Introduction
Palmer amaranth (Amaranthus palmeri S. Watson) is one of the most common, problematic, and economically detrimental weeds throughout the southern United States (Ward et al. Reference Ward, Webster and Steckel2013). It is one of the two most troublesome weeds in Arkansas, Louisiana, Mississippi, and Tennessee (Riar et al. Reference Riar, Norsworthy, Steckel, Stephenson, Eubank and Scott2013). Glyphosate-resistant A. palmeri infestations occurred in 16% of scouted areas in Louisiana and in 54% of scouted areas in Mississippi, Tennessee, and Arkansas (Riar et al. Reference Riar, Norsworthy, Steckel, Stephenson, Eubank and Scott2013). The average cost of hand weeding A. palmeri was US$59 ha−1 (Riar et al. Reference Riar, Norsworthy, Steckel, Stephenson, Eubank and Scott2013). Amaranthus palmeri emerges continuously from late spring to late summer as long as the soil temperature is favorable (between 22 and 32 C; Chahal et al. Reference Chahal, Barnes and Jhala2021; Keeley et al. Reference Keeley, Carter and Thullen1987).
The propensity of A. palmeri to evolve resistance to many herbicides has made it difficult to control. To date, it is resistant to 5-enolpyruvyl-shikimate-3-phosphate synthase–inhibiting herbicides (Culpepper et al. Reference Culpepper, Grey, Vencill, Kichler, Webster, Brown, York, Davis and Hanna2006; Norsworthy et al. Reference Norsworthy, Griffith, Scott, Smith and Oliver2008), acetolactate synthase (ALS)-inhibiting herbicides (Burgos et al. Reference Burgos, Kuk and Talbert2001; Gaeddert et al. Reference Gaeddert, Peterson and Horak1997; Horak and Peterson Reference Horak and Peterson1995), microtubule-inhibiting herbicides (Gossett et al. Reference Gossett, Murdock and Toler1992), 4-hydroxyphenylpyruvate dioxygenase–inhibiting herbicides (Jhala et al. Reference Jhala, Sandell, Rana, Kruger and Knezevic2014; Nakka et al. Reference Nakka, Godar, Wani, Thompson, Peterson, Roelofs and Jugulam2017b), photosystem II (PSII)-inhibiting herbicides (Nakka et al. Reference Nakka, Godar, Thompson, Peterson and Jugulam2017a), protoporphyrinogen oxidase (PPO)-inhibiting herbicides (Salas et al. Reference Salas, Burgos, Tranel, Singh, Glasgow, Scott and Nichols2016; Salas-Perez et al. Reference Salas-Perez, Burgos, Rangani, Singh, Refatti, Piveta, Tranel, Mauromoustakos and Scott2017; Varanasi et al. Reference Varanasi, Brabham and Norsworthy2018a, Reference Varanasi, Brabham, Norsworthy, Nie, Young, Houston, Barber and Scott2018b), and auxin mimic– and glutamine synthetase–inhibiting herbicides (Heap Reference Heap2021). Amaranthus palmeri has also evolved resistance to very-long-chain fatty acid (VLCFA)-inhibiting herbicides in Arkansas (Brabham et al. Reference Brabham, Norsworthy, Houston, Varanasi and Barber2019; Rangani et al. Reference Rangani, Noguera, Salas-Perez, Benedetti and Roma-Burgos2021).
VLCFAs are important components of lipids such as triacylglycerols (accumulated in seeds), some sphingolipids and phospholipids found in cell membranes, and cuticular waxes on plant aerial surfaces (Trenkamp et al. Reference Trenkamp, Martin and Tietjen2004). Therefore, VLCFAs are major components of hydrophobic polymers on the leaf surface, playing an important role in preventing desiccation (Trenkamp et al. Reference Trenkamp, Martin and Tietjen2004). Sphingolipids and phospholipids are required for cell division, polarity, and differentiation (Lechelt-Kunze et al. Reference Lechelt-Kunze, Meissner, Drewes and Tietjen2003). Herbicides that inhibit the VLCFAs target the condensing enzyme 3-ketoacyl-CoA synthase FAE1 within the elongase enzymatic complex bound to the endoplasmic reticulum (Boger Reference Boger2003; Busi Reference Busi2014; Matthes et al. Reference Matthes, Schmalfuss and Boger1998; Millar and Kunst Reference Millar and Kunst1997). By provoking a disruption of VLCFA levels in plants, these herbicides can inhibit growth or cause embryonic mortality (Du Granrut and Cacas Reference Du Granrut and Cacas2016). Herbicides that inhibit VLCFAs have been used for more than 60 yr (Busi Reference Busi2014). Important VLCFA-inhibiting herbicides include pyroxasulfone, dimethenamid-P, acetochlor, and S-metolachlor, with S-metolachlor labeled for use in more than 70 crops (O’Connell et al. Reference O’Connell, Harms and Allen1998). S-metolachlor effectively suppresses yellow nutsedge (Cyperus esculentus L.), annual grasses, and small-seeded broadleaf species, including A. palmeri (Barber et al. Reference Barber, Butts, Boyd, Cunningham, Selden, Norsworthy, Burgos and Bertucci2021). Despite the prevalent use of VLCFA-inhibiting herbicides, only five grasses had evolved resistance to them before resistance among Amaranthus species was reported (Busi Reference Busi2014; Heap Reference Heap2021) (Table 1).
Weed species that evolved resistance to very-long-chain fatty-acid–inhibiting herbicides globally, between 1982 and 2020. a
a Time span of resistance recorded by Heap (Reference Heap2021).
Weed resistance to herbicides is a major concern in modern agriculture, as it compromises producers’ efforts to sustainably manage crop production. Weeds generally cause greater yield reductions than other pests; therefore, weed management is mandatory in crop production (Oerke Reference Oerke2006). The use of synthetic herbicides has permitted simple and effective management of weeds in many cropping systems (Busi et al. Reference Busi, Porri, Gaines and Powles2018). However, resistance evolution in many weed species worldwide is reducing the effectiveness of chemical weed control (Beckie and Tardif Reference Beckie and Tardif2012; Busi et al. Reference Busi, Porri, Gaines and Powles2018; Powles and Yu Reference Powles and Yu2010; Roma-Burgos et al. Reference Roma-Burgos, Heap, Rouse, Lawton-Rauh, Korres, Burgos and Duke2019). Therefore, herbicide resistance is a key factor that spurs the search for new herbicide targets and intervention technologies (Burgos Reference Burgos2015) and the promotion of best management practices (Burgos Reference Burgos2015; Norsworthy et al. Reference Norsworthy, Ward, Shaw, Llewellyn, Nichols, Webster, Bradley, Frisvold, Powles, Burgos, Witt and Barrett2012). The loss of crucial herbicides and the need for immediate answers to growers’ needs require extensive research on weed resistance to enable proactive management of herbicide-resistant weeds (Burgos et al. Reference Burgos, Tranel, Streibig, Davis, Shaner, Norsworthy and Ritz2013).
For a comprehensive assessment of the resistance problem, other soil-applied herbicides need to be tested on populations deemed resistant to S-metolachlor. PPO-inhibiting herbicides such as fomesafen, flumioxazin, saflufenacil, and sulfentrazone have been extensively used as alternative herbicides to manage resistance to other herbicide modes of action (Umphres et al. Reference Umphres, Steckel and Mueller2018). They can be applied either preemergence or postemergence. Flumioxazin and fomesafen are effective on major weeds in field crop production such as common lambsquarters (Chenopodium album L.), common ragweed (Ambrosia artemisiifolia L.), A. palmeri, and morningglory species (Ipomoea spp.) (Askew et al. Reference Askew, Wilcut and Cranmer1999, Reference Askew, Wilcut and Cranmer2002; Clewis et al. Reference Clewis, Everman, Jordan and Wilcut2007; Niekamp et al. Reference Niekamp, Johnson and Smeda1999; Umphres et al. Reference Umphres, Steckel and Mueller2018). Flumioxazin can be applied with nonselective preplant burndown herbicides, preemergence alone or tank-mixed with other preemergence herbicides (Umphres et al. Reference Umphres, Steckel and Mueller2018). It is effective on glyphosate-resistant A. palmeri (Whitaker et al. Reference Whitaker, York, Jordan and Culpepper2010) or species resistant to ALS inhibitors or atrazine (Taylor-Lovell et al. Reference Taylor-Lovell, Wax and Bollero2002). Fomesafen, in combination with S-metolachlor or pendimethalin, can control glyphosate-resistant A. palmeri (Nandula et al. Reference Nandula, Ray, Ribeiro, Pan and Reddy2013). PSII-inhibiting herbicides are widely used for weed control in corn (Zea mays L.) and sorghum [Sorghum bicolor (L.) Moench] production (Norsworthy et al. Reference Norsworthy, Richburg, Barber, Roberts and Gbur2020). Many PSII-inhibiting herbicides have soil and foliar activity. Among the oldest PSII inhibitors with the broadest weed spectrum is atrazine (Senseman Reference Senseman2007). Together, the VLCFA, PPO, and PSII inhibitors comprise the most important groups of herbicides used in several production systems.
The extent of A. palmeri resistance to S-metolachlor in the midsouthern United States has not been investigated. The response of S-metolachlor–resistant populations to other soil-applied herbicides needs to be assessed to determine effective alternative chemical tools. The objectives of this research were to (1) evaluate the extent of A. palmeri resistance to S-metolachlor in the midsouthern United States, (2) determine the resistance level of accessions classified as resistant, (3) determine the change in resistance level from original populations to their progeny, and (4) investigate alternative preemergence herbicides for the control of resistant populations.
Materials and Methods
Amaranthus palmeri Seed Collection
Amaranthus palmeri seeds were collected in soybean [Glycine max (L.) Merr.] and cotton (Gossypium hirsutum L.) fields in 2017, 2018, and 2019 from midsouthern U.S. states Arkansas, Mississippi, and Tennessee (Figure 1). In Arkansas, samples were collected from 61 crop fields (15 counties) in 2017 and 35 crop fields (14 counties) in 2018. In Mississippi, samples were collected from 54 fields (17 counties) in 2017. In Tennessee, samples were collected from a total of 18 fields (10 counties) between 2018 and 2019. Samples were collected according to standard procedures (Burgos Reference Burgos2015) from fields reported by growers to university Extension agents as having a history of S-metolachlor use and A. palmeri at the end of the season. Inflorescences were harvested from at least 10 female plants and bagged to make one composite sample per field. The inflorescences were air-dried and threshed, and the seeds were cleaned. Seeds were stored at room temperature.
Amaranthus palmeri sampling sites in Arkansas, Mississippi, and Tennessee, USA, from 2017 to 2019.
During fall 2019, county Extension agents collected additional seeds from fields with accessions that were the most difficult to control among the 2018 collection (18CRI-D, 18PHI-C, and 18WOO-B). Accessions from these fields had high frequency of survivors in the resistance test (see “Results and Discussion”). The 2019 accessions were labeled 19CRI-D, 19PHI-C, and 19WOO-B, respectively, and included in subsequent dose–response studies.
Resistance Testing
A large-scale test for resistance was conducted in the greenhouse at the Milo J. Shult Agricultural Research & Extension Center (SAREC), University of Arkansas System Division of Agriculture, Fayetteville, AR, USA. Field soil (Roxana silt loam; coarse-silty, mixed, superactive, nonacid, thermic Typic Udifluvents), with no herbicide-use history, was collected from the Vegetable Research Station, Kibler, AR, USA. Greenhouse conditions for the study were 35/23 C day/night temperature and a 14-h photoperiod. Soil was air-dried and sieved. A subsample was submitted to the Agricultural Diagnostic Laboratory, MSAREC, Fayetteville, AR, USA, for analysis (Table 2). Soil pH and electrical conductivity (EC) were measured in a 1:2 soil:water mixture (Sikora and Kissel Reference Sikora and Kissel2014), and total nitrogen (N) was measured by thermal combustion analysis (Provin Reference Provin2014). Soil nutrients were analyzed using the Mehlich-3 method (Zhang et al. Reference Zhang, Hardy, Mylavarapu and Wang2014).
Chemical and physical characteristics of soil used for the greenhouse experiments conducted in 2018 to 2020 at the Shult Agricultural Research & Extension Center, University of Arkansas, Fayetteville, AR, USA. a
a Roxana silt loam soil from the Vegetable Research Station of the University of Arkansas, Kibler, AR, USA.
b Extracted using Mehlich-3 method.
c Soil pH and electrical conductivity (EC) measured in a 1:2 soil:water mixture.
d Measured by thermal combustion analysis.
The experimental units (flats) were arranged in a completely randomized design with three replicates, and the resistance test was repeated in time. The flats (12.2 cm by 9.5 cm by 5.7 cm; Insert TO standard, Hummert International, Earth City, MO, USA) were filled with 700 g of soil. The soil-filled flats were saturated with tap water the day before seeding and herbicide application and allowed to drain overnight to obtain uniform, water-holding capacity soil moisture. One hundred seeds were spread uniformly on the soil surface of each tray and were covered with a thin layer of soil. The assay had two treatments per accession (treated and nontreated). S-metolachlor (Dual II Magnum®, Syngenta Crop Protection, Greensboro, NC, USA) was applied at the field-labeled rate for soybean (1,120 g ai ha−1) in a spray chamber equipped with a motorized boom sprayer fitted with TeeJet® 1100067 nozzles (Spraying Systems, Wheaton, IL, USA) calibrated to deliver 187 L ha−1 at a pressure of 276 kPa in one pass and traveling at 0.45 m s−1. S-metolachlor was activated shortly after herbicide spraying by misting approximately 0.8 cm of water over the surface. The flats were misted overhead twice a day for the first week, after which the flats were subirrigated for the remainder of the study. Survivors of the labeled rate from the first resistance test (conducted during fall 2018) were grown, isolated within cages by accession, and allowed to interbreed for seed production to evaluate progression of herbicide resistance from parents to progeny. Two lines of progeny were produced (18PHI-C-F1 and 18WOO-B-F1).
S-Metolachlor Dose–Response Bioassays
Accessions with the least susceptibility to S-metolachlor, controlled less than 88% during the large-scale test, were subjected to a follow-up dose–response study. In 2019 and 2020, dose–response studies were conducted using nine rates of S-metolachlor (0, 0.125, 0.25×, 0.5×, 0.75×, 1×, 1.5×, 2×, 2.5×) for the putative resistant accessions, with the 1× rate being 1,120 g ha−1. A susceptible standard (SS), collected from an organic field in Woodruff County (AR, USA), was used as reference and treated with eight rates of S-metolachlor (0, 0.03125×, 0.125×, 0.25×, 0.5×, 0.75×, 1×, 1.5×). Overall, seven parent accessions were evaluated: five from Arkansas (17PRA-A, 17RAN-A, 18CRI-D, 18PHI-C, and 18WOO-B) and two from Mississippi (17TUN-A and 17TUN-D). The planting medium, seeding rate, herbicide application volume, watering, and plant maintenance were as described in “Resistance Testing.”
The “second-year” accessions—19CRI-D, 19PHI-C, and 19WOO-B—were included in the dose–response assay with the corresponding accessions collected from the same fields in 2018 and the respective progeny of survivors. The intent was to compare resistance levels between the 2018 and 2019 populations from the same fields and compare resistance levels between field-collected parents in 2018 and the progeny of plants surviving herbicide treatment in the greenhouse. Survivors of 18CRI-D did not produce enough seeds for a dose–response study of its progeny, so only field populations (18CRI-D and 19CRI-D) were studied. The dose–response rate structures were the same as those for the first year. The experimental design, plant establishment, and herbicide application details were as described in “Resistance Testing.” The assays were repeated in time.
Response of S-Metolachlor–Resistant Accessions to Other Soil-applied Herbicides
The response of the four accessions most resistant to S-metolachlor from dose–response assays (18CRI-D, 18WOO-B, 17TUN-A, and 17TUN-D) and one SS to five alternative residual herbicides representing three mechanisms of action (Table 3) was evaluated. These accessions (100 seeds per accession) were planted and treated with dimethenamid-P, pyroxasulfone, flumioxazin, fomesafen, and atrazine. Herbicides were applied at their respective field-use rates for soybean (dimethenamid-P, pyroxasulfone, flumioxazin, fomesafen) and corn (atrazine). Each accession had a nontreated control. The experiment was arranged in a completely randomized design with three replicates and was repeated in two greenhouses. Plant establishment and herbicide application details were as described earlier.
Herbicides used in resistance testing of Amaranthus palmeri from the midsouthern United States (Arkansas, Mississippi, Tennessee) in the greenhouse at the Shult Agricultural Research & Extension Center, University of Arkansas, Fayetteville, AR, USA.
a MOA, mechanism of action; PSII, photosystem II; PPO, protoporphyrinogen; VLCFA, very-long-chain fatty acid.
b Chemical names from Ransom (Reference Ransom2013).
Data Collection and Analysis
All bioassays were evaluated at 21 d after treatment (DAT). In each case, live plants were counted, and the data were converted to percent survival based on the number of live plants in the respective nontreated control. For the responses of S-metolachlor–resistant accessions to other soil-applied herbicides, survival rates were also evaluated at 14 DAT. The interaction between treatments and runs was not significant (P > 0.05); therefore, dose–response data were pooled across runs. Amaranthus palmeri percent survival in response to increasing rates of S-metolachlor, for parents and F1 progeny, were analyzed using a nonlinear regression equation. A three-parameter log-logistic model (Equation 1) was used to relate A. palmeri percent survival to S-metolachlor rates using nonlinear least-squares regression (nls) in R v. 4.0.0 (R Core Team 2020):
$$Y = {d \over {1 + {\rm{exp}}\left[ {b\left( {\log \left( x \right) - {\rm{log}}e} \right)} \right]}}$$
where Y is A. palmeri percent survival, d is the upper asymptotic value of Y, b is the slope of the curve, e is the rate of the herbicide required to reduce seedling emergence 50% (LD50), and x is the S-metolachlor dose.
For the resistance-profiling bioassay, A. palmeri percent control was subjected to ANOVA using the GLIMMIX procedure in SAS 9.4 (SAS Institute, Cary, NC, USA) assuming a beta distribution (Gbur et al. Reference Gbur, Stroup, McCarter, Durham, Young, Christman, West and Kramer2012). Greenhouses were considered random effects, while herbicides and accessions were considered fixed effects. Treatment means were separated at P ≤ 0.05 using Tukey’s honestly significant difference (HSD) adjustment.
Results and Discussion
Differential Responses to S-Metolachlor of Amaranthus palmeri from the Midsouthern United States
This research included 168 accessions covering 24, 17, and 10 counties in Arkansas (57% of accessions), Mississippi (32% of accessions), and Tennessee (11% of accessions), respectively. Out of 61 accessions from Arkansas in 2017, 3.3% were controlled less than 90%, 10% were controlled between 90% and 95%, and 87% were controlled 95% or more (Figure 2). Among 35 accessions collected in Arkansas in 2018, 23% were controlled less than 90%, 17% were controlled between 90% and 95% and 60% were controlled 95% or more. Of the 54 accessions from Mississippi in 2017, 4% were controlled less than 90%; the rest were controlled 90% or more. No accession from Tennessee was controlled less than 90%. Of the 18 Tennessee accessions evaluated, 6% were controlled between 90% and 95%. From experience, 5% to 10% escape is enough to start a cohort of resistant plants if some of these escapes carry a resistance trait (Salas et al. Reference Salas, Burgos, Tranel, Singh, Glasgow, Scott and Nichols2016).
Response of Amaranthus palmeri accessions to 1,120 g ai ha−1 S-metolachlor in the greenhouse, Milo J. Shult Agricultural Research & Extension Center (University of Arkansas, Fayetteville, AR, USA). (A) Arkansas 2017, (B) Arkansas 2018, (C) Mississippi 2017, and (D) Tennessee 2018 and 2019.
It is commonly understood that weed populations have differential tolerance to herbicides due to genetic background variation within and among populations (Radosevich et al. Reference Radosevich, Holt and Ghersa2007). The labeled rates of herbicides are set to ensure that the most-tolerant individuals, or populations of target species, are controlled 100% as consistently as possible across environments. In crop production, weed control ≥90% is considered excellent (Barber et al. Reference Barber, Butts, Boyd, Cunningham, Selden, Norsworthy, Burgos and Bertucci2021). Differential tolerance to labeled rate of herbicides has been documented among older (collected between 2008 and 2016) susceptible A. palmeri populations from Arkansas, for example, with respect to fomesafen (Salas et al. Reference Salas, Burgos, Tranel, Singh, Glasgow, Scott and Nichols2016), glufosinate (Salas-Perez et al. Reference Salas-Perez, Saski, Noorai, Srivastava, Lawton-Rauh and Nichols2018), mesotrione (Singh et al. Reference Singh, Roma-Burgos, Singh, Alcober, Salas-Perez and Shivrain2018), and ALS-inhibiting herbicides (Bond et al. Reference Bond, Oliver and Stephenson2006; Burgos et al. Reference Burgos, Kuk and Talbert2001). Significant variations in background response to herbicides were also documented among populations from Kansas with respect to glyphosate, 2,4-D, atrazine, and mesotrione (Kumar et al. Reference Kumar, Liu and Stahlman2020). In Arkansas, 34% of A. palmeri surveyed survived mesotrione applications with injury ranging from 61% to 90% (Singh et al. Reference Singh, Roma-Burgos, Singh, Alcober, Salas-Perez and Shivrain2018).
When a population starts having an increasing number of individuals surviving the labeled rate, this is an indication of evolving resistance, as was observed with A. palmeri populations resistant to PPO-inhibiting herbicides (Salas et al. Reference Salas, Burgos, Tranel, Singh, Glasgow, Scott and Nichols2016). The fact that a number of recent populations showed less than 90% control with the labeled rate of S-metolachlor indicates possible evolving resistance in those populations. The occurrence of resistance to S-metolachlor has already been confirmed in a few A. palmeri populations (Brabham et al. Reference Brabham, Norsworthy, Houston, Varanasi and Barber2019; Rangani et al. Reference Rangani, Noguera, Salas-Perez, Benedetti and Roma-Burgos2021). The current survey indicated that additional populations might have also evolved resistance to S-metolachlor.
Resistance Level to S-Metolachlor
The resistance level to S-metolachlor was evaluated for accessions that were controlled less than 88% during the large-scale test for resistance. In total, seven accessions were used for the dose–response studies: two accessions from Arkansas in 2017 (17PRA-A and 17RAN-A), three accessions from Arkansas in 2018 (18CRI-D, 18PHI-C, and 18WOO-B), and two accessions from Mississippi in 2017 (17TUN-A and 17TUN-D). The LD50 values (e) ranged between 73 and 443 g ha−1 for field populations of all seven accessions evaluated. The SS required 63 ± 16 g ha−1, while resistant accessions required 443 ± 36, 289 ± 12, 156 ± 16, 140 ± 11, 73 ± 21, 313 ± 54, and 242 ± 32 g ha−1 to reduce seedling emergence 50% for 18WOO-B, 18CRI-D, 17PRA-A, 17RAN-A, 18PHI-C, 17TUN-A, and 17TUN-D, respectively (Table 4; Figure 3; Supplemental Figure 1). The levels of resistance of 18WOO-B, 18CRI-D, 17RAN-A, 17PRA-A, 18PHI-C, 17TUN-A, and 17TUN-D to S-metolachlor were 7.0-, 4.6-, 2.2-, 2.5-, 1.2-, 5.0-, and 3.8-fold, respectively. Accession 18PHI-C was susceptible, while the rest were resistant to S-metolachlor. This survey confirmed resistance to S-metolachlor in four counties in Arkansas (Randolph, Prairie, Crittenden, Woodruff) and one county in Mississippi (Tunica). Brabham et al. (Reference Brabham, Norsworthy, Houston, Varanasi and Barber2019) had also reported two resistant populations from Marion and Crawfordsville (Crittenden County), while Rangani et al. (Reference Rangani, Noguera, Salas-Perez, Benedetti and Roma-Burgos2021) reported resistant populations in Crittenden, Woodruff, and Mississippi counties in 2014 and 2015. Resistant accessions reported by Brabham et al. (Reference Brabham, Norsworthy, Houston, Varanasi and Barber2019) required 156 and 133 g ai ha−1 S-metolachlor to attain 50% control and were 9.8 and 8.3 times less responsive to S-metolachlor than the susceptible standards. In a previous study, the LD50 values of resistant accessions were between 88 and 785 g ai ha−1 (Rangani et al. Reference Rangani, Noguera, Salas-Perez, Benedetti and Roma-Burgos2021), which equated to resistance levels between 3- and 29-fold. Results from this research documented, for the first time, S-metolachlor resistance in accessions collected from two crop fields in Tunica County, MS, USA. The dose–response studies produced survivors at a 2× rate of S-metolachlor. Should these types of individuals be allowed to produce seeds in the field owing to insufficient supplemental control measures, failure of the herbicide would be expected in a few years.
Resistance levels of A. palmeri populations to S-metolachlor in greenhouse experiments conducted at the Milo J. Shult Agricultural Research & Extension Center, University of Arkansas, Fayetteville, AR, USA.
a LD50, S-metolachlor rate that reduced seedling emergence by 50%. Values in parenthesis are standard errors of the mean.
b R/S, resistance index, ratio between the LD50 value of the S-metolachlor–resistant accessions and the LD50 value of the susceptible accession.
Dose–response studies of parental Amaranthus palmeri accessions collected in Arkansas (in 2018) and F1 progeny obtained in the greenhouse at the Milo J. Shult Agricultural Research & Extension Center (University of Arkansas, Fayetteville, AR, USA). Data were fit using a three-parameter log-logistic equation. Error bars represent A. palmeri % survival– associated standard errors.
Resistance Progression in the Progeny
The progeny of surviving plants from 18WOO-B (18WOO-B-F1) had the highest level of resistance to S-metolachlor at 9.2-fold compared with the SS (Figure 3), requiring 577 ± 52 g ha−1 of the herbicide to reduce seedling emergence 50%. The second F1 progeny (18PHI-C-F1) was only 2-fold resistant compared with SS. Therefore, the progression in resistance level from one cycle to the next is not always large. This most likely depends on the frequency and vigor of resistant plants in the field population. Vigorous resistant plants will produce more seed, and their seed will compose a large fraction of F1 seed, resulting in an increase in the resistance level of the F1 generation (Radosevich et al. Reference Radosevich, Holt and Ghersa2007). Accessions 19CRI-D and 19WOO-B required 327 ± 47 and 520 ± 64 g ha−1 to reduce seedling emergence 50%. Based on LD50 values, these populations were 5 and 8 times less sensitive to S-metolachlor compared with the SS (Figure 4). In both cases, the resistance level of the field population in the second year of sampling was the same as that of the same field in the first year. This indicates that whereas resistance level increases significantly after one cycle of “purification” in the greenhouse, the resistance progression could be slower in the field. One reason for this is the supplemental weed management measures done across seasons in the field. Accession 19PHI-C required 73 ± 19 g ha−1 to reduce seedling emergence 50% and was as sensitive as the SS.
Dose–response studies of parental Amaranthus palmeri accessions collected in Arkansas (in 2018) and accessions collected from the same fields in 2019: PHI-C (A), CRI-D (B), and WOOB-B (C). The test was conducted in the greenhouse at the Milo J. Shult Agricultural Research & Extension Center (University of Arkansas, Fayetteville, AR, USA). Data were fit using a three-parameter log-logistic equation. Error bars represent A. palmeri % survival–associated standard errors.
Resistance to VLCFA-inhibiting herbicides evolved more slowly compared with herbicides that target other sites of action (Heap Reference Heap2021), despite the extensive use of VLCFA-inhibiting herbicides in numerous crops and millions of hectares for decades. Several factors may explain the slower evolution of weed resistance to VLCFA-inhibiting herbicides, including the infrequent mutations in the condensing enzyme (Boger et al. Reference Boger, Matthes and Schmalfuss2000; Busi Reference Busi2014); the requirement of highly improbable simultaneous changes in several different targets to deliver resistance to VLCFA-inhibiting herbicides due to the interaction of these herbicides with multiple targets (Busi Reference Busi2014; Tanetani et al. Reference Tanetani, Kaku, Kawai, Fujioka and Shimizu2009; Trenkamp et al. Reference Trenkamp, Martin and Tietjen2004); and the low proportion of survivors of these herbicides that grow to maturity and produce seeds because of postemergence applications of herbicides with different modes of action (Busi Reference Busi2014). However, the occurrence of resistance to VLCFA-inhibiting herbicides has been increasing in recent years with five grasses: rigid ryegrass (Lolium rigidum Gaudin) (Busi et al. Reference Busi, Porri, Gaines and Powles2018), Italian ryegrass [Lolium perenne L. ssp. multiflorum (Lam.) Husnot] (Ducker et al. Reference Ducker, Zollner, Lummen, Ries, Collavo and Beffa2019a), slender meadow foxtail (Alopecurus myosuroides Huds.) (Ducker et al. Reference Ducker, Zollner, Parcharidou, Ries, Lorentz and Beffa2019b), barnyardgrass [Echinochloa crus-galli (L.) P. Beauv.] (Juliano et al. Reference Juliano, Casimero and Llewellyn2010), wild oat (Avena fatua L.) (Heap Reference Heap2021); and some broadleaf species, including wild radish (Raphanus raphanistrum L.) (Heap Reference Heap2021), waterhemp [Amaranthus tuberculatus (Moq.) Sauer], and A. palmeri] (Brabham et al. Reference Brabham, Norsworthy, Houston, Varanasi and Barber2019; Rangani et al. Reference Rangani, Noguera, Salas-Perez, Benedetti and Roma-Burgos2021; Strom et al. Reference Strom, Hager, Seiter, Davis and Riechers2020) reported to date.
Efficacy of Other Soil-applied Herbicides on Amaranthus palmeri Resistant to S-Metolachlor
Four S-metolachlor–resistant accessions (18CRI-D, 18WOO-B, 17TUN-A, and 17TUN-D) were evaluated. The three-way greenhouse-by-accession-by-herbicide interaction was not significant at 14 and 21 (P > 0.05) DAT. The two-way greenhouse-by-accession, greenhouse-by-herbicide, and accession-by-herbicide interactions were not significant at 14 and 21 DAT (P > 0.05) (Table 5). At full labeled rates, all soil-applied herbicides tested provided excellent control of S-metolachlor–resistant A. palmeri (≥ 90%), except for fomesafen, which had 89% control of 18WOO-B (Table 6). This level of control cannot be classified as resistant, but it is possible that resistance to soil-applied fomesafen is evolving in this population, just as had been discovered previously by Salas et al. (Reference Salas, Burgos, Tranel, Singh, Glasgow, Scott and Nichols2016) in other populations. The efficacy of soil-applied herbicides tested on the S-metolachlor–resistant accessions was the same as that on the SS. These results are consistent with previous research (Brabham et al. Reference Brabham, Norsworthy, Houston, Varanasi and Barber2019; Gonzalez-Torralva et al. Reference Gonzalez-Torralva, Norsworthy, Piveta, Varanasi, Barber and Brabham2020; Umphres et al. Reference Umphres, Steckel and Mueller2018). All five herbicides are viable options for the control of S-metolachlor–resistant A. palmeri, with a caveat that survivors of preemergence herbicides be controlled with follow-up herbicide applications and cultural management operations. Cross-resistance to other VLCFA inhibitors is possible. Brabham et al. (Reference Brabham, Norsworthy, Houston, Varanasi and Barber2019) reported reduced sensitivity of S-metolachlor–resistant accessions to dimethenamid-P, although the survivors were severely stunted at 0.25× the rate of dimethenamid-P. Still, the S-metolachlor–susceptible accessions were killed 100% at this rate of dimethenamid-P. All accessions were susceptible to other VLCFA inhibitors, but the reduced sensitivity to another herbicide in this MOA group, reported by Brabham et al. (Reference Brabham, Norsworthy, Houston, Varanasi and Barber2019) is noteworthy for planning resistance mitigation measures.
The F- and P-values for Amaranthus palmeri control (%) at 21 d after herbicide application (DAT) in a greenhouse experiment in Fayetteville, AR, USA.
Efficacy of other soil-applied herbicides on S-metolachlor–resistant Amaranthus palmeri accessions from Arkansas and Mississippi, USA.
a Pooled over two runs.
b Herbicide means within a column followed by the same letter are not significantly different based on Tukey’s honestly significant difference (HSD) test at α = 0.05.
c Accession means are not different based on Tukey’s HSD test at α = 0.05; the interaction effect between herbicide and accession was not significant.
In a larger survey of A. palmeri populations, atrazine remains an effective option for most A. palmeri accessions from Arkansas (Gonzalez-Torralva et al. Reference Gonzalez-Torralva, Norsworthy, Piveta, Varanasi, Barber and Brabham2020), likely aided by the small acreage of corn and grain sorghum produced in the state. Increasing the frequency of corn and grain sorghum in crop rotations would be a good strategy for delaying S-metolachlor resistance evolution in the midsouthern United States.
Umphres et al. (Reference Umphres, Steckel and Mueller2018) reported more than 90% control of A. palmeri by flumioxazin in a greenhouse study in Tennessee. Fomesafen and flumioxazin have both foliar and soil activity, but the former is primarily used as a postemergence herbicide (Senseman Reference Senseman2007), while the latter is primarily used as a preemergence herbicide (Senseman Reference Senseman2007; Umphres et al. Reference Umphres, Steckel and Mueller2018). In Arkansas, A. palmeri resistance to PPO-inhibiting herbicides has been documented in all major row crop–producing counties (Butts et al. Reference Butts, Barber and Norsworthy2019; Salas et al. Reference Salas, Burgos, Tranel, Singh, Glasgow, Scott and Nichols2016; Varanasi et al. Reference Varanasi, Brabham, Norsworthy, Nie, Young, Houston, Barber and Scott2018b). A foliar application of fomesafen to a fomesafen-resistant accession resulted in 55% survival (Varanasi et al. Reference Varanasi, Brabham and Norsworthy2018a), and 16% of 227 accessions collected throughout Arkansas had mortality ratings <90% (Varanasi et al. Reference Varanasi, Brabham, Norsworthy, Nie, Young, Houston, Barber and Scott2018b). Given the prevalence of A. palmeri resistance to PPO inhibitors in the U.S. Midsouth (Noguera et al. Reference Noguera, Rangani, Heiser, Bararpour, Steckel, Betz, Porri, Lerchl, Zimmermann, Nichols and Roma-Burgos2021), it can be assumed that some of these S-metolachlor–resistant populations are also resistant to PPO-inhibiting herbicides. However, resistance to foliar-applied fomesafen does not necessarily translate to loss of efficacy when it is applied preemergence. In the present study, flumioxazin applied preemergence provided >90% control of all accessions. Multiple factors could contribute to obtaining excellent control with soil-applied PPO herbicides, even if such accessions were resistant to foliar-applied PPO herbicides. Germinating seedlings have weak protective barriers (cuticular waxes) compared with seedlings used in foliar tests. Germinating seedlings are expected to absorb and accumulate more herbicide. Because seedlings do not have fully functional or sufficient level of protection mechanisms, it would take less herbicide to kill germinating seeds than fully developed (i.e., 4-leaf) seedlings.
Because A. palmeri resistance evolution to S-metolachlor is recent in the midsouthern United States, adoption of best management practices is critical for slowing the spread of resistance evolution. Adopting an integrated weed management program that involves the use of cultural and mechanical methods (Norsworthy et al. Reference Norsworthy, Ward, Shaw, Llewellyn, Nichols, Webster, Bradley, Frisvold, Powles, Burgos, Witt and Barrett2012), herbicide tank mixtures, sequential herbicide applications (preemergence followed by postemergence), and rotation of herbicides and crop traits will be beneficial for controlling S-metolachlor–resistant A. palmeri populations. For example, growing corn or grain sorghum in rotation with soybean/cotton will allow the use of atrazine, which continues to control S-metolachlor–resistant A. palmeri populations from the U.S. Midsouth. Because S-metolachlor resistance reported in Arkansas is metabolism based (Rangani et al. Reference Rangani, Noguera, Salas-Perez, Benedetti and Roma-Burgos2021), the addition of glutathione S-transferase inhibitors may help reverse resistance in these populations, a potential strategy to delay S-metolachlor resistance in A. palmeri. However, research is needed to validate this theory.
This research has documented resistance of A. palmeri to S-metolachlor in four counties in Arkansas and in one county in Mississippi. This evolving resistance is expected to increase weed management problems. The majority of populations in the U.S. Midsouth are currently susceptible to S-metolachlor, and the resistant ones exhibit resistance levels up to 7-fold. The level and frequency of resistance generally increased from parents to the first generation of progeny. The resistant populations reported here are not cross-resistant to other VLFCA inhibitors tested (dimethenamid-P and pyroxasulfone). These populations can also be controlled with soil-applied Group 14 herbicides tested here (flumioxazin and fomesafen) and atrazine. For now, there are effective herbicide options to manage S-metolachlor–resistant A. palmeri in various crops that could be grown in rotation.
Supplementary material
To view supplementary material for this article, please visit https://doi.org/10.1017/wsc.2022.37
Acknowledgments
Support for this research was provided by Arkansas soybean producers through check-off funds administered by the Arkansas Soybean Promotion Board and the Southern Integrated Pest Management Center. The authors thank the University of Arkansas System Division of Agriculture for all other personnel support and facilities. The following county Extension agents assisted in contacting growers, finding fields to sample, and in some cases, collecting seed samples: Stanley Baker, Ray Benson, Robert Goodson, Brett Gordon, Cody Griffin, Steven Kelley, Kevin Lawson, Russell Parker, Keith Perkins, Phil Sims, Jesse Taylor, and Jan Yingling. The authors also thank Matthew Janorschke, Diego Belapart, Nelson Diehl Kruse, Pâmela Carvalho-Moore, and Isabel Schlegel Werle for their help in planting and spraying the plants. The 2017 germplasm was maintained by Matheus Noguera and was part of a U.S. Midsouth project funded by Cotton Inc.
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