Details for Harvest Job Id: 80df33a0-5609-4e20-991a-ff7404c48b26

Job Info

Harvest Source:	usda-json
status:	complete
job_type:	harvest
date_created:	2025-12-03 07:31:21.717969
date_finished:	2025-12-03 07:33:49.529524
records_total:	2905
records_added:	0
records_updated:	0
records_deleted:	0
records_errored:	3
records_unchanged:	2902
records_validated:	0
id:	80df33a0-5609-4e20-991a-ff7404c48b26

Job Error Table

No job errors found

Record Error Details

Error type summary
Error type	Number of errors
ValidationError	3

90dfa87e-f3aa-4339-877b-5417865963a1

Identifier: 10.15482/USDA.ADC/27982133.v1

Title: Data from: Non-consumptive effects of parasitoids and predators in stored products: The case of Theocolax elegans and other field-collected predators on the foraging of lesser grain borer and rice weevil

Harvest Record ID: 08a36f5f-1589-4741-9322-9db823a3fe58

Error Message:

<ValidationError: '$.description, \'InsectsBeetles used in this study were obtained from stock colonies maintained at the USDA Agricultural Research Service’s (ARS) Center for Grain and Animal Health Research (CGAHR) in Manhattan, KS, USA. Colonies of R. dominica and S. oryzae were reared on organic whole wheat kernels that had been tempered to 15% grain moisture. To subculture, a total of 50 adult individuals were placed on 200 mL of grain in a mason jar (capacity: 473 mL) and given 14 d to mate and lay eggs. At the end of that period, adult hosts were removed by sieving with a #10 sieve (2.00 mm; W.S Tyler Inc., Mentor, Ohio), and colonies were allowed to age for 3-weeks prior to using beetles as hosts for parasitoid rearing. Theocolax elegans were maintained separately on two different hosts, either R. dominica or S. oryzae for at least three full generations. Freshly emerged, healthy T. elegans were used for the experiments below. All colonies of parasitoids were maintained in a separate environmental chamber than host-only colonies to prevent cross-contamination. Colonies were maintained in mason jars and stored in an environmental chamber under constant conditions (27.5°C, 60% RH, 14:10 L:D).Interactions with PredatorsLaboratory studies were performed in 2022 and 2023 at the USDA Center for Grain and Animal Health Research (Manhattan, KS, USA). From July–October of each year, predators were collected weekly from local post-harvest food facilities, including the Kansas State Agronomy Farm (GPS: 39.2062227, -96.5951959), where S. oryzae and other stored product pests are abundantly found (Morrison et al. 2025<a href="#_msocom_1" target="_blank">[1]</a> ). Most predators used in trials were collected by sweep netting (Bioquip Products, Inc., Rancho Dominguez, CA) sampling vegetation adjacent to grain bins or by hand collection and held temporarily in 1-gal (=3.98 L) Ziplocks, then immediately brought back to the lab in a cooler on insulated ice packs. In the lab, insects were processed by individually placing predators into a 950-mL mason jar with 10 S. oryzae from colonies. The predators were identified to family (Marshall 2006, Paquin et al. 2017). Mason jars with predators and S. oryzae were then placed on shelves in an environmental chamber set to constant conditions (27.5°C, 60% RH, 14:10 L:D). After 24 h, the jars were checked, and the number of S. oryzae consumed was recorded as well as the presence of any self-aggregation behavior of S. oryzae together and away from the predator, which was taken to be evidence for non-consumptive effects in the presence of the predator. The results of predators were only included when there were n = 3 or greater number of replicates.EthovisionVideo-tracking coupled with Ethovision software v.14.0 (Noldus, Inc., Leesburg, VA: Noldus et al. 2002) was used to investigate the impact of natural enemy kairomones on the mobility and orientation of R. dominica and S. oryzae over short distances. This system has previously been used for analyzing the mobility and foraging behaviors of stored product insects (Wilkins et al. 2020; Ponce et al. 2022). Six arenas consisting of Petri dishes (VWR Petri dishes, 100 × 15 mm) with an 85-mm filter paper (Grade 1, Whatman, GE Healthcare, Chicago, IL) adhered to the bottom using double-sided sticky tape were arranged 80 cm below a network video camera (GigE, Basler AG, Ahrensburg, Germany). The movement of individual insects within each arena was simultaneously recorded on an adjacent computer. Four zones were monitored in Ethovision, including the two halves of the Petri dish (i.e. treatment half vs control half) and two 1 cm diameter zones nested in the middle of each half where stimuli were applied (treatment stimulus zone and control stimulus zone). The position of treatments was randomized between replicates and a total of n = 12 replicate assays were conducted for each treatment. For each assay, a single insect was introduced into the center of an arena and its movement was tracked for a total of 10 min. Several measurements were summarized in Ethovision including cumulative distance moved (cm), instantaneous velocity (cm/s), frequency of entering each stimulus zone, latency to enter each stimulus zone, cumulative time in each stimulus zone, and cumulative time in each half of the arena.Parasitoid cues<a href="#_msocom_2" target="_blank">[2]</a>Both headspace extracts (wasp extract experiments) and adult wasps (adult wasp experiments) were employed as stimuli in experiments examining influence of parasitoid cues on R. dominica and S. oryzae movement and foraging. Treatment stimuli employed for wasp extract experiments consisted of clean solvent (control), headspace extract collected from 100 g of uninfested wheat (wheat), and headspace extract collected from colonies of conspecifics parasitized by T. elegans (parasitoid) applied in 10 μL aliquots to 10 mm filter paper discs. Prior to addition of filter paper to arenas, the solvent was allowed to evaporate for 15 s. Adult wasp experiments employed a single wheat kernel (wheat), two female T. elegans (parasitoid), and no stimulus (control) as treatment stimuli. Ethovision experiments were blocked by presence of wasps to account for potential spillover wasp odors to neighboring arenas. Control zones either lacked stimuli (adult wasp experiments) or contained a 10 mm filter paper disc to which 10 μl of clean dichloromethane solvent was applied (wasp extract experiments).Predator cues<a href="#_msocom_3" target="_blank">[3]</a>As Orthoptera were most commonly encountered in field plots and consumed S. oryzae at relatively high rates, experiments examining the response of S. oryzae and R. dominica to predator cues focused on one orthopteran family, namely Gryllidae. Gryllus pennsylvanicus (hereafter, gryllids) were collected from the Kansas State University Agronomy Farm by deploying 9 bottle traps (5 × 10 cm D:H)<a href="#_msocom_4" target="_blank">[4]</a> flush with the ground spaced 5 m apart among grain bins with S. oryzae documented in the area. The pitfall traps were 3D-printed (Lulzbot Taz 6) and baited with 5 g of cornmeal. Traps were checked daily during August–September 2024. Two experiments were conducted to assess the impact of gryllid cues on R. dominica and S. oryzae movement. The first experiment examined the impact of olfactory stimuli on R. dominica and S. oryzae movement, with treatment stimuli consisting of clean solvent and cricket headspace extracts. The cricket headspace extracts were prepared according to the headspace collections below. The second experiment examined the impact of predator visual cues with and without associated olfactory cues on R. dominica and S. oryzae movement. For this experiment, treatment stimuli consisted of clean solvent, clean solvent with visual cues, and cricket headspace extract with visual cues. Visual cues consisted of small (30 × 8 × 5 mm L:W:H) cricket models (Toyvian) that were first baked off at 75℃ for 30 min to ensure they were chemically inert.Headspace Volatile CollectionsTo determine the role of chemical cues in mediating nonconsumptive interactions between stored product pests and their natural enemies, headspace volatiles were collected from predators (5 crickets, Gryllidae), colonies of S. oryzae and R. dominica that were parasitized by T. elegans, and uninfested wheat kernels. All samples were collected using a headspace collection system (after Van Winkle et al. 2022). An activated carbon filter was employed to remove background volatiles from central air, which was then split between eight lines. Each piece of the system was connected using chemically inert PTFE tubing and fittings. Inline flowmeters (Volatile Collection Systems, Gainesville, FL) were employed to maintain a flow rate of 1 L/min through each line. Volatiles were collected on traps consisting of a drip tip borosilicate glass tube containing 20 mg of Poropak-Q absorbent between a stainless-steel screen (No. 316), borosilicate glass wool, and a PTFE compression seal (Volatile Collection Systems, Gainesville, FL). Volatiles were collected for 24 h, after which volatiles were eluted by pushing 150 µL of HPLC-grade dichloromethane (Sigma-Aldrich, St. Louis, MO) through the traps with N2 gas. The eluent was collected in 2 mL screw-cap GC vials (Item#5191-8121, Agilent Inc., Santa Clara, CA, USA) with 150-μL glass inserts with polymer feet (Item#5181-8872, Agilent Inc.). All samples were magnetic capped with PTFE-backed silicone septa (Item#XXX, Agilent Inc.), sealed with PTFE tape, and stored at -20°C prior to use in behavioral assays and chemical analysis.Chemical AnalysisHeadspace volatile samples of 50 µL aliquots of each sample were transferred to new GC vials with 150-µL inserts for analysis by GC-MS. Prior to chemical analysis, 190.5 ng of tetradecane was added to each sample as an internal standard. Sample extracts were then run on an Agilent 7890B gas chromatograph (GC) equipped with an Agilent Durabond HP-5 column (30 m length, 0.250 mm diameter and 0.25 µm film thickness) with He as the carrier gas at a constant 1.2 mL/min flow and 40 cm/s velocity, which was coupled with a single-quadrupole Agilent 5977B mass spectrometer (MS). The split/splitless inlet was operated in splitless mode and maintained at 250°C during injection. The initial oven temperature of 40°C was maintained for 3 min, before increasing to 280°C at a rate of 10°C/min, where it was held for 3 min. After a solvent delay of 5.5 min, mass ranges between 35 and 550 atomic mass units were scanned. A mixture containing C8-C20 alkanes was employed to calculate Kovats index for all peaks. Preliminary identification of peaks was achieved by comparing spectral data and Kovats index with references in the NIST 14 library. Data was compiled using Masshunter Unknowns Analysis (Agilent Inc., Santa Clara, CA, USA) and compounds were aligned with the R package uafR (Stratton et al., 2024).\' does not match any of the acceptable formats: max string length requirement'>

Type: ValidationError

Date Created: 2025-12-03 07:32:26.392675

9a2dbd72-ddf4-4446-9f53-7816d49d1f2f

Identifier: 10.15482/USDA.ADC/27898743.v1

Title: Data from: Development and evaluation of a rearing protocol for laboratory assays utilizing the blue orchard bee (Osmia lignaria Say, Hymenoptera: Megachilidae)

Harvest Record ID: b4ea3aed-e63c-444e-9f39-f3097621e4e5

Error Message:

<ValidationError: '$.description, \'The blue orchard bee (Osmia lignaria Say, Hymenoptera: Megachilidae) is a native solitary bee in North America. This pollinator species is crucial for orchard pollination, primarily apples, almonds, and cherries. Osmia lignaria is an increasingly managed commercial species sold to supplement honey bee pollination services or used alone. Consistent protocols to rear O. lignaria and other above-ground nesting solitary bee species are lacking. This makes comparisons to social species, such as honey bees and bumble bees, difficult, and data comparisons between solitary bee species are incompatible.We collected data from two study years, comprising three studies, where we followed O. lignaria’s development from grafting of eggs or first instars in the summer to adult emergence the following spring. The data presented were control bees that were fed sterilized sham inoculate treatments in a larger pathogen-pesticide study.Adult O. lignaria were first released into an apple orchard in Logan, Utah, USA, where they were allowed to pollinate and mate, and females created nests with provisioned offspring. We then took completed nests to the laboratory, where they were opened to obtain O. lignaria-collected provisions (pollen+nectar) and eggs/first instars. We retained these provisions and eggs/first instars in our rearing studies and to evaluate our protocol methods. We then grafted eggs/first instars onto homogenized provisions on a graft date inside 3-D printed well plates. 3-D printed well plates were desired for our protocol to provide enough space to allow O. lignaria to complete their life cycle to adult emergence the following spring.Our research proves that O. lignaria can be reared in 3-D-printed well plates and emerge as adults the following spring. This can allow researchers to evaluate the chronic effects of pathogen and/or pesticide exposure on immature solitary bees. Alterations to the protocol, including different kinds of treatment types, can allow researchers to evaluate synergisms, antagonisms, or additive effects that may influence the survival, development, or weight metrics of O. lignaria. The protocol is replicable and could be adapted for other above-ground nesting solitary bee species.Our O. lignaria rearing protocol is provided in full detail at: dx.doi.org/10.17504/protocols.io.eq2lyj4qplx9/v2Key findings include: (1) Determination of development in fine detail and near-exact dates for individual developing O. lignaria inside 3-D printed well plates, (2) a 3-D print file that can be altered for other species if desired, (3) Number of days between life stages and the total number of days to each life stage, (4) Life status at various immature and mature life stages, (5) Sex determination for bees that reached adulthood (male or female), (6) Final life stage reached (larva, prepupa, pupa, or live/dead adult), (7) Suggested weight metrics evaluate for O. lignaria, and (8) Different winter diapause durations may produce variable emergence and weight loss results from year-to-year or study-to-study.Additional variables in the dataset include: (1) Study year, (2) Study name, (3) Sample identifier), (4) Provision batch, (5) Graft date, and (6) Various dates that reflect temperature and relative humidity (RH) durations.Abbreviations and acronyms in the “RAWdata” dataset<ul><li>Year = year data was collected</li><li>Study_name = name of study data was collected</li><li>Sample_ID = sample identifier (one for each individual bee, some IDs may be replicated for both years depending on plate replicate or position replicate)</li><li>Provision_batch = homogenized O. lignaria-collected provisions provided to eggs and/or first instars on a given graft date</li><li>Graft = date eggs and/or first instars were grafted onto homogenized provisions (provision batch)</li><li>First = date first instar was observed</li><li>Second = date second instar was observed</li><li>Fifth = date fifth instar was observed</li><li>Cocoon_initiation = date first signs of silk were observed</li><li>Cocoon_completion = date cocoon was determined to complete</li><li>Pupation = date pupation was observed, determined using X-ray imaging</li><li>Adult_molt = date adult molt was observed, determined using X-ray imaging</li><li>Arbitrary_Adult_molt = arbitrary adult molt date for bees where adult molt may not have been easily identifiable (+30 days since pupation date)</li><li>Ramp_down = date bees were placed into temperature+RH ramp-down conditions</li><li>Winter_diapause = date bees were placed in winter diapause conditions</li><li>Arbitrary_Adult_death = arbitrary adult death date provided for adults that died before emergence conditions and did not emerge successfully the following spring</li><li>Ramp_up = date bees were placed into temperature+RH ramp-up conditions</li><li>Emergence_inc_start = date emergence incubation began</li><li>Emergence = date emergence was observed (adults completely chewed out of cocoons)</li><li>Date_pulled = date bees were pulled from the experiment and frozen at -80℃</li><li>Graft_First = number of days between graft and first instar</li><li>First_Second = number of days between first instar and second instar</li><li>Second_Fifth = number of days between second instar and fifth instar</li><li>Fifth_Cinitiation = number of days between fifth instar and cocoon initiation</li><li>Cinitiation_Ccompletion = number of days between cocoon initiation and cocoon completion</li><li>Ccompletion_Pupation = number of days between cocoon completion and pupation</li><li>Pupation_Adult = number of days between pupation and adult molt</li><li>Adult_ArbitraryDeath = number of days between adult molt and an arbitrarily assigned death date for adults</li><li>ArbitraryDeath_Emergence = number of days between an arbitrarily assigned death date for adults and emergence</li><li>Adult_Emergence = number of days between adult molt and emergence</li><li>Second_Pupation = number of days between second instar and pupation</li><li>Second_Emergence = number of days between second instar and emergence</li><li>Total_Dev_Second = total number of days from graft to second instar</li><li>Total_Dev_Fifth = total number of days from graft to fifth instar</li><li>Total_Dev_Cinitiation = total number of days from graft to cocoon initiation</li><li>Total_Dev_Ccompletion = total number of days from graft to cocoon completion</li><li>Total_Dev_Pupation = total number of days from graft to pupation</li><li>Total_Dev_Adult = total number of days from graft to adult molt</li><li>Total_Dev_Emergence = total number of days from graft to emergence</li><li>Total_Dev_Second_Pupation = total number of days from second instar to pupation</li><li>Total_Dev_Second_Emergence = total number of days from second instar to emergence</li><li>Alive_Dead_First = were bees alive or dead at the first instar stage?</li><li>Alive_Dead_Second = were bees alive or dead at the second instar stage?</li><li>Alive_Dead_Fifth = were bees alive or dead at the fifth instar stage?</li><li>Alive_Dead_Cinitiation = were bees alive or dead at cocoon initiation?</li><li>Alive_Dead_Ccompletion = were bees alive or dead at cocoon completion?</li><li>Alive_Dead_Pupation = were bees alive or dead at pupation?</li><li>Alive_Dead_Adult = were bees alive or dead at the adult molt stage?</li><li>Alive_Dead_Emergence = were bees alive or dead at emergence?</li><li>Status_First = 0 means bees were alive at the first instar stage and 1 means they were dead (used in survival analyses)</li><li>Status_Second = 0 means bees were alive at the second instar stage and 1 means they were dead (used in survival analyses)</li><li>Status_Fifth = 0 means bees were alive at the fifth instar stage and 1 means they were dead (used in survival analyses)</li><li>Status_Cinitiation = 0 means bees were alive at cocoon initiation and 1 means they were dead (used in survival analyses)</li><li>Status_Ccompletion Status_Pupation = 0 means bees were alive at pupation and 1 means they were dead (used in survival analyses)</li><li>Status_Adult Status_Emergence = 0 means bees were alive at emergence and 1 means they were dead (used in survival analyses)</li><li>Pre_diapause_weight = weight in milligrams obtained for adults in cocoons before being placed into winter diapause (only live adults at the end of emergence are provided weights)</li><li>Post_diapause_weight = weight in milligrams obtained for adults in cocoons after winter diapause (only live adults at the end of emergence are provided weights)</li><li>Percent_weight_loss_X100 = weight loss calculated for each adult (only live adults at the end of emergence are provided weight loss calculations); calculated as post-diapause weight subtracted from pre-diapause weight divided by pre-diapause weight then multiplied by 100 to obtain a percentage (%) of weight loss</li><li>Sex = sex determined for bees that reached the adult stage (female or male)</li><li>Final_life_stage = final life stage recorded for each bee</li><li>Instar = if the bee’s final life stage was a larval stage, which larval stage was the final one recorded?</li><li>Required_more_time = did adults require more time than the allowed emergence period to emerge successfully? (adults that were still alive when cut out of cocoons, they were considered live adults but not included in emergence analyses)</li><li>Final_life_stage_2 = life stage for adults further categorized as live or dead</li><li>Sex_2 = males and females further categorized into live or dead</li></ul>Abbreviations and acronyms in the "Death_graft" dataset: The number of samples per year and study that did not survive past the first instar stage. The second instar stage was used to standardize survival and development since they begin to feed on provisions. Eggs and first instars were used as the initial grafting life stage because they are non-feeding stages of O. lignaria; therefore, they should be excluded from analyses unless desired.<ul><li>Year = year data was collected</li><li>Study_name = name of study data was collected</li><li>Sample_ID = sample identifier (one for each individual bee, some IDs may be replicated for both years depending on plate replicate or position replicate)</li><li>Provision_batch = homogenized O. lignaria-collected provisions provided to eggs and/or first instars on a given graft date</li><li>Graft = date eggs and/or first instars were grafted onto homogenized provisions (provision batch)</li><li>First = date first instar was observed</li><li>Death_graft = did sample experience death due to grafting? (likely via mechanical injury)</li><li>Graft_First = number of days between graft and first instar</li><li>Final_life_stage = final life stage recorded for each bee, for all these samples the final life stage reached was larva</li><li>Instar = if the bee’s final life stage was a larval stage, which larval stage was the final one recorded? For all these samples, the final instar reached was first</li></ul>\' does not match any of the acceptable formats: max string length requirement'>

Type: ValidationError

Date Created: 2025-12-03 07:33:00.986030

1a685d76-ed19-4a25-b9db-5f036f625744

Identifier: https://www.arcgis.com/home/item.html?id=4e6b0400575340d189aa6344c99026b4

Title: Legacy Aerial Fire Retardant Avoidance Area Products Deprecation & Retirement

Harvest Record ID: bc3d9b04-8aee-48bd-b3fb-e54688697959

Error Message:

<ValidationError: "$.description, 'background-color:rgb(255,255,255); font-family:Roboto; font-size:x-large;' does not match any of the acceptable formats: max string length requirement">

Type: ValidationError

Date Created: 2025-12-03 07:33:05.955864