Research Article

Predictive Markers of Honey Bee Colony Collapse

  • Benjamin Dainat mail,

    Affiliation: Swiss Bee Research Centre, Agroscope Liebefeld-Posieux Research Station ALP, Bern, Switzerland

  • Jay D. Evans,

    Affiliation: Bee Research Laboratory, United States Department of Agriculture-Agricultural Research Service, Beltsville, Maryland, United States of America

  • Yan Ping Chen,

    Affiliation: Bee Research Laboratory, United States Department of Agriculture-Agricultural Research Service, Beltsville, Maryland, United States of America

  • Laurent Gauthier,

    Affiliation: Swiss Bee Research Centre, Agroscope Liebefeld-Posieux Research Station ALP, Bern, Switzerland

  • Peter Neumann

    Affiliations: Swiss Bee Research Centre, Agroscope Liebefeld-Posieux Research Station ALP, Bern, Switzerland, Department of Zoology and Entomology, Rhodes University, Grahamstown, South Africa

  • Published: February 23, 2012
  • DOI: 10.1371/journal.pone.0032151


Across the Northern hemisphere, managed honey bee colonies, Apis mellifera, are currently affected by abrupt depopulation during winter and many factors are suspected to be involved, either alone or in combination. Parasites and pathogens are considered as principal actors, in particular the ectoparasitic mite Varroa destructor, associated viruses and the microsporidian Nosema ceranae. Here we used long term monitoring of colonies and screening for eleven disease agents and genes involved in bee immunity and physiology to identify predictive markers of honeybee colony losses during winter. The data show that DWV, Nosema ceranae, Varroa destructor and Vitellogenin can be predictive markers for winter colony losses, but their predictive power strongly depends on the season. In particular, the data support that V. destructor is a key player for losses, arguably in line with its specific impact on the health of individual bees and colonies.


Agricultural pollination should integrate wild species, which provide pollination as an ecosystem service, and managed pollinator introduction as crop management practices [1]. Amongst the managed pollinators, the Western honey bee, Apis mellifera, is clearly a cornerstone, because pollination of many crops in most parts of the world relies on this species [1]. However, managed honey bee colonies are currently affected by a syndrome corresponding to an abrupt depopulation during winter [2]. Many biotic and abiotic factors are suspected to be involved in this condition, either alone or in combination [2][3]. Among them, parasites contribute to weakening colony health, leaving room to secondary infections. In particular, the ectoparasitic mite Varroa destructor [4] is now considered to be the main candidate involved in winter colony losses in Europe [5][8]. This parasite originates from South-East Asia and has now become widespread across most of the continents [4]. It has been shown that V. destructor or its associated microbes can affect the immune system of parasitized bees [9][12]. In addition, viral infections linked with V. destructor are generally considered as a major cause of bee losses. Indeed, V. destructor plays a central role as a mechanical and biological vector of several viruses [12][17]. In addition V. destructor appears to accelerate the replication of latent viral infections [12], [17][20]. Although more than 19 different viruses have been detected in A. mellifera, only three have been associated with winter losses on a large scale [5], [21][23], namely Deformed wing virus [24], Acute bee paralysis virus [25], [26] and Israeli acute bee paralysis virus [27]. These viruses are positive stranded RNA viruses belonging to the Iflaviridae and Dicistroviridae families and are suspected to enhance the deleterious action of V. destructor on bee colonies by their strong association with this mite [20], [28], [29]. In the United States, IAPV was first identified as a predictive factor for producing CCD symptoms [21]. However, subsequent surveys indicate that this virus was not the main factor responsible for losses but only one of multiple possible factors involved [30], [31]. In Europe, DWV and ABPV are generally suspected to be involved in winter colony losses [5], [22], [23]. Both are transmitted by the mite after feeding on bee pupae or adults [20], [29]. ABPV is highly virulent for bees when injected directly into the hemolymph [25], [29], [32]. On the contrary, DWV is much less virulent and generates typical symptoms of deformed wings only in bees from colonies highly infested with Varroa mites [33]. Despite its low virulence for bees, DWV infects a large range of bee tissues and can produce high titers in infected bees, suggesting a potential impact on bee physiology [34], [35].

Another potential candidate involved in colony losses is the microsporidian Nosema ceranae [36], [37] although the impact of this parasite on colony health in Europe still remains controversial [5], [38], [39].

Despite the fact that several studies have pointed out the potential involvement of pathogens on colony losses, no common pattern has yet emerged. This is probably due in part to the different parameters present in these studies such as climate, bee races, beekeeping practices or sampling methods. Indeed sampling often consists of bees collected once from either healthy, weak or dead colonies. In this context long term monitoring appears crucial, especially because pathogens causing colony death may have disappeared leaving room for opportunistic infections.

In this study, we aimed to identify predictive markers of winter honey bee colony losses. Although the up- or down-regulation of a marker in a sample may not be related to the principal cause(s) of the disease, such markers would help beekeepers or bee inspectors to set up a reliable diagnostic tool and to standardize bee colony monitoring all around the world. For this purpose we performed a survey of bee colonies in Switzerland over six months and checked for the presence and loads of eleven honey bee pathogens in the samples, as well as the levels of expression of three A. mellifera genes involved in bee immunity.

Materials and Methods

1. Experimental design

In summer 2007, 29 queenright colonies were selected from our local bee stocks (predominantly A. m. carnica) of similar strength (~14'000 workers each) at the Swiss Bee Research Centre in Bern, Switzerland. In order to get sufficiently different parasitism levels with the ectoparasitic mite V. destructor, 18 colonies were adequately and timely treated in winter 2006–2007 and in summer and fall 2007 against this mite using organic acids following the Liebefelder alternative treatment (twice with formic acid by evaporation using the FAM diffuser in summer and late summer and oxalic acid by droplets in Fall) [40], while the others were left untreated. Both groups were otherwise managed in exactly the same way prior to and during the experiment. In the experiment, the two groups were physically separated by 250 m and one four-storied building to minimize mite movement between colonies (e.g. via drifting and/or robbing; [4], [41]), but nevertheless had similar foraging conditions. Mite infestation levels were monitored weekly in each colony using the natural mite fall method [4], [42], distinguishing colonies with high and low mite infestations. Pooled worker samples (N = 100) were collected alive in the brood nest in summer (18-08-2007) at the beginning of the experiment and in fall (22/11/2007). These two samplings were called “Summer” and “Fall”. Another sampling, “Winter”, was ultimately performed during winter but at different times according to the destiny of the colony: in colonies which survived winter, bees were collected on 28/01/2008 while for the colonies that did not survive, this sampling was done just before collapsing from 30/11/2007 to 28/01/2008. Colony-level traits (areas covered with bees, number of cells with open, sealed brood, honey and pollen) were estimated in dm2 every 3 weeks from September until the end of October and at the beginning of March until May using the Liebefelder standard method [43].

2. Molecular approaches

Pools of 100 workers were collected alive from the brood nests of each colony and immediately frozen at −20°C. For total RNA extraction, bees were first homogenized in 20 ml of Tris-NaCl buffer (Tris 10 mM; NaCl 400 mM; pH 7.5). An aliquot of 50 µl of the homogenate was used for RNA extraction with the NucleoSpin RNA II Kit® (Macherey-Nagel) following the recommendations of the supplier. Then, cDNA was immediately processed using M-MLV reverse transcriptase (Invitrogen) and random hexamers [44]. These samples were checked for the presence of eight honey bee viruses (DWV, ABPV, IAPV, Chronic bee paralysis virus, Kashmir bee virus, Black queen cell virus, Sacbrood virus and Slow bee paralysis virus), using a qualitative PCR assay [31], [44], [45] with viral cDNA for positive control and water for the negative control. DWV, BQCV and ABPV positive samples were further processed for the quantification of viral titers using quantitative PCR (qPCR). The microsporidians N. ceranae and N. apis were quantified as well in each sample using qPCR [31]. In parallel, the expression levels of A. mellifera transcripts including vitellogenin, eater and hymenoptaecin were monitored using qPCR [46]. In order to normalize the data according to the amount of RNA in the sample, analysis of the β-actin gene was performed in parallel for each sample [47]. For all the targets except DWV, normalization was done using the comparative quantification method (delta CT method) [48]. DWV loads in samples were quantified by absolute quantification method using standard curves made of serial dilutions of known amounts of the amplicons [49] and presented as equivalent copies of DWV genome. All qPCR reactions were conducted using a thermal profile of: 50°C (2 min) then 95°C (10 min) followed by 40 cycles of 95°C (15 s), 60°C (1 min). Because qPCR assays were performed using SYBR-Green (Eurogentec), a melting curve was performed at the end of each run to ascertain the amplification of the target.

3. Data analyses

The bee colony samples were divided into two groups according to their winter survival. The first group (DC: dead colonies) consisted of 13 colonies which died during winter; most of these (11 out of 13) belonged to the set of colonies that received no treatment against V. destructor. The second group (SC: surviving colonies) included the 16 colonies that survived winter and coincided with the colonies that received a treatment against the mite. The variation estimates of transcript abundance of the studied variable between different groups were evaluated by using two tailed t-tests and non-parametric Kruskal–Wallis test as appropriate. Since DWV values covered a wide range, the data were transformed as the log10 DWV. For survival analysis, a Kaplan–Meier survival analysis was performed and used to compare the groups using Mantel-Hansel tests. Linear Models were also performed using Standard Least squares fitting in the Fit Model platform of JMP software to test the effects of colony status when nested within season. To visualize the results, regression diagnostics were performed with the model leverage plot. This allowed us to test if the variables are predictive on overwintering abilities and also to check the influence of each point on each hypothesis test. Multivariate Spearman correlations were performed between the variables (Pathogens and physiological markers). P-values below 0.05 were considered significant. The analyses were performed using Systat 12® and JMP® software.


1. Bee population measurements and timing of colony collapse

While the colony size did not differ significantly in September between SC and DC groups (Figure 1; Mean: 12743.75 bees and 13376.92 respectively, Mann-Whitney test P = 0.07), a significant decrease in population was observed in October (29/10/2007) in the group of colonies that died during winter (Mann-Whitney test, P<0.01, Figure 1 A). In the untreated group most of the colonies collapsed during December 2007 (N = 9) and two out of 11 died before February 2008. Two colonies properly treated against V. destructor mites died during winter but later in the season (end of February) and obviously because of queen failure (these colonies became drone layers). The rest of the colonies did develop with an increased population as expected in this season (Figure 1 A). The V. destructor infestation levels and timing of treatments are indicated in Figure 1 B. After each mite treatment, we had considerable treatment Varroa fall confirming the treatment efficacy. From August to September, the natural daily mite fall in the surviving colonies decreased from [average ± SE] 8.13±1.95 to 5.21±0.5 per day with 0.377±0.089 after the last oxalic acid treatment.


Figure 1. Colony strength and V. destructor natural mite fall.

A) Colony strength (Y-axis) by sampling month in 2007/2008 (X-axis) for the colonies that died during winter (DC, black boxes) and the ones that survived (SC, grey boxes). P value is indicated (Mann-Whitney test): **P<0.01. Number of live colonies is given (N). B) Natural average V. destructor mite fall in 2007/2008 on the hive bottom boards per day per colony (Y-axis) for the two groups Dying Colonies (DC) and Surviving Colonies (SC) over the experimental period. (X-axis) Infestation levels [average ± SD] are shown for each month and timing of treatments (OA = Oxalic Acid, FA = Formic acid) is indicated by arrows (n.v. = no value).


2. Parasites and Pathogens

The number of V. destructor mites collected during the course of the experiment in the DC group exceeded those collected in the SC group (Figure 1 B and 2 C). The mite level in the DC increased constantly until October before decreasing slightly thereafter. Mite loads in the surviving colonies dropped substantially from October to the winter sample.


Figure 2. Seasonal variability in Summer, Fall and Winter.

A) Pathogens B) Gene expression profiles C) V. destructor. The Y-axis shows the relative quantities except for DWV, where it shows equivalent genome copies and the X-axis displays the groups Dying Colonies DC (N = 13) and Surviving Colonies SC (N = 16). Significant differences (Two tailed t-test) are indicated with * = P<0.05 and ** = P<0.01.


Only five honey bee viruses (DWV, BQCV, ABPV, SBV and SPV) were detected in the experimental colonies (Table 1). The viruses CBPV, KBV and IAPV were not detected. DWV had 56.25% prevalence for SC and 61.5% for DC in summer. Almost all colonies were positive for this virus in fall (93.75% for SC and 100% for DC). Conversely, BQCV and SBV displayed a lower prevalence during the cold season, with no detectable SBV sample in the fall sample. We failed to detect SPV in summer and this virus was identified in less than 20% of the samples collected in fall in both DC and SC groups. No SPV could be detected in the bees that survived winter although the virus was detected in three colonies of the DC just before colony collapse. Although all colonies were positive for N. ceranae, N. apis could not be detected. The prevalence of N. ceranae was equivalent between the groups in all seasons and ranged between 18.75% and 50% (Table 1). No distinction could be made in terms of numbers of the detected investigated pathogens between the SC and DC groups in any season as shown in table 1 (Mann-Whitney U-tests, Summer: P = 0.729; Fall: P = 0.854, Winter: P = 0.359).


Table 1. Proportion of colonies with detectable levels of pathogens as measured by PCR and qPCR in surviving (SC) and dying (DC) colonies.


3. Expression levels of bee pathogens and genes related to the bee immunity

As none of the qualitative PCR analysis showed significant differences between surviving colonies and colonies that died during winter (Table 1), we conducted quantitative analyses from samples collected in summer, fall and winter in order to point out potential differences. Because winter samples from the DC group were collected just before collapsing and therefore at different time points during winter, data analyses are presented separately for DC and SC groups (Fig. 2). We measured the expression levels of three pathogens (DWV, BQCV and N. ceranae) based on their high prevalence in our samples and their potential pathogenic effects at the colony level. ABPV was excluded from these assays because only three samples were found infected by this virus. In addition, we completed these analyses by measuring in parallel the expression levels of three A. mellifera genes involved in bee immune defenses (hymenoptaecin and eater) or bee life expectancy (vitellogenin).

Seasonal variation.

Without considering the outcome of the colonies (death or survival during winter), seasonal variation was observed between summer and fall (Figure 3). DWV expression was higher in fall than in summer (P<0.001), but conversely BQCV titers were lower in fall than in summer (P<0.001). N. ceranae quantification showed equivalent titers between summer and fall (P = 0.479). Vitellogenin mRNA titers remained stable between summer and fall (P = 0.544) while hymenoptaecin mRNA levels were higher in fall than in summer (P<0.001). Conversely, eater expression was significantly reduced in fall compared to summer (P<0.001).


Figure 3. Overall seasonal variability of colonies (N = 29) from Summer to Winter.

A) Pathogens B) Genes C) V. destructor. The Y-axis show the relative quantities except for DWV, where it shows equivalent genome copies [log10]. The seasons summer, fall and winter are shown on the X-axis. (Mann-Whitney test with Bonferoni correction,* P<0.05; **P<0.01; ***P<0.001).


Such comparisons between fall and winter were more difficult to address, especially for colonies that died during winter, because the sampling was done just before the population decline and thus for this group, winter sampling encompassed several weeks, from December, when most of these colonies died, to January. In contrast, all samples were collected by the end of January in colonies that survived winter. The results are presented in table 2. In the group that died during winter, significant differences could be observed between samples collected in fall and those collected upon collapsing but only for BQCV which displayed increasing levels (P<0.001) and the eater gene for which expression conversely decreased (P<0.05). The levels of N. ceranae remained stable (P = 0.94). In the surviving group, significant variations were observed between fall and winter: N. ceranae levels decreased (P<0.001) as well as eater (P<0.001) and vitellogenin (P<0.001) mRNA levels. In contrast, DWV increased (P<0.05) as well as BQCV (P<0.05). Levels of hymenoptaecin were stable (P = 0.981).


Table 2. Seasonal variability for all colonies together from Summer to Winter for pathogen loads, Varroa destructor (Vd) and expression levels for vitellogenin and immune genes.

Comparisons between DC and SC groups.

Significant variations were observed in the fall between DC and SC groups, but only for DWV, N. ceranae and vitellogenin mRNA (Figure 2). No differences in any of the targets analyzed here were observed in summer between the two groups. DWV loads were higher in fall in the collapsing colonies than in the surviving ones (P<0.01). In fall, colonies that collapsed during winter displayed lower levels of N. ceranae than surviving ones (P<0.05).while in the summer N. ceranae levels were similar in both DC and SC groups (P = 0.483).Variations in BQCV titers between SC and DC groups were only observed in winter (P<0.05). While no vitellogenin differences could be observed in summer between both SC and DC groups, this gene displayed significantly higher expression levels in fall in the surviving colonies than in the DC group (P<0.05).

4 Correlations between markers

Correlations between the six markers were observed (Figure 4). In summer, DWV vs. hymenoptaecin (rs = 0.50, P<0.01), hymenoptaecin vs. eater (rs = 0.46; P<0.05), vitellogenin vs. eater (rs = 0.88, P<0.001) and vitellogenin vs. hymenoptaecin (rs = 0.37, P<0.05) showed significantly positive correlations. In fall, these correlations were not observed anymore but BQCV showed a positive correlation with N. ceranae (rs = 0.44, P<0.05). In fall, the number of V. destructor mites collected on bottom boards was significantly correlated with both DWV (positively) and vitellogenin (negatively) expression levels (rs = 0.57, P<0.05 and rs = −0.37, P<0.05, respectively). In contrast, V. destructor correlated positively in winter with N. ceranae (rs = 0.41, P<0.05), Eater (rs = 0.58, P<0.01) and vitellogenin (rs = 0.45, P<0.05). Full data are presented in Figure 4.


Figure 4. Spearman rank correlations for the different variables who showed significant P values (P<0.05, indicated in bold) for the three seasons summer, fall and winter (N = 29 colonies).

The variables shown are: Hym = Hymenoptaecin, Vg = Vitellogenin, Eater, NCer = Nosema ceranane, DWV, BQCV and Vd = Varroa destructor.


5. Identification of predictive markers for colony collapse

Using a linear model (see M&M) the results show that over all seasons, DWV (P<0.05), V. destructor (P<0.001), N. ceranae (P<0.001) and vitellogenin (P<0.001) could be considered as predictive markers for winter losses. This was not the case for BQCV (P = 0.467), eater (P = 0.173) and hymenoptaecin (P = 0.376) which displayed few variations between DC and SC groups either in summer or in fall. However, the model showed that there is a significant seasonal impact on the expression of these markers (DWV: P<0.05; V. destructor: P<0.01, N. ceranae: P<0.05 and vitellogenin: P<0.01). Then in summer only V. destructor (P<0.01) could be considered as a significant predictive marker while in fall, DWV (increased; P<0.01), V. destructor (increased; P<0.01), N. ceranae (decreased; P<0.05) and Vitellogenin (decreased; P<0.05) could be considered as significant predictors of colony collapse.


Here we showed that both V. destructor and DWV are strong predictive markers for honey bee colony death during winter.

Among the high number of microorganisms which are coexisting with honey bee colonies, most are opportunistic and induce troubles under as-yet undefined environmental conditions. It is then crucial for establishing a proper diagnosis of bee diseases to be able to distinguish between a normal situation and a pathogenic one. This can be partly achieved by measuring the expression levels of pathogens in honey bees using quantitative techniques, although data can only be recorded when clinical signs are detected or after colony collapse. Here we present a novel approach, which consists of identifying markers which could predict the destiny of the colony during winter. These markers may help to establish reliable diagnostic tools in relation with field observations, and ultimately to identify the causes of colony mortality.

1. Varroa destructor is strongly associated with colony collapse during winter

In our assay, all of the colonies which were left untreated died during winter, while only two colonies collapsed despite proper treatment. These two colonies collapsed late in the season (in February) in comparison with the majority of the other colonies which died before the end of December. These two colonies had an over-abundance of male bees, arguably a sign of failing queen fecundity. Colonies that died during winter had significantly more mites than the surviving group either in summer, fall or winter. V. destructor loads were thus very predictive of colony death and, in fact, provided the only predictive marker in summer. The mite level in the colonies which died during winter increased to reach a peak in October and decreased thereafter following the drop in colony size.

2. DWV is a predictive marker of colony collapse

Several bee viruses were identified. Apart from SPV which was only detected in highly mite-infested colonies here and rarely in previous surveys of European bees [45], [50], DWV, SBV and BQCV are commonly detected in western honey bee colonies all around the world, most of the time in the absence of clinical signs, although these viruses can be pathogenic under favorable environmental circumstances [20]. We found a significant increase of DWV titers between summer and fall. This result is consistent with previous reports showing an increase in DWV titers in fall [49], which probably reflects the close link between DWV and V. destructor since mite numbers climb rapidly from summer to fall. It is also illustrated with the significant positive correlation in fall between V. destructor and DWV. This mite is indeed an efficient vector of DWV, transmitting it upon feeding on bee pupae or during the phoretic phase of its biological cycle on adult bees [14], [51], [52]. The mite seems also competent for replication of the virus thereby increasing DWV prevalence and titers in mite infested colonies [33], [53]. Proper treatments of bee colonies against V. destructor drastically reduced DWV titers in colonies supporting arguments that this virus is not efficiently horizontally transmitted in the absence of mites [54] and that vertical transmission routes are unlikely to generate heavy loads in bee progeny. We found higher DWV titers in collapsing colonies than in the surviving group suggesting that this virus might be involved in the process of collapsing. DWV was shown to replicate in various bee tissues including fat body, a key tissue involved in many physiological processes including immune defenses [34], [55]. In particular, the fat body is the site for production of the egg yolk protein vitellogenin [34], [56]. Vitellogenin is involved in immunity and ageing through hormonal regulatory pathways and is therefore a common molecular marker for the overall health and lifespan of individual bees [57]. One can hypothesize that DWV replication impairs the expression of vitellogenin in fat body cells, which could explain why we found significantly less vitellogenin mRNA titers in collapsing colonies than in surviving ones. In addition, V. destructor infestation levels and vitellogenin were significant negatively correlated in fall. The data agree well with a previous study showing a reduction of Vitellogenin titers in mite infested workers [58], although DWV quantification was not addressed in the prior study. Put together, this reinforces the hypothesis of an impact of DWV on fat body function.

3. Nosema ceranae titers are higher in healthy colonies

N. ceranae is a microsporidian intracellular parasite suspected to have replaced its common relative N. apis during the last decade [59], [60], although there are some reports showing that N. ceranae has been present in western honey bees for greater than twenty years [59], [61]. This parasite replicates in the bee gut and is therefore a potent pathogen of bee colonies even if its pathogenicity has only been observed in experimental conditions. These infections are very common in the absence of clinical symptoms and recent reports have shown that this parasite is not involved in bee colony collapses in Europe [5], [39] except in Spain [36], [62]. Our results support that N. ceranae is not involved in colony collapse, because no significant differences were observed between colonies that died during winter and those which survived. Likewise, we did not observe an increase of N. ceranae titers from summer to fall, even in December when colonies were about to die. No N. apis were detected in any sample in spite of the fact that this species has a lower temperature preference than N. ceranae and might therefore be favored in temperate climates such as in Switzerland [60], [63]. In a case study in Switzerland, N. apis was detected only in mixed infections with N. ceranae [64], consistent with these results.

4. Immune genes are upregulated in dying colonies

We monitored the expression of three A. mellifera genes involved in humoral and cellular immune defenses to identify physiological responses that may occur before colony collapse. In workers, in addition to being the precursor of royal jelly proteins produced by nurses to feed the larvae, the egg yolk glycoprotein vitellogenin displays multiple functions affecting important physiological pathways [65]. Among these, it has been shown that vitellogenin plays a role in bee immunity as a zinc transporter [66]. Hymenoptaecin is an antimicrobial peptide, which is highly expressed in the bee hemolymph after challenge with bacterial infections [48], [67]. Eater is a major phagocytic receptor for a broad range of bacterial pathogens in Drosophila [68] and its homolog was identified in the honey bee genome [48], [69].

The analysis of such markers from pooled individuals is complex, especially for samples collected in summer, which contained a mix of workers of different ages, because the expression of these genes might also vary according to the age-related task of worker bees. In foragers it has been shown that the vitellogenin titers as well as the number of hemocytes were strongly reduced compared to the nurse bees [70], [71]. Furthermore, no data are available concerning the gene expression patterns of winter bees. Despite that, we observed significant seasonal variations among these genes. While vitellogenin expression remained stable from summer to fall, hymenoptaecin and eater displayed opposite expression patterns in both groups of colonies (surviving and non surviving colonies). The rapid decrease of eater from summer to fall suggests that hemocyte numbers are reduced in winter bees while humoral immune responses are activated. Data analyses from fall to winter in samples collected from colonies that did not survive winter (mostly collected in December before collapsing) showed no variation in either vitellogenin or hymenoptaecin mRNA levels while eater displayed a slight increase. In contrast, samples collected from colonies that survived winter showed a very high increase of both vitellogenin and eater transcripts while hymenoptaecin kept stable. Since these samples were collected at the end of January, these results may point out a different physiological state of bees collected in winter clusters two months apart. One can hypothesize that V. destructor – DWV – N. ceranae may induce different immune signaling transduction pathways than the pathway, leading to the immune transcript hymenoptaecin [48]. As such, none of the immune genes could be identified as significant predictive markers, while vitellogenin does seem to be a viable marker.

5. Varroa destructor and DWV are strong predictive markers for colony collapse during winter

From the putative investigated markers, four of them were shown to be good predictive ones but seasonal. Among them, V. destructor and DWV were already identified during summer as strong predictive markers for collapsing during winter. As winter bees are reared as soon as mid-summer until mid-September in Switzerland [72], these data suggest that V. destructor infestations levels in colonies should be estimated by beekeepers as soon as summertime in order to anticipate winter colony losses. Therefore, recording of DWV loads might not be as suitable since DWV was shown to be a strong marker of winter colony collapse in fall but not in summer.

In general, the results presented here are in line with those of several studies showing that V. destructor and DWV are associated with colony losses in winter [5], [6], [8], [22], and in contrast to analyses of the enigmatic Colony Collapse Disorder in the U.S., for which mite numbers were a poor correlate with CCD risk [31].

6. Conclusion

This study provides evidence that Varroa destructor is a key player for winter colony losses and highlights the urgent need for efficient treatments against this parasite. The data suggest an indirect effect of mite infestation on honeybee overwintering abilities through the promotion of opportunistic viral infections, which eventually lead to the impairment of critical physiological functions. The knowledge gathered in this work will help to improve our understanding of bee losses, standardize methods for biomarkers of disease and finally to mitigate causes of bee declines.


We would like to address our thanks to Hélène Berthoud, Monika Haueter, Alexandra Roetschi and Rolf Kuhn for their valuable assistance. Our thanks are also addressed to Dawn Lopez for technical assistance in USA and Virginia Williams for editorial comments. Use of commercial names in this paper is for informational purposes only.

Author Contributions

Conceived and designed the experiments: BD PN. Performed the experiments: BD. Analyzed the data: BD JDE YPC. Contributed reagents/materials/analysis tools: BD LG PN. Wrote the paper: BD JDE YPC LG PN.


  1. 1. Aebi A, Vaissière BE, vanEngelsdorp D, Delaplane K, Roubik DW, et al. (2012) Back to the future: Apis vs. non-Apis pollination. Trends Ecol Evol 27: In press.
  2. 2. Neumann P, Carreck NL (2010) Honey bee colony losses. J Apic Res 49: 1–6. doi:10.3896/IBRA.
  3. 3. Potts SG, Biesmeijer JC, Kremen C, Neumann P, Schweiger O, et al. (2010) Global pollinator declines: drivers and impacts. Trends Ecol Evol 25: 345–353.
  4. 4. Rosenkranz P, Aumeier P, Ziegelmann B (2010) Biology and control of Varroa destructor. J Invertebr Pathol 103: 96–119. doi:10.1016/j.jip.2009.07.016.
  5. 5. Genersch E, von der Ohe W, Kaatz H, Schroeder A, Otten C, et al. (2010) The German bee monitoring project: a long term study to understand periodically high winter losses of honey bee colonies. Apidologie 41: 332–352. doi:10.1051/apido/2010014.
  6. 6. Schäfer MO, Ritter W, Pettis JS, Neumann P (2010) Winter losses of honeybee colonies (Hymenoptera: Apidae): The role of infestations with Aethina tumida (Coleoptera: Nitidulidae) and Varroa destructor (Parasitiformes: Varroidae). J Econ Entomol 103: 10–16.
  7. 7. Dahle B (2010) The role of Varroa destructor for honey bee colony losses in Norway. J Apic Res 49: 124–125. doi:10.3896/IBRA.
  8. 8. Guzman-Novoa E, Eccles L, Calvete Y, Mcgowan J, Kelly PG, et al. (2010) Varroa destructor is the main culprit for the death and reduced populations of overwintered honey bee (Apis mellifera) colonies in Ontario, Canada. Apidologie 41: 443–450. doi:10.1051/apido/2009076.
  9. 9. Ball BV (1988) The impact of secondary infections in honey-bee colonies infested with the parasitic mite Varroa jacobsoni. In: Needham GR, Page RE, Delfinado-Baker M, Bowman CE, editors. Africanized Honeybees and Bee Mites. Chichester, London, UK: Ellis Horwood. pp. 457–461.
  10. 10. Yang XL, Cox-Foster DL (2005) Impact of an ectoparasite on the immunity and pathology of an invertebrate: Evidence for host immunosuppression and viral amplification. Proc Natl Acad Sci U S A 102: 7470–7475.
  11. 11. Gregory PG, Evans JD, Rinderer T, de Guzman L (2005) Conditional immune-gene suppression of honeybees parasitized by Varroa mites. J Insect Sci 5: 7.
  12. 12. Yang X, Cox-Foster D (2007) Effects of parasitization by Varroa destructor on survivorship and physiological traits of Apis mellifera in correlation with viral incidence and microbial challenge. Parasitology 134: 405–412.
  13. 13. Ball BV, Allen MF (1988) The prevalence of pathogens in honey bee Apis mellifera colonies infested with the parasitic mite Varroa jacobsoni. Ann Appl Biol 113: 237–244.
  14. 14. Bowen-Walker PL, Martin SJ, Gunn A (1999) The transmission of deformed wing virus between honeybees (Apis mellifera L.) by the ectoparasitic mite Varroa jacobsoni Oud. J Invertebr Pathol 73: 101–106.
  15. 15. Chen YP, Pettis JS, Evans JD, Kramer M, Feldlaufer MF (2004) Transmission of Kashmir bee virus by the ectoparasitic mite Varroa destructor. Apidologie 35: 441–448.
  16. 16. Shen MQ, Cui LW, Ostiguy N, Cox-Foster D (2005) Intricate transmission routes and interactions between picorna-like viruses (Kashmir bee virus and sacbrood virus) with the honeybee host and the parasitic varroa mite. J Gen Virol 86: 2281–2289.
  17. 17. Shen MQ, Yang XL, Cox-Foster D, Cui LW (2005) The role of varroa mites in infections of Kashmir bee virus (KBV) and deformed wing virus (DWV) in honey bees. Virology 342: 141–149.
  18. 18. Dall DJ (1985) Inapparent infection of honey bee pupae by Kashmir and sacbrood bee viruses in Australia. Ann Appl Biol 106: 461–468.
  19. 19. Anderson DL, Gibbs AJ (1988) Inapparent virus infections and their interactions in pupae of the honey bee (Apis mellifera Linnaeus) in Australia. J Gen Virol 69: 1617–1625.
  20. 20. Chen YP, Siede R (2007) Honey bee viruses. Advances in Virus Research Vol 70: 33–80.
  21. 21. Cox-Foster DL, Conlan S, Holmes EC, Palacios G, Evans JD, et al. (2007) A metagenomic survey of microbes in honey bee colony collapse disorder. Science 318: 283–287.
  22. 22. Highfield AC, El Nagar A, Mackinder LCM, Noel LMLJ, Hall MJ, et al. (2009) Deformed wing virus implicated in overwintering honeybee colony losses. Appl Environ Microbiol 75: 7212–7220.
  23. 23. Berthoud H, Imdorf A, Haueter M, Radloff S, Neumann P (2010) Virus infections and winter losses of honey bee colonies (Apis mellifera). J Apic Res 49: 60–65. doi:10.3896/IBRA.
  24. 24. Lanzi G, de Miranda JR, Boniotti MB, Cameron CE, Lavazza A, et al. (2006) Molecular and biological characterization of deformed wing virus of honeybees (Apis mellifera L.). J Virol 80: 4998–5009.
  25. 25. Bailey L, Gibbs AJ, Woods RD (1963) Two viruses from adult honey bees (Apis mellifera Linnaeus). Virology 21: 390–395.
  26. 26. Govan VA, Leat N, Allsopp M, Davison S (2000) Analysis of the complete genome sequence of acute bee paralysis virus shows that it belongs to the novel group of insect-infecting RNA viruses. Virology 277: 457–463.
  27. 27. Maori E, Lavi S, Mozes-Koch R, Gantman Y, Peretz Y, et al. (2007) Isolation and characterization of Israeli acute paralysis virus, a dicistrovirus affecting honeybees in Israel: evidence for diversity due to intra- and inter-species recombination. J Gen Virol 88: 3428–3438.
  28. 28. Di Prisco G, Pennacchio F, Caprio E, Boncristiani HF, Evans JD, et al. (2011) Varroa destructor is an effective vector of Israeli acute paralysis virus in the honeybee, Apis mellifera. J Gen Virol 92: 151–155. doi:10.1099/vir.0.023853-0.
  29. 29. Ribière M, Ball BV, Aubert M (2008) Natural history and geographic distribution of honey bee viruses. In: Aubert M, Ball BV, Fries I, Moritz R, Milani N, et al., editors. Virology and the honey bee. Luxembourg: European Communities. pp. 15–84.
  30. 30. vanEngelsdorp D, Hayes J, Underwood RM, Pettis J (2008) A survey of honey bee colony losses in the US, fall 2007 to spring 2008. Plos One 3: e4071.
  31. 31. vanEngelsdorp D, Evans JD, Saegerman C, Mullin C, Haubruge E, et al. (2009) Colony collapse disorder: A descriptive study. Plos One 4: e6481.
  32. 32. de Miranda JR, Cordoni G, Budge G (2010) The acute bee paralysis virus - Kashmir bee virus - Israeli acute paralysis virus complex. J Invertebr Pathol 103: 30–47. doi:10.1016/j.jip.2009.06.014.
  33. 33. de Miranda JR, Genersch E (2010) Deformed wing virus. J Invertebr Pathol 103: S48–S61. doi:10.1016/j.jip.2009.06.012.
  34. 34. Fievet J, Tentcheva D, Gauthier L, de Miranda J, Cousserans F, et al. (2006) Localization of deformed wing virus infection in queen and drone Apis mellifera L. Virology Journal 3: 1–5.
  35. 35. Boncristiani HF, Di Prisco G, Pettis JS, Hamilton M, Chen YP (2009) Molecular approaches to the analysis of deformed wing virus replication and pathogenesis in the honey bee, Apis mellifera. Virology Journal 6: 1–9. doi:10.1186/1743-422X-6-221.
  36. 36. Higes M, Martin-Hernandez R, Botias C, Bailon EG, Gonzalez-Porto AV, et al. (2008) How natural infection by Nosema ceranae causes honeybee colony collapse. Environ Microbiol 10: 2659–2669.
  37. 37. Higes M, Martin-Hernandez R, Martinez-Salvador A, Garrido-Bailon E, Gonzalez-Porto AV, et al. (2010) A preliminary study of the epidemiological factors related to honey bee colony loss in Spain. Environ Microbiol Rep 2: 243–250. doi:10.1111/j.1758-2229.2009.00099.x.
  38. 38. Chauzat MP, Martel AC, Zeggane S, Drajnudel P, Schurr F, et al. (2010) A case control study and a survey on mortalities of honey bee colonies (Apis mellifera) in France during the winter of 2005–6. J Apic Res 49: 40–51. doi:10.3896/IBRA.
  39. 39. Gisder S, Hedtke K, Mockel N, Frielitz MC, Linde A, et al. (2010) Five-Year Cohort Study of Nosema spp. in Germany: Does Climate Shape Virulence and Assertiveness of Nosema ceranae? Appl Environ Microbiol 76: 3032–3038. doi:10.1128/AEM.03097-09.
  40. 40. Imdorf A, Charrière JD, Kilchenmann V, Bogdanov S, Fluri P (2003) Alternative strategy in central Europe for the control of Varroa destructor in honey bee colonies. Apiacta 38: 258–278.
  41. 41. Goodwin RM, Taylor MA, McBrydie HM, Cox HM (2006) Drift of Varroa destructor-infested worker honey bees to neighbouring colonies. J Apic Res 45: 155–156.
  42. 42. Imdorf A, Charrière JD (1998) What is the Varroa population in my colonies ? Bee Biz 7: 37.
  43. 43. Imdorf A, Bühlmann G, Gerig L, Kilchenmann V, Wille H (1987) Überprüfung der Schätzmethode zur Ermittlung der Brutfläche und der Anzahl Arbeiterinnen in freifliegenden Bienenvölkern. Apidologie 18: 137–146.
  44. 44. Tentcheva D, Gauthier L, Zappulla N, Dainat B, Cousserans F, et al. (2004) Prevalence and seasonal variations of six bee viruses in Apis mellifera L. and Varroa destructor mite populations in France. Appl Environ Microbiol 70: 7185–7191.
  45. 45. de Miranda JR, Dainat B, Locke B, Cordoni G, Berthoud H, et al. (2010) Genetic characterization of slow bee paralysis virus of the honeybee (Apis mellifera L.). J Gen Virol 91: 2524–2530. doi:10.1099/vir.0.022434-0.
  46. 46. Evans JD (2006) Beepath: An ordered quantitative-PCR array for exploring honey bee immunity and disease. J Invertebr Pathol 93: 135–139.
  47. 47. Lourenco AP, Mackert A, Cristino AD, Simoes ZLP (2008) Validation of reference genes for gene expression studies in the honey bee, Apis mellifera, by quantitative real-time RT-PCR. Apidologie 39: 372-U33.
  48. 48. Evans JD, Aronstein K, Chen YP, Hetru C, Imler JL, et al. (2006) Immune pathways and defence mechanisms in honey bees Apis mellifera. Insect Mol Biol 15: 645–656.
  49. 49. Gauthier L, Tentcheva D, Tournaire M, Dainat B, Cousserans F, et al. (2007) Viral load estimation in asymptomatic honey bee colonies using the quantitative RT-PCR technique. Apidologie 38: 426–436.
  50. 50. Ball BV, Bailey L (1997) Viruses. In: Morse RA, Flottum K, editors. Honey bee pests, predators & diseases. Medina, OH: A.I. Root Company. pp. 11–31.
  51. 51. Santillan-Galicia MT, Ball BV, Clark SJ, Alderson PG (2010) Transmission of deformed wing virus and slow paralysis virus to adult bees (Apis mellifera L.) by Varroa destructor. J Apic Res 49: 141–148. doi:10.3896/IBRA.
  52. 52. Mockel N, Gisder S, Genersch E (2011) Horizontal transmission of deformed wing virus: pathological consequences in adult bees (Apis mellifera) depend on the transmission route. J Gen Virol 92: 370–377. doi:10.1099/vir.0.025940-0.
  53. 53. Gisder S, Aumeier P, Genersch E (2009) Deformed wing virus: replication and viral load in mites (Varroa destructor). J Gen Virol 90: 463–467.
  54. 54. Sumpter DJT, Martin SJ (2004) The dynamics of virus epidemics in Varroa-infested honey bee colonies. J Anim Ecol 73: 51–63.
  55. 55. Trenczek T, Faye I (1988) Synthesis of immune proteins in primary cultures of fat body from Hyalophora cecropia. Insect Biochem 18: 299–312.
  56. 56. Tufail M, Takeda M (2008) Molecular characteristics of insect vitellogenins. J Insect Physiol 54: 1447–1458.
  57. 57. Munch D, Amdam GV, Wolschin F (2008) Ageing in a eusocial insect: molecular and physiological characteristics of life span plasticity in the honey bee. Funct Ecol 22: 407–421.
  58. 58. Amdam GV, Hartfelder K, Norberg K, Hagen A, Omholt SW (2004) Altered physiology in worker honey bees (Hymenoptera : Apidae) infested with the mite Varroa destructor (Acari : Varroidae): A factor in colony loss during overwintering? J Econ Entomol 97: 741–747.
  59. 59. Paxton RJ, Klee J, Korpela S, Fries I (2007) Nosema ceranae has infected Apis mellifera in Europe since at least 1998 and may be more virulent than Nosema apis. Apidologie 38: 558–565.
  60. 60. Fries I (2010) Nosema ceranae in European honey bees (Apis mellifera). J Invertebr Pathol 103: S73–S79. doi:10.1016/j.jip.2009.06.017.
  61. 61. Chen Y, Evans JD, Smith IB, Pettis JS (2008) 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 97: 186–188.
  62. 62. Higes M, Martin-Hernandez R, Garrido-Bailon E, Gonzalez-Porto AV, Garcia-Palencia P, et al. (2009) Honeybee colony collapse due to Nosema ceranae in professional apiaries. Environ Microbiol Rep 1: 110–113. doi:10.1111/j.1758-2229.2009.00014.x.
  63. 63. Higes M, Garcia-Palencia P, Botias C, Meana A, Martin-Hernandez R (2010) The differential development of microsporidia infecting worker honey bee (Apis mellifera) at increasing incubation temperature. Environ Microbiol Rep 2: 745–748.
  64. 64. Dainat B, vanEngelsdorp D, Neumann P (2012) CCD in Europe?. Environ Microbiol Rep. doi:10.1111/j.1758-2229.2011.00312.x.
  65. 65. Amdam GV, Norberg K, Hagen A, Omholt SW (2003) Social exploitation of vitellogenin. Proc Natl Acad Sci U S A 100: 1799–1802.
  66. 66. Amdam GV, Simoes ZLP, Hagen A, Norberg K, Schroder K, et al. (2004) Hormonal control of the yolk precursor vitellogenin regulates immune function and longevity in honeybees. Exp Gerontol 39: 767–773.
  67. 67. Chan QWT, Melathopoulos AP, Pernal SF, Foster LJ (2009) The innate immune and systemic response in honey bees to a bacterial pathogen, Paenibacillus larvae. Bmc Genomics 10: 387.
  68. 68. Kocks C, Cho JH, Nehme N, Ulvila J, Pearson AM, et al. (2005) Eater, a transmembrane protein mediating phagocytosis of bacterial pathogens in drosophila. Cell 123: 335–346.
  69. 69. Simone M, Evans JD, Spivak M (2009) Resin Collection and Social Immunity in Honey Bees. Evolution 63: 3016–3022.
  70. 70. Wilson-Rich N, Dres ST, Starks PT (2008) The ontogeny of immunity: Development of innate immune strength in the honey bee (Apis mellifera). J Insect Physiol 54: 1392–1399.
  71. 71. Schmid MR, Brockmann A, Pirk CWW, Stanley DW, Tautz J (2008) Adult honeybees (Apis mellifera L.) abandon hemocytic, but not phenoloxidase-based immunity. J Insect Physiol 54: 439–444.
  72. 72. Merz R, Gerig L, Wille H, Leuthold R (1979) Das Problem der Kurz- und Langlebigkeit bei der Ein- und Auswinterung im Bienenvolk (Apis mellifica L.): eine Verhaltensstudie. Rev Suisse Zool 86: 663–671.