Aedes aegypti, the yellow fever mosquito, is an efficient vector of arboviruses and a convenient model system for laboratory research. Extensive linkage mapping of morphological and molecular markers localized a number of quantitative trait loci (QTLs) related to the mosquito's ability to transmit various pathogens. However, linking the QTLs to Ae. aegypti chromosomes and genomic sequences has been challenging because of the poor quality of polytene chromosomes and the highly fragmented genome assembly for this species.
Based on the approach developed in our previous study, we constructed idiograms for mitotic chromosomes of Ae. aegypti based on their banding patterns at early metaphase. These idiograms represent the first cytogenetic map developed for mitotic chromosomes of Ae. aegypti. One hundred bacterial artificial chromosome clones carrying major genetic markers were hybridized to the chromosomes using fluorescent in situ hybridization. As a result, QTLs related to the transmission of the filarioid nematode Brugia malayi, the avian malaria parasite Plasmodium gallinaceum, and the dengue virus, as well as sex determination locus and 183 Mbp of genomic sequences were anchored to the exact positions on Ae. aegypti chromosomes. A linear regression analysis demonstrated a good correlation between positions of the markers on the physical and linkage maps. As a result of the recombination rate variation along the chromosomes, 12 QTLs on the linkage map were combined into five major clusters of QTLs on the chromosome map.
This study developed an integrated linkage, chromosome, and genome map—iMap—for the yellow fever mosquito. Our discovery of the localization of multiple QTLs in a few major chromosome clusters suggests a possibility that the transmission of various pathogens is controlled by the same genomic loci. Thus, the iMap will facilitate the identification of genomic determinants of traits responsible for susceptibility or refractoriness of the mosquito to diverse pathogens.
About half of the human population is under risk of dengue infection. Because of the absence of a vaccine or drug treatment, the prevention of this disease largely relies on controlling its major vector mosquito Aedes aegypti. Availability of the complete genome sequence for this mosquito offers the potential to help in the identification of novel disease control strategies. An efficient vector of arboviruses, Ae. aegypti is also a convenient model for laboratory studies. A number of genetic loci related to the remarkable ability of this mosquito to transmit various pathogens were genetically mapped to the three linkage groups corresponding to the three individual chromosomes of the mosquito. However, the exact physical positions of the genetic loci and genomic sequences on the chromosomes were unknown. In this study, we developed maps for mitotic chromosomes of Ae. aegypti and localized 100 clones carrying major genetic markers, which were previously used for mapping genetic loci associated with the pathogens' transmission. Finally, linkage, chromosome, and genome maps of Ae. aegypti were integrated. Anchoring of the genomic sequences associated with genetic markers to the chromosomes of Ae. aegypti will help to identify candidate genes that might be utilized for developing advanced genome-based strategies for vector control.
Citation: Timoshevskiy VA, Severson DW, deBruyn BS, Black WC, Sharakhov IV, et al. (2013) An Integrated Linkage, Chromosome, and Genome Map for the Yellow Fever Mosquito Aedes aegypti. PLoS Negl Trop Dis 7(2): e2052. doi:10.1371/journal.pntd.0002052
Editor: Jesus G. Valenzuela, National Institute of Allergy and Infectious Diseases, United States of America
Received: October 16, 2012; Accepted: December 21, 2012; Published: February 14, 2013
Copyright: © 2013 Timoshevskiy et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: The research was funded by grant R21-AI088035 from the National Institutes of Health/National Institute of Allergy and Infectious Diseases (NIH/NIAID) to MVS. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Mosquitoes are vectors of numerous human pathogens such as malaria parasites transmitted by the subfamily Anophelinae; lymphatic filarial worms transmitted by both Anophelinae and Culicinae subfamilies; and arboviruses whose transmission is largely associated with the subfamily Culicinae. Aedes aegypti is recognized as a principal vector of dengue and yellow fever viruses. These two diseases have a significant world-wide impact on human health. Dengue fever is currently considered the most important vector-borne arboviral disease of the 21st century . The disease is a threat to 3.6 billion people with an annual incidence of 230 million cases of infection resulting in 21,000 deaths per year. Since the 1950s, the incidence of dengue fever has expanded globally. The World Health Organization (WHO) estimated a 30-fold increase in the incidence of dengue infections over the past 50 years . The disease became endemic in 100 countries in Africa, West Asia, and America  and is a growing threat to the United States . In addition to dengue, yellow fever, a devastating disease of the 19th century in North America and Europe, still affects up to 600 million lives and remains responsible for about 30,000 deaths annually . The disease is currently endemic in 32 countries in Africa and 13 in South America. The spread of the pathogens is associated with the extremely tight connection of their major vector Ae. aegypti to humans. Despite all control campaigns, Ae. aegypti currently occupies most subtropical and tropical regions in the world.
Ae. aegypti represents both an efficient vector of arboviruses and a convenient model system for experimental laboratory research. This species can be easily colonized and is highly tolerant to inbreeding . Unlike Anopheles eggs, Ae. aegypti eggs are resistant to desiccation and can be stored in a dry place for several months. As a result of these advantages, genetic (linkage) mapping conducted on Ae. aegypti was very successful. The genetic mapping was originally inspired from the study of the inheritance of dichlorodiphenyltrichloroethane (DDT) resistance as a single dominant trait . A similar mechanism of inheritance, as a single gene or a single block of chromosome material, was demonstrated for sex determination . The sex determination alleles were described as Mm in males and mm in females and linked to homomorphic chromosome 1 . In addition, 28 of 87 morphological mutations described for Ae. aegypti were mapped to the three linkage groups corresponding to the three chromosomes of this mosquito . The linkage map was extended by additional mapping of physiological and enzyme loci . The classical linkage map included about 70 loci of morphological mutants, insecticide resistance, and isozyme markers .
A possibility of using DNA molecular markers opened a new era in genetic mapping of mosquito genomes. The first molecular-marker-based linkage map for Ae. aegypti was constructed using restriction-fragment-length polymorphism (RFLP) of complementary DNA (cDNA) clones . This map included 50 DNA markers and covered 134 centimorgan (cM) across the three linkage groups. Thereafter, the polymerase chain reaction (PCR) was used to generate a map based on random-amplified polymorphic DNA (RAPD) loci which consisted of 96 RAPD loci covering 168 cM . Linkage maps based on single-strand conformation polymorphism (SSCP) and single nucleotide polymorphism (SNP) markers were also constructed. A composite map for RFLP, SSCP, and SNP markers incorporated 146 loci and covered 205 cM . Later, an additional map using amplified fragment-length polymorphism (AFLP) was also developed for 148 loci and covered about 180 cM of the genome . Finally, the genetic map of Ae. aegypti was extended by incorporating microsatellite loci . The linkage map was used as a tool to localize several quantitative trait loci (QTLs) related to pathogen transmission: the filarioid nematode Brugia malayi , the avian malaria parasite Plasmodium gallinaceum , , and dengue virus , . Among all mosquitoes, the map developed for Ae. aegypti is the most densely populated.
Cytogenetic mapping on Ae. aegypti and other culicine species is difficult due to the absence of high-quality, easily spreadable polytene chromosomes ,  The majority of cytogenetic studies for Ae. aegypti have been conducted on mitotic chromosomes from brain ganglia or meiotic chromosomes from male testis –. These studies led to the conclusion that Ae. aegypti has a karyotype consisting of three pairs of metacentric chromosomes . The chromosomes first numbered as chromosomes I, II, and III in order of increasing size  were later renumbered as chromosomes 1, 2, and 3 in correspondence to the linkage map developed for Ae. aegypti, resulting in the longest chromosome III becoming chromosome 2 . Chromosomes from brain ganglia of Ae. aegypti were first utilized for the successful nonfluorescent in situ hybridization of two ribosomal genes . Fluorescent in situ hybridization (FISH) technique has been developed using mitotic chromosomes from the ATC-10 cell line of Ae. aegypti, resulting in direct positioning of 37 cosmid clones onto chromosomes . In addition, 21 cDNA genetic markers and 8 cosmid clones containing the RFLP markers have been mapped to the chromosomes from this line . This map was the first attempt to integrate linkage and physical maps for Ae. aegypti.
The genome of Ae. aegypti was among the first three mosquito genomes sequenced in the last decade . As compared with Anopheles gambiae  and Culex quinquefasciatus  genomes, the genome of Ae. aegypti is the largest and consists of 1,376 Mb. The availability of the Ae. aegypti genome provides an opportunity to integrate linkage, chromosome, and genome maps for this mosquito. A total of 106 bacterial artificial chromosome (BAC) clones carrying major genetic markers have been identified by screening an Ae. aegypti BAC library prepared from the Liverpool strain . In addition, a new cytogenetic approach based on mitotic chromosomes from imaginal discs (IDs) of 4th instar larvae has been recently developed . Instead of using cell lines, which usually accumulate chromosomal rearrangements , this method utilizes live larvae for cytogenetic analysis. A preparation slide of one ID contains ~175 chromosome spreads. This number is 6-fold greater than that of two brain ganglia. Clearly visible banding patterns of mitotic chromosomes from IDs allowed the construction of preliminary idiograms without numbered divisions for the chromosomes at mid-metaphase . A FISH technique was optimized for using BAC clones as probes  resulting in the assignment of 10 BAC clones and ribosomal 18S DNA to bands on the idiograms .
In the current study, we constructed new idiograms for the longer early-metaphase chromosomes with numbered divisions and subdivisions. These idiograms facilitated assignment of 100 BAC clones carrying major genetic markers to chromosomal bands. BAC clones within each band on the chromosomes were additionally ordered based on multicolor FISH on higher resolution prophase or polytene chromosomes. Finally, because each BAC clone also represents a supercontig in the Ae. aegypti genome assembly, the total of 183 Mb or 13.3% of the genomic sequences was also incorporated into the map. We define our map as integrated linkage, chromosome, and genome map or an iMap of Ae. aegypti.
This study was performed on the Liverpool IB12 strain of Ae. aegypti, which was previously used for the genome sequencing project . This strain originated from the Liverpool strain (LVP) following several rounds of inbreeding. LVP was a major strain for conducting genetic and QTL mapping in the past , , . Originally, mosquitoes for this strain were collected in West Africa and then kept by the Liverpool School of Medicine .
Chromosome preparations were prepared from imaginal discs (IDs) or salivary glands of the 4th instar larvae of Ae. aegypti (Timoshevskiy et al., 2012). For ID dissection larvae were placed on ice for several minutes for immobilization. Individual larva was decapitated in a drop of cold hypotonic solution (0.5% sodium citrate). Then the thoracic part of the larva was dissected, and cuticle from the ventral side of the larval thorax was cut by dissecting scissors (Fine Science Tools, USA) and opened. The gut and fat body particles were removed, and a new drop of hypotonic solution was applied. After 10 min., the hypotonic solution was removed using filter paper, and a drop of fixative solution (ethanol/acetic acid in 3:1 ratio) was applied. IDs were isolated using dissecting needles (Fine Science Tools, USA), placed in a drop of 50% propionic acid for maceration, and squashed under a cover slip (22×22 mm). Salivary glands were dissected from the larvae prefixed in fixative solution (ethanol/acetic acid in 3:1 ratio) for at least 24 hrs and then squashed in a drop of 50% propionic acid. Presence of chromosomes on the slide was determined by using a phase-contrast microscope Olympus CX41 (Olympus America, Inc., USA) at 200× magnification. Slides suitable for further applications were placed in liquid nitrogen and cover slips were removed. Finally, slides were dehydrated in an ethanol series (70, 80, 100%) and stored at −20°C.
Probe/Cot fraction DNA preparation
BAC clone DNA was prepared by the Clemson University Genomics Institute in 96-well plates. For the probe preparation, BAC clone DNA was labeled by nick-translation. The reaction mix with final volume of 25 µl contained 0.5 µg of DNA, 0.05 mM each of unlabeled dATP, dCTP, and dGTP, and 0.015 of mM dTTP, 0.5 µl of Cy3-, or Cy5-dUTP (GE Healthcare UK Ltd, Buckingham-shire, UK), or 1 µl fluorescein-12-dUTP (Fermentas, Inc., USA), 0.05 mg/ml BSA, 2.5 µl of 10× nick translation buffer, 10 u of DNA polymerase I, and 0.0006 u of DNAse I (Fermentas, Inc., USA). DNA polymerase/DNAse ratio was selected empirically to obtain the probe with a size range from 300 to 500 base pair. For performing FISH with additional colors (besides Cy3, Cy5, and fluorescein), a pair combination of equal volumes of differently labeled probes was used.
Optimized methods for isolation of the repetitive DNA fraction for Ae. aegypti was described by Timoshevskiy et al., 2012. Genomic DNA was isolated from adult mosquitoes using Qiagen Blood & Cell Culture DNA Maxi Kit (Qiagen Science, USA). For individual extractions, approximately 500 mg of adult mosquitoes were taken. For further manipulation, DNA was dissolved in 1.2× SSC buffer to final concentration of 1 µg/µl. For shearing, a denatured DNA solution was heated at 120°C for 2 min. Reassociation of the DNA was performed at 60°C for 10 min or 15 min. After reannealing, samples were placed in ice, and 10× S1-nuclease buffers and S1 nuclease (100 U per 1 mg DNA) were added. Nuclease treatment was performed at 42°C for 1 hr. Isolated repetitive DNA fractions were precipitated by isopropanol and dissolved in TE-buffer. According to our estimation, the repetitive fractions isolated using this approach correspond to Cot2 or Cot3 DNA fraction and contained all highly repetitive and part of medium-repetitive DNA fragments (Trifonov et al., 2009). Final outcome of Cot DNA fraction accounts for ~30% of the Aedes genomic DNA. Repetitive DNA fractions of genomic DNA were utilized to suppress repetitive sequences in hybridizations to the chromosomes.
In situ hybridization was performed using a modified standard human protocol (Timoshevskiy et al., 2012). Slides were placed in 2× SSC for 30 min at 37°C, pretreated with 0.1 mg/ml of pepsin for 5 min at 37°C, denaturated in 70% formamide in 2× SSC at 72°C for 2 min, and dehydrated in a series of cold (−20°C) ethanol (70, 80, 100%) for 3–5 min each. Hybridization mix contained: 50% formamide, 10% dextran sulfate, 100 ng of each probe per slide, and 3 µg of unlabeled repetitive DNA fractions per probe. DNA/probe mix was precipitated by adding 1/10 volume of sodium acetate and 2 volumes of 100% ethanol. The DNA pellet was dissolved in “master mix” (10 µl per slide) that contained 50% formamide, 10% dextransulfate, and 1.2× SSC. After that, DNA was denatured at 96°C for 7 min. Denatured DNA was placed on ice for 1 min and incubated at 37°C for 30 min for pre-hybridization with unlabeled repetitive DNA fractions. Ten µl of hybridization mix was placed on a slide, which had been preheated to 37°C, under a 22×22 mm cover slip, and glued by rubber cement. Slides were hybridized at 37°C in a dark humid chamber overnight. After hybridization, slides were dipped for washing in a Coplin jar with 0.4× SSC, 0.3% Nanodept-40 at 72°C for 2 min, and then in 2× SSC, 0.1% Nanodept-40 at RT for 5 min. Thereafter, slides were counterstained using Prolong with DAPI (Invotrogen Corporation, USA) or incubated with 1 µM YOYO-1 solution in 1× PBS for 10 min in the dark, rinsed in 1× PBS, and then enclosed in antifade Prolong Gold (Invitrogen Corporation, USA) under a cover slip. Slides were analyzed using a Zeiss LSM 510 Laser Scanning Microscope (Carl Zeiss Microimaging, Inc., USA) at 1000× magnification.
To develop idiograms, the best images of the chromosomes from IDs stained with YOYO-1 were selected. The colored images were converted into black and white images and contrasted in Adobe Photoshop as described previously . The chromosomal images were straightened using ImageJ program  and were aligned for comparison. In total, ~90 chromosomes at early metaphase were analyzed. FISH images were also filtered using ImageJ program . For ordering genetic markers, chromosomes at various levels of condensation were used. Prometaphase and early metaphase chromosomes were utilized for assigning genetic markers to the particular chromosome bands. Prophase and polytene chromosomes were used for ordering markers within the same chromosome band. From 10 to 20 images were analyzed to obtain reproducible ordering patterns.
Measurements and statistics
Chromosomes were measured as described previously  using Zen 2009 Light Edition software . The relationship between the physical locations of markers and their linkage positions was assessed by assigning genes of known physical position an integer score. These scores were 1–26 (1p3.4–1q4.4) on chromosome 1, 1–36 (2p4.4–2q4.4) on chromosome 2, and 1–32 (3p4.4–3q4.4) on chromosome 3. This integer score was then regressed upon the cM position of the gene as determined in a number of previous independent linkage mapping studies and F1 intercross families. Linear regression analysis was performed using R (2.14.1) . These regression models were then used to predict the physical position of the markers for which we have linkage positions in cM.
Results and Discussion
Cytogenetic map of mitotic chromosomes of Ae. aegypti
Our previous study developed preliminary idiograms – diagrammatic representations of the chromosome banding patterns – for the mid-metaphase chromosomes of Ae. aegypti . This stage of mitosis is the most representative in any chromosome preparation. At mid metaphase, chromosomes and chromosome arms can be easily distinguished from each other based on their length and presence of specific landmarks. Chromosomes on preliminary idiograms were not divided into divisions and subdivisions, and these idiograms served only for chromosome and chromosome arm identification. In the current study, we developed idiograms for the chromosomes of Ae. aegypti at an earlier stage of mitosis – early metaphase. The average chromosome lengths at this stage are 11.86, 16.19, and 13.64 µm for chromosomes 1, 2, and 3, respectively, or ~5.5 µm longer than at mid metaphase. At stages of mitosis previous to metaphase, such as prophase and prometaphase, homologous chromosomes of Ae. aegypty are usually tightly paired . Although chromosomes at these stages are longer than at early metaphase, the banding patterns of the chromosomes are variable. At early metaphase, chromosomes finally segregate from each other, resulting in a visible number of chromosomes becoming equal to 6 and chromosome patterns becoming more reproducible (Figure 1A). We consider this stage of mitosis as the most reliable for the development of the chromosome map, which can be used for the detailed physical mapping.
Figure 1. The construction of idiograms for mitotic chromosome of Aedes aegypti.
Early metaphase chromosomes of Ae. aegypti stained with YOYO-1 iodide (A) were utilized for idiogram (B) development. Chromosome numbers are shown on the top of each chromosome. Chromosomal arms p and q and numbered divisions and subdivisions are shown on the left side of the idiograms. Landmarks are indicated by asterisks.doi:10.1371/journal.pntd.0002052.g001
Similarly to our previous study , we used chromosome images stained with YOYO-1 iodide. This dye provides much clearer banding patterns as compared with the most commonly used DAPI (4′,6-diamidino-2-phenylindole fluorescent stain). Images of the chromosomes were converted into black and white images (Figure 1A) and straightened. Similarly to the idiograms of human chromosome , we identified chromosome bands of 4 different intensities – intense, medium intensity, low intensity, and negative (Figure 1B). Chromosomes were finally subdivided into 23 numbered divisions and 94 bands. The following regions can be considered as landmarks for the chromosome arm recognition: intense band in division 1q21; intense double band in divisions 2q21–23; and 2 low-intensity bands in region 3q32, 3q34. These regions are shown by asterisks on Figure 1. Large negative bands indicate the boundaries between all divisions on the chromosomes.
Chromosome idiograms constructed in this study represent the first cytogenetic map developed for mitotic chromosomes of Ae. aegypti. In studies conducted before on chromosomes from cell lines of Ae. aegypti, the positions of the markers on the chromosomes were measured by FLpter: a fractional length from the short-arm telomeric end p-terminus . As a result, this mapping provides only approximate coordinates for the markers. The idiograms recently developed for mid-metaphase chromosome  were designed mostly for individual chromosome and chromosome arm recognition. The map for early metaphase chromosome presented here is designed for the more detailed band-based mapping. It finally permits assignment of the location of the specific DNA signals to the particular numbered subdivision on the chromosomes.
A “two-step” approach to physical mapping
Previous efforts identified 106 BAC clones that carry genetically mapped marker sequences . We used a “two-step” physical mapping approach for 1) assigning BAC clones to the chromosomal bands and 2) ordering them within the band. For the first step, we utilized FISH on chromosomes stained with the green dye YOYO-1 iodide. BAC clone DNA was labeled with Cy3 (red) and Cy5 (infrared) fluorescent dyes. Examples of FISH results on early metaphase chromosomes are shown in Figure 2. Each FISH allowed us to place two BAC clones to a specific band on idiograms. Eight BAC clones produced more than one hybridization signal. In these cases, the most intense signal was considered as a major position of the BAC clone on the chromosomes. In total, 100 out of 106 BAC clones were successfully assigned to specific bands on Ae. aegypti chromosomes (Table 1).
Figure 2. FISH on early metaphase chromosomes of Aedes aegypti.
BAC DNA probes labeled by CY3 (red) and Cy5 (blue) were hybridized to the chromosomes stained with YOYO-1 iodide. Positions of the BAC clones on chromosomes 1 (A), 2 (B), and 3 (C) are indicated by arrows.doi:10.1371/journal.pntd.0002052.g002
Table 1. Chromosome locations of genetic markers and genomic supercontigs.doi:10.1371/journal.pntd.0002052.t001
For ordering BAC clones within one band, FISH was performed on prophase chromosomes from imaginal discs or, for higher resolution, on polytene chromosomes from salivary glands of 4th instar larvae of Ae. aegypti. Probes were labeled with three different dyes: fluorescein (green), Cy3 (red), and Cy5 (infrared), or with a combination of these dyes (Figure 3). Chromosomes after FISH were stained with DAPI (ultraviolet). This approach allowed mapping of up to 6 BAC clones simultaneously. Our FISH results showed that two probes have to be separated by a distance of ~0.5 Mb on prophase chromosomes in order to be distinguished from each other (Figure 3A). The resolution of mapping using polytene chromosomes was even higher, ~300 kb (Figure 3D). As a result of this additional mapping, all 100 BAC clones were placed in correct order on the chromosomes (Figure 4).
Figure 3. Multicolor FISH on mitotic and polytene chromosomes of Aedes aegypti.
DNA probes labeled with fluorescein, Cy3, Cy5, and combinations of these dyes were hybridized to the prophase (A, B, C) and polytene chromosomes (D) stained by DAPI. The maximum resolutions of ~0.5 Mb between markers LF179 and LF314 (A) and 300 kb between markers LF407 and Amyl (C) are obtained on prophase and polytene chromosomes, respectively.doi:10.1371/journal.pntd.0002052.g003
Figure 4. Integrated linkage, chromosome, and genome map–iMap of Ae. aegypti.
Chromosome divisions and subdivisions are indicated on the left sides of the idiograms. The positions of genetic markers are shown on the right sides of the idiograms. The numbers of supercontigs in brackets are indicated by last 2–4 digits of supercontig ID. Anchor markers for dengue virus 2 (DEN2) midgut infection barrier (MIB) QTL are in purple; for DEN2 midgut escape barrier (MEB) QTL – in brown; filarial worm QTL - in blue; malaria parasite QTL – in green; for sex determination locus - in red. LF 98 is QTL anchor marker for both filarial worm and malaria parasite pathogens. The orientations of 4 supercontigs are demonstrated by arrows. Major locations of the BAC clones with multiple signals on the chromosomes are indicated by asterisks. Two BAC clones and 3 supercontigs in conflict with previous genetic mapping/genome assembly are in bold.doi:10.1371/journal.pntd.0002052.g004
The physical map constructed in this study is the most populated physical map developed for Ae. aegypti thus far. Our current mapping effort placed 100 BAC clones and an 18S rDNA probe to their particular regions on the chromosomes. The “two-step” mapping approach significantly improved the resolution of the mapping. Using long prophase chromosomes and low-polytenized chromosomes from salivary glands, in addition to early metaphase chromosomes, provided the resolution similar to that obtained on polytene chromosomes from ovaries of An. gambiae, which is equal to ~100 kb . The current study developed a simple and robust technique for high-resolution physical mapping that can be further applied for more detailed physical mapping of the Ae. aegypti genome and other mosquito genomes. Similar to studies conducted on Drosophila –, the physical mapping approach based on the banding patterns of mitotic chromosomes can also be used for the additional mapping of An. gambiae heterochromatin, which is under-replicated in normal polytene chromosomes.
Integrating chromosome map with linkage and genome map of Ae. aegypti
Mapping of the BAC clones that carry particular genetic markers allowed us to clarify the order of the genetic markers (Figure 4). Genetic markers physically mapped in this study span the entire chromosome complement. The longest chromosome 2 was the most densely populated with 45 genetic markers. The highest number of markers was found in areas close to the telomeres, especially on the p arm of chromosome 2. In contrast to the previous study , some markers were located around the centromeres. Surprisingly, two areas in the middle of the short arms on chromosome 1 and 2 (regions 1p2 and 2p2) had extremely low density of markers. A linear regression analysis demonstrated a good overall correlation between positions of the markers on the physical and linkage maps: R2 equaled to 0.69, 0.73, and 0.86 for chromosomes 1, 2, and, 3 respectively (Figure 5). On average, 1 cM on the linkage map corresponds to the half of a cytogenetic band or to 6.88 Mbs on the physical genome map. However, we found large discrepancies between the two maps with respect to the distances among markers located in areas near the centromeres and telomeres. These discrepancies probably caused by the high rate of recombination near telomeres and the low rate of recombination near the centromeres.
Figure 5. Linear regression analyses of the physical position of a gene as a function of its cM position.
For chromosomes 1 (A), 2 (B), and 3 (C), the linear regression model is provided along with the probability that the slope is zero and the proportion of the total variance accounted for by the linear model (R2).doi:10.1371/journal.pntd.0002052.g005
Based on previous studies, we were able to physycally map the positions of the QTLs related to the ability of Ae. aegypti to transmit different pathogens. The QTLs associated with the transmission of dengue virus 2 (DEN2) , ; filarioid nematode Brugia malayi  and the avian malaria parasite Plasmodium gallinaceum ,  are indicated by different colors on Figure 4. As a result of physical mapping, 12 QTLs on the linkage map “collapsed” into five clusters of QTLs on the chromosome map in regions: 1p31–34; 2p33–42; 2q31–32 and 3p31–32 (Figure 6). Interestingly, four QTLs on 2p arm related to the transmission of various pathogens, such as filarioid nematode, avian malaria parasite, and dengue virus 2, were placed by different studies within a large region on the linkage map (31.8 cM or about 50% of chromosome 2). However, they were physically mapped within four chromosomal bands, which encompass only ~11% of chromosome 2. These results suggest that the susceptibility of Ae. aegypti to diverse pathogens is controlled by fewer genomic loci than it was previously considered.
Figure 6. Localization of QTLs to various pathogens on linkage and chromosome maps of Aedes aegypti.
The linkage positions of QTLs in cM on linkage groups I, II, and III are indicated on the left side. QTLs to dengue virus 2 (DEN2), midgut infection barrier (MIB), DEN2 midgut escape barrier (MEB), malaria parasite, and filarial worm are shown on the right sides of chromosomes 1, 2, and 3.doi:10.1371/journal.pntd.0002052.g006
In addition to QTLs, the location of marker LF284, an anchoring marker for the sex determination locus , was also determined on chromosome 1 (Figure 4). This marker was localized in the intensively stained band in region 1q21. This region is located next to the ribosomal locus in negative band 1q22 that usually forms secondary constriction and can be easily identified on the chromosomes. Two BAC clones with markers AEGI10 and LF231 were found in conflict with previous mapping positions on different chromosomes. This result is not unexpected, as the genetic linkage map is a composite based on results of multiple independent genetic crosses .
Finally, the availability of the Ae. aegypti genome allowed us to map 100 genomic supercontigs to the chromosomes (Figure 4). Four supercontigs—1.123, 1.219, 1.14, and 1.1, which contained two or more genetic markers,—were oriented on the chromosomes. The orientation of these supercontigs is indicated by arrows on Figure 4. Physical mapping also helped us to identify potentially misassembled supercontigs if two or more BAC clones located in the same genomic supercontigs were mapped to different chromosomes. Our data suggests that three genomic supercontigs 1.148, 1.1, and 1.209 were misassembled in the previous study . Potentially misassembled supercontigs are indicated in bold on Figure 4. In total, our mapping effort placed 183 Mb of genomic supercontigs, which is equal to 13.3% of the genome, to the chromosomes. The chromosome-based genome map for Ae. aegypti developed in this study is the second after the An. gambiae genome map developed for mosquitoes , , .
The genomes of the three most dangerous for the human health species of mosquitoes—Aedes aegypti, Anopheles gambiae, and Culex quinquefasciatus—were sequenced in the last decade. The genome of Ae. aegypti is the largest among the three species and consists of 1,376 Mb. Our physical mapping effort incorporated 94 cytogenetic bands, 100 molecular genetic markers, and 183 Mb of the genome into one iMap of Ae. aegypti. The locations of anchor markers for QTLs related to dengue virus, filarial nematode, and malaria parasite transmission were determined on the chromosomes, as well as for the sex determination locus. Our discovery of the localization of multiple “unrelated” QTLs in a few major chromosome clusters suggests a possibility that the transmission of different pathogens is controlled by the same genomic loci. The study also demonstrated that physical mapping can orient genomic supercontigs and identify potential mistakes in genome assembly. Thus, the iMap developed here will facilitate the identification of genomic determinants of traits responsible for susceptibility or refractoriness of the mosquito to diverse pathogens and will also guide future efforts to improve the assembly of Ae. aegypti genome.
Conceived and designed the experiments: MVS DWS. Performed the experiments: VAT BSD. Analyzed the data: VAT WCB IVS. Contributed reagents/materials/analysis tools: DWS. Wrote the paper: MVS IVS.
- 1. Gubler DJ (2012) The economic burden of dengue. Am J Trop Med Hyg 86: 743–744. doi: 10.4269/ajtmh.2012.12-0157
- 2. WHO (2009) Dengue. Guidelines for Diagnosis, Treatment, Prevention and Control. World Health Organization Geneva, Switzerland.
- 3. Halasa YA, Shepard DS, Zeng W (2012) Economic cost of dengue in puerto rico. Am J Trop Med Hyg 86: 745–752. doi: 10.4269/ajtmh.2012.11-0784
- 4. Morens DM, Fauci AS (2008) Dengue and hemorrhagic fever: a potential threat to public health in the United States. Jama 299: 214–216. doi: 10.1001/jama.2007.31-a
- 5. Gould EA, Solomon T (2008) Pathogenic flaviviruses. Lancet 371: 500–509. doi: 10.1016/s0140-6736(08)60238-x
- 6. Severson DW (2008) Mosquito. In: Kole C, Hunter W, editors. Genome Mapping and Genomics in Animals. Berlin Heidelberg: Springer-Verlag. pp. 69–91.
- 7. Coker WZ (1958) The inheritance of DDT resistance in Aedes aegypti. Ann Trop Med Parasitol 52: 443–455.
- 8. McClelland GAH (1962) Sex-linkage in Aedes aegypti. Trans roy Soc trop Med Hyg 56: 4.
- 9. McDonald PT, Rai KS (1970) Correlation of linkage groups with chromosomes in the mosquito Aedes aegypti. Genetics 66: 475–485.
- 10. Craig GBJ, Hickey WA (1967) Genetics of Aedes aegypti; Wright JW, Pal R, editors. Amsterdam, London, New York: Elsevier.
- 11. Munstermann LE, Craig GBJ (1979) Genetics of Aedes aegypti. Updating the linkage map. The Journal of Heredity 70: 291–296.
- 12. Munstermann L (1990) Linkage map for yellow fever mosquito, Aedes aegypti; O'Brein S, editor. New York: Cold Spring Harbor Laboratories, Cold Spring Harbor.
- 13. Severson DW, Mori A, Zhang Y, Christensen BM (1993) Linkage map for Aedes aegypti using restriction fragment length polymorphisms. J Hered 84: 241–247.
- 14. Antolin MF, Bosio CF, Cotton J, Sweeney W, Strand MR, et al. (1996) Intensive linkage mapping in a wasp (Bracon hebetor) and a mosquito (Aedes aegypti) with single-strand conformation polymorphism analysis of random amplified polymorphic DNA markers. Genetics 143: 1727–1738.
- 15. Zhong D, Menge DM, Temu EA, Chen H, Yan G (2006) Amplified fragment length polymorphism mapping of quantitative trait loci for malaria parasite susceptibility in the yellow fever mosquito Aedes aegypti. Genetics 173: 1337–1345. doi: 10.1534/genetics.105.055178
- 16. Chambers EW, Meece JK, McGowan JA, Lovin DD, Hemme RR, et al. (2007) Microsatellite isolation and linkage group identification in the yellow fever mosquito Aedes aegypti. J Hered 98: 202–210. doi: 10.1093/jhered/esm015
- 17. Severson DW, Mori A, Zhang Y, Christensen BM (1994) Chromosomal mapping of two loci affecting filarial worm susceptibility in Aedes aegypti. Insect Mol Biol 3: 67–72. doi: 10.1111/j.1365-2583.1994.tb00153.x
- 18. Severson DW, Thathy V, Mori A, Zhang Y, Christensen BM (1995) Restriction fragment length polymorphism mapping of quantitative trait loci for malaria parasite susceptibility in the mosquito Aedes aegypti. Genetics 139: 1711–1717. doi: 10.1534/genetics.105.055178
- 19. Bosio CF, Fulton RE, Salasek ML, Beaty BJ, Black WC (2000) Quantitative trait loci that control vector competence for dengue-2 virus in the mosquito Aedes aegypti. Genetics 156: 687–698.
- 20. Gomez-Machorro C, Bennett KE, del Lourdes Munoz M, Black WC (2004) Quantitative trait loci affecting dengue midgut infection barriers in an advanced intercross line of Aedes aegypti. Insect Mol Biol 13: 637–648. doi: 10.1111/j.0962-1075.2004.00522.x
- 21. Sharma GP, Mittal OP, Chaudhry S, Pal V (1978) A preliminary map of the salivary gland chromosomes of Aedes (Stegomyia) aegypti (Culicadae, Diptera). Cytobios 22: 169–178.
- 22. Campos J, Andrade CF, Recco-Pimentel SM (2003) A technique for preparing polytene chromosomes from Aedes aegypti (Diptera, Culicinae). Mem Inst Oswaldo Cruz 98: 387–390. doi: 10.1590/s0074-02762003000300017
- 23. Rai KS (1963) A comparative study of mosquito karyotypes. Ann Entomol Soc Amer 56: 160–170.
- 24. Motara MA, Rai KS (1977) Chromosomal differentiation in two species of Aedes and their hybrids revealed by Giemsa C-banding. Chromosoma 64: 125–132. doi: 10.1007/bf00327052
- 25. Motara MA, Rai KS (1978) Giemsa C-banding patterns in Aedes (Stegomia) mosquitoes. Chromosoma 70: 51–58. doi: 10.1007/bf00292215
- 26. Newton ME, Southern DI, Wood RJ (1974) X and Y chromosmes of Aedes aegypti (L.) distiguished by Giemsa C-banding. Chromosoma 49: 41–49. doi: 10.1007/bf00284986
- 27. Motara MA, Pathak S, Satya-Prakash KL, Hsu TC (1985) Agrentophilic structures of spermatogenesis in the yellow fever mosquito. J Hered 76: 295–300.
- 28. Kumar A, Rai KS (1990) Chromosomal localization and copy number of 18S+28S ribosomal RNA genes in evolutionary diverse mosquitoes (Diptera, Culicidae). Hereditas 113: 277–289. doi: 10.1111/j.1601-5223.1990.tb00094.x
- 29. Brown SE, Menninger J, Difillipantonio M, Beaty BJ, Ward DC, et al. (1995) Toward a physical map of Aedes aegypti. Insect Mol Biol 4: 161–167. doi: 10.1111/j.1365-2583.1995.tb00021.x
- 30. Brown SE, Severson DW, Smith LA, Knudson DL (2001) Integration of the Aedes aegypti mosquito genetic linkage and physical maps. Genetics 157: 1299–1305.
- 31. Nene V, Wortman JR, Lawson D, Haas B, Kodira C, et al. (2007) Genome sequence of Aedes aegypti, a major arbovirus vector. Science 316: 1718–1723. doi: 10.1126/science.1138878
- 32. Holt RA, Subramanian GM, Halpern A, Sutton GG, Charlab R, et al. (2002) The genome sequence of the malaria mosquito Anopheles gambiae. Science 298: 129–149. doi: 10.1126/science.1076181
- 33. Arensburger P, Megy K, Waterhouse RM, Abrudan J, Amedeo P, et al. (2010) Sequencing of Culex quinquefasciatus establishes a platform for mosquito comparative genomics. Science 330: 86–88. doi: 10.1126/science.1191864
- 34. Jimenez LV, Kang BK, deBruyn B, Lovin DD, Severson DW (2004) Characterization of an Aedes aegypti bacterial artificial chromosome (BAC) library and chromosomal assignment of BAC clones for physical mapping quantitative trait loci that influence Plasmodium susceptibility. Insect Mol Biol 13: 37–44. doi: 10.1046/j.0962-1075.2004.00456.x
- 35. Sharakhova MV, Timoshevskiy VA, Yang F, Demin S, Severson DW, et al. (2011) Imaginal discs–a new source of chromosomes for genome mapping of the yellow fever mosquito Aedes aegypti. PLoS Negl Trop Dis 5: e1335. doi: 10.1371/journal.pntd.0001335
- 36. Steiniger GE, Mukherjee AB (1975) Insect chromosome banding: technique for G- and Q-banding pattern in the mosquito Aedes albopictus. Can J Genet Cytol 17: 241–244.
- 37. Timoshevskiy VA, Sharma A, Sharakhov IV, Sharakhova MV (2012) Fluorescent in situ Hybridization on Mitotic Chromosomes of Mosquitoes. J Vis Exp doi: 10.3791/4215
- 38. Macdonald WW (1962) Selection of a strain of Aedes aegypti susceptible to infection with semi-periodic Brugia malayi. Ann Trop Med Parasotol 56: 368–372.
- 39. Demin S, Pleskach N, Svetova M, Solovjeva L (2010) High-resolution mapping of interstitial teleomeric repeats in Syrian hamster metaphase chromosomes. Cytogenetic and Genome Research DOI: 10.1159/000321676: 1–5. doi: 10.1159/000321676
- 40. NIH website. Available: http://rsb.info.nih.gov/ij/. Accessed 2011 Mar 10.
- 41. Zeiss website. Available: http://www.zeiss.de. Accessed 2010 Dec 5.
- 42. R Development Core Team (2008) A language and environment for statistical computing. R Foundation for Statistical Computing Vienna, Austria, ISBN 3-900051-07-0, URL. Available: http://www.R-project.org. Accessed 2012 Oct 26.
- 43. Shaffer LG, Slovak ML, Campbell LJ (2009) An international system for human cytogenetic nomenclature. Basel (Switzerland): Karger.
- 44. Sharakhova MV, Hammond MP, Lobo NF, Krzywinski J, Unger MF, et al. (2007) Update of the Anopheles gambiae PEST genome assembly. Genome Biol 8: R5. doi: 10.1186/gb-2007-8-1-r5
- 45. Hoskins RA, Smith CD, Carlson JW, Carvalho AB, Halpern A, et al. (2002) Heterochromatic sequences in a Drosophila whole-genome shotgun assembly. Genome Biol 3: RESEARCH0085.
- 46. Corradini N, Rossi F, Verni F, Dimitri P (2003) FISH analysis of Drosophila melanogaster heterochromatin using BACs and P elements. Chromosoma 112: 26–37. doi: 10.1007/s00412-003-0241-9
- 47. Dimitri P, Corradini N, Rossi F, Verni F, Cenci G, et al. (2003) Vital genes in the heterochromatin of chromosomes 2 and 3 of Drosophila melanogaster. Genetica 117: 209–215. doi: 10.1023/a:1022996112742
- 48. Rossi F, Moschetti R, Caizzi R, Corradini N, Dimitri P (2007) Cytogenetic and molecular characterization of heterochromatin gene models in Drosophila melanogaster. Genetics 175: 595–607. doi: 10.1534/genetics.106.065441
- 49. Severson DW, Meece JK, Lovin DD, Saha G, Morlais I (2002) Linkage map organization of expressed sequence tags and sequence tagged sites in the mosquito, Aedes aegypti. Insect Mol Biol 11: 371–378. doi: 10.1046/j.1365-2583.2002.00347.x
- 50. George P, Sharakhova MV, Sharakhov IV (2010) High-resolution cytogenetic map for the African malaria vector Anopheles gambiae. Insect Mol Biol 19: 675–682. doi: 10.1111/j.1365-2583.2010.01025.x