International Journal of Agronomy

International Journal of Agronomy / 2012 / Article

Research Article | Open Access

Volume 2012 |Article ID 305764 |

Chance W. Riggins, Patrick J. Tranel, "Will the Amaranthus tuberculatus Resistance Mechanism to PPO-Inhibiting Herbicides Evolve in Other Amaranthus Species?", International Journal of Agronomy, vol. 2012, Article ID 305764, 7 pages, 2012.

Will the Amaranthus tuberculatus Resistance Mechanism to PPO-Inhibiting Herbicides Evolve in Other Amaranthus Species?

Academic Editor: Robert J. Kremer
Received15 Sep 2011
Accepted10 Jan 2012
Published15 Mar 2012


Resistance to herbicides that inhibit protoporphyrinogen oxidase (PPO) has been slow to evolve and, to date, is confirmed for only four weed species. Two of these species are members of the genus Amaranthus L. Previous research has demonstrated that PPO-inhibitor resistance in A. tuberculatus (Moq.) Sauer, the first weed to have evolved this type of resistance, involves a unique codon deletion in the PPX2 gene. Our hypothesis is that A. tuberculatus may have been predisposed to evolving this resistance mechanism due to the presence of a repetitive motif at the mutation site and that lack of this motif in other amaranth species is why PPO-inhibitor resistance has not become more common despite strong herbicide selection pressure. Here we investigate inter- and intraspecific variability of the PPX2 gene—specifically exon 9, which includes the mutation site—in ten amaranth species via sequencing and a PCR-RFLP assay. Few polymorphisms were observed in this region of the gene, and intraspecific variation was observed only in A. quitensis. However, sequencing revealed two distinct repeat patterns encompassing the mutation site. Most notably, A. palmeri S. Watson possesses the same repetitive motif found in A. tuberculatus. We thus predict that A. palmeri will evolve resistance to PPO inhibitors via the same PPX2 codon deletion that evolved in A. tuberculatus.

1. Introduction

Herbicides that inhibit protoporphyrinogen oxidase (PPO) have been used for many years for control of broadleaf weeds in large-scale crop production systems in the United States. Their use began to slowly decline during the late 1990s due to the introduction and subsequent widespread adoption of glyphosate-resistant crop varieties, such as Roundup Ready soybean, corn, and cotton. Glyphosate-resistant crops currently dominate throughout much of the United States and elsewhere in the world, and these systems rely almost exclusively on glyphosate as the sole means for weed management [1]. Unfortunately, the continuous broad-scale use of glyphosate over time has triggered the evolution of glyphosate-resistant biotypes among an increasing diversity of weed species [2]. In many cases, these glyphosate-resistant biotypes have been selected from weed populations that already had resistance to one or more other herbicide families, such as ALS inhibitors, triazines, and, less frequently, PPO inhibitors. As glyphosate resistance continues to increase in frequency, distribution, and the number of species [2], growers are once again relying on PPO-inhibiting herbicides as an alternative approach to control weeds.

The enzyme protoporphyrinogen oxidase (EC is one of the most important targets for herbicide development [3, 4]. PPO is the last common enzyme in the tetrapyrrole biosynthesis pathway and is responsible for converting protoporphyrinogen IX (Protogen) to protoporphyrin IX (Proto). In plants, two isoforms of the PPO enzyme are encoded by two different nuclear genes, PPX1 and PPX2. These two enzymes share little sequence identity and are functionally compartmentalized, with PPX1 being targeted to plastids and PPX2 targeted to the mitochondria. Inhibition of PPO disrupts the synthesis of chlorophylls and hemes, which results in the damaging photodynamic effect characteristic of PPO inhibiting herbicides [3].

Natural resistance to PPO-inhibitors has been slow to evolve [3, 5], yet it has been confirmed in four weed species [2]. The first weed to evolve resistance to PPO herbicides was Amaranthus tuberculatus (Moq.) Sauer (waterhemp) in 2000 [6]. PPO resistance has subsequently been confirmed in Euphorbia heterophylla L. (wild poinsettia) and Amaranthus quitensis Kunth, both from South America, and Ambrosia artemisiifolia L. (common ragweed). The mechanism of PPO-inhibitor resistance, a unique target-site amino acid deletion, was first elucidated in a biotype of A. tuberculatus from Illinois [7]. This mechanism involves the loss of a glycine at position 210 in the mitochondrial isoform of the PPO enzyme. Loss of this amino acid is considered to have occurred via a slippage-like mechanism within a trinucleotide repeat of the PPX2 gene [7, 8]. Specifically, the sequence motif spanning position 210 (i.e., …TGTGGTGGA…) contains both a GTG and a TGG bi-repeat. Loss of either one of these repeat elements results in a loss of a glycine codon (GGT) without affecting the reading frame. This glycine deletion alters the binding domain of the enzyme without negatively affecting substrate affinity, and thus overall sensitivity to PPO-inhibiting herbicides is reduced by at least 100-fold [3]. The presence of a short repetitive motif at the mutation site, together with the favorable biochemical consequences of the deletion, seems to have predisposed A. tuberculatus to evolving this unique resistance mechanism, which thus far is the only identified mechanism of evolved PPO-inhibitor resistance. Despite being an unusual mutation, it is found commonly in A. tuberculatus populations across the Midwestern United States [911]. Assuming a slippage mechanism is responsible for evolved PPO resistance in A. tuberculatus, the question arises whether other weedy amaranth species possess the same sequence repeat and thus are also predisposed to acquiring this mutation.

It is unknown how conserved the PPX2 gene is among weed species or whether other weedy members of the genus Amaranthus, such as A. hybridus L., A. retroflexus L., A. powellii S. Watson, and most notably Palmer amaranth (A. palmeri S. Watson), share the same repeat motif as in A. tuberculatus. These species are aggressive and pernicious weeds in their own right and have evolved resistances to multiple herbicides [2], though as of yet not to PPO inhibitors. However, there is growing concern that over-reliance on the PPO herbicides for controlling glyphosate-resistant A. palmeri in Roundup Ready crops (soybean, cotton, and corn) in the Southeastern United States will promote PPO resistance in this species [12]. In addition to glyphosate, populations of A. palmeri have evolved resistance to ALS inhibitors, dinitroanilines, and triazines [2, 13, 14], so the threat of a multiple-resistant individual or population is real and will be much more difficult to control once PPO resistance occurs in this species.

In this paper, we investigate inter- and intraspecific variability of the PPX2 gene among weedy amaranths with conventional PCR and sequencing methods in conjunction with a newly developed PCR-RFLP (restriction fragment length polymorphism) assay. Our primary objective was to determine if the repeat motif encompassing Gly210 of PPX2 from A. tuberculatus is shared among other weedy amaranth species. A second objective was to obtain baseline sequence information for future genetic and molecular studies of evolved PPO-inhibitor resistance in weedy amaranths.

2. Materials and Methods

Plant species and populations sampled for this study are listed in Table 1. Genomic DNA of some accessions utilized in this study was previously isolated for analysis of genetic similarity [15] and herbicide target-site genes [16, 17]. Source material for additional Amaranthus accessions was obtained either from herbarium specimens (for A. acanthochiton Sauer and A. caudatus L.) or from germplasm collections of the authors. In the case of A. quitensis, seed was obtained from the North Central Regional Plant Introduction Station (NCRPIS) in Ames, Iowa, and represented semi domesticated types from the Pacific side of South America and field weeds collected from Brazil. Seeds were initially sown in containers with 3 : 1 : 1 : 1 mixture of commercial potting mix to soil to peat to sand. When seedlings exhibited true leaves, the plants were thinned and transplanted into new containers of the same size to ensure ample material for DNA extractions. Plants were fertilized as necessary with slow-release fertilizer and grown under mercury halide and sodium vapor lamps along with incident sunlight. Lamps were programmed for a 16-hour photoperiod and the temperature maintained at 22 C at night and 28 C daytime. Leaf material for DNA extraction was harvested from one individual mature plant per accession and flash frozen in liquid nitrogen prior to DNA extraction using the modified CTAB method [18].

SpeciesAccession no. Location information PCR-RFLP result

A. acanthochiton Sauer398443New Mexico, USAUncleaved
A. albus L.MH36Washington, USAUncleaved
(Tumble pigweed)MH38Mississippi, USAUncleaved
PT70Illinois, USAUncleaved
A. caudatus L.CAUBoliviaCleaved
A. hybridus L.MH154North Carolina, USACleaved
(Smooth pigweed)PT12Illinois, USACleaved
MH165Ohio, USACleaved
A. palmeri S. WatsonAlex 1Illinois, USAUncleaved
(Palmer amaranth)Alex 2Illinois, USAUncleaved
S1 unionIllinois, USAUncleaved
S1 pulIllinois, USAUncleaved
Mass 1Illinois, USAUncleaved
GA-5Georgia, USAUncleaved
GA-7Georgia, USAUncleaved
GA-8Georgia, USAUncleaved
GA-10Georgia, USAUncleaved
MH253New Mexico, USAUncleaved
MH247California, USAUncleaved
MH254Texas, USAUncleaved
A. powellii S. WatsonMH234Washington, USACleaved
(Powell’s amaranth)MH237New York, USACleaved
MH242Ontario, CanadaCleaved
A. quitensis Kunth511736BoliviaCleaved
568154Tarija, BoliviaCleaved
652421Goias, BrazilCleaved
652423Goias, BrazilCleaved
652426Federal District, BrazilCleaved
652429Federal District, BrazilCleaved
652430Federal District, BrazilCleaved
A. retroflexus L.MH84New Mexico, USACleaved
(Redroot pigweed)PT25Illinois, USACleaved
PT67Illinois, USACleaved
A. spinosus L.MH267Puerto RicoUncleaved
(Spiny amaranth)MH203Texas, USAUncleaved
MH205Louisiana, USAUncleaved
A. tuberculatus (Moq.) SauerPT43Illinois, USAUncleaved
(Waterhemp)ACRAdams Co., IL, USAUncleaved
WCSWayne Co., IL, USAUncleaved
MH320Ohio, USAUncleaved
MO-aMissouri, USAUncleaved
MO-bMissouri, USAUncleaved
MO-cMissouri, USAUncleaved
MO-1Missouri, USAUncleaved

PCR amplifications were performed using MJ Research thermal cyclers in 25 μL volumes with 1x buffer (GoTaq Flexi Buffer, Promega Corp., Madison, WI, USA), 2.5 mM MgCl2, 200 μM dNTPs, 0.4 μM each primer, 1.0 μL total genomic DNA (10–50 ng), and 1.25 units of GoTaq polymerase. Parameters for PCR featured an initial denaturation of 95 C for 2 min, followed by 37 cycles (95 C for 45 sec, 55 C for 30 sec, and 72 C for 90 sec) and a final extension of 72 C for 5 min. Three primer sets were used for amplifications of the exon 9 region of PPX2. Since genomic PPX2 information with intron sizes and sequence identity was limited, we initially used the primer set ARMS7-F (5′-TCTGATGAGCATGTTCAGGAAAGGCAAG) and PPX2ex10-R (5′-CTGGAAATGTATGGTGCATC) to amplify a large fragment (~1200 bp) between exons 7 and 10 for all species. Following sequence comparisons to identify conserved motifs in the introns adjacent to exon 9, the primer sets PPX2int8-F1 (5′-CAACTTGCCATGCTCTATTCC) and PPX2int9-R1 (5′-ATGGCGAAATGAGTTAAGGTTC), or PPX2int8-F2 (5′-ATTGCCATGCTCTATTCATTCC) and PPX2int9-R2 (5′-CGCCTATTCAAATCAAAT GTCC), were used to amplify smaller fragments of ~500 bp and ~400 bp, respectively. PCR products were visualized on a 1% agarose gel containing 0.5 μg mL−1 ethidium bromide and cleaned using an E.Z.N.A. Cycle-Pure Kit (Omega Bio-Tek, Inc., Norcross, GA, USA) following the manufacturer’s instructions. Purified PCR products were directly sequenced using an ABI Prism BigDye Terminator Kit v3.1 (Applied Biosystems, Foster City, CA, USA), and run on an ABI 3730XL capillary sequencer at the W. M. Keck Center for Comparative and Functional Genomics at the University of Illinois. Sequencing reactions were prepared in 13–16 μL volumes and contained 1.8 μL ddH2O, 5.2 μL 12.5% glycerol, 2.0 μL 5x sequencing buffer, 2.0 μL 10 μM primer, 1.0 μL BigDye Terminator v3.1, and 1.0–4.0 μL PCR product. Cycle sequencing conditions started at 96 C for 1 min, followed by 30 cycles of (96 C for 30 sec, 50 C for 15 sec, 60 C for 4 min) and final extension of 60 C for 4 min. Forward and reverse sequences were manually edited and assembled into contiguous sequences (contigs) using the Alignment Explorer in MEGA5 [19]. Alignment of coding regions and exon-intron boundaries were determined by comparison with published genomic and cDNA PPX2 sequences of A. tuberculatus (DQ394875, DQ394876, DQ386113, DQ386114, DQ386116, DQ386117, DQ386118) and A. hypochondriacus L. (EU024569) from GenBank.

Comparative sequence alignments of exon 9 of the PPX2 gene showed nucleotide variations at the Gly210 mutation site. To facilitate the screening of additional accessions of each species for variation at this site, a PCR-RFLP assay was developed using the restriction enzyme EciI (New England Biolabs Inc., USA). Amplified products from all primers sets were digested and analyzed for fragment patterns. Following PCR, 10 μL of each reaction was added to 10 μL of a digestion mixture and incubated at 37 C for 1.5 hrs. The digestion mixture contained EciI (1 unit μL−1) and 1x concentrations of the supplied buffer (NEB2) and BSA. After digestion, the fragments were separated on a 1% agarose gel and visualized under UV with ethidium bromide staining. PCR amplifications and digestions for each sample were replicated at least twice to validate the assay.

3. Results and Discussion

Sequence comparisons between a PPO-inhibitor-sensitive biotype (i.e., wild-type) of A. tuberculatus (GenBank accession DQ394875) and A. hypochondriacus (GenBank accession EU024569) revealed the presence of a single-nucleotide polymorphism (SNP) in the third position of the Gly210 codon in exon 9 of the genomic PPX2 gene. Although this SNP is a synonymous substitution, its position is significant in being part of a codon that, when deleted, confers resistance to PPO-inhibiting herbicides in A. tuberculatus [7]. In biotypes of A. tuberculatus, the thymine present at this site creates a bi-GTG or bi-TGG nucleotide repeat that spans the Gly210 codon. In the nucleotide sequence of A. hypochondriacus, a cytosine rather than a thymine is present, so no repeat motifs are formed. Repetitive sequences are thought to be more prone to slippage during replication, and it would not matter in this case if the deleted triplet was a TGG or a GTG since the reading frame is maintained in both instances [8]. Moreover, the resultant loss of a glycine at this position imparts herbicide resistance without adversely affecting the normal functions of the PPO enzyme [3].

The initial PCR experiments tested for cross-species amplification of the PPX2 gene using primers based on sequence data from A. tuberculatus. The primers ARMS7-F and PPX2ex10-R produced a single product of approximately 1200 bp in the five amaranth species tested (Figure 1(a)). The amplified products for each species were fairly uniform in size with only minor differences in length being attributable to short indel (insertion/deletion) mutations located in the introns. Digestion of these PCR products with the restriction enzyme EciI produced two smaller fragments of approximately 500 and 580 bp in A. hybridus, A. retroflexus, and A. powellii, but no fragments in the multiple accessions of A. tuberculatus and A. palmeri (Figure 1(b)). Sequencing these PCR products confirmed the digestion patterns by showing that both accessions of A. palmeri had the same repeat motif as A. tuberculatus and thus lacked the restriction site. Conversely, a single restriction site was present in the sequences of the three other species since they possessed a cytosine substitution similar to A. hypochondriacus rather than a thymine as in A. tuberculatus and A. palmeri. The uncut bands observed for A. hybridus, A. retroflexus, and A. powellii in Figure 1(b) were determined to be the result of incomplete digestion rather than heterozygosity as their intensity decreased, but was not completely eliminated, through additional digestion experiments with different enzyme and template concentrations and longer incubation times. Sequencing evidence also confirmed that none of these accessions were heterozygous for the CT polymorphism. Subsequent PCR experiments using the primers ARMS7-F and PPX2ex10-R produced single bands of ~1200 bp in A. albus L., A. quitensis, and A. spinosus L., which again suggested that this portion of the gene is relatively conserved across amaranth species. Digestion with EciI produced cleaved products only for the accessions of A. quitensis (data not shown).

Based on sequence data from the first series of experiments, two additional primer sets were designed that are positioned in relatively conserved regions of the introns immediately flanking exon 9 (Figure 2(a)). The first primer set, PPX2int8-F1 and PPX2int9-R1, worked well for amplifying and sequencing exon 9 in all species except some accessions of A. tuberculatus. In this case, the modified primers PPX2int8-F2 and PPX2int9-R2 were successfully used. PCR experiments with both primer sets resulted in single amplified products of the expected size (~500 bp) in all accessions tested (data not shown). Results of the digestion analyses conducted with the different primer sets were in complete agreement with one another and with the sequencing evidence for every accession tested (Table 1). No infraspecific variation was observed in the PCR-RFLP fragment patterns for any species, although infraspecific variation was detected in A. quitensis after sequencing four randomly chosen accessions. In accession 511751 of this species, sampled from a Peruvian population, a silent T→C nucleotide mutation was observed in the codon immediately preceding Gly210, which in effect produced a bi-CGG sequence repeat spanning the resistance mutation site (Figure 2(b)). The position of this polymorphism has not been directly implicated in resistance to PPO herbicides, but it does open the possibility for an alternative repeat motif that could lead to the same Gly210 mutation.

Sequence comparisons among the remaining accessions, including wild-type and confirmed PPO-resistant A. tuberculatus (i.e., biotypes without and with the deletion mutation), revealed six additional SNPs in exon 9, but only one resulted in a nonsynonymous substitution (Figure 2(b)). This substitution occurred at position 47 in the sequence of A. acanthochiton (a dioecious species) and resulted in an inferred change of glycine to valine (amino acid position 211). Only one accession sequenced appeared heterozygous, and this too was from a sample of a dioecious species (i.e., A. palmeri Mass1). This polymorphism was in the third position of codon 215 (serine) and thus did not result in an amino acid change. These observations are not surprising as dioecious species are obligately outcrossing and thus expected to have higher levels of sequence polymorphisms compared to the primarily self-pollinated monoecious species [20, 21]. Nonetheless, additional sampling of these widespread and ecologically diverse species is needed to determine the extent of sequence variability present in natural populations.

Although the experimental results were not in conflict with one another, it is important to point out some limitations of the PCR-RFLP assay. This test cannot be used to screen plants for the same target-site deletion mutation responsible for PPO-inhibitor resistance in A. tuberculatus. For example, PCR-amplified products for both the wild-type and PPO-resistant biotypes of A. tuberculatus were uncut by EciI. However, mutated alleles can be detected using an allele-specific PCR method [9]. This allele-specific marker should theoretically work in other amaranth species (e.g., Palmer amaranth) that have the same repeat motif and, of course, the same deletion mechanism as operative in A. tuberculatus. On the other hand, supposing a similar codon deletion mutation occurred at the Gly210 site in an aberrant biotype of Amaranthus that normally possesses a cytosine SNP in the wild-type (A. quitensis, for example), then the PCR-RFLP test would be able to distinguish between the mutated and non-mutated alleles. There is a risk, however, of generating false positives or negatives due to other mutations within the EciI recognition site. Furthermore, the likelihood of mutations occurring outside the recognition site and endowing resistance must also be considered [22]. Even with these caveats, the PCR-RFLP assay is one more molecular tool that can be used in conjunction with other molecular markers to monitor the evolution of PPO-inhibitor resistance in weedy amaranths.

4. Conclusions

Even though resistance to PPO-inhibiting herbicides has been slow to evolve, it may be expected to occur in weedy species with large populations that are under strong and continuous selection pressure [23]. Inherently high levels of genetic variation also help to increase the likelihood that mutated alleles conferring resistance will be selected under strong herbicide pressure. Although PPX2 variability was relatively low among the ten species investigated in this study, the results do show that two groups can be recognized: species with and species without a repeat motif. It is noteworthy that the PPX2 gene of Palmer amaranth shared the same repeat motif as waterhemp, which suggests that Palmer amaranth will evolve resistance to PPO inhibitors via the Gly210 deletion mutation. Of course, the possibility of Palmer amaranth evolving another resistance mechanism (e.g., a different target-site mutation or a non-target-site mechanism) cannot be ruled out. In fact, preliminary evidence for a different target-site mutation in the PPX2 gene of common ragweed was recently reported [24]. The occurrence of a second repeat pattern in A. quitensis is also noteworthy, especially since this species is one of the four known with PPO-inhibitor resistance. Further studies with resistant and sensitive biotypes of this species will be useful in linking sequence patterns with the likelihood of evolving PPO-inhibitor resistance. Finally, the information provided in this study will facilitate the use and further development of molecular markers for screening amaranth populations suspected of PPO-inhibitor resistance for target-site-based mechanisms.


  1. R. G. Wilson, B. G. Young, J. L. Matthews et al., “Benchmark study on glyphosate-resistant cropping systems in the United States—part 4: weed management practices and effects on weed populations and soil seedbanks,” Pest Management Science, vol. 67, no. 7, pp. 771–780, 2011. View at: Publisher Site | Google Scholar
  2. I. Heap, “International Survey of Herbicide Resistant Weeds,” 2011, View at: Google Scholar
  3. F. E. Dayan, P. R. Daga, S. O. Duke, R. M. Lee, P. J. Tranel, and R. J. Doerksen, “Biochemical and structural consequences of a glycine deletion in the α-8 helix of protoporphyrinogen oxidase,” Biochimica et Biophysica Acta, vol. 1804, no. 7, pp. 1548–1556, 2010. View at: Publisher Site | Google Scholar
  4. K. Grossmann, J. Hutzler, G. Caspar, J. Kwiatkowski, and C. L. Brommer, “Saflufenacil (Kixor): biokinetic properties and mechanism of selectivity of a new protoporphyrinogen ix oxidase inhibiting herbicide,” Weed Science, vol. 59, no. 3, pp. 290–298, 2011. View at: Publisher Site | Google Scholar
  5. S. B. Powles and Q. Yu, “Evolution in action: plants resistant to herbicides,” Annual Review of Plant Biology, vol. 61, pp. 317–347, 2010. View at: Publisher Site | Google Scholar
  6. D. E. Shoup, K. Al-Khatib, and D. E. Peterson, “Common waterhemp (Amaranthus rudis) resistance to protoporphyrinogen oxidase-inhibiting herbicides,” Weed Science, vol. 51, no. 2, pp. 145–150, 2003. View at: Publisher Site | Google Scholar
  7. W. L. Patzoldt, A. G. Hager, J. S. McCormick, and P. J. Tranel, “A codon deletion confers resistance to herbicides inhibiting protoporphyrinogen oxidase,” Proceedings of the National Academy of Sciences of the United States of America, vol. 103, no. 12, pp. 329–334, 2006. View at: Publisher Site | Google Scholar
  8. J. Gressel and A. A. Levy, “Agriculture: the selector of improbable mutations,” Proceedings of the National Academy of Sciences of the United States of America, vol. 103, no. 12, pp. 215–216, 2006. View at: Publisher Site | Google Scholar
  9. R. M. Lee, A. G. Hager, and P. J. Tranel, “Prevalence of a novel resistance mechanism to PPO-inhibiting herbicides in waterhemp (Amaranthus tuberculatus),” Weed Science, vol. 56, no. 3, pp. 371–375, 2008. View at: Publisher Site | Google Scholar
  10. K. A. Thinglum, C. W. Riggins, A. S. Davis, K. W. Bradley, K. Al-Khatib, and P. J. Tranel, “Wide distribution of the waterhemp (Amaranthus tuberculatus) ΔG210 PPX2 mutation, which confers resistance to PPO-inhibiting herbicides,” Weed Science, vol. 59, no. 1, pp. 22–27, 2011. View at: Publisher Site | Google Scholar
  11. P. J. Tranel, C. W. Riggins, M. S. Bell, and A. G. Hager, “Herbicide resistances in Amaranthus tuberculatus: a call for new options,” Journal of Agricultural and Food Chemistry, vol. 59, no. 11, pp. 5808–5812, 2011. View at: Publisher Site | Google Scholar
  12. L. M. Sosnoskie, J. M. Kichler, R. D. Wallace, and A. S. Culpepper, “Multiple resistance in palmer amaranth to glyphosate and pyrithiobac confirmed in Georgia,” Weed Science, vol. 59, no. 3, pp. 321–325, 2011. View at: Publisher Site | Google Scholar
  13. T. A. Gaines, D. L. Shaner, S. M. Ward, J. E. Leach, C. Preston, and P. Westra, “Mechanism of resistance of evolved glyphosate-resistant palmer amaranth (Amaranthus palmeri),” Journal of Agricultural and Food Chemistry, vol. 59, no. 11, pp. 5886–5889, 2011. View at: Publisher Site | Google Scholar
  14. P. Neve, J. K. Norsworthy, K. L. Smith, and I. A. Zelaya, “Modelling evolution and management of glyphosate resistance in Amaranthus palmeri,” Weed Research, vol. 51, no. 2, pp. 99–112, 2011. View at: Publisher Site | Google Scholar
  15. J. J. Wassom and P. J. Tranel, “Amplified fragment length polymorphism-based genetic relationships among weedy Amaranthus species,” Journal of Heredity, vol. 96, no. 4, pp. 410–416, 2005. View at: Publisher Site | Google Scholar
  16. R. M. Lee, J. Thimmapuram, K. A. Thinglum et al., “Sampling the waterhemp (Amaranthus tuberculatus) genome using pyrosequencing technology,” Weed Science, vol. 57, no. 5, pp. 463–469, 2009. View at: Publisher Site | Google Scholar
  17. C. W. Riggins, Y. Peng, C. N. Stewart, and P. J. Tranel, “Characterization of de novo transcriptome for waterhemp (Amaranthus tuberculatus) using GS-FLX 454 pyrosequencing and its application for studies of herbicide target-site genes,” Pest Management Science, vol. 66, no. 10, pp. 1042–1052, 2010. View at: Publisher Site | Google Scholar
  18. J. J. Doyle and J. L. Doyle, “Isolation of plant DNA from fresh tissue,” Focus, vol. 12, pp. 13–15, 1990. View at: Google Scholar
  19. K. Tamura, D. Peterson, N. Peterson, G. Stecher, M. Nei, and S. Kumar, “MEGA5: molecular evolutionary genetics analysis using maximum likelihood, evolutionary distance, and maximum parsimony methods,” Molecular Biology and Evolution, vol. 28, no. 10, pp. 2731–2739, 2011. View at: Publisher Site | Google Scholar
  20. M. J. Murray, “The genetics of sex determination in the family Amaranthaceae,” Genetics, vol. 25, pp. 409–431, 1940. View at: Google Scholar
  21. M. Costea, S. E. Weaver, and F. J. Tardif, “The biology of Canadian weeds. 130. Amaranthus retroflexus L., A. powellii S. Watson and A. hybridus L,” Canadian Journal of Plant Science, vol. 84, no. 2, pp. 631–668, 2004. View at: Google Scholar
  22. C. Délye, K. Boucansaud, F. Pernin, and V. Le Corre, “Variation in the gene encoding acetolactate-synthase in Lolium species and proactive detection of mutant, herbicide-resistant alleles,” Weed Research, vol. 49, no. 3, pp. 326–336, 2009. View at: Publisher Site | Google Scholar
  23. M. Jasieniuk, A. L. Brule-Babel, and I. N. Morrison, “The evolution and genetics of herbicide resistance in weeds,” Weed Science, vol. 44, pp. 176–193, 1996. View at: Google Scholar
  24. S. L. Rousonelos, J. L. Luecke, J. M. Stachler, and P. J. Tranel, “Resistance to PPO-inhibiting herbicides in common ragweed: one mechanism or many?” North Central Weed Science Society, vol. 39, abstract 65, 2010. View at: Google Scholar

Copyright © 2012 Chance W. Riggins and Patrick J. Tranel. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

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