Genome sequencing and comparative genomics of honey bee microsporidia, Nosema apis reveal novel insights into host-parasite interactions
© Chen et al.; licensee BioMed Central Ltd. 2013
Received: 14 March 2013
Accepted: 1 July 2013
Published: 5 July 2013
The microsporidia parasite Nosema contributes to the steep global decline of honey bees that are critical pollinators of food crops. There are two species of Nosema that have been found to infect honey bees, Nosema apis and N. ceranae. Genome sequencing of N. apis and comparative genome analysis with N. ceranae, a fully sequenced microsporidia species, reveal novel insights into host-parasite interactions underlying the parasite infections.
We applied the whole-genome shotgun sequencing approach to sequence and assemble the genome of N. apis which has an estimated size of 8.5 Mbp. We predicted 2,771 protein- coding genes and predicted the function of each putative protein using the Gene Ontology. The comparative genomic analysis led to identification of 1,356 orthologs that are conserved between the two Nosema species and genes that are unique characteristics of the individual species, thereby providing a list of virulence factors and new genetic tools for studying host-parasite interactions. We also identified a highly abundant motif in the upstream promoter regions of N. apis genes. This motif is also conserved in N. ceranae and other microsporidia species and likely plays a role in gene regulation across the microsporidia.
The availability of the N. apis genome sequence is a significant addition to the rapidly expanding body of microsprodian genomic data which has been improving our understanding of eukaryotic genome diversity and evolution in a broad sense. The predicted virulent genes and transcriptional regulatory elements are potential targets for innovative therapeutics to break down the life cycle of the parasite.
KeywordsMicrosporidia Nosema Honey bees Genome Comparative genomics
Microsporidia are obligate intracellular parasites that comprise over 1,200 described species belonging to 143 genera and infect members of almost all animal phyla [1–3]. Until recently, microsporidia were regarded as primitive amitochondriate protozoa, because they do not possess typical eukaryotic organelles such as mitochondria, peroxisomes, and classical stacked Golgi apparati. In addition, ribosomal RNAs of microsporidia present some prokaryote-like features by harboring 16S and 23S rRNA genes and lacking the 5.8S rRNA in their large ribosomal subunit that is characteristic of eukaryotes . However, this putatively ancient origin of microsporidia has been contested and redefined. Recent data has shown the presence of a mitosome, a mitochondrion-derived organelle , and genes encoding proteins of mitochondrial origin such as heat shock protein 70 in microsporidia [6, 7]. This suggests that microsporidia once had mitochondria and lost them through the course of evolution. Based on the aforementioned factors, in conjunction with their possession of characteristic traits of closed mitosis and spores that contain chitin and trehalose, as fungi do , microsporidia have been classified as the earliest diverging clade of sequenced fungi  that underwent substantial genetic changes during adaptive evolution.
Nosema apis and N. ceranae (Family: Nosematidae, Genus: Nosema) are two microsporidia species that infect honey bees. Like other microsporidia, the infective form of the Nosema is the resistant spore, which is surrounded by an outer layer consisting of an electron-dense glycoprotein exospore and an electron-lucent chitinous endospore layer separated from the cell by a thin plasma membrane. The spore possesses a polar tubule which is considered to be a specialized product of the Golgi apparatus and the posterior vacuole at the posterior pole of the spore has been postulated to function as a peroxisome [10–12]. In the midgut of the host, the spore germinates and extrudes its polar tubule and injects the infective sporoplasm into the host intestinal epithelium. Inside the host cell cytoplasm, the sporoplasm undergoes divisions by binary fission (merogony) or multiple fission (schizogony) and spore production by formation of a thick wall around the spore (sporogony). Repeated multiplication results in the host cell becoming completely filled with spores and eventually rupturing to release the spores into surroundings cells  and to spread to other tissues [14, 15]. Mature spores excreted in feces can also infect other hosts, providing new sources of the infection in bee colonies . Parasitism by Nosema impairs the host’s metabolism and reproduction, and causes a destructive disease known as nosemosis, a digestive disorder that shortens honey bee lifespan, retards colony development, decimates bee populations, and causes colony queen supersedure [17–22]. N. ceranae as a destructive intracellular parasite not only directly causes a serious disease in honey bees but also has the potential to compromise the physical and immunological barriers of honey bees toward disease, leaving bees more susceptible to other pathogens and senescence [23–25]. New evidence shows that interactions between N. ceranae and neuro-active pesticides, neonicotinoids which have been used for controlling pests in the IPM system, could synergistically and negatively affect honey bee survival and significantly contribute to colony depopulation [26–30]. So far, the only registered treatment for Nosema disease is fumagillin, whose use is forbidden in Europe because it has no established Maximun Residue Level (MRL). With prolonged use of fumagillin, disease resistance to treatment has become an issue . As a result, additional therapeutic options are urgently needed.
European honey bees, Apis mellifera, are the most important insect pollinator and are responsible for the pollination of one third of agricultural food crops in the world with an estimated value of $216/€153 billion per year . For decades, nosema disease was exclusively attributed to N. apis, first described in 1909 . In 2005, a natural infection of another microsporidia species, N. ceranae, which was first found in the Asian honey bee Apis cerana, was identified in A. mellifera colonies [35, 36]. Subsequently, N. ceranae has become the predominant infection of two bee species [37–41] and has been implicated in honey bee Colony Collapse Disorder (CCD) [15, 19, 42–44], a malady that has decimated honey bee colonies across the U.S. and around the world [45–47]. The emergence of N. ceranae has changed the epidemiological pattern of honey bee nosemosis, resulting in an urgent need for elucidating the genetic basis that defines the epidemiology and pathogenicity of the Nosema species.
Microsporidia genomes are highly reduced and compact in nature. The size of microsporidia genomes has been determined for sixteen microsporidia species mostly based on karyotyping analysis and EST surveys and varies considerably, ranging from 2.3 to 23 Mbp (reviewed in [48, 49]). The first full genome sequence of a microsporidia species, Encephalitozoon cuniculi, marked a significant milestone in the study of microsporidia biology . The genome organization and gene content of E. cuniculi represents the first evidence of microsporidia genomic reduction (2.9 Mb) and has provided considerable functional insight on the evolution of microsporidia-host relationships at the biochemical and molecular levels. Since then, seven additional microsporidia genomes have been sequenced [51–57].
In 2009, using the whole-genome shotgun (WGS) sequencing approach, we sequenced, annotated, and analyzed the complete genome of N. ceranae at 25X coverage , which represents a second full genome sequence of microsporidia. Like many microsporidia, N. ceranae has a highly reduced and compact genome with a draft assembly of 7.86 Mbp. A total of 2,641 putative protein-coding genes were identified based on computational analysis of the N. ceranae genome sequences. By comparing the N. ceranae putative protein-coding genes with those of fully sequenced E. cuniculi as well as with yeast, Saccharomyces cerevisiae, about 50% of N. ceranae genes appeared to be conserved among microsporidia. These microsporidia specific genes are of special interest for identification of potential virulence factors and elucidation of molecular mechanisms of intracellular invasion of these obligate intracellular parasites. We have now extended our efforts for genome-wide analysis of insect microsporidia to a second species, N. apis which is the first described microsporidia species of honey bees. In this report, we present a draft sequence of the N. apis genome and an annotation of the N. apis genome at the nucleotide and protein levels. We undertake comparative analyses of N. apis with its sympatric congener N. ceranae in order to identify candidates of species-specific coding sequences that may be associated with adaptation and virulence of the intracellular parasites. We hope that our genomic studies of honey bee microsporidia parasites will lead to greater understanding of the biology and pathogenesis of these difficult-to-treat fungal pathogens and contribute to the worldwide efforts to manage honey bee diseases and improve pollination services provided by honey bees.
Results and discussion
Species specificity of N. Apis
General features of N. Apisgenome assembly
N. apis genome assembly statistics
Number of Total Scaffold
Minimum Scaffold Span
Maximum Scaffold Span
Mean Span of Scaffolds
Total Bases in Scaffold
Number of Total Contigs
Minimum Contig Length
Maximum Contig Length
Mean Contig Length
Contents of the N. Apisgenome
Main features of the N. apis genome in comparison with N. ceranae
GC percentage (total genome) (%)
GC percentage in coding sequences (%)
GC percentage in 3rd position
tRNA genes (#)
Protein coding genes (CDSs)
Gene density (genes/kb)
Percent coding (%)
The N. apis genome is very AT rich, with an overall GC content of 18.78%, 7.2% lower than that of N. ceranae. The protein coding regions have significantly higher GC content (25%) compared to the overall GC content for the entire genome, indicating that GC content is not uniformly distributed across the genome and supporting the notion that GC content is higher in coding regions than in non-coding regions. The GC content also varies by codon position, with the 1st and 2nd positions of the coding regions having greater GC content than the third (synonymous) position.
The predictions by SignalP and TMHMM showed that 399 proteins contained putative signal peptides with over 70% of the probability and significantly high C, S and Y scores and that 348 proteins contained putative transmembrane segments of some form with a score of equal or more than 0.3. Of 348 proteins that had membrane-spanning domains, 114 were predicted to contain an amino-terminal signal peptide. The signal peptides, and transmembrane motifs are also included in the dataset (Additional file 4: Table S1).
The combination of noncoding RNA (ncRNA) prediction programs and BLAST similarity search algorithms identified tRNA genes, rRNA gene clusters (16S, 23S and 5S), and small nuclear RNA (snRNA) genes. Both ARAGORN and tRNAscan-SE yielded similar results for tRNA prediction and showed a diversity of tRNA genes in the N. apis genome. There were 62 tRNA genes from ARAGORN and 58 genes from tRNAscan-SE as well as 16 tRNA-derived pseudogenes in tRNAscan-SE. By combining predictions from two tRNA prediction programs, there were 60 overlapping tRNAs with 42 distinct anticodons and gene lengths of 57 to 68 nucleotides. The 16S, 23S, and 5S rRNA genes were organized as a typical co-transcribed operon and arranged in order of 16S-23S-5S separated by two internal transcribed spacers (ITSs) in a tandemly repeated manner. The 16S, 23S, and 5S genes were identified in twenty-six scaffolds and four scaffolds contain a complete locus of 16S, 23S, and 5S genes. The sequence comparisons revealed polymorphisms among copies of rRNA genes and ITSs with the majority of polymorphisms found in the IGS region. The degree of intragenomic variability observed in 23S rRNA genes was greater than in 16S and 5S rRNA genes. While both 16S and 5S genes displayed 2% intragenomic variability, the average intragenomic variability observed it the 23S genes was about 10% with one 23S rRNA gene showing extreme divergence and sharing only 82% nucleotide sequence homology with the other 23S rRNA genes. While sequence alignment identified short conserved sequence motifs in ITSs, the intragenomic variability observed in ITSs was demonstrated not only by nucleotide substitutions but also by length variance across the genome.
The comparison of the 2,771 putative N. apis proteins with the 2,614 N. ceranae proteins revealed a broadly similar gene set shared between N. apis and N. ceranae. The reciprocal best BLAST search comparing the N. apis gene set and N. ceranae gene set yielded 1,356 one-to-one orthologs that were each other’s mutual best matches; thus, the orthologs corresponded to 49% of N. apis genes and 52% of N. ceranae gene sets. Of 1,356 ortholog pairs for both N. apis and N. ceranae, 137 orthologs had multiple hits in N. apis, suggesting the presence of paralogous proteins. The list of ortholog pairs in the genome of N. apis and N. ceranae can been found in Additional file 5: Table S2.
Functional annotation of protein coding genes
N. apis s equences that show homology to annotated and experimentally verified pathogenicity and virulence genes of microsporidia species
Homologous to N. ceranae
Organism whose annotated sequence has top BlastP hit
1) Polar Tube Protein
Host cell invasion
2) Spore Wall Protein
Structural capacity &
host cell adhesion
4) Chitin synthase
6) Mitogen-activated protein kinase
7) ATP/ADP Translocase
9) Splicing machinery
9) Putative secretive proteins (399 proteins listed in Additional file 4: Table S1)
Virulence factors are molecules expressed and secreted by parasites that are keys for causing disease in the host as the parasites enter into and exit out of host cells, and inhibit certain host functions. Genome analysis of N. apis has identified genes encoding a wide array of potential virulence determinants. These potential virulence factors of N. apis include genes encoding 1) polar tube proteins defining structure and invasion mechanisms; 2) spore wall and anchoring proteins involved in host tissue recognition and the initiation of host cell invasion; 3) endochitinase and chitin synthase involved in spore-host cell attachment; 4) proteins involved in pathogenicity regulations and energy parasitism, 5) components of the spliceosome machinery that plays a major role in the generation of proteomic diversity and proteins regulating splicing activity, and 6) putative secretive proteins that are involved in interactions with the host and are essential for modulation of host immunity towards successful completion of the parasite lifestyle in the host (Table 3).
Functional conservation and divergence of protein sequences between N. Apis and N. Ceranae
While putative proteins of N. apis share significant sequence homology and functional similarity for enriched GO terms with N. ceranae, the comparison of the GO terms based on Fisher’s exact test after a false discovery rate correction (p < 0.05) displayed some differences between the two species. Comparison of biological processes (Figure 8A) showed that genes involved in the developmental process, organismal development, signaling, kinase activity, translational activity were on the same level of abundance for both species. However, genes that are functionally linked to cell amino acid derivative metabolic process and reproduction were significantly more common in N. apis than in N. ceranae. In contrast, genes involved in metabolic processes and stress response were greatly expanded in N. ceranae. The protein transport genes were also found to have greater representation in N. ceranae than in N. apis. N. apis and N. ceranae also displayed different protein profiles responsive to stress and stimuli. Genes responsive to stress were over represented in N. ceranae compared to N. apis, while N. apis contained a slightly greater number of genes responding to abiotic stimuli. Both species had about the same number of genes related to responses to endogenous stimuli. While cell homeostasis and response to external stimulus genes were only identified in N. ceranae, symbiosis and encompassing, mutualism through parasitism genes were unique to N. apis. The genes related to response to external stimuli were present only in N. ceranae and absent in N. apis. These gene families may therefore represent species-specific proteins. For molecular function GO terms, a number of differences were observed between the two Nosema species (Figure 8B). Structure molecule activity proteins that contribute to the structural integrity of a complex or assembly within or outside a cell were found significantly reduced in N. ceranae, compared to N. apis. The calcium binding protein that was not in N. apis was present in N. ceranae. An enrichment test of cellular components showed that genes encoding nucleolus, Golgi apparatus, cytosol, nuclear chromosome, mitochondrion and plasma membrane were at approximately similar levels of abundance for both species. However, intracellular membrane-bounded organelles including mitochondrion and endoplasmic reticulum were overrepresented in N. ceranae relative to N. apis. In contrast, nucleoplasm was significantly more common in N. apis than in N. ceranae. The ribosome was also found to be more represented in N. ceranae in relation to N. apis. The vacuole and vesicle proteins were present in N. ceranae but absent in N. apis, suggesting species-specific genes involved in structure and function of cellular components.
Nosema disease is regarded as one of the most destructive and widespread adult honey bee diseases in existence and has become a serious problem in the beekeeping industry worldwide because of an alarming increase in the disease’s prevalence as well as its association with the widespread collapse of honey bee colonies. The sequencing and annotation of the N. apis genome provide a comprehensive overview of genetic content, structure and organization of the parasite and give some interesting insights into the complex biological and molecular processes of the parasite. The comparison of the N. apis genome to its sympatric congener, N. ceranae, provides an opportunity to define a subset of genes and their associated pathways that may be responsible for the pathogenesis of Nosema disease and identify potential virulence factors that could be used as potential drug targets and for the development of novel antimicrobial agents. The identification of an overrepresented (ACCCTT) motif in the upstream promoter regions of 37% of N. apis genes led us to wonder if these genes have similar patterns of promoter activity and are regulated by the same transcriptional factors. Post-genomic experimental investigations are warranted to identify possible transcriptional factors and to determine the roles of the motif in the gene expression profile of Nosema, parasitic processes of development and host invasion. The transcription factors may offer an attractive opportunity to exploit RNAi-based targets for therapeutic intervention of Nosema disease.
Genomic data of N. apis and N. ceranae showed that overall genetic structure, contents, coding capacity and proteome complexity of N. apis and N. ceranae are similar, suggesting a shared evolutionary history for the two species. Previous studies have shown that variability in codon usage is correlated strongly with GC content, particularly at the third codon position (GC3), and also that highly expressed genes exhibit very high levels of codon bias. The evolution and functional significance of the genome variation in GC content and codon usage bias have been widely reported between organisms and also within a genome; however, the underlying causes of these variations remain poorly elucidated and there has been a long debate over whether these variations are selected or neutral traits . It is hard to define whether selection plays a role in codon usage bias in N. apis with observed weak correlation between codon usage bias and the GC content at the third site (GC3). The slight difference in correlation of genomic GC content and codon usage between N. apis and N. ceranae may reflect an evolutionary divergence or may simply be due to gene length effects of the two species.
The large number of orthologous protein groups shared by N. apis and N. ceranae and similar biochemical pathways encoded by N. apis and N. ceranae suggests that the core genes and their associated functions have been retained in the genus Nosema. The inferences of biological process, molecular function and cellular component categorizations based on predicted gene products, however, distinguish the two species. Although N. apis and N. ceranae lack the sophisticated biosynthetic pathways that are necessary for energy production, biochemical analyses showed that ATP transporter proteins are enriched in both parasites, largely reflecting their host-dependent intracellular lifestyle. The key enzymes involved in energy transporter activity and metabolic process are more represented in N. ceranae than N. apis, suggesting that N. ceranae may have a greater capacity for biosynthesis and better ability to obtain energy from its host, compared with N. apis. Although N. ceranae is a comparatively recent introduction into populations of European honey bees, N. ceranae is the more prevalent of the two Nosema species in honey bees and appears to be replacing N. apis in some populations of A. mellifera[37, 43, 59, 60]. The high survival capacity of N. ceranae would allow the parasite to consume the host for its own growth and multiplication and therefore reduce the host’s fitness over time but generally not kill it. In contrast to the distinctive disease symptoms caused by N. apis, such as dysentery and crawling behavior, N. ceranae infection is generally not associated with external symptoms. Instead, infected colonies have been found to decline gradually and collapse over a period of time. The differences in host pathogenicity between N. apis and N. ceranae may be, in part, a result of their differences in molecular function and biological process. The novel sequences of N. apis without detectable homologs in N. ceranae and vice versa suggests that there has been gene shuffling along the evolutionary pathway separating N. apis and N. ceranae from their common ancestor.
The success of the parasite also relates to its ability to respond to stress and endogenous stimuli within hosts. The result that proteins involved in response to stress and endogenous stimulus were more represented in N. ceranae than N. apis suggests that N. ceranae may have a better ability to survive under stressful conditions such as host immune functions. Alternatively, N. apis may be able to sense and respond rapidly to abiotic stimuli such as environmental changes, as categories related to the response to abiotic stimuli were more represented in N. apis than in N. ceranae. This assumption is supported by recent findings that N. ceranae and N. apis responded differently to decreasing fumagillin levels  and that N. apis was more resistant to cold temperatures than N. ceranae.
Discovering virulence factors is a key to understanding microsporidia pathogenesis and their interactions with their host and for identifying targets of novel drugs. The data from the genome sequences of N. apis as well as N. ceranae have allowed us to identify a number of putative virulence factors. For example, host tissue recognition and polar tube extrusion for initiating cell invasion are important factors in the pathogenesis of microsporidia parasites. Parasite spore wall and polar tube proteins that are essential for host cell specificity and cell invasion processes therefore could be potential targets for development of antigen-based diagnostic tests, antimicrobials and siRNA molecules. The proteins secreted from cells into the extracellular space mediate important parasite-host interactions and therefore are also interesting targets for innovative therapeutics. Future experimental evaluation of these virulence factors of microsporidia through molecular manipulations such as RNA interference (RNAi)  should provide valuable insight into their usefulness in drug development.
Although they share some morphological, biological and genetic features, as well as invasive strategies, the genome sequences of N. apis and N. ceranae revealed that these microsporidia species are highly diversified and that not all microsporidia genomes are characterized by reductions in size and complexity. Nosema genomes appear to be much less compact than the smallest microsporidia genomes, such as E. cuniculi, providing new insight into the adaptive evolution caused by the host-parasite relationship across the microsporidan groups. The availability of draft sequences of the N. apis genome is a significant addition to the rapidly expanding body of microsprodian genomic data which has been improving our understanding of eukaryotic genome diversity and evolution in a broad sense.
Bee sample collection and spore purification
Adult worker bees infected with N. apis were collected from an apiary infected exclusively with N. apis in Beaverlodge, Alberta, Canada in 2007. The species status of the Nosema infection was determined by a combination of morphological and molecular methods. In order to purify spores of N. apis from the infected bees, alimentary tracts were individually removed by grasping the stinger with forceps and pulling it out with gentle traction. The infected alimentary tracts were homogenized in 3 ml sterile water using a conical ground-glass homogenizer with a rough grinding surface and filtered through a Corning (Lowell, MA) Netwell insert (24 mm diameter, 74 mm mesh size) to remove large-sized tissue debris. The filtered suspension was centrifuged (Rotor: Sorvall RC-5B) at 3,000 g for 5 minutes to pelletize the spores. The resuspended pellet was then purified on a discontinuous Percoll (Sigma-Aldrich, St. Louis, MO) gradient consisting of 10 ml each of 30%, 60%, and 90% Percoll solution by overlaying the spore suspension onto the gradient and centrifuging at 8,000 g for 10 minutes. The pelleted spores were further purified with 30 ml of 100% Percoll solution by centrifuging at 5,000 g for 2–3 minutes to separate the spores and lighter cellular debris into the top and bottom layers, respectively. The spore-containing supernatant was collected and diluted with water in the ratio of 1:1 and centrifuged at 8,000 g for 10 minutes to pellet the spores. The purity and size of spores were examined under a light microscope (Nikon, Eclipse TE 300) and photographed with a Nikon Digital Camera (DXM 1200).
Genomic DNA isolation and N. Apis species confirmation
The genomic DNA was isolated using CTAB (hexadecyltrimethylammonium bromide) extraction buffer following spore disruption. Approximately 106 N. apis spores were suspended in 500 ml CTAB buffer (100 mM Tris–HCl, pH 8.0; 20 mM EDTA, pH 8.0; 1.4 M sodium chloride; 2% cetyltrimethylammonium bromide, w/v; 0.2% 2-mercaptoethanol) and broken by adding 500 mg of glass beads (425–600 mm, Sigma-Aldrich, St. Louis, MO) into the tube and disrupting the mixture at maximum speed for 3–5 minutes using a FastPrep Cell Disrupter (Qbiogene, Carlsbad, CA). The mixture was then incubated with proteinase K (200 mg/ml) at 55°C for five hours and treated with chitinase (0.4 U) with an extended incubation period of 16 hours at 55°C. The genomic DNA was twice extracted in an equal volume of phenol/chloroform/isoamyl alcohol (25:24:1), followed by a single extraction in chloroform. The purified DNA was precipitated with isopropanol, washed in 70% ethanol, and dissolved in 100 μl sterile water. The concentration and purity of the DNA were determined by spectrophotometric absorption at 260 nm, and ratios of absorption at 260 nm and 280 nm.
The Nosema species specificity of extracted genomic DNA was confirmed by a PCR assay prior to 454 pyrosequencing. Primers specific to N. apis and to N. ceranae were used individually in the PCR-mediated amplification of genomic DNA isolated from purified spores. The sequences of N. apis primers that amplified 269-bp fragment of the 18S rRNA were as follows: apisF 5′- CCATTGCCGGATAAGAGAGT -3′ and apisR 5′- CCACCAAAAACTCCCAAGAG -3′. The PCR reaction mixture, thermal conditions, and sequences of N. ceranae primers used were as previously described . The amplified PCR products were purified using the Wizard PCR Prep DNA Purification System (Promega, Madison, WI) and the nucleotide sequence identity of the PCR fragments was determined using a Basic Local Alignment Sequence Tool (BLAST) homology search.
Library construction, sequencing, and assembly
Although the high% AT vs.% GC ratio of this genome poses challenges for all high-throughput sequencing platforms, a successful sequencing library was constructed, sequenced and assembled through protocol optimizations. The 454 Titanium sequencing platform offers an ideal combination of throughput and long read length to enable de novo sequence assembly of whole genomes. A paired-end library was constructed according to the manufacturer’s protocol, with modifications and optimizations to enable robotic automation of crucial steps and manipulation of limited, high-% AT starting material. An initial sample of 500 ng DNA was sheared using a Covaris E210 high-performance ultra-sonicator. Following adaptor ligation and double AMPure SPRI bead-based size selection, the resulting library had an average fragment size of 2,072 bp with a standard deviation of 208 bp. This library was sequenced on a full two-region 454 Titanium run resulting in 1,070,575 passed-filter sequence reads with an average quality-trimmed length of 304 bp. During data quality control procedures, 126,461 reads, or 11.8% of the total, were eliminated as PCR-induced duplicates. This represents a typical duplicate read percentage for the 454 sequencing platform. An additional 10% of the reads were eliminated as too short for assembly or containing an inconsistent or partial paired-end linker sequence. Of the remaining reads, 360,731 were bisected at the linker to form successful pairs, while 475,944 remained as unpaired shotgun reads.
These data were assembled using the Celera Assembler (http://sourceforge.net/projects/wgs-assembler/) version 6.1 using the CABOG module, an overlap-layout-consensus sequence assembler that has been recently optimized for use with 454 Titanium paired-end sequence data. The Celera Assembler uses a stringent algorithm that heavily weighs paired-end read constraints and favors shorter, higher-confidence contigs over longer, potentially misassembled contigs. This approach ensures a highly accurate result with minimal mis-assembly.
Repetitive element identification
Genome analysis of N. ceranae showed the presence of a large proportion of the repetitive elements which could interfere with the accuracy of de novo gene prediction. We therefore used RepeatMasker (http://www.repeatmasker.org), Tandem Repeat Finder , and LTR Finder  in an ab initio manner with the default settings to identify the repetitive elements. Repetitive elements and low complexity DNA sequences in the N. apis genome were then masked for elimination. To avoid the incorrect identification of repetitive elements and low complexity from DNA sequences, manual inspection of the list of repeats was carried out. The repeats that had significant Basic Local Alignment Search Tool (BLAST) hits to the NCBI protein database (E-value cutoff of 1.0E-5) were kept for subsequent gene prediction and annotation.
Protein-coding gene prediction and regulatory motif identification
After the exclusion of a few contaminating honey bee host sequences identified through BLASTN searches against the bee genome, a combination of two programs was used for identification of protein-coding sequences (CDSs) in the masked N. apis genome: GeneMark.hmm.ES (version 3.0) using non-supervised training procedures and Augustus trained with E. cuniculi, and S. cerevisiae. The GeneMark.hmm  and AUGUSTUS  programs for eukaryotic genomes access the coding potential of DNA sequence based on Hidden Markov Models (HMM). Next, outputs of supervised gene prediction based on sequence similarity to reference organisms (extrinsic method) and ab initio gene prediction relying on intrinsic features of the DNA sequence (intrinsic method) were merged and reconciled with other gene models. The CD-HIT-2D  was used for identifying overlapping and unique sets of proteins from different gene prediction programs. For overlapping predictions produced by different programs, the prediction with BLAST evidence was kept. If the overlapping predictions by different programs did not have BLAST evidence or if they all had BLAST evidence, the longest prediction was chosen. To verify the correct prediction of protein-coding genes, all inferred genes larger than 50 aa were further compared across an NCBI non-redundant protein database using BLASTP program with default parameters. Frame-shifts and point mutations were detected and corrected where appropriate. Candidates with a protein identity match ≥ 30%, and BLASTP value ≤ 10–5 were retained as protein-encoding gene candidates.
Nucleotide composition and synonymous codon usage of protein coding genes were investigated using the program INCA2.0 by . The maximum-likelihood codon bias (MCB) was used as a measure for codon usage bias where the contribution to the index of the bias of each amino acid is weighted by an estimation of the likelihood of occurrence of bias on each amino acid . The relative synonymous codon usage (RSCU) of individual codons between N. apis and N. ceranae were compared. Putative transcriptive regulators were searched by identifying over-represented motifs in the 100-bp upstream region of the start codon of each protein-coding gene. The MEME 3.0 software program  was used for the motif identification.
Signal peptide and transmembrane region prediction
The N-terminal amino acid sequence of predicted protein from this study was analyzed for the presence of putative signal peptides using the SignalP 3.0 program , and a neural network and HMM trained on eukaryotes. The transmembrane regions of predicted protein were identified with TMHMM 2.0, a HMM based transmembrane helix prediction program. The architecture of the hidden Markov model and the neural network algorithm was applied for prediction of the signal peptide and transmembrane region of each translated protein. The default parameters were used for both programs.
tRNA genes were detected using two tRNA identification programs, tRNAScan-SE version 123 (Lowe and Eddy, 1997) and ARAGORN  at the default settings. The tRNAScan-SE search was based on tRNA training data from a mixed general tRNA model. The ARAGORN search was based on the homology of recognized tRNA consensus sequences by specifying a yeast nuclear genome (NC_001133-NC_001148) and the ability of input data to form a base-paired cloverleaf to predict tRNA secondary structure. Two programs are also able to distinguish tRNA pseudogenes from true genes with high sensitivity.
Ribosomal genes coding rRNA in a full genome sequence were identified using both RNAmmer 1.2 server  with the default parameters and BlastN searches. Matches were defined as those sequences having greater than 90% similarity and greater than 90% of the query length. Small nuclear RNAs (snRNA) were also identified by BlastN searches. rRNA sequences were annotated based on homology to previously published rRNA sequences deposited in GeneBank.
Ortholog and paralog identification
The possible orthologs of N. apis in N. ceranae, E. cuniculi or S. cerevisiae genomes were predicted by searching for the best reciprocal BLASTP matches with InParanoid . In each of the between-species comparisons, we aligned protein sequences from one species to protein sequences from the other, and corresponding best matches were then aligned back to the original species. On the basis of all of the possible between-species sequence pairs, we reported orthologs and in-paralogs that had multiple hits in the same genome with a bit score cutoff of 40 and an aligned region larger than 50% of the longer query sequence in each pair. We also performed bootstrap analysis to obtain confidence for each ortholog identified. Gene duplications were identified with a focus on proteins in the data set that had a better match within the N. apis genome they reside (excluding the self match) when compared against all other genomes used in the study. In order to avoid assigning paralogs to ortholog pairs, the top hit had to have an E-value 105 times lower (more significant) than the next best hit. In addition, the complete genome sequence of N. apis was aligned individually to the complete genome of N. ceranae to find the corresponding orthologous blocks in the genomes and to illustrate homologs between genomes by using the Mauve 2.2. .
Protein domain functional annotation
The predicted proteins were analyzed using the BLASTP algorithm to search for homolog sequences and functionally annotated by gene ontology (GO) terms, InterPro terms (Conserved patterns in sequences, InterProScan, EBI), enzyme classification (EC) codes, and metabolic pathways (Kyoto Encyclopedia of Genes and Genomes, KEGG) using the Blast2GO (B2G) software suite v2.4.2 (http://www.BLAST2go.org, . The functional annotation in B2G was performed using the following steps: 1) performing BlastP to final homologous sequences to the query set; 2) mapping to collect gene ontology terms (GO) associated to the hits after a BLASTP search; 3) selecting GO terms from the GO pool collected in the mapping step and assigning them to the query sequence; 4) grouping the descriptions into ‘GOslim” categories for biological process, molecular function, and cellular component, and 5) performing Enzyme code and InterPro annotations support language by GO terms. Finally, an enrichment analysis was performed to assess the differences in functional classes between N. apis and N. ceranae using one-way Fisher’s Exact Tests. The default settings of B2G were used in every annotation step. The false discovery rate (FDR) at level α = 0.05 was applied for controlling procedures. Gene product names are assigned based on sequence homology to known genes in NCBI databases. The putative proteins without GO annotation were classified as “hypothetical protein with no significant database hit”.
The apiaries for bee sample collection are the property of the USDA-ARS Beltsville Bee Research Laboratory, MD, USA and the Agriculture & Agri-Food Canada, Beaverlodge Research Farm, Beaverlodge, AB, Canada; therefore, no specific permits were required for the described studies. Studies involved the European honey bee (Apis mellifera), which is neither an endangered nor protected species.
We thank Dr. Kevin J. Hackett for facilitating the project, Drs. Christina Grozinger and Katherine Aronstein for critical reviews and helpful comments on an earlier version of this manuscript, and Dr. Thomas C. Webster for providing Nosema-infected bees.
- Didier ES: Microsporidiosis: an emerging and opportunistic infection in humans and animals. Acta Trop. 2005, 94: 61-76. 10.1016/j.actatropica.2005.01.010.View ArticlePubMedGoogle Scholar
- Keeling PJ, Fast NM: Microsporidia: biology and evolution of highly reduced intracellular parasites. Annu Rev Microbiol. 2002, 56: 93-116. 10.1146/annurev.micro.56.012302.160854.View ArticlePubMedGoogle Scholar
- Wittner M, Weiss LM: The microsporidia and microsporidosis. 1999, Washington, DC: ASM Press, 553-Google Scholar
- Vossbrinck CR, Maddox JV, Friedman S, Debrunner-Vossbrinck BA, Woese CR: Ribosomal RNA sequence suggests microsporidia are extremely ancient eukaryotes. Nature. 1987, 326: 411-414. 10.1038/326411a0.View ArticlePubMedGoogle Scholar
- Williams BA, Hirt RP, Lucocq JM, Embley TM: A mitochondrial remnant in the microsporidian trachipleistophora hominis. Nature. 2002, 418: 865-869. 10.1038/nature00949.View ArticlePubMedGoogle Scholar
- Hirt RP, Healy B, Vossbrinck CR, Canning EU, Embley TM: A mitochondrial Hsp70 orthologue in vairimorpha necatrix: molecular evidence that microsporidia once contained mitochondria. Curr Biol. 1997, 7: 995-998. 10.1016/S0960-9822(06)00420-9.View ArticlePubMedGoogle Scholar
- Arisue N, Sánchez LB, Weiss LM, Müller M, Hashimoto T: Mitochondrial-type hsp70 genes of the amitochondriate protists, Giardia intestinalis, Entamoeba Histolytica and two microsporidians. Parasitol Int. 2002, 51: 9-16. 10.1016/S1383-5769(01)00093-9.PubMed CentralView ArticlePubMedGoogle Scholar
- James TY, Kauff F, Schoch CL, Matheny PB, Hofstetter V, Cox CJ, Celio G, Gueidan C, Fraker E, Miadlikowska J, et al: Reconstructing the early evolution of fungi using a six-gene phylogeny. Nature. 2006, 443: 818-822. 10.1038/nature05110.View ArticlePubMedGoogle Scholar
- Capella-Gutiérrez S, Marcet-Houben M, Gabaldón T: Phylogenomics supports microsporidia as the earliest diverging clade of sequenced fungi. BMC Biol. 2012, 10: 47-10.1186/1741-7007-10-47.PubMed CentralView ArticlePubMedGoogle Scholar
- Sokolva V, Snigirevskaya E, Morzhina E, Skarlato S, Mironov A, Komissarchik Y: Visualization of early golgi compartments at proliferate and sporogenic stages of a microspordian nosema grylli. J Eukaryot Microbiol. 2001, 48: 86s-87s.View ArticleGoogle Scholar
- Takvorian PM, Call A: Enzyme histochemical identification of the golgi apparatus in the microsporidian glugea stephani. J Eukaryot Microbiol. 1994, 41: 63S-64S.PubMedGoogle Scholar
- Weidner E, Findley A: Catalase in microsporidian spores before and during discharge. Biol Bull. 2003, 205: 236-237. 10.2307/1543272.View ArticlePubMedGoogle Scholar
- Bailey L, Ball BV: Honey bee pathology. 1997, London: Academic Press, 2Google Scholar
- Chen YP, Evans JD, Murphy C, Gutell R, Zuker M, Gundensen-Rindal D, Pettis JS: Morphological, molecular, and phylogenetic characterization of nosema ceranae, a microsporidian parasite isolated from the european honey bee, apis mellifera. J Eukaryo Microbiol. 2009, 56: 142-147. 10.1111/j.1550-7408.2008.00374.x.View ArticleGoogle Scholar
- Higes M, Garcia-Palencia P, Martin-Hernandez R, Meana A: Experimental infection of apis mellifera honeybees with nosema ceranae (microsporidia). J Invertebr Pathol. 2007, 94: 211-217. 10.1016/j.jip.2006.11.001.View ArticlePubMedGoogle Scholar
- Smith ML: The honey bee parasite nosema ceranae: transmissible via food exchange?. PLoS One. 2012, 7 (8): e43319-10.1371/journal.pone.0043319.PubMed CentralView ArticlePubMedGoogle Scholar
- Farrar CL: Nosema losses in package bees as related to queen supersedure and honey yield. J Econ Entomol. 1947, 40: 333-338.View ArticlePubMedGoogle Scholar
- Hassanein MH: The influence of nosema apis on the larval honeybee. Ann Appl Biol. 1953, 38: 844-846.View ArticleGoogle Scholar
- Higes M, Martín-Hernandez R, Garrido-Bailón E, Gonzales-Porto A, García-Palencia P, Meana A, Del Nozal MJ, Mayo R, BJ L: Honeybee colony collapse due to nosema ceranae in professional apiaries. Environ Microbiol Reports. 2009, 1: 110-113. 10.1111/j.1758-2229.2009.00014.x.View ArticleGoogle Scholar
- Malone LA, Giacon HA, Newton MR: Comparison of the responses of some New zealand and australian honey bees (apis mellifera L) to nosema apis Z. Apidologie. 1995, 26: 495-502. 10.1051/apido:19950606.View ArticleGoogle Scholar
- Rinderer TE, Sylvester HA: Variation in response to nosema apis, longevity, and hoarding behavior in a free-mating population of the honey bee. Ann Entomol Soc Am. 1978, 71: 372-374.View ArticleGoogle Scholar
- Furgala B: The effect of the intensity of nosema inoculum on queen supersedure in the honey bee, apis mellifera L. J Insect Pathol. 1962, 4: 427-432.Google Scholar
- Antunez K, Martin-Hernandez R, Prieto L, Meana A, Zunino P, Higes M: Immune suppression in the honey bee (apis mellifera) following infection by nosema ceranae (microsporidia). Environ Microbiol. 2009, 11 (9): 2284-2290. 10.1111/j.1462-2920.2009.01953.x.View ArticlePubMedGoogle Scholar
- Dussaubat C, Brunet JL, Higes M, Colbourne JK, Lopez J, Choi JH, Martin-Hernandez R, Botias C, Cousin M, McDonnell C, et al: Gut pathology and responses to the microsporidium nosema ceranae in the honey bee apis mellifera. PLoS One. 2012, 7 (5): e37017-10.1371/journal.pone.0037017.PubMed CentralView ArticlePubMedGoogle Scholar
- Costa C, Tanner G, Lodesani M, Maistrello L, Neumann P: Negative correlation between nosema ceranae spore loads and deformed wing virus infection levels in adult honey bee workers. J Invertebr Pathol. 2011, 108 (3): 224-225. 10.1016/j.jip.2011.08.012.View ArticlePubMedGoogle Scholar
- Alaux C, Brunet JL, Dussaubat C, Mondet F, Tchamitchan S, Cousin M, Brillard J, Baldy A, Belzunces LP, Le Conte Y: Interactions between nosema microspores and a neonicotinoid weaken honeybees (apis mellifera). Environ Microbiol. 2010, 12 (3): 774-782. 10.1111/j.1462-2920.2009.02123.x.PubMed CentralView ArticlePubMedGoogle Scholar
- Pettis JS, Van Engelsdorp D, Johnson J, Dively G: Pesticide exposure in honey bees results in increased levels of the gut pathogen nosema. Die Naturwissenschaften. 2012, 99 (2): 153-158. 10.1007/s00114-011-0881-1.PubMed CentralView ArticlePubMedGoogle Scholar
- Wu JY, Smart MD, Anelli CM, Sheppard WS: Honey bees (apis mellifera) reared in brood combs containing high levels of pesticide residues exhibit increased susceptibility to nosema (microsporidia) infection. J Invertebr Pathol. 2012, 109 (3): 326-329. 10.1016/j.jip.2012.01.005.View ArticlePubMedGoogle Scholar
- Vidau C, Diogon M, Aufauvre J, Fontbonne R, Vigues B, Brunet JL, Texier C, Biron DG, Blot N, El Alaoui H, et al: Exposure to sublethal doses of fipronil and thiacloprid highly increases mortality of honeybees previously infected by nosema ceranae. PLoS One. 2011, 6 (6): e21550-10.1371/journal.pone.0021550.PubMed CentralView ArticlePubMedGoogle Scholar
- Aufauvre J, Biron DG, Vidau C, Fontbonne R, Roudel M, Diogon M, Vigues B, Belzunces LP, Delbac F, Blot N: Parasite-insecticide interactions: a case study of nosema ceranae and fipronil synergy on honeybee. Sci Rep. 2012, 2: 326-PubMed CentralView ArticlePubMedGoogle Scholar
- Huang WF, Solter LF, Yau PM, Imai BS: Nosema ceranae escapes fumagillin control in honey bees. PLoS Pathog. 2013, 9 (3): e1003185-10.1371/journal.ppat.1003185.PubMed CentralView ArticlePubMedGoogle Scholar
- Gallai N, Salles JM, S J, V B: Economic valuation of the vulnerability of word agriculture confronted with pollinator decline. Ecol Econ. 2008, 68: 810-821.View ArticleGoogle Scholar
- Zander E: Tierische parasiten als krankenheitserreger bei der biene. Münchener Bienenzeitung. 1909, 31: 196-204.Google Scholar
- Fries I, Feng F, Silva AD, Slemenda SB, Pieniazek NJ: Nosema ceranae n. sp. (Microspora, nosematidae), morphological and molecular characterization of a microsporidian parasite of the asian honey bee apis cerana (hymenoptera, apidae). Europ J Protistol. 1996, 32: 356-365. 10.1016/S0932-4739(96)80059-9.View ArticleGoogle Scholar
- Fries I, Martín R, Meana A, García-Palencia P, Higes M: Natural infections of nosema ceranae in european honey bees. J Apic Res. 2006, 45: 230-233.View ArticleGoogle Scholar
- Huang WF, Jiang JH, Chen YW, Wang CH: A nosema ceranae isolate from the honeybee apis mellifera. Apidologie. 2007, 38: 30-37. 10.1051/apido:2006054.View ArticleGoogle Scholar
- Fries I: Nosema ceranae in european honey bees (apis mellifera). J Invertebr Pathol. 2010, 103: S73-S79.View ArticlePubMedGoogle Scholar
- Higes M, Martín-Hernandez R, Meana A: Nosema ceranae, a new microsporidian parasite in honeybees in europe. J Invertebr Pathol. 2006, 92: 81-83.View ArticleGoogle Scholar
- Klee J, Besana AM, Genersch E, Gisder S, Nanetti A, Tam DQ, Chinh TX, Puerta F, Ruz JM, Kryger P, et al: Widespread dispersal of the microsporidian nosema ceranae, an emergent pathogen of the western honey bee, apis mellifera. J Invertebr Pathol. 2007, 96: 1-10. 10.1016/j.jip.2007.02.014.View ArticlePubMedGoogle Scholar
- Paxton RJ, Klee J, Korpela S, Fries I: Nosema ceranae has infected apis mellifera in europe since at least 1998 and may be more virulent than nosema apis. Apidologie. 2007, 38: 558-565. 10.1051/apido:2007037.View ArticleGoogle Scholar
- Chen YP, Evans JD, Smith JB, Pettis JS: Nosema ceranae is a long-present and wide-spread microsporidian infection of the european honey bee (apis mellifera) in the united states. J Invertebr Pathol. 2008, 97: 186-188. 10.1016/j.jip.2007.07.010.View ArticlePubMedGoogle Scholar
- Higes M, Martín-Hernandez R, Botias C, Bailon EG, Gonzales-Porto A, Barrios L, Del Nozal MJ, Palencia PG, Meana A: How natural infection by nosema ceranae causes honeybee colony collapse. Environ Microbiol. 2008, 10: 2659-2669. 10.1111/j.1462-2920.2008.01687.x.View ArticlePubMedGoogle Scholar
- Higes M, Martín-Hernández R, Meana A: Nosema ceranae in europe: an emergent type C nosemosis. Apidologie. 2010, 41: 375-392. 10.1051/apido/2010019.View ArticleGoogle Scholar
- Paxton RJ: Does infection by nosema ceranae cause “colony collapse disorder” in honey bees ( apis mellifera)?. J Apic Res. 2010, 49: 80-84. 10.3896/IBRA.18.104.22.168.View ArticleGoogle Scholar
- Cox-Foster DL, Conlan S, Holmes E, Palacios G, Evans JD, Moran NA, Quan PL, Briese T, Hornig M, Geiser DM, et al: A metagenomic survey of microbes in honey bee colony collapse disorder. Science. 2007, 318: 283-287. 10.1126/science.1146498.View ArticlePubMedGoogle Scholar
- Neumann P, Carreck NL: Honey bee colony losses. J Apic Res. 2010, 49: 1-6. 10.3896/IBRA.1.49.1.01.View ArticleGoogle Scholar
- Van Engelsdorp D, Underwood R, Caron D, Hayes JJ: An estimate of managed colony losses in the winter of 2006–2007: a report commissioned by the apiary inspectors of america. Am Bee J. 2007, 147: 599-603.Google Scholar
- Belkorchia A, Biderre C, Militon C, Polonais V, Wincker P, Jubin C, Delbac F, Peyretaillade E, Peyret P: In vitro propagation of the microsporidian pathogen brachiola algerae and studies of its chromosome and ribosomal DNA organization in the context of the complete genome sequencing project. Parasitol Int. 2008, 57: 62-71. 10.1016/j.parint.2007.09.002.View ArticlePubMedGoogle Scholar
- Keeling PJ, Fast NM, Law JS, Williams BA, Slamovits CH: Comparative genomics of microsporidia. Folia Parasitologia. 2005, 52: 8-14.View ArticleGoogle Scholar
- Katinka MD, Duprat S, Cornillot E, Metenier E, Thomarat F, Prensier G, Barbe V, Peyretaillade E, Brottier P, Wincker P, et al: Genome sequence and gene compaction of the eukaryote parasite encephalitozoon cuniculi. Nature. 2001, 414: 450-453. 10.1038/35106579.View ArticlePubMedGoogle Scholar
- Akiyoshi DE, Morrison HG, Lei S, Feng X, Zhang Q, Corradi N, Mayanja H, Tumwine JK, Keeling PJ, Weiss LM, et al: Genomic survey of the non-cultivatable opportunistic human pathogen. Enterocytozoon bieneusi. PLoS pathogens. 2009, 5: e1000261-10.1371/journal.ppat.1000261.View ArticlePubMedGoogle Scholar
- Cornman RS, Chen YP, Schatz MC, Street C, Zhao Y, Desany B, Egholm M, Hutchison S, Pettis JS, Lipkin WI, et al: Genomic analyses of the microsporidian nosema ceranae, an emergent pathogen of honey bees. PLoS Pathog. 2009, 5: e1000466-10.1371/journal.ppat.1000466.PubMed CentralView ArticlePubMedGoogle Scholar
- Corradi N, Pombert JF, Farinelli L, Didier ES, Keeling PJ: The complete sequence of the smallest known nuclear genome from the microsporidian encephalitozoon intestinalis. Nat Commun. 2010, 1: 77-PubMed CentralView ArticlePubMedGoogle Scholar
- Cuomo CA, Desjardins CA, Bakowski MA, Goldberg J, Ma AT, Becnel JJ, Didier ES, Fan L, Levin JZ, Young S, et al: Microsporidian genome analysis reveals evolutionary strategies for obligate intracellular growth. Genome Res. 2012, 22: 2478-2488. 10.1101/gr.142802.112.PubMed CentralView ArticlePubMedGoogle Scholar
- Peyretaillade E, Parisot N, Polonais V, Terrat S, Denonfoux J, Dugat-Bony E, Wawrzyniak I, Biderre-Petit C, Mahul A, Rimour S, et al: Annotation of microsporidian genomes using transcriptional signals. Nat Commun. 2012, 3: 1137-View ArticlePubMedGoogle Scholar
- Pombert J, Selman M, Burki F, Bardell FT, Farinelli L, Solter LF, Douglas WW, Weiss LM, Corradi N, Keeling PJ: Gain and loss of multiple functionally related, horizontally transferred genes in the reduced genomes of two microsporidian parasites. Proc Natl Acad Sci USA. 2012, 109: 12638-12643. 10.1073/pnas.1205020109.PubMed CentralView ArticlePubMedGoogle Scholar
- Heinz E, Williams TA, Nakjang S, Noel CJ, Swan DC, Goldberg AV, Harris SR, Weinmaier T, Markert S, Becher D, et al: The genome of the obligate intracellular parasite trachipleistophora hominis: new insights into microsporidian genome dynamics and reductive evolution. PLoS Pathog. 2012, 8 (10): e1002979-10.1371/journal.ppat.1002979.PubMed CentralView ArticlePubMedGoogle Scholar
- Ermolaeva MD: Synonymous codon usage in bacteria. Curr Issues Mol Biol. 2001, 3 (4): 91-97.PubMedGoogle Scholar
- Chen YP, Huang ZY: Nosema ceranae, a newly identified pathogen of apis mellifera in the U.S. And asia. Apidologie. 2010, 41: 364-374. 10.1051/apido/2010021.View ArticleGoogle Scholar
- Huang WF, Solter LF: Comparative development and tissue tropism of nosema apis and nosema ceranae. J Invertebr Pathol. 2013, 113 (1): 35-41. 10.1016/j.jip.2013.01.001.View ArticlePubMedGoogle Scholar
- Higes M, Garcia-Palencia P, Botias C, Meana A, Martin-Hernandez R: The differential development of microsporidia infecting worker honey bee (apis mellifera) at increasing incubation temperature. Environ Microbiol Reports. 2010, 2: 745-748. 10.1111/j.1758-2229.2010.00170.x.View ArticleGoogle Scholar
- Paldi N, Glick E, Oliva M, Zilberberg Y, Aubin L, Pettis JS, Chen YP, Evans JD: Effective gene silencing of a microsporidian parasite associated with honey bee (apis mellifera) colony declines. Appl Environ Microbiol. 2010, 76: 5960-5964. 10.1128/AEM.01067-10.PubMed CentralView ArticlePubMedGoogle Scholar
- Benson G: Tandem repeats finder: a program to analyze DNA sequences. Nucleic Acid Res. 1999, 27: 573-580. 10.1093/nar/27.2.573.PubMed CentralView ArticlePubMedGoogle Scholar
- Xu Z, Wang H: LTR_FINDER: an efficient tool for the prediction of full-length LTR retrotransposons. Nucleic Acids Res. 2007, 35: W265-W268. 10.1093/nar/gkm286.PubMed CentralView ArticlePubMedGoogle Scholar
- Besemer J, Borodovsky M: GeneMark: web software for gene finding in prokaryotes, eukaryotes and viruses. Nucleic Acids Res. 2005, 33: W451-W454. 10.1093/nar/gki487.PubMed CentralView ArticlePubMedGoogle Scholar
- Stanke M, Steinkamp R, Waack S, Morgenstern B: AUGUSTUS: a web server for gene finding in eukaryotes. Nucl Acids Res. 2004, 32: W309-W312. 10.1093/nar/gkh379.PubMed CentralView ArticlePubMedGoogle Scholar
- Huang Y, Niu B, Gao Y, Fu L, Li W: CD-HIT suite: a web server for clustering and comparing biological sequences. Bioinformatics. 2010, 26: 680-682. 10.1093/bioinformatics/btq003.PubMed CentralView ArticlePubMedGoogle Scholar
- Supek F, Vlahovicek K: INCA: synonymous codon usage analysis and clustering by means of self-organizing map. Bioinformatics. 2004, 20: 2329-2330. 10.1093/bioinformatics/bth238.View ArticlePubMedGoogle Scholar
- Urrutia AO, Hurst LD: The signature of selection mediated by expression on human genes. Genome Res. 2003, 13 (10): 2260-2264. 10.1101/gr.641103.PubMed CentralView ArticlePubMedGoogle Scholar
- Bailey TL, Williams N, Mislech C, Li WW: MEME: discovering and analyzing DNAand protein sequence motifs. Nucleic Acids Res. 2006, 34: W369-W373. 10.1093/nar/gkl198.PubMed CentralView ArticlePubMedGoogle Scholar
- Bendtsen JD, Nielsen H, Von Heijne G, Brunak S: Improved prediction of signal peptides: SignalP 3.0. J Mol Biol. 2004, 340: 783-795. 10.1016/j.jmb.2004.05.028.View ArticlePubMedGoogle Scholar
- Laslett D, Canback B: ARAGORN, a program to detect tRNA genes and tmRNA genes in nucleotide sequences. Nucleic Acids Res. 2004, 32: 11-16. 10.1093/nar/gkh152.PubMed CentralView ArticlePubMedGoogle Scholar
- Lagesen K, Hallin PF, Rødland E, Stærfeldt HH, Rognes T, Ussery DW: RNammer: consistent annotation of rRNA genes in genomic sequences. Nucleic Acids Res. 2007, 35: 3100-3108. 10.1093/nar/gkm160.PubMed CentralView ArticlePubMedGoogle Scholar
- O'Brien KP, Remm K, Sonnhammer ELL: Inparanoid: a comprehensive database of eukaryotic orthologs. Nuclic Acids Res. 2005, 33: D476-D480.View ArticleGoogle Scholar
- Darling AC, Mau B, Blattner FR, Perna NT: Mauve: multiple alignment of conserved genomic sequence with rearrangements. Genome Res. 2004, 14: 1394-1403. 10.1101/gr.2289704.PubMed CentralView ArticlePubMedGoogle Scholar
- Cornesa A, Gőtz S, García-Gómez JM, Terol J, Talón M, Robles M: Blast2go: a universal tool for annotation, visualization and analysis in functional genomic research. Bioinfomratics. 2005, 21: 3674-3676. 10.1093/bioinformatics/bti610.View ArticleGoogle Scholar
- Li Z, Pan G, Li T, Huang W, Chen J, Geng L, Yang D, Wang L, Zhou Z: SWP5, A spore wall protein, interacts with polar tube proteins in the parasitic microsporidian nosema bombycis. Eukaryot Cell. 2012, 11: 229-237. 10.1128/EC.05127-11.PubMed CentralView ArticlePubMedGoogle Scholar
- Wu Z, Li Y, Pan G, Tan X, Hu J, Zhou Z, Xiang Z: Proteomic analysis of spore wall proteins and identification of two spore wall proteins from nosema bombycis (microsporidia). Proteomics. 2008, 8: 2447-2461. 10.1002/pmic.200700584.View ArticlePubMedGoogle Scholar
- Wu Z, Li Y, Pan G, Zhou Z, Xiang Z: SWP25, A novel protein associated with the nosema bombycis endospore. J Eukaryot Microbiol. 2009, 56: 113-118. 10.1111/j.1550-7408.2008.00375.x.View ArticlePubMedGoogle Scholar
- Li Y, Wu Z, Pan G, He W, Zhang R, Hu J, Zhou Z: Identification of a novel spore wall protein (SWP26) from microsporidia nosema bombycis. Int J Parasitol. 2008, 39: 391-398.View ArticlePubMedGoogle Scholar
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.