The glassy cutworm has occasionally caused serious damage to grass seed fields in the U.S. Pacific Northwest and the Canadian prairie provinces. Previous outbreaks of this species in grass occurred in the mid-1960s and 1970s in the Peace River Region.

The glossy, semi-translucent greenish-white or grey larva lacks body markings, but has a prominent reddish brown head and neck shield (Figure 1). Mature larvae are 35 to 40 mm (about 1.5 inches) in length and pupate in the soil near the host plant.

Pupae: the spindle-shaped pupae, within which the transformation to the adult moth occurs, is reddish-brown in colour and about 20 mm in length.

Adult: the adult cutworm is a nondescript, medium sized (35-40 mm wing span) greyish miller moth with a scattering of dark markings on the forewings (Figure 2).

Eggs: cutworm eggs, which are 0.55 mm in diameter, are usually laid on the upper surface of a grass leaf, near the base (Figure 3). Newly laid eggs are glistening white, but progressively darken until they hatch after about one week.

Photo of Glassy cutworm larvae

Figure 1. Glassy cutworm larvae

Photo of an adult glassy cutworm (pinned specimen)

Figure 2. Adult glassy cutworm (pinned specimen)

Photo of a glassy cutworm eggs on leaf blades

Figure 3. Glassy cutworm eggs on leaf blades

Life cycle

There is one generation per year.

Glassy cutworm moths are in flight from July to early September, although most eggs are laid during August (Figure 4).

After hatching, the larvae immediately begin to feed on the host plant and will usually be about half grown by freeze-up. The cutworm overwinters as a partly grown larva and resumes feeding again early the next spring as soon as new green growth appears. The larvae feed underground, or in the case of bunch grasses, within the crown and rarely come to the surface. They pupate in the soil by the end of June.

If the soil temperature is warm enough for grass to grow, the larvae will be active and feeding. Larvae start off very small and will not cause much damage until late in the fall. The extent of fall damage probably varies considerably between years, depending on the weather.

Photo of the glassy cutworm lifecycle

Figure 4. Glassy cutworm lifecycle

Hosts and damage

The glassy cutworm is most commonly associated with grasses and turf but may attack cereals, corn and vegetables, particularly if these crops are planted on newly broken sod or in crops infested with grassy weeds the previous fall. Larvae damage grass stands in the fall and following spring by feeding on stems and crown at or below the soil surface. Apparently, larvae sometimes pull severed leaf below the soil surface until it is entirely consumed. Commonly infested grasses are tall and creeping red fescues, timothy, bluegrass and brome. Low, and even moderate, infestations may not cause noticeable damage if growing conditions are favourable.

Drought appears to be an important factor favouring population increases of glassy cutworm. The severe outbreak in the Peace River Region in 2000 was followed 2 years of drought.

Photo of damaged creeping red fescue seed stand (left) and pasture stand (right) in June 2000

Figure 5. Damaged creeping red fescue seed stand (left) and pasture stand (right) in June 2000

Any fresh grass or cereal growth present between July until early September may be attractive to the female moths for egg laying. Newly hatched larvae will feed on whatever green plant material is present until freeze-up. They will then resume feeding the following spring. Crops affected in the Peace in 2000 were creeping red fescue, tall fescue, timothy, and meadow brome. In one case, seedling meadow brome was attractive for egg laying and the subsequent larval population destroyed a promising stand. Foxtail barley was frequently infested as was quackgrass in some pastures.

Damage will vary according to plant vigour, moisture levels and larval abundance. Healthy, vigorous stands can tolerate more cutworms than stands that are under environmental stress.

The larval stage feeds on the plant. Although they are referred to as cutworms, the pest is not a worm but a juvenile moth also referred to as a larva or caterpillar.


  • Pheromone trap monitoring is not possible at present because no glassy cutworm pheromone is commercially available. Furthermore, no baseline data is available that would enable interpretation of trap catches.
  • Monitoring for larvae in the fall and early spring can provide information on the pest potential. However, larvae will be extremely small and difficult to detect in the fall. Fall monitoring should not be attempted until the larvae have reached at least 10 mm in length.
Photo of Timothy stand near Debolt in June 2000

Figure 6. Timothy stand near Debolt in June 2000

Glassy cutworm females lay eggs on green leaves of host plants. In 1999, one portion of a field (left) was cut for hay, but plant material in the remainder of the field (right) was left standing so plants could set seed. Glassy cutworm damage occurred only where plant material was left standing.


There is no established economic threshold for glassy cutworms in crops or pastures.

Cultural practices

Newly broken land and summer fallow with grassy weeds should be well cultivated during August to prevent new growth suitable for egg laying. Fields at risk should be monitored for evidence of browning-off or unusually poor growth during both the fall and early the next spring. Damaged or sickly plants should be dug up and the roots and surrounding soil searched for the presence of cutworms.

Biological control

Numerous beneficial insects, including both predatory ground beetles and parasitic wasps and flies, were observed in the outbreak populations of glassy cutworm in the Peace River Region in 2000. In some fields, 50% of cutworms were parasitized. These natural enemies are often effective in suppressing cutworm populations below damaging levels. Therefore, unnecessary use of insecticides should be avoided.

Chemical control

  • Glassy cutworm larvae rarely come above the soil surface. This makes them very difficult to control with contact insecticide applications.
  • Late-instar stages exhibit a degree of resistance to insecticide applications whereas younger larvae are relatively more susceptible.
  • High water volume (³ 200 L/ha) is recommended when applying an insecticide. This should provide better penetration of spray droplets into the grass crowns where the larvae are feeding. Light to moderate rain within a week after application will enhance efficacy.

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