid Lariophagus distinguendus and its controlling effect on S. zeamais were studied by Li et al. (1998). L. distinguendus was found to have five generations each year in the laboratory, with final-instar larvae of the parasitoid over-wintering in larvae of S. zeamais. The parasitoid Theocolax elegans has also been recorded to attack S. zeamais (Helbig, 1998).

The effect of different isolates and formulations of Beauveria bassiana on S. zeamais in stored maize are reported by Adane et al. (1996); Moino and Alves (1997); Hidalgo et al. (1998); and Junior and Alves (1998). B. bassiana can be an effective microbial control agent if used as a preventative treatment (Moino et al., 1998).

The fungal pathogens of maize storage pests in Kenya were surveyed by Oduor et al. (2000). Between 0.08 and 0.94% of the insects collected (mostly S. zeamais) were found to be infected.

Botanical Insecticides

The toxicity of a large number of essential oils and plant parts of various spices and herbs have been assessed against S. zeamais.

A number of citrus oils have vapour toxicity to adults of S. zeamais; lime, mandarin and grapefruit peel oils reduce oviposition and larval emergence (Don-Pedro, 1996). Garlic oil is toxic to adults (Ho et al., 1997), and oils of coconut, sunflower, sesame and mustard, alone and in combination with eucalyptol, eugenol or camphor have been found to be toxic to S. zeamais in wheat and maize-treated grains (Obeng-Ofori and Reichmuth, 1999).

Plants or extacts from a considerable number of other plants have exhibited toxicity to S. zeamais. These include: Ocimum suave (Bekele et al., 1996); Ocimum kenyense (Bekele et al., 1997); Ocimum kilimandscharicum (Obeng-Ofori et al., 1998); Dennettia tripetala, Piper guineense, Monodora myristica and Xylopia aethiopica (Okonkwo and Okoye, 1996); Ricinus communis, Gaura coccinea, Larrea tridentata, Ribes ciliatum, Castilleja tenuiflora, Alchemilla procumbens and Guazuma tomentosa (Araya-Gonzalez et al., 1996); Juniperus sabina (Gao and Zhang, 1997); Chrysanthemum cinerariaefolium (Saggar et al., 1997); Tagetes minuta (Weaver et al., 1997); cinnamon, garlic, coriander, Capsicum annuum and Murraya paniculata (Ho et al., 1997); Eucalyptus (Obeng-Ofori et al., 1997); Cinnamomum aromaticum (Huang and Ho, 1998); Pachyrhizus erosus (Alavez-Solano et al., 1998); Allium sativum (Chiam et al., 1999); Evodia rutaecarpa (Liu and Ho, 1999); Canaga odorata (Huang et al., 1999); Baccharis genistelloides (Prates, 1999); Aloe marlothii (Achiano et al., 1999); Securidaca longipedunculata (Belmain et al., 1999); Cleome hirta; cardamom (Huang et al., 2000); Basella alba, Operculina turpethum and Calotropis gigantea (Haque et al., 2000).

References

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