USDA-APHIS-PPQ

Asian Gypsy Moth Survey and 

Response Guidelines

Photo Credit: John H. Ghent, USDA Forest Service, Bugwood.org

January 2014
USDA APHIS PPQ Asian Gypsy Moth Survey and Response Guidelines

January 2014

Dedicated to Roeland Elliston, PPQ Western Region Gypsy Moth Program Manager

Acknowledgements: 

PPQ Developers: Vic Mastro, Dave Lance, Clinton Campbell, Roeland Elliston, Mitchell Nelson, John 

Molongoski, Gary Brown, Joseph Beckwith, Patrick McPherren, Julie Spaulding, and Paul Chaloux

Reviewers: PPQ: David Kaplan and Scott Pfister, Bob Rabaglia (US Forest Service), Helmuth Rogg

(OR), Robert Leavitt (CA), Dan Kenny (OH), Jim Marra (WA)

Purpose 

The information contained in these response guidelines is intended for use when surveying and 

controlling introductions of Asian gypsy moth (AGM, L. dispar japonica, L. dispar asiatica, L. umbrosa, 

L. albescens and L. postalba). These guidelines provide technical and general guidelines for detection, 

delimiting, eradication treatment, and follow-up delimiting survey activities for occurrences of AGM 

beyond Department of Homeland Security Customs and Border Protection finds during port of entry 

inspections. 

To avoid the establishment of AGM, the nationwide PPQ response policy for any AGM detection is 

eradication as outlined in the 1995 USDA Asian Gypsy Moth Policy (Appendix A). These guidelines 

support this policy with the addition of a decision table to determine the appropriate response method. 

Authority and Statutes

The Plant Protection Act, Public Law 106-224, June 2000, provides authority to the United States 

Department of Agriculture to order treatment or quarantine of an area when the Secretary considers such 

action necessary to prevent the dissemination of a plant pest. 

The choice of treatment material for the Asian Gypsy Moth is governed by the Supplemental 

Environmental Impact Statement (SEIS) that was filed with the United States Environmental Protection 

Agency on October 12, 2012.

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Contents

I. Pest Information ........................................................................................................................................3

A. Description and classification..............................................................................................................3

B. History and risk of AGM in North America ........................................................................................4

C. Life cycle .............................................................................................................................................5

D. Biology ................................................................................................................................................6

E. Host range ............................................................................................................................................6

F. Spread of infestation.............................................................................................................................7

II. Identification ............................................................................................................................................7

A. Handling and submission of suspect AGM specimens for identification............................................7

B. Morphological description of AGM ....................................................................................................9

C. Molecular methods and DNA markers ..............................................................................................11

D. Rearing...............................................................................................................................................13

III. Survey ...................................................................................................................................................13

A. Traps and lures...................................................................................................................................13

B. AGM detection survey.......................................................................................................................14

C. Egg masses.........................................................................................................................................16

D. Trap deployment................................................................................................................................17

IV. Eradication Actions ..............................................................................................................................19

A. Determining response ........................................................................................................................19

B. Size of area to be treated....................................................................................................................22

C. Proven eradication treatment options.................................................................................................22

D. Precision delimiting...........................................................................................................................23

E. Treatment considerations...................................................................................................................23

F. Degree-day modeling .........................................................................................................................24

V. Post Treatment Delimiting Surveying to Verify Treatment Effectiveness............................................26

A. Area and density to be surveyed........................................................................................................26

B. Duration of surveying necessary to declare successful eradication ...................................................26

VI. Environmental Assessment...................................................................................................................26

VII. Collaboration with State Government Entities....................................................................................26

VIII. Glossary .............................................................................................................................................27

IX. References.............................................................................................................................................29

Appendix A - USDA ASIAN GYPSY MOTH POLICY ...........................................................................33

Appendix B – AGM Trapping Submission Guidelines..............................................................................34

Appendix C – PPQ Form 305 .....................................................................................................................35

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I. Pest Information

A. Description and classification

Adult Asian gypsy moth (AGM) males have grayish-brown wings with black markings and a 11⁄2 to 2 

inch (3.8-5 cm) wingspan. Adult female AGM are heavy-bodied and can have a wingspan of 31⁄2 inches

(8.9 cm) or more. Female wings are white with black markings (Figure 1); however, they rarely exhibit 

color morphs and appear almost black (PPQ, 2003). Early-instar AGM larvae appear black and have long 

hair-like setae. Older instars (IV through VI) have distinctive markings on the head capsule and are gray 

with five pairs of raised blue to blackish spots and six pairs of raised red to brownish-red spots along their 

back (CAPS, 2008). Occasionally, the instars express color morphs. There are several different types, 

with the most common being a black or nearly black stripe along the dorsal surface (Figure 2) (Mastro, 

2009).

Figure 1. Male (left) and female (right) adult Asian gypsy moths (PPQ).

Figure 2. Late instar Asian gypsy moth larvae exhibiting typical coloration (top) and color morphs (bottom)

(PPQ).

Lymantria dispar is a moth in the family Lymantriidae (some recent classifications consider Lymantriinae 

to be a subfamily of Noctuiidae; see Pogue and Schaefer, 2007). In a recent review of the genus 

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Lymantria, Pogue and Schaefer (2007) recognized three subspecies of Lymantria dispar: L. d. dispar (L.) 

(European gypsy moth), L. d. asiatica Vnukovskij, and L. d. japonica (Motschulsky). For regulatory 

purposes, the latter two subspecies are both considered Asian gypsy moths (AGM). L. d. asiatica occurs 

in temperate Asia from the Ural Mountains east to China, Korea and the Russian Far East (north of the 

Himalayans). L. d. japonica is found on several major Japanese islands including Honshu, Shikoku, 

Kyushu, and parts of Hokkaido. 

Pogue and Schaefer (2007) also described three new or revised/re-described species that had previously 

been considered subspecies of L. dispar. These are L. umbrosa (Lymantria dispar 

hokkaidoensis/umbrosa/nesiobia), L. albescens (L. dispar albescens), and L. postalba (L. d. 

postalba/tsushimensis, L. albescens tsushimensis). All three are native to Japan (though their 

distributions are generally more limited than that of L. d. japonica). All three species, like L. dispar, use

disparlure as the major, if not sole, component of their sex-attractant pheromone and thus may be caught 

in gypsy moth monitoring traps. 

Pogue and Schaefer indicate that regardless of the changes in nomenclature, “Asian Gypsy Moths” are 

those that have females capable of flight. Therefore, for regulatory purposes, USDA considers all three 

newly classified species to be AGM in addition to L. d. asiatica Vnukovskij, and L. d. japonica 

(Motschulsky) (Table 1). DNA analysis is used to determine what type of moth is trapped; Section XX 

covers the submission process of samples.

Table 1. Asian Gypsy Moth. Winged and flight-capable females.

B. History and risk of AGM in North America

AGM was first discovered in North America in 1991 in British Columbia, having arrived as egg masses 

on cargo ships from Russia (Savotikov, 1995). Immediately after this discovery, traps were set around 

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ports in Washington and Oregon where additional AGM were caught. In 1993, AGM were found on the 

east coast when females started flying off of a military cargo vessel that had arrived from Germany and 

docked in Sunny Point, North Carolina. Eradication protocols were immediately put into effect in these 

areas and the populations were successfully eradicated (PPQ, 2003). Recent studies have revealed that 

AGM as well as European gypsy moth (EGM) are capable of surviving in all temperate regions of the 

world with the exception of sub-alpine and desert regions (Peterson, 2007). As of 2008, AGM has been 

detected and subsequently eradicated in Washington, Oregon, California, Idaho, Texas, and North 

Carolina. AGM is not known to be established in any areas of the United States. 

C. Life cycle

AGM has four life stages: egg, larva (caterpillar), pupa and adult (moth). Females lay one batch of eggs 

in a single mass on a host tree or inanimate object. The size of the egg mass varies depending on what the 

female fed on while in the larval stage (among other factors), but can range up to 1500 eggs. AGM are 

attracted to light; therefore, eggs are frequently laid near light sources (Figure 3) (Savotikov, 1995). Egg 

masses are covered with yellowish to tan hairs (appearing fuzzy) but can bleach out to near white after 

prolonged exposure to direct sunlight. On average they are 11⁄2 inches (3.8 cm) long and 3⁄4 inch (1.9 cm)

wide (Figure 4) (PPQ, 2003). In 4-6 weeks, embryos develop into larvae but remain unhatched, in the 

egg, until spring. Time of hatch in the spring is temperature-dependent, but typically larvae emerge from 

eggs approximately when buds on host trees have just broken. AGM larvae feed on leaves and are the 

only stage that causes damage (Doane et al. 1981, Wallner et al. 1989). After five or six molts as larvae, 

AGM enter the pupal stage which typically lasts 10-14 days (Figure 5). When the moths emerge they do 

not feed. Females release a sex pheromone to attract males and, after mating, search for a place to lay 

their eggs (PPQ, 2003). The moth stage is very short, lasting only 2-3 days (Mastro, 2009).

Figure 3. Asian gypsy moth egg masses laid on a light aboard a shipping vessel (PPQ).

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Figure 4. Asian gypsy moth egg mass (Canadian Food Inspection Agency).

Figure 5. Asian gypsy moth female (left) and male pupae (PPQ).

D. Biology

Female gypsy moths of the European subspecies do not fly; however, the Asian variety can fly distances 

up to 25 miles (40 km) (Savotikov, 1995). AGM also require a shorter number of days of exposure to 

low temperatures to complete diapause (Reineke, 1998). AGM hatch can be induced when ships from 

infested areas with cold climates reach our much warmer southern ports, even during winter months 

(Mastro, 2009).

E. Host range

AGM larvae have been known to feed on more than 600 plant species, covering more than 100 botanical 

families. AGM prefer deciduous trees but can develop on conifers. As a result, they have a broader host 

range than the European subspecies. Large infestations of AGM can completely defoliate trees, which 

weaken the trees and expose them to attack by secondary organisms. If defoliation is repeated for two or 

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more years, it can lead to the death of large sections of forest as well as orchards and plantations

(Savotikov, 1995). 

F. Spread of infestation

Because females have the ability to fly long distances, they spread rapidly into and through uninfested 

areas. In addition, newly hatched AGM larvae disperse by “ballooning,” which consists of climbing a 

tree or other object, dropping on a silken thread, and becoming wind-borne. Humans are also a potential

source of long-range spread. Eggs can be laid on ships, shipping containers, outdoor furniture, firewood, 

timber, rail cars, automobiles and other inanimate objects. While in the egg stage, gypsy moth is in 

diapause and can remain quiescent and viable for long periods of time. This provides a long opportunity 

for these contaminated vehicles and materials to be transported to new areas. Also, AGM egg masses are

extremely hardy and their tolerance of temperature and moisture extremes enhances the risk of spread

(APHIS, 1992). Once hatched in a new location, the broad host range and the ability of the larvae to 

disperse enhances their ability to establish. 

II. Identification

A. Handling and submission of suspect AGM specimens for identification

Specimens that are suspected of being AGM should be submitted to the Center for Plant Health Science 

and Technology (CPHST) Otis Laboratory for testing (see Appendix B). All specimens collected outside 

of the EGM quarantine areas will be analyzed. Specimens collected within generally-infested areas will 

be analyzed based on sub-samples of total catch because of the large number of insects which can be 

caught in some areas. It is critical that samples be collected regularly, stored properly, and 

submitted to the Otis Lab as soon as possible to maintain the integrity of the DNA. If traps cannot be 

checked regularly, it may be considered to trap when flight is expected rather than spreading resources 

out across the whole season. As a general rule, traps should be checked and samples removed every two 

weeks in order to reduce the degradation of the specimen’s DNA. High temperatures and high humidity 

speed degradation of specimens and trapping schedules should be adjusted accordingly. If stored 

unfrozen the specimens should be in containers (paper bags or boxes) which will promote drying. Plastic 

containers retain moisture that favors the growth of bacteria and fungi, which will quickly degrade the 

DNA. Specimens should be stored in a freezer if possible (if not, in a cool dry area) and shipped to Otis 

as soon as practical. Specimens should not be stored unfrozen for extended periods. A PPQ Form 305

(Appendix C) should be sent with each trap, stating the trap number, collection site, number of specimens 

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(estimates okay), life stage, collection date, and date of last (previous) trap check (to determine maximum 

time that the moth may have been in the trap prior to the check). Specimens should be shipped via next 

day delivery for Tuesday through Friday arrival (PPQ, 2008) to: 

Molecular Diagnostics Unit-Otis Laboratory

USDA, APHIS, PPQ

1398 West Truck Road

Buzzards Bay, MA 02542-1329

Questions can be directed to John Molongoski (phone: 508-563-0929; email: 

john.j.molongoski@aphis.usda.gov; or fax: 508-563-0903).

The CPHST Otis Laboratory will communicate negative results directly back to the submitter. For any 

positive AGM confirmations, they will complete a PPQ form 391 and send an e-mail narrative about the 

detection and PDF of the completed PPQ form 391 to ppq.nis.urgents@aphis.usda.gov. The data will be 

entered into the Pest ID system and confirmation communicated by the National Identification Service’s

Domestic Diagnostics Coordinator to the National Survey Coordinator with Emergency and Domestic 

Programs staff at APHIS headquarters. According to the agreed upon communication protocol, the 

National Survey Coordinator will forward the confirmation to the list of contacts including the State Plant 

Health Director and State Plant Regulatory Officer of the state of origin, and the AGM national and 

regional program managers.

Milk Carton Trap

• Layer moths loosely between wadded paper towels or tissue paper in a paper bag (brown lunch 

bag size) to prevent motion and specimen damage during shipment (one bag per trap; if more than 

one bag is required per trap, label appropriately). Label paper bag clearly with trap numbers 

matching paperwork. 

• Staple or tape paper bag closed. 

• Do not attach paperwork to individual bags. 

• Do not use plastic bags or paper envelopes as these do not allow moisture release and thus 

promote fungal growth and decomposition of the moths. 

• Do not send traps or paperwork for traps which contain no specimens.

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Delta Traps

• Label each trap clearly with trap numbers matching paperwork.

• Package traps to avoid crushing during shipment.

• Do not attach paperwork to individual traps.

• Do not use Styrofoam peanuts or other small packaging materials that could potentially enter the 

traps.

• Do not disassemble the traps or remove moths from the trap.

• Do not ship traps with sharp staples exposed.

Egg Masses

To ensure that useful molecular information can be extracted, DNA must be able to be recovered. In 

order to achieve this, please adhere to the following protocols.

• Egg masses that are being shipped to Otis should not be treated with oil.

• If egg masses are wet, air dry before shipping.

• Ship individual egg masses in separate Ziploc bags; do NOT mix egg masses. 

• Include a shipping permit with any shipment of viable eggs (permit obtained from Otis). 

• If practical, notify Otis Lab via email or phone (508-563-9303) that egg masses are being 

shipped.

B. Morphological description of AGM

1. Distinguish from non-Lymantriids

L. dispar can be most easily distinguished from other non-Lymantriids by their medium sized, nontranslucent, intricately patterned, wings (USDA, 1981). Their eggs are large (>1 mm diameter), covered 

in buff-colored hair, and laid in masses that may contain as many as 1500 eggs. Masses are laid on 

surfaces such as tree trunks, rocks, cars, and shipping containers (Mastro, 2009).

2. Distinguish from other Lymantriids

L. dispar can be easily confused with L. monacha, the nun moth, as well as other Lymantriids. The nun 

moth is also a defoliator and native to Eurasia. It can be distinguished from L. dispar by its wide range in 

color variation, from chalk white to dark brown, covered with intricate patterns. The exception is the dark 

phase males which are especially difficult to separate. Also, the female nun moths have a narrower 

abdomen and long ovipositor which L. dispar lacks. Nun moth eggs are deposited in clusters, not in a 

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single mass and without a covering of hair (USDA, 1981). Because of the similarities between AGM and 

other Lymantriids, it is best to send all suspect samples to an identifier.

Figure 6. L. dispar asiatica (AGM) male Figure 7. L. monacha (Nun moth) male

(John H. Ghent, USDA Forest Service, (Peter Lillywhite).

Bugwood.org)

Figure 8. L. monacha (Nun moth) female Figure 9. L. mathura (Rosy moth

and male. (Melody Keena, USDA Forest female) (PPQ)

Service, Bugwood.org)

3. Distinguish AGM from European gypsy moth

AGM adults are similar enough to EGM that the two cannot be reliably distinguished by visual 

examination alone. AGM tend to be larger than EGM, and AGM females, unlike female EGM, usually 

have wings that are large enough to completely cover the abdomen when closed, but these differences do 

not provide definitive identification. In addition, the subspecies can hybridize to produce moths that 

intermediate in a number of traits including flight (Keena et al., 2001). As a result, DNA analysis is 

routinely used to distinguish between the subspecies.

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Figure 10. European gypsy moth (L. dispar dispar) Figure 11. Asian gypsy moth (L. dispar japonica) 

(CAPS). (CAPS).

C. Molecular methods and DNA markers

Two genetic markers are routinely used to assess the genotype of submitted gypsy moth specimens: the 

nuclear marker FS1 (Garner and Slavicek, 1996) and a mitochondrial marker (Bogdanowicz et al., 1993). 

Two alleles or variations occur at the FS1 loci, designated as North American (NA) or Asian (A) 

respectively. As gypsy moths are diploid organisms, each moth contains two non-identical copies of each 

autosomal (non-sex) chromosome. The two copies or alleles of FS1 can be identical (homozygous) or 

different (heterozygous) in a given specimen. Thus, three combinations are possible: a moth can be 

homozygous North American (possessing two copies of the North American allele), homozygous Asian, 

or heterozygous (containing one copy each of the North American and Asian allele). As the designation 

implies, the North American FS1 allele is the allele most frequently found in gypsy moths from North 

America while the Asian allele is the only FS1 allele present in moths from eastern Asia. The Asian 

allele is, however, also detected in the US population at a low percentage (approximately 3 to 6% 

depending upon geographic location in the continental US). Both of the FS1 alleles, on the other hand, 

are present in high abundance in gypsy moths from Europe and Western Russia.

Unlike nuclear DNA, mitochondrial DNA is always maternally inherited. Thus, the mitochondrial DNA 

analysis of any given gypsy moth reflects the mitochondrial DNA of its mother. The mitochondrial 

marker is characterized by four possible haplotypes or variations defined by restriction site 

polymorphisms. After completion of PCR (DNA amplification), the amplified DNA fragment is 

incubated in the presence of the restriction enzymes Nla III and Bam H I respectively. For the North 

American haplotype (NA), neither of the enzymes cut nor digest the amplified DNA (Nla and Bam 

negative). For the A1 haplotype (commonly found in moths originating in Europe and Western to Central 

Russia), Nla III cuts the DNA fragment into two pieces (Nla positive), but Bam H I does not cut the DNA 

fragment (Bam negative). For the A2 haplotype (common to Far East Russia and the Orient), both 

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Band Size (bp) 

produced in FS1 PCR

FS1 

Designation

Band Size (bp) 

produced in 

Mitochondrial 

RFLP

Mitochondrial DNA 

RFLP Data

Mitochondrial DNA 

Haplotype Distribution Determination Additional Analysis Advised

207 NA 500 Nla-Bam- NA Prevalent genotype in 

North America North American None 

207 NA 350/150 Nla+Bam- A1

 Europe and North 

America (E>NA); % varies 

with location in North 

America)

Subject to further 

analysis

Microsatellite 

Analysis

207 NA 300/150/50 Nla+Bam+ A2

Rare; 2 in Austria,1 in 

Slovak Republic, 15 in 

Tunisia all from 1990's

Subject to further 

analysis

Microsatellite 

Analysis

207 NA 450/50 Nla-Bam+ A3

Very rare: 1 moth found 

in North America 

(Delaware, 2009)

Subject to further 

analysis

Microsatellite 

Analysis

207/312 H 500 Nla-Bam- NA North America (% varies 

with location)

Subject to further 

analysis

Microsatellite 

Analysis

207/312 H 350/150 Nla+Bam- A1

 Europe and North 

America (E>NA); varies 

with location in North 

America

Subject to further 

analysis

Microsatellite 

Analysis

207/312 H 300/150/50 Nla+Bam+ A2 Rare; 2 in Austria, 1 each 

in China, Korea, & Tunisia 

Subject to further 

analysis

Microsatellite 

Analysis

207/312 H 450/50 Nla-Bam+ A3 Not found to date None None 

312 A 500 Nla-Bam- NA North America (% varies 

with location)

Subject to further 

analysis

Microsatellite 

Analysis

312 A 350/150 Nla+Bam- A1 Europe and Asia (E>A) Asian Microsatellite 

Analysis

312 A 300/150/50 Nla+Bam+ A2 Prevalent genotype in 

Asia Asian Microsatellite Analysis

312 A 450/50 Nla-Bam+ A3 Rare; 8 found in China; 1 

in Japan Asian Microsatellite Analysis

enzymes cut the DNA fragment (Nla and Bam positive). The fourth possible haplotype (Nla negative and 

Bam positive) has only been detected to date in a few moths from China and is rare. This haplotype is 

designated A3. Similar to the FS1 A allele, the A1 mitochondrial haplotype is also found in the US 

population at a low percentage. In both cases, the exact percentage varies depending upon location within 

the United States. It is important to keep in mind that these designations for the nuclear FS1 marker and 

the mitochondrial marker are not meant to indicate the evolutionary origin of the moths tested, but rather 

implies the geographic region where they are found in the highest abundance (Table 2). 

Table 2. Gypsy Moth Genotype Determination

Genetic markers termed “microsatellites” are available to provide more precise information on the

possible origins of captured or intercepted gypsy moths. Microsatellites are repeated sequences of 

typically 2 to 4 base pairs in length (for example, [GTT]n or [AT]n or similar repeats). They are found in 

nuclear DNA but are not in portions of the DNA that actually code for proteins. Consequently, mutations 

in microsatellites are typically not “weeded out” by selection, and thus numerous alleles of a given 

microsatellite can accumulate in a species’ genome. This makes microsatellites potentially useful for 

answering within-species questions relating to such things as geographic or population-level origins of an 

individual. In humans, they are used for determining paternity. Microsatellites are inherited in 

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Mendelian fashion; i.e., an individual has two copies of each microsatellite – one from each parent. For 

analysis, they are amplified (many copies are made) using PCR primers that adhere to the flanking 

regions of each microsatellite. To determine which alleles the individual has, the lengths of the 

microsatellite DNA are then measured, as the various alleles differ only in the number of times the basic 

2- to 4-base sequence is repeated. Data generated using multiple microsatellite markers (6-12 markers 

minimum) are subject to analysis using population assignment software such as STRUCTURE (Pritchard 

et. al., 2000). STRUCTURE is a Bayesian-based clustering method for inferring population structure; the 

program uses allele data from multiple microsatellites to identify distinct genetic populations (termed 

clusters) and assigns individual specimens into those populations. The use of microsatellites may 

potentially provide information relating to the country of origin of AGM intercepts, the possible 

relatedness of multiple AGM interceptions, and the possible infiltration of AGM genes into the 

established North American gypsy moth population. 

D. Rearing

Immature insects can be difficult to identify taxonomically, and for this and other reasons it may 

occasionally be advantageous to rear out suspect AGM that were intercepted as eggs or early-instar 

larvae. EGM have been reared routinely in large numbers for such purposes as virus production and pilot 

sterile insect release programs (Bell et al. 1981), and these methods are applicable to AGM. Within the 

U.S., however, suspect AGM must be reared under permit and within a PPQ-approved quarantine facility. 

Contact the CPHST Otis laboratory for shipping instructions for live egg masses and other viable life 

forms, and to obtain a copy of the permit, which must accompany the shipment.

III. Survey

A. Traps and lures

Pheromone baited traps are used for detecting and delimiting AGM populations in North America. With 

rare exception, these traps capture only males. Black-light traps can capture AGM of both sexes and are

used to monitor AGM in port environs in Asia, but they are not considered sensitive or specific enough 

for detection and delimitation survey purposes.

Gypsy moth pheromone lures contain 0.5 milligrams of disparlure in either a PVC-coated string or

laminated plastic strip. These dispensers provide slow release of the attractant into the air over a period 

of several months. The lures are used in delta or milk-carton traps. Delta traps are used outside of areas 

that are generally infested with gypsy moth, where catch is expected to be less than 10 moths per trap. 

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They are prism-shaped traps made of plastic-coated cardboard; moths enter through openings on the 

triangular ends and are captured in a sticky substance that coats two of the three inner surfaces. Milk 

carton traps resemble basic 0.5 gallon (2 quart) paper milk cartons, but contain small entry ports on each 

side as well as a trap hood around the carton which serves as a behavioral stop for males so they will enter 

the ports. The lure hangs inside the carton at approximately the same height as the entry ports. Moths 

that enter the milk carton trap are killed by an insecticide (DDVP) that is released from a laminated

plastic strip which is also hung inside the carton. Milk carton traps can hold as many as 1000 moths.

B. AGM detection survey 

Detecting insect populations with traps is probabilistic in nature. All other things equal, the closer a moth 

is to a trap, the more likely it is to be captured. Because of that, the sensitivity of a detection trapping 

grid, that is, the probability of detecting a relatively small population, improves with increases in the 

number of traps per unit area (Figure 12). 

Figure 12. Percentages of marked male European gypsy moths captured in grids of disparlure-baited traps 

at various densities in testing conducted from the mid-1970s through 2002 (Lance, et al. 2003). 

Ideally, moths will be detected in the same year they are introduced. Trap density will vary depending on 

the local risk, which is based on pathways of introduction and spread, host availability, and other factors 

as determined by local managers. General guidelines are provided below.

0

4

8

12

16

0 20 40 60 80 100

Traps per square mile

% of male GM captured

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Areas at risk should be surveyed using pheromone traps. Ports and other high risk areas should set up to 

25-36 traps per square mile (2.6 square km) within a two-mile (3.2 km) radius of docking areas and other 

high risk sites. An additional 16 traps per square mile (2.6 square km) should be set out to a distance of 5 

miles (8 km), where there is host vegetation (Figure 13 below). Areas within 1 mile (1.6 km) from the 

banks of high-risk waterways should be set with up to 25-36 traps per square mile (2.6 square km). 

Figure 13. Sample trap density grid for high risk areas

In other risk areas, traps should be set at 9 traps per square mile (2.6 square km) out to a 1 mile (1.6 km)

radius from docking areas and other sites at risk. An additional 4 traps per square mile (2.6 square km) 

should be set out to a distance of 3 miles (4.8 km), where there is host vegetation (Figure 14 below). 

Waterways should be set with 9 traps per square mile (2.6 square km) along the water out to 1 mile (1.6

km) inland on each side of the waterway (APHIS, 1992).

Figure 14. Sample trap density grid for risk areas

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C. Egg masses

1. Egg masses to determine hatch dates

If male gypsy moths are treated with the proper substerilizing dose of radiation and mated to an 

unirradiated female, a portion of the resulting eggs will hatch, but the larvae will develop into fully sterile 

adults. These egg masses can be placed in areas with newly detected gypsy moth populations to help 

estimate timing of hatch without risk of adding to the incipient population. The egg masses are caged as 

an added security measure, to protect the egg mass, and to avoid possible confusion over the origin of any 

males that are subsequently captured. The Otis laboratory provides sterile EGM egg masses and can also 

provide cages or guidance on cage construction.

Egg masses should be placed outdoors in the area where suspect AGM were captured. This should be 

done as early as possible, preferably during the fall following the summer when the AGM were trapped. 

Cages should be placed in a variety of locations near the ground, but in places where they will not be 

disturbed by the public. Masses should be checked for hatch three times weekly starting about 3 weeks 

before phenological models or other indices indicate that hatch is expected. In areas with warm winters 

(e.g., coastal California or the Gulf Coast), masses should also be checked weekly through the winter.

An alternative, if available, is to monitor hatch of wild egg masses that are found in the area. This 

reduces possible environmental differences that could affect timing of hatch and would also eliminate 

possible differences in timing of hatch between the laboratory (EGM) insects and the target (AGM) 

population. However, a high degree of security would be required to ensure that no larvae escape. Eggs 

should be carefully scraped from their substrate, keeping the mass intact as much as possible and placed 

in a cage (as above) in a secure area.

2. Egg mass surveys

Various types of egg mass surveys, all based on visual search, have been designed for, and used in, 

managing gypsy moth, but they are typically used in dealing with outbreak-level populations (KolodnyHirsch 1986, Buss et al. 1999). Female European GM doesn’t fly and typically deposits egg masses near 

their pupation sites, which are often in relatively hidden locations such as under bark flaps, in the interior 

of wood piles, or under decks. AGM females may also do this but instead often fly some distance prior to 

oviposition. Searching for egg masses in indiscriminate and often cryptic locations is much less efficient 

than pheromone trapping for finding and characterizing Asian gypsy moth populations, especially at the 

low population levels typical of incipient populations. As a result, AGM egg mass surveys are not 

16 | Page
recommended for detecting or delimiting a newly introduced population. In addition, eradication 

protocols are based on data from trapping grids.

Egg mass searches, however, may be desirable if resources are available and masses would be considered 

useful for such tasks as confirming the presence of a locally reproducing population, molecular 

characterization of a population, or timing control measures. Tree trunks, as well as the cryptic types of 

locations noted above, should be systematically searched in the vicinity of trap captures. In addition, 

AGM females in many areas tend to fly to lights at night, and searches of well-lit light poles and 

architectural surfaces can prove successful.

D. Trap deployment

1. Timing for start and end in different geographic areas

Traps should be set out before male gypsy moths emerge; however, times conducive to adult flight at 

various U.S. port areas and months when male moths from various sources could potentially be present

vary. The highest risk would come from any moths that had left ships or cargo in previous seasons and 

were reproducing locally. The second highest risk would come from moths that dispersed away from 

ships or containers, either as adults that had pupated prior to transit or, earlier in the season, as newly 

hatch larvae. Note that this risk would also be present throughout the period when flight of local 

populations could be occurring. 

A lesser but non-zero risk is present through other portions of the year when temperatures at a port allow 

for flight. This occurs because ships coming from foreign ports in the northern hemisphere sometimes 

transit southern hemisphere ports before coming to the U.S. In those cases, the reversal of season could 

affect temperature conditioning of egg masses on the ships, causing eggs to hatch at unusual times of 

year. Under this scenario, larvae in sub-tropical ports could potentially disperse from ships, find host 

material, and develop into adults at most any time (an alternative possibility is transport of AGM from 

breeding populations in the southern-hemisphere, though none are known at this time). While the risk of 

such an occurrence is low, managers at southern ports can consider keeping traps in place, if resources are 

available to do so. 

Trap lures can draw in moths for up to one year in the field, so, in general, they will last throughout a 

year’s trapping period, and setting them out early will not decrease their effectiveness (APHIS, 1992). 

17 | Page
However, if trapping is conducted year-around, lures should be changed every six months to ensure 

optimum effectiveness.

2. Trap placement

Trap locations should focus on high risk ports and waterways, first and foremost, as determined by the 

SPHD and SPRO. Determinations should be based on past experience of interceptions, volume of ships 

arriving from Asia, and other factors. Other risk areas should be trapped as resources allow.

Milk carton traps should be hung using a string, tied to a branch of a host tree (Figure 15). Delta traps are 

most effective when attached directly to the bole of a host tree. The most efficient way of doing this is by 

stapling a binder clip to the bole of a host tree then clipping the trap in place. However, if a homeowner 

objects to this method, it can also be hung using a paper clip (Figure 16) or by tying a string around the 

tree and hanging the clip on the string. The traps should be hung at breast height unless vandalism is a 

problem in which case they should be hung higher (Lance, 2009). If a trap cannot be hung on a host tree, 

another vertical surface, such as a telephone pole, can be used to hang the trap, preferably within 100 

meters of a host. Never hang the traps on branch tips.

 

 

 Figure 15. Milk carton trap Figure 16. Delta trap (PPQ).

 (William A. Carothers).

3. Trap monitoring, frequency, and timing

Generally, traps should be monitored as often as possible. Past experience has shown that vandalism 

usually occurs soon after a trap is set; therefore, it is desirable to check traps at least once before male 

moths would be expected to emerge. Pheromone traps should be checked every two weeks if possible. 

Collected specimens should be sent to the Otis Diagnostic Laboratory in Massachusetts (section II.A.). 

18 | Page
4. Detection of suspected AGM in trapping season

If a suspect AGM is identified during the trapping season, it is recommended that the number of traps be 

increased within the detection grid to help delimit the population. In addition, staff can visually survey

light structures in the area around the trap and/or ports for female moths or egg masses.

IV. Eradication Actions

A. Determining response

A Technical Working Group (TWG) will be convened or consulted as soon as a diagnostic test confirms

AGM are trapped. The TWG will consider each situation prior to rendering a response plan. This 

includes reviewing prior trapping densities and grids, vegetation, obvious introduction points, etcetera. 

The TWG will assist in the determination if the population is at a sufficient level to require eradication 

and the scope of such eradication. If eradication is recommended, the TWG will work with the local 

federal regulatory managers to determine the best eradication and trapping methodologies. Local federal 

officials will communicate with their respective state counterparts and other federal and state agencies to 

determine the type of response. 

Consult Tables 4 and 5, which represent an array of time (single season (Table 4), multiple seasons (Table 

5)) and situations (single moth catch in a port grid, multiple moth catch in a port grid, etc.) that shows the 

various levels of response available within an eradication framework. “Level two” listings for land-based 

detections are shown as either proven eradication treatments or “precision delimiting”. Precision 

delimiting (see part D of this section) is not a treatment itself, but, as with any form of delimiting 

trapping, is part of the eradication process. Based on input from the TWG and the possible responses 

outlined in Tables 4 and 5, apply the appropriate levels of response for the situation. In addition, 

quarantines may be considered beyond what is listed below if needed to control the spread of AGM.

19 | Page
Table 4. Single season situations and response steps for AGM detections beyond standard detection surveys

Scale Scenario 

type

Situation Type of 

response

First step of 

response

Second step 

of response

Third step of 

response

Fourth step of 

response

Foreign Single 

season 

scenarios

AGM populations 

high in Asia

Detection Maximum 

inspection 

intensity by 

CBP

Increase 

detection 

trapping 

intensity

Outreach & 

Public 

Information

Domestic 

(national)

AGM shipinterceptions 

“low”

Eradication CBP 

eradicates life 

stages found 

onboard vessel

Maintain 

normal highrisk trapping 

grids

AGM shipinterceptions 

“high”

Eradication or 

Detection

CBP 

eradicates life 

stages found 

onboard vessel

Increase 

detection 

trapping 

intensity

Outreach & 

Public 

Information

Single 

season 

scenarios

One moth in a 

Port/Waterway 

(P&W) trap grid

Eradication or 

Delimiting

Outreach & 

Public 

Information

Eradication 

treatment or

Precision 

Delimiting

Delimiting 

trapping for 3 

years posttreatment

One moth outside 

a Port/Waterway 

trap grid

Eradication or 

Delimiting

Outreach & 

Public 

Information

Eradication 

treatment or

Precision

Delimiting

Delimiting 

trapping for 3-

4 years posttreatment

Multiple moths in 

the same trap grid 

or finite locality

Eradication or 

Delimiting

Outreach & 

Public 

Information

Eradication

treatment or 

Precision

Delimiting

Delimiting 

trapping for 3 

years posttreatment

If/when 

possible, 

determine 

“relatedness”

One moth and 

other life stage(s) 

in the same trap 

grid

Eradication Outreach & 

Public 

Information

Eradication 

treatment

Quarantine Delimiting 

trapping for 3 

years posttreatment

20 | Page
Table 5. Multiple season situations and response steps for AGM detections beyond standard detection surveys

Scale Scenario 

type

Situation Type of 

response

First step of 

response

Second step 

of response

Third step of 

response

Fourth step of 

response

Multiple 

season 

scenarios

One moth in 

season 1 plus one 

moth in season 2 –

in the same

Port/Waterway 

(P&W) trapping 

grid 

Eradication or 

Delimiting 

(continues 

across both 

seasons)

Outreach & 

Public 

Information

(increased)

Season 1 –

Eradication 

treatment or

Precision 

Delimiting

Delimiting 

trapping for 3 

years posttreatment

If/when 

possible, 

determine 

“relatedness” of 

season 1 moth 

and season 2 

moth

Season 2 –

Eradication 

treatment or

Precision 

Delimiting

continues

Delimiting 

trapping for 3 

years posttreatment; 

[the 3-year 

clock resets to 

zero with 

season 2]

One moth in 

season 1 plus one 

moth in season 2 –

outside a P&W 

grid

Eradication or 

Delimiting

(continues 

across both 

seasons)

Outreach & 

Public 

Information 

(increased)

Season 1 –

Eradication 

treatment or

Precision 

Delimiting

Delimiting 

trapping for 3 

years posttreatment

If/when 

possible, 

determine 

“relatedness” of 

season 1 moth 

and season 2 

moth

Season 2 –

Eradication 

treatment or

Precision 

Delimiting

continues

Delimiting 

trapping for 3 

years posttreatment

Multiple moths in 

the trap grid (or 

finite locality) 

Eradication Outreach & 

Public 

Information 

(maximum)

Treatments –

i.e. multiple 

tactics

Quarantine Delimiting 

trapping for 3 

years posttreatment

21 | Page
B. Size of area to be treated

A minimum of a half mile (0.8 km) radius around the capture site should be treated with a proven 

eradication treatment (AGM SAP, 2007). If adjacent traps with positive captures are 1 mile (1.6 km) or 

less apart, the area between the traps should be treated with a proven eradication treatment as well as the 

half mile (0.8 km) radius. If adjacent traps further than 1 mile (1.6 km) apart both have positive captures, 

site parameters such as host type, host density, and trap placement would need to be evaluated by the 

program manager.

C. Proven eradication treatment options

1. Btk

Btk (Bacillus thuringiensis kurstaki) has repeatedly been proven efficacious against gypsy moth. It is 

short-lived in the field, so multiple applications (typically 3) should be made either by air or by ground at 

intervals of 7 to 10 days (AGM SAP, 2007). The spray zone should extend at least a half-mile (0.8 km) 

radius from all capture sites. Btk is effective only against young caterpillars (instars I and II and, to a 

lesser degree, III), so it is critical to apply the material when these stages are present in the field. Btk is 

more specific than other insecticides; it will kill some non-target caterpillars (Lepidoptera) if they ingest 

sufficient materials but has little toxicity on other organisms. The bacteria occur naturally and can be 

found in soil (AGM SAP, 2004). Btk works by disrupting the caterpillar’s digestive system, which leads 

to death in 7-10 days (PPQ, 2003).

2. Diflubenzuron

Diflubenzuron (trade name of Dimilin) is an insect growth regulator that interferes with development by 

inhibiting synthesis of chitin, a major component of the insect exoskeleton. Dimilin is highly effective 

against gypsy moth larvae. In comparison with Btk, it has a longer field life (requires fewer applications) 

and is more effective against older larvae (timing is less critical), but kills a much wider range of insects 

and other arthropods (APHIS, 2006, TX). 

Other eradication treatment options are available in the 2012 Supplemental Final Environmental Impact 

Statement, which is entitled “Gypsy Moth Management in the United States – a cooperative approach.” 

22 | Page
D. Precision delimiting

Delimiting for AGM, when applied post-treatment, normally involves a grid with a 5-mile radius and the 

following trap densities: 25-36 traps per square mile for the first two miles (from center) and 16 traps per 

square mile for the last three miles (Figure 13). However, precision delimiting may be applied in certain 

circumstances, such as in an area with limited host material or low trap catches often involved in a port or 

waterway detection (Tables 4 and 5), to determine the necessity of or prepare for an eradication treatment 

at the recommendation of the Technical Working Group. The trapping grid for precision delimitation

would take on the following enhanced densities—49 traps per square mile for the first two miles (from 

center) and 25 traps per square mile for the last three miles (Figure 17). No post-treatment delimiting 

survey is required since no treatment is being applied.

25 25 25 25 25 25 25 25 25 25

25 25 25 25 25 25 25 25 25 25

25 25 25 25 25 25 25 25 25 25

25 25 25 49 49 49 49 25 25 25

25 25 25 49 49 49 49 25 25 25

25 25 25 49 49 49 49 25 25 25

25 25 25 49 49 49 49 25 25 25

25 25 25 25 25 25 25 25 25 25

25 25 25 25 25 25 25 25 25 25

25 25 25 25 25 25 25 25 25 25

Figure 17. Precision delimiting grid showing trap densities per sq. mile

E. Treatment considerations

When treating, special consideration must be given to people living and working in the area. Notices,

with information about when an area will be sprayed, what will be sprayed, and any possible side effects, 

should be sent to residents and businesses and posted in public areas. People should be encouraged to 

stay indoors at the time the spraying should occur. Open houses and a well-staffed toll free hot line 

should also be used to help educate the public. 

23 | Page
1. Aerial insecticide treatment

Aerial applications of diflubenzuron or Btk are the best-tested and most effective tools available for 

eradicating isolated gypsy moth populations. Aerial application provides more thorough coverage than 

ground-based sprayers and is the only viable option for applying insecticides to forested areas and/or 

areas with very tall vegetation that is beyond the reach of ground-based sprayers. Of the two insecticides 

listed, diflubenzuron is generally more effective against gypsy moth and requires fewer applications and 

less precise timing compared to Btk. Btk, however, has fewer non-target effects and is used more often 

against gypsy moth.

2. Ground-based insecticide treatment

If aerial application of pesticides is not feasible, treatment using ground-based equipment such as 

hydraulic sprayers may be an alternative. Ground-based equipment allows targeting of host trees while 

avoiding non-hosts and objects such as houses, cars, and buildings. Along with coverage issues, ground 

spraying is labor and time intensive and treatments typically have to be made during daylight hours. This

can create more exposure to humans than aerial spraying which can be scheduled early mornings. 

Ground spraying can also be problematic because spray trucks and/or operators often require access to 

private land (BCMFR, 2007).

F. Degree-day modeling

1. Use of degree-day projections

Degree-day models are phenological simulation models that use temperature data to predict when 

biological events will occur. Gypsy moth degree-day models are available that use daily minimum and 

maximum temperatures to estimate the timing of events such as egg hatch or adult flight. In programs to 

eradicate isolated GM populations, wild egg masses and other immature stages are often difficult to 

impossible to find, and these models are valuable aids in determining the proper time to apply control 

measures such as Btk sprays (which are only effective against early instars) or mating disruption 

applications. Predictions of dates when adult flight will occur can also be used to time placement and 

removal of disparlure-baited traps. Note that for detection programs, however, trapping periods should 

generally be much broader than the flight periods predicted by models. Moths that arrived in an area 

recently may have been exposed, during much of their lives, to temperatures very different from local 

conditions. As a result, the models would be poor predictors of dates when their flight would occur. 

24 | Page
The most commonly used gypsy moth phenology model is GMPHEN (Sheehan 1992). The model was 

based on data from EGM and is thought to be generally applicable to AGM, although temperature-related 

differences in development among strains have been demonstrated (Keena 1996). Studies are currently 

underway to develop better data on potential differences among Asian, Japanese, and European strains, 

especially with regard to predicting hatch dates. However, the movement of AGM egg masses around the 

world, from one climate to another complicates the application of a model. 

Weather data for GMPHEN typically consist of daily minimum and maximum temperature readings 

throughout one calendar year (January 1 to December 31), or at least from the first of the year until late in 

the expected flight season (GMPHEN allows for other options). Daily min/max temperature data, and a 

variety of related information, are available for many weather stations throughout the United States. The 

data can be obtained at no charge in comma-delimited files from sites such as www.wunderground.com. 

Typically, these files are pasted into a spreadsheet such as MS-Excel, placed into the basic format for a 

GMPHEN data file, and then exported to Notepad or a similar editor for final formatting. For initial 

planning of program activities, data from one or more locations near the program area can be 

downloaded, averaged across multiple years if desired, and run in GMPHEN. For finer estimates of 

gypsy moth phenology at the program site, temperatures can be monitored on-site and used to replace the 

historical data as the season progresses. GMPHEN can be obtained online from the Forest Service 

(http://www.fs.fed.us/ne/morgantown/4557/gypsymth/download.html) or by contacting the CPHST Otis 

Laboratory.

2. Predicting gypsy moth hatch

For AGM programs, one shortcoming of using sterile egg masses is that hatch patterns of AGM may 

differ somewhat from those of European-type GM, and especially those of EGM from a lab-adapted strain 

that has been irradiated. If wild-type egg masses are found in the program area and the program deems it 

worth the risk, they can similarly be sealed in escape-proof cages and followed to monitor hatch.

3. Historic hatch data 

In some instances, AGM populations will be detected in areas where gypsy moths (AGM or EGM) had 

been detected in earlier years, and data on timing of hatch of wild eggs had been collected. These data 

can be used in conjunction with the above methods to improve confidence in date-of-hatch estimates.

25 | Page
4. Phenological indicators 

Timing of hatch of gypsy moth eggs tends to coincide in various locales with botanical events. For 

example, in New England, hatch is said to occur when shadbush (or serviceberry, Amelanchier sp.) 

bloom. More critical to the gypsy moths’ ecology, hatch of EGM typically occurs at approximately the 

time of bud break in members of the red oak subgroup (Quercus sp.). 

V. Post Treatment Delimiting Surveying to Verify Treatment Effectiveness

A. Area and density to be surveyed

Area within a five mile (8 km) radius of any traps that captured AGM should be trapped at 16-36 traps per 

square mile (2.6 sq. km) the following year or, if possible, at the end of the season when initial captures 

occurred (AGM SAP, 2007). These traps should be in place for at least 3 months (and longer in warmer 

areas) starting several weeks before adult flight is expected to start (AGM SAP, 2004). See Section III.D.

for guidance on trapping dates. 

B. Duration of surveying necessary to declare successful eradication

Trapping in the five mile (8 km) radius area should be continued for three years, including the year of 

treatment, to provide assurance that no population remains. If a positive capture takes place during these 

3 years, reset delimiting survey.

VI. Environmental Assessment

Though treatment options are included in the 2012 Supplemental Final Environmental Impact Statement, 

a site-specific Environmental Assessment is required to analyze the specific conditions of the proposed 

treatment area and what effects an eradication treatment might have on the area.

VII. Collaboration with State Government Entities

Each State in which a suspect AGM is captured has in common with PPQ an interest in detection and 

control of the pest. The partnerships between PPQ and State Departments of Agriculture are essential. 

PPQ understands each State's interest in protecting resources that may be threatened by AGM. 

26 | Page
VIII. Glossary

Asian gypsy moth (AGM)—For regulatory purposes, Asian gypsy moths include the following species: 

Lymantria albescens, Lymantria dispar asiatica, Lymantria dispar japonica, Lymantria postalba, and 

Lymantria umbrosa.

Btk—The abbreviation used for the biological insecticide Bacillus thuringiensis var. kurstaki.

Delimiting survey— A survey to determine the limits of an infestation and the approximate size of the 

infestation.

Delta trap—A triangular shaped trap made of plastic coated cardboard which uses a sticky surface to 

capture insects. For gypsy moth, disparlure is used to attract male moths to the trap.

Detection survey—A survey to determine if a species is present in an area where it is not known to 

exist. For gypsy moth, detection surveys most often consist of a systematic deployment of pheromonebaited traps.

Disparlure— The chemical cis-7,8-epoxy-2-methyloctadecane, which is the only known active 

component of the female gypsy moth’s sex attractant pheromone.

Eradication—Action taken to eliminate all members of a population or to drive a population to 

extinction.

GMPHEN—Phenology model used to determine potential for capturing male moths in different areas of 

the country throughout the year. Based on data from European gypsy moth, and thought to be generally 

applicable to AGM, although temperature-related differences in development among strains have been 

demonstrated.

High risk areas—Areas where AGM is most likely to be introduced. These may include, but are not 

limited to, ports, international or state border crossings, inland waterways, rivers used for transportation 

of goods, warehouse districts, inspection stations, major highways and railways, rest areas and weigh 

stations, parks, and inland container storage and intermodal sites.

27 | Page
Isolated infestation—A population that is isolated geographically from other populations of the same 

species

Lymantria albescens—Found on Okinawa and the southern Ryukyu Islands of Japan. Females are 

capable of flight. Considered AGM for regulatory purposes. Formerly known as Lymantria dispar 

albescens.

Lymantria dispar asiatica— A subspecies of L. dispar found in Asia, mostly east of the Ural Mountains, 

China, and Korea. Females are capable of flight. Considered AGM for regulatory purposes. 

Lymantria dispar dispar—The scientific name for the European gypsy moth, which is established in 

areas of North America. The females have wings but are flightless.

Lymantria dispar japonica—A subspecies of L. dispar found on all of the main islands of Japan. 

Females are capable of flight. Considered AGM for regulatory purposes. 

Lymantria postalba— Found on southern Kyushu and northern Ryukyu Islands of Japan. Females are 

capable of flight. Considered AGM for regulatory purposes. Formerly known as Lymantria dispar 

postalba, L. d. tsushimensis, and L. albescens tsushimensis.

Lymantria umbrosa— Found in Hokkaido, Japan. Females are capable of flight. Considered AGM for 

regulatory purposes. Formerly known as Lymantria dispar hokkaidoensis, L. d. umbrosa, and L. d. 

nesiobia. 

Maritime Waterway—An inland waterway, such as Puget Sound, San Francisco Bay, or the Columbia 

River, that is transited by trans-oceanic vessels.

Milk carton trap—A milk carton shaped trap made of plastic coated cardboard that uses insecticide to 

kill insects and has a larger capacity than a delta trap. For gypsy moth trapping, milk carton traps are 

placed where you can expect to trap 20 or more moths. 

Post treatment delimiting survey—A delimiting survey conducted after an eradication program to 

determine if eradication was successful.

28 | Page
Precision delimiting survey—A more intensive delimiting survey than is usually applied due to 

circumstances of the detection such as finding one moth or the environment in which the moth was found. 

May be used to determine the necessity of or prepare for an eradication treatment at the recommendation 

of the Technical Working Group. 

Ship interceptions “high”–When interceptions of the number of ships with egg masses are higher than 

the average for a location.

Treatment—Any action taken that is intended to control a pest

IX. References

Animal and Plant Health Inspection Service (APHIS). 2006. Asian gypsy moth cooperative eradication 

program Orange County, CA; Environmental Assessment. 

http://www.aphis.usda.gov/plant_health/ea/downloads/gypsymothorangecountyfinal.pdf

Animal and Plant Health Inspection Service (APHIS). 2006. Asian gypsy moth cooperative eradication 

program Travis County, Texas; Environmental Assessment. 

http://www.aphis.usda.gov/plant_health/ea/downloads/gypsymoth-txfinal.pdf

Animal and Plant Health Inspection Service (APHIS). 1992. Asian Gypsy Moth Emergency Program 

Manual. 

Asian gypsy moth Science Advisory Panel. 2007. Asian Gypsy Moth Science Advisory Panel Report. 

Asian gypsy moth Science Advisory Panel. 2006. Asian gypsy moth Science Advisory Panel Report. 

http://www.aphis.usda.gov/plant_health/plant_pest_info/sirex/downloads/sirex-sap-report.pdf

Asian gypsy moth Science Advisory Panel. 2004. Asian Gypsy Moth Science Advisory Panel Comments 

and Recommendations. 

Bell, R. A., C. D. Owens, M. Shapiro, and J. R. Tardif. 1981. Development of mass-rearing technology, 

pp. 598-633. In C. C. Doane and M. L. McManus [eds.], The gypsy moth: research toward integrated 

pest management. USDA Technical Bulletin 1584, Washington, D. C.

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Bogdanowicz, S.M., W.E. Wallner, J. Bell, T.M. Odell, and R.G. Harrison. 1993. Asian Gypsy Moths 

(Lepidoptera: Lymantriidae) in North America: Evidence From Molecular Data. Ann. Entomol. Soc. 

Am. 86, 710-715.

British Columbia Ministry of Forestry and Range (BCMFR). 2007. Ground spraying Btk for gypsy moth 

eradication in British Columbia. http://www.for.gov.bc.ca/hfp/gypsymoth/ground.htm

Buss, L.J., D.G. McCullough, and C.W. Ramm. 1999. Comparison of three egg mass survey methods in 

relation to gypsy moth (Lepidoptera: Lymantriidae) defoliation in Michigan. Environmental 

Entomology 28, 485-495.

Cooperative Agriculture Pest Survey (CAPS). 2008. Asian gypsy moth pest alert. United 

States Department of Agriculture. 

http://www.agmkt.state.ny.us/caps/pdf/Asian%20Gypsy%20Moth%20Pest%20Alert.pdf

Doane, C. C. & M. L. McManus (eds). 1981. The gypsy moth: research toward integrated pest 

management. USDA Technical Bulletin 1584. Washington, DC, USA. 757 p.

Garner, K.J., and J.M. Slavicek. 1996. Identification and Characterization of a RAPD-PCR marker for 

Distinguishing Asian and North American Gypsy Moths. Insect Molecular Biology. 5, 81-91.

Keena, M. A. 1996. Comparison of the hatch of Lymantria dispar (Lepidoptera: Lymantriidae) eggs from 

Russia and the United States after exposure to different temperatures and durations of low 

temperature. Annals of the Entomological Society of America. 89, 564-572.

Keena, M.A., W.E. Wallner, P.S. Grinberg and R.T. Carde. 2001. Female flight propensity and capability 

in Lymantria dispar (Lepidoptera: Lymantriidae) from Russia, North America, and their reciprocal f1 

hybrids. Environmental Entomology 30, 380-387.

Kolodny-Hirsch, D.M. 1986. Evaluation of methods for sampling gypsy moth (Lepidoptera: 

Lymantriidae) egg mass populations and development of sequential sampling plans. Environmental 

Entomology 15, 122-127.

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Lance, D.R. 2009. Asian gypsy moth (Lymantria dispar). Personal communication.

Lance, D. R., and D. O. McInnis. 2005. Biological basis of the Sterile Insect Technique. 69-94. In V. A. 

Dyck, J. Hendrichs and A. S. Robinson [eds.], Sterile Insect Technique: principles and practice in 

area-wide integrated pest management. Springer, Dordrecht, The Netherlands.

Lance, D., M. White, V. Mastro, A. Sawyer, M. Connor, K. Connors & S. Burks. 2003. Male (gypsy) 

moth trapping in Minnesota. Presented at the 14th USDA Interagency Research Forum on Gypsy 

Moth and Other Invasive Species, Annapolis, MD, 14-17 January.

Lance, D. R., and D. B. Gates. 1994. Sensitivity of detection trapping systems for Mediterranean fruit 

flies (Diptera: Tephritidae) in southern California. Journal of Economic Entomology 87, 1377-1383.

Lance, D. R., T. C. Holler, D. B. Gates, V. C. Mastro, and A. J. Sawyer. 2007. Strategies for optimizing 

detection trapping systems. Poster presentation at the 55th Annual Meeting of the Entomological 

Society of America, San Diego, CA, 9-12 December. 

Lance, D. R., T. M. ODell, V. C. Mastro, and C. P. Schwalbe. 1988. Temperature-mediated programming 

of activity rhythms in male gypsy moths (Lepidoptera: Lymantriidae): implications for the sterile 

male technique. Environmental Entomology. 17, 649-653.

Maksimovic, M. 1972. Two releases of sterile gypsy moth males (Lymantria dispar L.) in the park of 

Jelsa on the island of Hvar. Zastita Bilja. 23, 37-48.

Mastro, Vic. 2009. Asian gypsy moth (Lymantria dispar). Personal communication. 

Peterson, A.T., R. Williams and G. Chen. 2007. Modeled global invasive potential of Asian gypsy moths, 

Lymantria dispar. Entomologia Experimentalis et Applicata. 125, 39-44.

Plant Protection and Quarantine (PPQ). 2008. Asian gypsy moth trapping submission guidelines.

Plant Protection and Quarantine (PPQ). 2007. Taking Emergency Action for Suspect Asian Gypsy Moth 

Ships. Manual for Agricultural Clearance. 

http://www.aphis.usda.gov/plant_health/plant_pest_info/gypsy_moth/downloads/guidelines.pdf

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Plant Protection and Quarantine (PPQ). 2003. Asian gypsy moth fact sheet. 

http://www.aphis.usda.gov/lpa/pubs/fsheet_faq_notice/fs_phasiangm.html

Pogue, M. G. & P. W. Schaefer. 2007. A review of selected species of Lymantria Hübner [1819] 

including three new species (Lepidoptera: Noctuidae: Lymantriinae). USDA Forest Service, FHTET 

2006-07. 

Pritchard, J.K., P. Stephens, and P. Donnelly. (2000). Inference of Population Structure using Multilocus 

Genotype Data. Genetics. 155: 945-959.

Reardon, R. C., and V. C. Mastro. 1993. Development and status of the sterile insect technique for 

managing gypsy moth. AIPM Tech.Transfer. NA-TP-13-93, 17.

Reineke, A. and C.P.W. Zebitz. 1998. Flight ability of gypsy moth females (Lymantria dispar): a 

behavioural feature characterizing moths from Asia? Journal of Applied Entomology. 122(6), 307.

Robinet, C., D. R. Lance, K. W. Thorpe, K. S. Onufrieva, P. C. Tobin, and A. M. Liebhold. 2008. 

Dispersion in time and space affect mating success and Allee effects in invading gypsy moth 

populations. Journal of Animal Ecology 77, 966-973.

Savotikov, I.F., A.I. Smetnik, and A.D. Orlinskii. 1995. Situation of the Asian form of gypsy moth 

(Lymantria dispar) in Russia and the world. European Plant Protection Organization Bulletin. 25(4), 

617-622. 

Sheehan, K. A. 1992. User's guide for GMPHEN: gypsy moth phenology model. USDA, Forest Service 

Northeastern Forest Experiment Station, General Technical Report. NE-158, 29.

United States Department of Agriculture. 1981. The gypsy moth: research toward integrated pest

management. 

Wallner, W. E. & K. A. McManus (eds). 1989. Lymantriidae: a comparison of features of new and old 

world tussock moths. USDA Forest Service, Northeastern Forest Experiment Station, General 

Technical Report NE-123.

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Appendix A - USDA ASIAN GYPSY MOTH POLICY

It is well documented that gypsy moths (Lymantria dispar) display considerable variation in behavior 

throughout their range. Most Asian strains of gypsy moth are characterized by females capable of strong 

directed flight and host ranges broader than that of the gypsy moth strain currently established in North 

America (narrow genetic range based on isolation of population originally introduced from Europe in 

1869; characterized by non-flying female moths). In recognition of these significant behavioral 

differences, it has been determined that Asian Gypsy Moth (AGM) warrants status as a significant, exotic 

pest of economic importance. Contrary to USDA’s North American gypsy moth (NAGM) policy of not 

conducting eradication activities within the generally infested area, action will be taken against confirmed 

AGM infestations in the generally infested area when the source of the introduction is known. 

Knowledge of the time, location and extent of an Asian introduction will be required to trigger treatment 

activities. In cases where deductive, circumstantial or investigative information can be developed about 

an introduction of uncertain origin, appropriate action may also be recommended and taken. The goal of 

such treatments will be to eliminate all of the gypsy moths that exhibit traits characteristic of AGM.

USDA’s current policy of excluding the introduction and preventing the establishments of exotic 

economic pests will be applied to AGM, regardless of whether an introduction occurs within or outside of 

the area generally infested with NAGM.

The consequences of an AGM introduction into the United States will be determined by several factors, 

the most important of which are: 1) source of the introduced AGM, 2) site of introduction and 3) size of 

introduction relative to any resident North American population. Operational responses to mitigate these 

consequences will be based upon the specific circumstances of each occurrence to maximize the 

effectiveness of treatment strategies.

Recent studies indicate that several Asian strains are sexually compatible with NAGM, resulting in hybrid 

progeny that possess a mixture of behavioral characteristics and demonstrate observed hybrid vigor. 

While the exact effects of such hybridization are not well defined, the presence of NAGM in superior 

numbers is believed to dilute the expression of noxious Asian behaviors (i.e. female flight and a broader 

host range) in mixed populations. However, the possible retention of these traits at some low level

requires mitigation measures where feasible to prevent or reduce the likelihood of introducing Asian 

genetic material into NAGM populations.

In recognition of the behavioral differences between AGM and NAGM, standard programmatic 

operations used outside of the generally infested area will be modified. Pretreatment delimiting surveys 

will not be conducted for AGM due to the potential increase in size and scope an AGM population can 

achieve in a single year. Control measures will commence as soon as possible after confirmation of an 

Asian introduction based upon the best information available, followed by extensive post-treatment 

delimiting surveys.

In order reduce the likelihood of future introductions, USDA will conduct multifaceted exclusionary 

activities, supported by effective detection surveys at high risk introduction sites. These sites will include 

ports of entry, selected military bases, and other locations as needed.

Future policy changes will be determined by scientific advances that provide new information required 

for informed decision making and improved operational support.

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Appendix B – AGM Trapping Submission Guidelines

Asian Gypsy Moth Trapping Submission Guidelines

Specimens trapped in the field can be analyzed for the presence of Asian genetic markers by submitting the 

specimens to the CPHST Otis Laboratory. All specimens submitted from outside the generally-infested area 

will be analyzed. Because of the quantity of specimens submitted from within the generally-infested area, only 

a small fraction can be analyzed. Collect captured moths a minimum of every two weeks to minimize DNA 

degradation of the specimens, more frequently in warm climates.

Store specimens in a cool, dry location (frozen if possible). 

Ship ASAP after collection

MILK CARTON TRAPS

DO layer loose moths between wadded paper

towels or tissue paper in paper bag (brown lunch 

bag size) to prevent motion and specimen damage 

during shipment.

DO label paper bag clearly with trap numbers 

matching paperwork. 

DO staple or tape paper bag closed.

DO NOT attach paperwork to bags.

DO NOT use plastic bags or paper envelopes as 

these promote fungal growth and do not allow 

moisture release.

DO NOT send traps or paperwork for traps 

which contain no specimens.

DELTA TRAPS

DO label each trap clearly with trap numbers 

matching paperwork.

DO package traps to avoid crushing during 

shipment.

DO NOT attach paperwork to traps.

DO NOT use Styrofoam peanuts for packaging.

DO NOT disassemble the traps or remove moths 

from the trap.

SHIPPING

DO send a PPQ Form 305 for each trap sent.

Include: • Trap number • Collection Date

• Collection Site • Life Stage

• No. of specimens (estimates OK)

DO package moths / traps to prevent crushing or 

motion during shipping. Moths must be received 

whole with antennae and legs attached to body.

DO ship via next day delivery for Tuesday 

through Friday arrival.

DO ship ASAP after each collection.

DO keep moths frozen until shipment.

DO keep specimens dry.

DO NOT attach paperwork to traps or bags.

DO NOT use Styrofoam peanuts with delta traps.

DO NOT send traps or paperwork for traps with 

no specimens.

SHIP TO: 

 John Molongoski 

 USDA, APHIS, PPQ 

 CPHST Otis Laboratory 

 1398 West Truck Road

 Buzzards Bay, MA 02542-1329

 • Voice: (508) 563-9303 ext 218

 • Fax: (508) 564-4398

 • Email: john.j.molongoski@aphis.usda.gov

 PPQ Form 305 can be obtained from the Otis Lab via phone or email requests. Please do not hesitate to contact 

us if you have any questions.

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Appendix C – PPQ Form 305

Longitude  Eggs

 Larvae

 Pupae

 Female

PPQ FORM 305

FOR LABORATORY USE ONLY

Buzzards Bay, MA 02542

16. Date Sent:

Fax: 508-563-0903

Date Received: Otis MSC ID Number:

15. Send to:

13. Other Life Stages Collected:

Phone: 

14. Special Treatments of Specimens: (e.g. freezing conditions, use of alcohol, prolonged storage conditions, host if no trap used, etc.)

12. Number of Specimens in trap:

Latitude

Tel: 508-563-0929

Other Coordinates

Molecular Diagnostics

USDA, APHIS,PPQ

CPHST Otis Lab

1398 West Truck Road

State

County Number of Specimens

Address

City

Genotype Analysis

11. Trap Location:

Fax: 

5. Submitting Agency:

U.S. Department of Agriculture Animal and Plant Health Inspection Service Plant Protection and Quarantine

Insect Collection Worksheet for

Public reporting burden for this collection of information is estimated to average .17 hours per response, including the time for reviewing

instructions, searching existing data sources, gathering & maintaining the data needed, & completing and review the collection of

information, including suggestions for reducing this burden, to Department of Agriculture, Clearance Officer, OIRM, AG Box 7630,

Complete for each trap containing specimens

Washington, D.C. 20250, & to the Office of Information and Regulatory Affairs, Office of Management and Budget, Washington, D.C. 205

1. Insect Name:

2. Submitter's Name: 3. Submitter's Address:

4. Email Address:

TRAP DATA

10. Trap Type:

6. Date Collected: 7. Date of Last Trap Check: 8. Trap Number: 9. Nearest Port of Entry

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