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23 January 2020 Biodiversity, Bugs, and Barcodes: The Cicadellidae Associated with Grassland and Phytoplasmas in the Sabana de Bogotá, Colombia
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Abstract

The leafhoppers (Cicadellidae) are a diverse and cosmopolitan group of Hemiptera that feed on plants, and occasionally cause losses due to the direct damage they inflict to their hosts, or by transmission of viruses and phytoplasmas. Phytoplasmas are plant pathogenic bacteria that can adversely affect many plant families. In the Sabana de Bogotá, Colombia, several species of urban trees, potatoes, and strawberry crops are affected by phytoplasma diseases. The family Cicadellidae contains the largest number of known vectors of phytoplasmas, but in Colombia, knowledge of their biology is scarce. The objective of this work was to characterize the diversity of Cicadellidae associated with kikuyu grass Cenchrus clandestinus (Hochst. ex Chiov.) Morrone (Poaceae) in the grasslands of the Sabana de Bogotá, at an urban site of the Universidad Nacional de Colombia and a semirural site at the Universidad Militar Nueva Granada, located in Bogotá and Cajicá, Colombia, respectively. Species richness, abundance, and cicadellid dominance were compared for the 2 sampling sites, using alpha and beta diversity estimators. In total, 3,334 leafhoppers were collected, represented by subfamilies Deltocephalinae (82.3%), Cicadellinae (15.8%), Aphrodinae (1.2%), Iassinae (0.6%), Idiocerinae (0.03%), and Typhlocybinae (0.03%). Of the 15 leafhopper species present, 6 were identified to the species level. DNA barcodes were established for 12 morphotypes, including 6 species and 6 superior taxa by amplification of the COI gene. In both locations, the sampling effort was deemed insufficient. Species richness at Universidad Militar Nueva Granada was greater (n = 13) than at Universidad Nacional de Colombia (n = 10), but abundance was higher at Universidad Nacional de Colombia (n = 1,982) than at Universidad Militar Nueva Granada (n = 1,352). The 2 most abundant species were Amplicephalus funzaensis Linnavuori and Exitianus atratus Linnavuori (both Hemiptera: Cicadellidae), both recorded as vectors of phytoplasmas. Other common leafhopper species in collections were Haldorus sp. and Dalbulus sp. (both Hemiptera: Cicadellidae) and are considered possible phytoplasma vectors. Because C. clandestinus is host to several cicadellid species, it may play an important role in the epidemiology of phytoplasma transmission in the Sabana de Bogotá.

Cicadellidae is a worldwide cosmopolitan group of about 20,000 species (Dietrich 2013a). Because leafhoppers feed from the xylem, mesophyll, or phloem of their hosts they can have a significant negative impact on their host plants, reducing plant growth, producing damage by oviposition, and acting as vectors of viruses and phytoplasmas (Nielson 1968; Ammar & Nault 2002; Weintraub & Beanland 2006). The ecologic interactions of pathosystems that involve phytoplasmas, insect vectors, suitable plant hosts, and a conducive environment are very complex (Lee et al. 2000; Weintraub & Beanland 2006). In order to successfully control phytoplasmal diseases, 2 aspects should be addressed: strengthening plant defense mechanisms and a reduction in transmittal efficiency of the pathogen by the insect vectors (Weintraub & Wilson 2010).

The Sabana de Bogotá consists of a plateau located in the center of the Colombian Andes that is interspersed with urban, rural, and forested areas where plant diseases associated with phytoplasmic groups 16SrI-B and 16SrVII-A have been described. The presence of phytoplasmas has been reported in native and introduced symptomatic urban trees from these areas, such as Acacia melanoxylon R.Br. (Fabaceae), Croton spp. (Euphorbiaceae), Eugenia neomyrtifolia M. Sobral (Myrtaceae), Fraxinus uhdei (Wenz.) Lingelsh. (Oleaceae), Liquidambar styraciflua L. (Altingiaceae), Magnolia grandiflora L. (Magnoliaceae), Pittosporum undulatum Guill. (Pittosporaceae), Populus nigra L. (Salicaceae), and Quercus humboldtii Bonpl. (Fagaceae) (Perilla-Henao et al. 2012; Perilla-Henao & Franco-Lara 2013; Franco-Lara & Perilla-Henao 2014; Franco-Lara et al. 2017). In addition, physiological alterations associated with phytoplasma infection have been described in potato and strawberry crops in the Sabana de Bogotá (L. Franco-Lara unpublished data). In addition to the environmental and economic cost of replacing infected urban trees, a considerable amount of concern also has arisen regarding the potential negative impact of phytoplasmas in the food production and urban environment. Information regarding the diversity and abundance of Cicadellidae inhabiting the Sabana de Bogotá is scarce but needed to define strategies for surveillance and management of phytoplasma diseases. The objective of our study was to characterize the species richness and composition of grassland Cicadellidae of the Sabana de Bogotá, as well as generate DNA barcodes for these species in order to complement their taxonomic identification for future studies.

Materials and Methods

INSECT SAMPLING AND IDENTIFICATION

Leafhoppers were collected at 2 sites of the Sabana de Bogotá. The first site was an urban location in Bogotá, Colombia, on the campus of the Universidad Nacional de Colombia (???4.640333°N, 74.081500°W; 2,559 masl) with an average temperature of 13.6 °C and average relative humidity of 79.6%. The habitat sampled encompassed 121.3 ha of which about 80% was covered in Cenchrus clandestinus (Hochst. ex Chiov.) Morrone (Poaceae) grassy areas with 13% trees and bushes. The second site was a semirural location at Cajicá, Cundinamarca, Colombia, on the campus of Universidad Militar Nueva Granada (4.944055°N, 74.008722°W; 2,447 masl). The Universidad Militar Nueva Granada campus encompasses 78 ha with an average annual temperature of 13.9 °C and average relative humidity of 87.9%. The predominant plant species is C. clandestinus, which covers about 70% of the campus, less than 10% is dedicated to trees and bushes.

Insect sampling was carried out twice per mo from Feb 2016 to Jan 2017, between 11:30 A.M. and 12:30 P.M. On each campus, 1 location was sampled that consisted of three 25 m2 quadrants further subdivided into five 1 m × 5 m sub-quadrants. On each sample date, 3 randomly selected sub-quadrants were sampled. Sampling sites at both campuses corresponded to areas with little disturbance except in cases where the grass was cut; in those cases new quadrants were established near the original location. At Universidad Nacional de Colombia, the first quadrant was sampled from Feb to Apr 2016, the second quadrant from May to Jun 2016, and the third from Jul 2016 to Jan 2017. At Universidad Militar Nueva Granada, the first quadrant was sampled from Feb to May 2016, the second from May to Oct 2016, and the third from Oct 2016 to Jan 2017. Leafhoppers were captured with an entomological sweep net and mouth aspirator, sweeping 25 times in each sub-quadrant for a total of 900 samples per site. Specimens were preserved in 90% ethanol. Adults were identified based on male external morphological characters with male genitalia cleared in 10% KOH (Oman 1949) based on Dietrich (2005). The following taxonomic keys were used for identifications: Linnavuori (1959), Young (1977), Dietrich (2005), Zahniser & Dietrich (2008, 2013), Beltrán et al. (2011), and Krishnankutty et al. (2016). Some morphotypes were not identified to the species level because only females were collected, or due to insufficient taxonomic keys for the Cicadellidae of Colombia.

DNA BARCODES

Half of leafhopper abdomens were used for DNA extraction while the remainder was preserved as voucher specimens. Extractions were performed using the protocol of Hung et al. (2004) with minor modifications. The DNA pellet was air dried and finally re-suspended in 25 µL of TE (10 mM Tris HCl pH 8.0, 1 mM EDTA). DNA extracts were stored at –20 °C. The PCR amplification of the COI gene was performed with primers LCO1490 (???5′-GGTCAACAAATCATAAAGATATTGG-3′) and HCO2198 (5′-TAAACTTCAGGGTGACCAAAAAATCA-3′), which produce an expected band of about 710 bp (Folmer et al. 1994). Samples that did not amplify with primers LCO1490/HCO2198 were tested with primers LepF2_t1 (5′-TGTAAAACGACGGCCAGAATCATAARGATATYGG-3′) and LepR1 (5′-TAAACTTCTGGATGTCCAAAAAATCA-3′), which produce an expected band of about 658 bp (Hebert et al. 2004; Foottit et al. 2014). Reactions were carried out at a final volume of 15 µL, with 1X reaction buffer, 2.5 mM Cl2Mg, 0.3 mM dNTPs, 0.3 mM of each set of primer, 2 µL of DNA template, 0.05 U of Taq DNA polymerase (Bioline, London, United Kingdom), and MiliQ (Merk KGaA, Darmstadt, Germany) sterile water. The thermic cycle for both pairs of primers was: 1 cycle at 95 °C 10 min; 35 cycles of denaturation at 95 °C for 60 s, annealing at 45.6 °C for 45 s, and extension at 72 °C for 45 s, and a final extension at 72 °C for 10 min. When using LCO1490 and HCO2198 in the Idiocerinae sp. samples, the annealing temperature was increased to 48.4 °C in order to obtain a single band. Amplicons were analyzed by standard gel agarose at 1% in 0.5X TBE buffer (Tris-Borate-EDTA). Samples used for sequencing were amplified by PCR as described, but at final volume of 30 µL.

PCR products were cleaned with the “UltraClean PCR Clean-up” kit (MoBio, Carlsbad, California, USA) and sequenced bi-directionally at Macrogen, Seoul, Korea. Sequences were edited manually, and the forward and reverse sequences aligned with MUSCLE (Edgar 2004) using the Geneious 10.2.3 software (Kearse et al. 2012) to generate consensus sequences of each sample. The sequences were compared by BLASTn with the NCBI ( https://www.ncbi.nlm.nih.gov/) and BOLD (Barcode of Life Data System) databases. Genetic distances were estimated and a sequence tree constructed with the neighbor joining algorithm using the Kimura-2-parameters model (Kimura 1980) with 1,000 bootstrap (Felsenstein 1985) in Mega 7.0.26 software (Kumar et al. 2016), using as an outgroup Tylocentrus quadricornis Funkhouser (Hemiptera: Membracidae). The sequences produced in this work were aligned with sequences of Cicadellidae species obtained from BOLD. A Barcode gap analysis was performed for these sequences using Mega 7.0.26 to estimate the intra- and interspecific genetic distances. Voucher specimens were placed in the entomological collection of Universidad Militar Nueva Granada and the DNA barcode sequences submitted to BOLD.

BIODIVERSITY STUDIES

Cicadellid males and females were used in all biodiversity analyses. The alpha diversity of the 2 sampling sites was calculated as the relative abundance per mo using the Margalef index (DMg), the dominance index Simpson (λ), and the equity index Shannon-Wiener (H′), using the PAST 3.15 software (Hammer et al. 2001). To determine if sampling effort was adequate for each site, accumulation curves for the collected species were built with EstimateS 9.1.0 (Colwell 2013) and compared with the accumulative curves of non-parametric estimators Chao 2, Jackknife 1, Jackknife 2, and Bootstrap (Magurran 2004; Chao et al. 2005). Hill numbers N0, N1, and N2 were calculated to determine the effective number of species. Beta diversity was based on Bray-Curtis (Ss), Jaccard (IJ), and Sørensen (IS) indices (Magurran 2004).

Results

LEAFHOPPER DIVERSITY

During the period of study, a total of 3,334 leafhopper adults and 1,175 nymphs were captured at both sample sites (Universidad Nacional de Colombia: n = 1,982 adults, n = 856 nymphs; Universidad Militar Nueva Granada: n = 1,352 adults, n = 919 nymphs). The most abundant subfamily was Deltocephalinae (82.3%), followed by Cicadellinae (15.8%), Aphrodinae (1.2%), Iassinae (0.6%), Idiocerinae (0.03%), and Typhlocybinae (0.03%) that belonged to 15 taxonomic groups (Table 1). Identification to species level was possible for 6 of them: Amplicephalus funzaensis Linnavuori; Borogonalia impressifrons Signoret; Draeculacephala soluta Gibson; Exitianus atratus Linnavuori; Paracatua rubrolimbata (Signoret), and Xestocephalus desertorum Berg (all Hemiptera: Cicadellidae). The sex ratio of these species is presented in Table 1. Images of the collected morphotypes are presented in the Supplementary Material.

Table 1.

Number of Cicadellidae captured at Universidad Nacional de Colombia (UNAL) and Universidad Militar Nueva Granada (UMNG) and their taxonomic identification.

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The semirural environment of Universidad Militar Nueva Granada contained a greater number of taxonomic groups (n = 13) than the urban environment of Universidad Nacional de Colombia (n = 10); however, the Chao 2 index estimated n = 13 for both sampling sites. For Universidad Militar Nueva Granada, Jackknife 1 and Jackknife 2 estimators calculated an expected number of species of n = 15, and for Universidad Nacional de Colombia n = 13 and n = 16, respectively (Fig. 1). The Simpson index showed that Universidad Nacional de Colombia species dominance was greater than Universidad Militar Nueva Granada due to the fact that A. funzaensis was an abundant species (n = 1,334). For both sites the similarity was > 53% (Table 2).

Abundance of monthly leafhopper capture rates varied for different species depending on mo and site. Amplicephalus funzaensis, the most abundant species, was collected infrequently at Universidad Nacional de Colombia during the first sample period, but the number of captured individuals increased up to 4 times from Oct 2016 to Jan 2017; at Universidad Militar Nueva Granada the number of captures was similar throughout the yr (Fig. 2A). Exitianus atratus, the second most frequent species, had a high rate of capture at Universidad Nacional de Colombia from Apr to May and Nov. Individuals of this species at Universidad Militar Nueva Granada were most abundant during Feb to Oct with a decrease in the last of mo of the yr (Fig. 2B). For B. impressifrons, collections from Universidad Nacional de Colombia were very low but in Universidad Militar Nueva Granada this species was abundant from Nov to Jan (Fig. 2C). Capture rates of Dalbulus sp. at Universidad Nacional de Colombia were very high during Feb, but remained very low the following mo until a peak was observed from Nov to Dec. At Universidad Militar Nueva Granada, no individuals of this genus were collected in sweep net samples obtained during Feb to Sep but peaked in Nov (Fig. 2D). Haldorus sp. collections at Universidad Militar Nueva Granada peaked in Sep with a lesser peak in May and very low captures in Jul, Aug, Nov, and Dec 2016, and Jan 2017, which appeared to coincide with the precipitation periods. At Universidad Nacional de Colombia, more leafhoppers of this genus occurred in samples during May and Jun (Fig. 2E). In both sample locations, abundance of the remaining species was too low in both locations to determine seasonality.

Fig. 1.

Accumulation curves for the observed species (S) and for the non-parametric estimators Chao 2, Jack 1 = Jackknife 1, Jack 2 = Jackknife 2, and Bootstrap from Universidad Nacional de Colombia (UNAL) and Universidad Militar Nueva Granada (UMNG).

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Table 2.

Index values for specific richness, dominance, equitability, effective number of species (N0, N1, and N2), similarity and dissimilarity for Universidad Nacional de Colombia (UNAL) and Universidad Militar Nueva Granada (UMNG).

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During the study, 3 closely located quadrants were sampled at each location. Interestingly, the spatial distribution of B. impressifrons, Dalbulus sp. and D. soluta was not homogeneous. These 3 species were collected together from 1 quadrant, unlike E. atratus and Haldorus sp. where they occurred in any quadrant. Amplicephalus funzaensis was an interesting case because at Universidad Militar Nueva Granada, the number of collected individuals was more or less homogenous among quadrants, but at Universidad Nacional de Colombia, a marked heterogeneity was observed (Table 3).

Fig. 2.

Capture rate per month of Exitianus atratus, Amplicephalus funzaensis, Borogonalia impressifrons, Dalbulus sp., and Haldorus sp. at Universidad Nacional de Colombia (UNAL) and Universidad Militar Nueva Granada (UMNG).

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DNA BARCODES

PCR reactions using primers LCO1490/HCO2198 produced amplicons of approximately 600 bp for A. funzaensis, Dalbulus sp., D. soluta, E. atratus, Haldorus sp., P. rubrolimbata, and X. desertorum, including those of Portanini sp., Gyponini sp., and Idiocerinae sp. For B. impressifrons and Empoasca (Hemiptera: Cicadellidae) sp., LepF2_t1/LepR1 produced amplicons or about 600 bp. However, with these 2 primer sets no amplification of the COI gene was observed for individuals of Amplicephalus sp., Borogonalia sp., or Deltocephalini sp. In some cases, the LCO1490/HCO2198 primers amplified sequences of the bacteria Wolbachia spp. (Rickettsiales: Anaplasmataceae) from A. funzaensis and Dalbulus sp. From 45 sequenced COI amplicons, 36 showed good quality reads. For B. impressifrons, D. soluta, E. atratus, Haldorus sp., and P. rubrolimbata, 2 haplotypes per species were found, but for the rest of the taxonomic groups only 1 haplotype was obtained. Sequences, trace files, collection data, and specimen photographs were deposited in the Barcode of Life Data System (BOLD,  http://www.bold-systems); processes ID are shown in fig. 3.

A neighbor joining sequence tree was constructed including 12 sequences of leafhoppers from Universidad Nacional de Colombia, 24 from Universidad Militar Nueva Granada, with 42 sequences downloaded from BOLD (Fig. 3). In all cases, sequences belonging to the same taxa clustered together. Furthermore, all sequences of Deltocephalinae species clustered in a single clade, and the Cicadellinae, Typhlocybinae, and Idiocerinae were grouped in a second clade. A third clade contained the sequences from Portanini sp. that belong to the subfamily Aphrodinae. A fourth clade contained the subfamily Iassinae, whereas a fifth clade contained individuals of the tribe Xestocephalini that belong to subfamily Aphrodinae.

In order to evaluate the utility of sequences as DNA barcodes, a Barcode gap analysis was performed. The average intraspecific divergence of sequences was 0.3%, with a minimum value of 0% and a maximum of 2.4%; average interespecific divergence was 25.1% with a minimum of 10.7% and a maximum value of 33.7%. Sequences of Portanini sp., Gyponini sp., and Idiocerinae sp. showed an intraspecific divergence of 0% while that of B. impressifrons, D. soluta, E. atratus, Haldorus sp., and P. rubrolimbata was of 0.08%, 0.1%, 0.04%, 0.1%, and 0.3%, respectively. All sequences used in our analyses fulfilled the barcode gap criterion (results not shown).

Discussion

We found that the biodiversity of Cicadellidae in Sabana de Bogotá showed greater richness at the semirural Universidad Militar Nueva Granada campus, compared with the urban Universidad Nacional de Colombia campus. This geographic area is located in a tropical zone where meteorological seasons do not exist, maximum and minimum daily temperatures are similar throughout the yr with a bimodal precipitation regime from Apr to May, and Sep to Nov the rainiest mo (Guzmán et al. 2014). Cicadellid species, as well as abundance in collections fluctuated during the yr, but only in the case of Haldorus sp. did the fluctuation show a correlation with the dry and rainy periods. More observations and finer measurements of the climatic variables are needed to make correlations with the population dynamics of these species. However, observations indicate that for different mo, different vector species prevailed, and that during an entire yr there are insect vectors present to transmit phytoplasmas.

Table 3.

Number of leafhoppers captured per quadrant, per site at Universidad Nacional de Colombia (UNAL) and Universidad Militar Nueva Granada (UMNG).

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Non-parametric estimators showed that the sampling effort performed was not enough in either site. In a previous study (A. F. Silva-Castaño unpublished results), 13 species were collected from the Universidad Militar Nueva Granada campus, of which 4 (Agalliana sp., Gyponana sp., Stehlikiana crassa [Walker], and Xerophloea sp.) (all Hemiptera: Cicadellidae) were not captured in our current study. We found the diversity indices difficult to interpret from our datasets; therefore, the effective number of species was calculated (Magurran 2004). Hill series values indicated that at Universidad Nacional de Colombia, A. funzaensis was a dominant species, but at Universidad Militar Nueva Granada, greater equitability occurred because several abundant species were observed, such as A. funzaensis, B. impressifrons, Dalbulus sp. E. atratus, and Haldorus sp. We also found that the most abundant subfamilies represented in collections were Cicadellinae and Deltocephalinae. Both families have many representatives that are grass feeders (Dietrich 2000). The number of individuals of Idiocerinae, Iassinae, and Typhlocybinae, which are usually reported as tree and bush inhabitants, was low in our sweep net collections (Dietrich 2000; Dietrich 2013b). However, observations from the current study suggest that Idiocerinae sp. and Empoasca sp. may be casual visitors of C. clandestinus, because males and females of these species were observed during sampling in nearby Eugenia neomyrtifolia Sobral (Myrtaceae) and Acacia decurrens (J.C. Wendl.) Willd. (Fabaceae). A few individuals of X. desertorum were captured at Universidad Nacional de Colombia and Universidad Militar Nueva Granada. This species of Aphrodinae usually is associated with the roots of grasses (Cwikla & Blocker 1981).

The most abundant species in both sampling sites were A. funzaensis and E. atratus, both of which are known to transmit phytoplasmas of groups 16SrI-B and 16rVII-A under experimental conditions (Perilla-Henao et al. 2016). Haldorus sp. and Dalbulus sp. also were abundant in our sweep net collections. Perilla-Henao et al. (2016) showed that Haldorus sp. from the Sabana de Bogotá was infected with phytoplasmas of the 16SrI group. Dalbulus spp., on the other hand, has been reported as the vector of Maize rayado fino virus (Tymovirales: Tymoviridae) (Gámez 1973) maize bushy stunt phytoplasmas (group16SrI-B) (Nault 1980), and Spiroplasma kunkelii Whitcomb et al. (Entomoplasmatales: Spiroplasmataceae), the ethiological agent of corn stunt disease in maize in the US (Whitcomb et al. 1986). Amplicephalus funzaensis, E. atratus, Haldorus sp., and Dalbulus sp. are abundant inhabitants of the Sabana de Bogotá grassland and may be involved in the dispersal of phytoplasmas.

The ecosystem of the Sabana de Bogotá has changed dramatically from native low Andean forests in pre-Hispanic times, to the present situation of semirural areas intermingled with urban zones (Pérez-Preciado 2000). Cenchrus clandestinus was introduced into Colombia in the 1920s, becoming one of the predominant grass species of the Andes in urban and rural zones, replacing many native plant species (Mears 1970; Nepstad et al. 2013). In the Sabana de Bogotá, C. clandestinus is an asymptomatic host of phytoplasmas of 16SrI-A and 16SrVII-B groups (Perilla-Henao et al. 2016; L. Franco-Lara unpublished results). Therefore, C. clandestinus plays an important role in the epidemiology of phytoplasmas in the region because it serves as hosts to several Cicadellidae species incriminated as vectors.

The main goal of the DNA Barcode system is to generate short DNA sequences that allow the identification of species by comparing them with a cured database such as BOLD ( http://v3.boldsystems.org/) (Hebert et al. 2004). To complement the conventional taxonomic identification of the cicadellids from our collection, DNA barcodes for the 12 morphotypes were obtained. The neighbor joining tree built with those sequences clustered individuals of the same species and separate species in different clades, showing the usefulness of the barcodes. To our knowledge these are the first DNA barcode reports for Colombian Cicadellidae published in the BOLD database. However, no amplicons or sequences were obtained for the Amplicephalus sp., Borogonalia sp., or Deltocephalini sp. specimens. Failure to amplify those individuals with primers designed for the COI gene of invertebrates has been reported before (Palomera et al. 2012; Sharma & Kobayashi 2014). In 3 cases, the primers we used amplified the COI gene of Wolbachia from A. funzaensis and Dalbulus sp. samples. Wolbachia belongs to a genus of endosymbiotic bacteria of many arthropod species, which affects the sex-ratio and reproductive compatibility of its hosts. Insect COI primers can amplify the Wolbachia COI gene, but it is not considered to compromise the accuracy of the DNA barcode system (Smith et al. 2012). A Barcode gap analysis also was performed for sequences obtained in this work with additional Cicadellidae sequences retrieved from other databases. This analysis refers to the separation between mean intra- and interspecific sequence variability for congeneric COI sequences. If a gap exists between these 2, a cut value for the species delimitation can be established that would illustrate the usefulness of this method, as indicated by Meyer and Paulay (2005). We found that barcode gap analysis from all the taxonomic groups in our study met this criterion. However, this is a limited assessment because sequences of close phylogenetic species were not included because they are not available in the databases. This limitation has been pointed out, but it will be solved as the databases are being fed more information (Collins & Cruickshank 2012). DNA barcodes are useful for the routine identification of adult or immature arthropods, determination of cryptic or atypical species, including taxonomic and phylogenetic studies (Hajibabaei et al. 2007; Foottit et al. 2014; Čandek & Kuntner 2015). In our case, the availability of DNA barcodes will enhance our ability to study the biology of cicadellids, particularly vectors of phytoplasmas.

Fig. 3.

COI gene neighbor joining tree using Kimura-two-parameter (K2P) with 1,000 Bootstrap. The tree includes 77 leafhopper sequences. Red Circles indicate the sequences of species captured at Universidad Militar Nueva Granada (UMNG) and triangles at Universidad Nacional de Colombia (UNAL).

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Acknowledgments

We thank the Universidad Militar Nueva Granada for funding the project INV-CIAS-2046, as well as the Universidad Nacional de Colombia for allowing us to perform the sweep net collections. We also are grateful to Christopher H. Dietrich for his suggestions during the preparation of this paper, the students of the Plant Biotechnology laboratory, and particularly Adriana Fonseca for her permanent technical support.

References Cited

1.

Ammar ED, Nault LR. 2002. Virus transmission by leafhoppers, planthoppers and treehoppers (Auchenorrhyncha, Homoptera). Advances in Botanical Research 36: 141–167. Google Scholar

2.

Beltrán CE, Vargas Rojas JM, Freytag PH. 2011. A new species of Paracatua Melichar (Cicadellidae: Cicadellinae) from Colombia. Entomological News 122: 214–222. Google Scholar

3.

Čandek K, Kuntner, M. 2015. DNA barcoding gap: reliable species identification over morphological and geographical scales. Molecular Ecology Resources 15: 268–277. Google Scholar

4.

Chao A, Chazdon RL, Colwell RK, Shen TJ. 2005. A new statistical approach for assessing similarity of species composition with incidence and abundance data. Ecology Letters 8: 148–159. Google Scholar

5.

Collins RA, Cruickshank RH. 2012. The seven deadly sins of DNA barcoding. Molecular Ecology Resources 13: 969–975. Google Scholar

6.

Colwell R. 2013. EstimateS: statistical estimation of species richness and shared species from samples. Version 9.1.0, User's Guide and Application.  http://purl.oclc.org/estimates (last accessed 12 May 2019). Google Scholar

7.

Cwikla PS, Blocker HD. 1981. An annotated list of the leafhoppers (Homoptera: Cicadellidae) from tallgrass prairie of Kansas and Oklahoma. Transactions of the Kansas Academy of Science 1903: 89–97. Google Scholar

8.

Dietrich CH. 2000. Guide to the subfamilies of leafhoppers (Cicadellidae). Center for Biodiversity, Illinois Natural History Survey, Champaign, Illinois, USA.  https://www.inhs.illinois.edu/collections/insect/data/leafhoppers/guide (last accessed 11 Jun 2019). Google Scholar

9.

Dietrich CH. 2005. Keys to the families of Cicadomorpha and subfamilies and tribes of Cicadellidae (Hemiptera: Auchenorrhyncha). Florida Entomologist 88: 502–517. Google Scholar

10.

Dietrich CH. 2013a. Overview of phylogeny, taxonomy and diversity of the leafhopper (Hemiptera: Auchenorrhyncha: Cicadomorpha: Membrac-oidea: Cicadellidae) vectors of plant pathogens. Proceedings of the International Symposium on Insect Vectors and Insect-Borne Diseases, Taiwan, 2013.  https://pdfs.semanticscholar.org/6df4/eb1e6649cb824db1f1511c681921afeef032.pdf (last accessed 11 June 2019). Google Scholar

11.

Dietrich CH. 2013b. South American leafhoppers of the tribe Typhlocybini (Hemiptera: Cicadellidae: Typhlocybinae). Zoologia (Curitiba) 30: 519–568. Google Scholar

12.

Edgar RC. 2004. MUSCLE: multiple sequence alignment with high accuracy and high throughput. Nucleic Acids Research 32: 1792–1797. Google Scholar

13.

Felsenstein J. 1985. Confidence limits on phylogenies: an approach using the bootstrap. Evolution 39: 783–791. Google Scholar

14.

Folmer O, Black M, Hoeh W, Lutz R, Vrijenhoek R. 1994. DNA primers for amplification of mitochondrial cytochrome c oxidase subunit I diverse metazoan invertebrates. Molecular Marine Biology and Biotechnology 3: 294–299. Google Scholar

15.

Foottit RG, Maw E, Hebert PDN. 2014. DNA barcodes for Nearctic Auchenorrhyncha (Insecta: Hemiptera). PLoS ONE 9: e101385.  https://doi.org/10.1371/journal.pone.0101385  Google Scholar

16.

Franco-Lara L, Perilla Henao LM. 2014. Phytoplasma diseases in trees of Bogotá, Colombia: a serious risk for urban trees and crops, pp. 90–100 In Bertaccini A [ed.], Phytoplasmas and Phytoplasma Disease Management: How to Reduce Their Economic Impact. International Phytoplasmologist Working Group, Bologna, Italy. Google Scholar

17.

Franco-Lara L, Contaldo N, Mejia JF, Paltrinieri S, Duduk B, Bertaccini A. 2017. Detection and identification of phytoplasmas associated with declining Liquidambar styraciflua trees in Colombia. Tropical Plant Pathology 42: 352–361. Google Scholar

18.

Gámez R. 1973. Transmission of rayado fino virus of maize (Zea mays) by Dalbulus maidis . Annals of Applied Biology 73: 285–292. Google Scholar

19.

Guzmán D, Ruíz JF, Cadena M. 2014. Regionalización de Colombia según la estacionalidad de la precipitación media mensual, a través análisis de componentes principales (acp). Grupo de Modelamiento de Tiempo, Clima y Escenarios de Cambio Climático, Subdirección de Meteorología–IDEAM.  http://www.ideam.gov.co/documents/21021/21141/Regionalizacion+de+la+Precipitacion+Media+Mensual/1239c8b3-299d-4099-bf52-55a414557119 (last accessed 11 Jun 2019). Google Scholar

20.

Hajibabaei M, Singer GA, Hebert PD, Hickey DA. 2007. DNA barcoding: how it complements taxonomy, molecular phylogenetics and population genetics. TRENDS in Genetics 23: 167–172. Google Scholar

21.

Hammer Ø, Harper DAT, Ryan PD. 2001. PAST: PAleontological STatistics software package for education and data analysis. Palaeontologia Electronica 4: 1–9.  https://www.uv.es/∼pardomv/pe/2001_1/past/pastprog/past (last accessed 12 May 2019). Google Scholar

22.

Hebert PD, Penton EH, Burns JM, Janzen DH, Hallwachs W. 2004. Ten species in one: DNA barcoding reveals cryptic species in the Neotropical skipper butterfly Astraptes fulgerator. Proceedings of the National Academy of Sciences of the United States of America 101: 14812–14817. Google Scholar

23.

Hung TH, Hung SC, Chen CN, Hsu MH, Su HJ. 2004. Detection by PCR of Candidatus Liberibacter asiaticus, the bacterium causing citrus huanglongbing in vector psyllids: application to the study of vector-pathogen relationships. Plant Pathology 53: 96–102. Google Scholar

24.

Kearse M, Moir R, Wilson A, Stones-Havas S, Cheung M, Sturrock S, Buxton S, Cooper A, Markowitz S, Duran C, Thierer T, Ashton B, Mentjies P, Drummond A. 2012. Geneious Basic: an integrated and extendable desktop software platform for the organization and analysis of sequence data. Bioinformatics 28: 1647–1649. Google Scholar

25.

Kimura M. 1980. A simple method for estimating evolutionary rates of base substitutions through comparative studies of nucleotide sequences. Journal of Molecular Evolution 16: 111–120. Google Scholar

26.

Krishnankutty SM, Dietrich CH, Dai W, Siddappaji MH. 2016. Phylogeny and historical biogeography of leafhopper subfamily Iassinae (Hemiptera: Cicadellidae) with a revised tribal classification based on morphological and molecular data. Systematic Entomology 41: 580–595. Google Scholar

27.

Kumar S, Stecher G, Tamura K. 2016. MEGA7: Molecular Evolutionary Genetics Analysis, Version 7.0 for bigger datasets. Molecular Biology and Evolution 33: 1870–1874. Google Scholar

28.

Lee IM, Davis RE, Gundersen-Rindal DE. 2000. Phytoplasma: phytopathogenic mollicutes. Annual Reviews in Microbiology 54: 221–255. Google Scholar

29.

Linnavuori R. 1959. Revision of the Neotropical Deltocephalinae and some related subfamilies (Homoptera). Societas Zoologica Botanica Fennica “Vanamo” 20: 1–370. Google Scholar

30.

Magurran AE. 2004. Measuring Biological Diversity. Blackwell Publishing, Malden, Massachusetts, USA. Google Scholar

31.

Mears PT. 1970. Kikuyu (Pennisetum clandestinum) as a pasture grass. A review. Tropical Grasslands 4: 139–152. Google Scholar

32.

Meyer CP, Paulay G. 2005. DNA barcoding: error rates based on comprehensive sampling. PLoS Biology 3: 1–10. Google Scholar

33.

Nault LR. 1980. Maize bushy stunt and corn stunt: a comparison of disease symptoms, pathogen host ranges, and vectors. Phytopathology 70: 659–662. Google Scholar

34.

Nepstad DC, Bezerra T, Tepper D, McCann K, Stickler C, McGrath DG, Barrera MX, Lowery S, Armijo E, Higgins ML, Monschke J, Gomez R, Velez S, Tejada M, Tejada M, Killeen T, Schwalbe K, Ruedas A. 2013. Addressing agricultural drivers of deforestation in Colombia: increasing land-based production while reducing deforestation, forest degradation, greenhouse gas emissions and global poverty.  https://www.gov.uk/government/uploads/system/uploads/attachment_data/file/274185/drivers_of_deforestation_in_colombia.pdf (last accessed 12 May 2019). Google Scholar

35.

Nielson MW. 1968. The leafhopper vectors of phytopathogenic viruses (Homoptera, Cicadellidae): taxonomy, biology, and virus transmission. USDA, Agricultural Research Service, Technical Bulletin #1382).  https://naldc.nal.usda.gov/download/CAT87201370/PDF (last accessed 12 May 2019). Google Scholar

36.

Oman PW. 1949. The Nearctic Leafhoppers (Homoptera: Cicadellidae). A Generic Classification and Check List. Entomological Society of Washington, Laurel, Maryland, USA. Google Scholar

37.

Palomera V, Bertin S, Rodríguez A, Bosco D, Virla E, Moya-Raygoza G. 2012. Is there any genetic variation among native Mexican and Argentinian populations of Dalbulus maidis (Hemiptera: Cicadellidae)? Florida Entomologist 95: 150–155. Google Scholar

38.

Pérez-Preciado A. 2000. La estructura ecológica principal de la Sabana de Bogotá. Sociedad Geográfica de Colombia – Academia de Ciencias Geográficas.  https://www.sogeocol.edu.co/documentos/est_eco.pdf (last accessed 12 May 2019). Google Scholar

39.

Perilla-Henao LM, Franco-Lara L. 2013. Especies arbóreas de las familias Euphorbiaceae, Pittosporaceae y Salicaceae son infectadas por ‘Ca. Phytoplasma fraxini' y ‘Ca. Phytoplasma asteris’ en infecciones mixtas en Bogotá, Colombia. Revista Facultad de Ciencias Básicas 9: 248–265. Google Scholar

40.

Perilla-Henao LM, Dickinson M, Franco-Lara L. 2012. First report of ‘Candidatus Phytoplasma asteris’ affecting woody hosts (Fraxinus uhdei, Populus nigra, Pittosporum undulatum and Croton spp.) in Colombia. Plant Disease 96: 1372.  https://www.apsnet.org/publications/plantdisease/2012/September/Pages/96_9_1372.2.aspx (last accessed 12 May 2019). Google Scholar

41.

Perilla-Henao L, Wilson MR, Franco-Lara L. 2016. Leafhoppers Exitianus atratus and Amplicephalus funzaensis transmit phytoplasmas of groups 16SrI and 16SrVII in Colombia. Plant Pathology 65: 1200–1209. Google Scholar

42.

Sharma P, Kobayashi T. 2014. Are “universal” DNA primers really universal? Journal of Applied Genetics 55: 485–496. Google Scholar

43.

Smith MA, Bertrand C, Crosby K, Eveleigh ES, Fernandez-Triana J, Fisher BL, Gibbs J, Hajibabaei M, Hallwachs W, Hind K, Hrcek J, Huang DW, Janda M, Janzen DH, Li Y, Miller SE, Packer L, Quicke D, Ratnasingham S, Rodriguez J, Rougerie R, Shaw MR, Sheffield C, Stahlhut JK, Steinke D, Whitfield J, Wood M, Zhou X. 2012. Wolbachia and DNA barcoding insects: patterns, potential, and problems. PLoS One 7: e36514. https://doi.org/10.1371/journal.pone.0036514 Google Scholar

44.

Weintraub PG, Beanland L. 2006. Insect vectors of phytoplasmas. Annual Review of Entomology 51: 91–111. Google Scholar

45.

Weintraub PG, Wilson MR. 2010. Control of phytoplasma diseases and vectors, pp. 233–249 In Weintraub PG, Jones P [eds.], Phytoplasmas: Genomes, Plant Hosts and Vectors. CABI, Wallingford, Oxfordshire, United Kingdom. Google Scholar

46.

Whitcomb RF, Chen TA, Williamson DL, Liao C, Tully JG, Bové JM, Mouches C, Rose D, Coan ME, Clark TB. 1986. Spiroplasma kunkelii sp. nov.: characterization of the etiological agent of corn stunt disease. International Journal of Systematic and Evolutionary Microbiology 36: 170–178. Google Scholar

47.

Young DA. 1977. Taxonomic study of the Cicadellinae (Homoptera: Cicadellidae). 2. New World Cicadellini and the genus Cicadella. North Carolina Agricultural Experiment Station (USA) Technical Bulletin 239. Raleigh, North Carolina, USA. Google Scholar

48.

Zahniser JN, Dietrich C. 2013. A review of the tribes of Deltocephalinae (Hemiptera: Auchenorrhyncha: Cicadellidae). European Journal of Taxonomy 45: 1–211. Google Scholar

49.

Zahniser JN, Dietrich CH. 2008. Phylogeny of the leafhopper subfamily Deltocephalinae (Insecta: Auchenorrhyncha: Cicadellidae) and related subfamilies based on morphology. Systematics and Biodiversity 6: 1–24. Google Scholar
Andrés Felipe Silva-Castaño, Michael R. Wilson, Helena Luisa Brochero, and Liliana Franco-Lara "Biodiversity, Bugs, and Barcodes: The Cicadellidae Associated with Grassland and Phytoplasmas in the Sabana de Bogotá, Colombia," Florida Entomologist 102(4), 755-762, (23 January 2020). https://doi.org/10.1653/024.102.0413
Published: 23 January 2020
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