Lymphatic filariasis (LF) is a socio-economically devastating mosquito-borne Neglected Tropical Disease caused by parasitic filarial nematodes. The interaction between the parasite and host, both mosquito and human, during infection, development and persistence is dynamic and delicately balanced. Manipulation of this interface to the detriment of the parasite is a promising potential avenue to develop disease therapies but is prevented by our very limited understanding of the host-parasite relationship. Exosomes are bioactive small vesicles (30–120 nm) secreted by a wide range of cell types and involved in a wide range of physiological processes. Here, we report the identification and partial characterization of exosome-like vesicles (ELVs) released from the infective L3 stage of the human filarial parasite Brugia malayi. Exosome-like vesicles were isolated from parasites in culture media and electron microscopy and nanoparticle tracking analysis were used to confirm that vesicles produced by juvenile B. malayi are exosome-like based on size and morphology. We show that loss of parasite viability correlates with a time-dependent decay in vesicle size specificity and rate of release. The protein cargo of these vesicles is shown to include common exosomal protein markers and putative effector proteins. These Brugia-derived vesicles contain small RNA species that include microRNAs with host homology, suggesting a potential role in host manipulation. Confocal microscopy shows J774A.1, a murine macrophage cell line, internalize purified ELVs, and we demonstrate that these ELVs effectively stimulate a classically activated macrophage phenotype in J774A.1. To our knowledge, this is the first report of exosome-like vesicle release by a human parasitic nematode and our data suggest a novel mechanism by which human parasitic nematodes may actively direct the host responses to infection. Further interrogation of the makeup and function of these bioactive vesicles could seed new therapeutic strategies and unearth stage-specific diagnostic biomarkers.
Lymphatic filariasis is caused by parasitic nematodes that invade and occupy the host lymphatic system. The extent of lymphatic filariasis is staggering, with over 120 million people infected in 73 endemic countries and an estimated 40 million people suffering from a range of disfiguring and debilitating clinical manifestations of this disease. The mechanisms by which these medically important parasites navigate the host immune response to establish infection are not yet fully understood. In this study, we identify exosome-like vesicles (ELVs) that are abundantly released from infective stage L3 Brugia malayi, an etiological agent of human lymphatic filariasis. We show that these vesicles have a narrow size distribution and morphology consistent with classical exosomes, and that they contain common exosomal protein markers, putative effector proteins, as well as small regulatory RNAs. We show that ELVs are enriched with microRNAs that are perfectly conserved between parasite and host, suggesting a potentially novel mechanism by which filarial worms can actively manipulate host gene expression. We demonstrate that parasite ELVs are internalized by macrophages and elicit a classically activated phenotype in these host cells. The discovery of exosome-like vesicle release by human nematode parasites newly enlightens the roadmap to understanding the pathology of LF and related helminthiases. These vesicles also present promising new targets for intervention and diagnostics.
Citation: Zamanian M, Fraser LM, Agbedanu PN, Harischandra H, Moorhead AR, Day TA, et al. (2015) Release of Small RNA-containing Exosome-like Vesicles from the Human Filarial Parasite Brugia malayi. PLoS Negl Trop Dis9(9): e0004069. https://doi.org/10.1371/journal.pntd.0004069
Editor: Achim Hoerauf, Institute of Medical Microbiology, Immunology and Parasitology, GERMANY
Received: March 10, 2015; Accepted: August 18, 2015; Published: September 24, 2015
Copyright: © 2015 Zamanian et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited
Data Availability: All relevant data are within the paper and its Supporting Information files.
Funding: This work was supported by National Institute of Food and Agriculture Award 1001501 to MJK. URL: www.csrees.usda.gov. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
The parasitic filarial nematodes Wuchereria bancrofti, Brugia malayi and B. timori are etiological agents of Lymphatic filariasis (LF), a chronic and debilitating disease infecting over 120 million people in 73 endemic countries . Adult parasites reside in the lymphatic vasculature of infected individuals and release larvae called microfilariae, which are taken up by vector mosquitoes during the blood meal. Parasites rapidly develop within the mosquito, molting twice to the infective L3 stage [2, 3] before transmission to the definitive host during a subsequent blood meal. Following penetration of the vertebrate host via the puncture wound left by the mosquito, L3 stage parasites migrate to the lymphatics and undergo further growth and development, molting to the L4 stage and again to adulthood. The longevity of patent infection is remarkable; adults live for at least 8–10 years by general consensus. The ability of larval stages to successfully invade the host, and for adult worms to maintain infection for such an extended period of time, suggest filarial worms have developed strategies to both facilitate the establishment of infection and evade or manipulate the host immune response. Although the immunomodulatory capabilities of infecting larval and adult stage filarial worms have been well documented and reviewed [4–8], the parasite effector molecules responsible for manipulating host biology and their mechanisms of release have been difficult to define. Actively secreted proteins have historically been considered the principal candidates and several secreted proteins have been identified with demonstrable bioactivity at the host-parasite interface [9–12]. Adding to these, the characterization of parasitic nematode secretomes has revealed a complex array of potential proteinaceous effectors [13–16]. Other types of effector, including molecules expressed on the parasite surface may have a role  and the emergence of small noncoding RNAs as cell-to-cell agents of genetic regulation [18–22] hint at exciting alternative mechanisms.
Exosomes are a subtype of extracellular vesicle categorized by size (30–120 nm diameter) and defined by a particular biogenic pathway ; exosomes are formed by inward budding of vesicles in the late endosomal pathway to create multivesicular endosomes that fuse with the plasma membrane to effect release [24, 25]. Originally thought to be a means of cellular waste disposal, exosomes are now considered highly bioactive extracellular vesicles that facilitate cell-to-cell communication and are the focus of renewed investigation. The cargo of exosomes is complex and variable, containing bioactive proteins, functional mRNA, miRNA and other small non-coding RNA species [18, 26], likely reflecting both source and target environments. Fusion of the exosome to a target cell delivers this heterogeneous bioactive cargo and selectively alters the biology of the target tissue [19, 21, 26, 27]; the isolation of exosomes from circulatory systems and an array of biofluids suggests effector sites can be far from the point of release. Parasites are known to release exosome-like vesicles [27–30] and it is compelling to hypothesize that bioactive molecules secreted by parasitic nematodes, packaged in exosomes, function as cell-to-cell effectors in the host-parasite interaction. Indeed recently, extracellular vesicles secreted by the gastrointestinal nematode Heligmosomoides polygyrus, containing proteins and small RNA species, have been shown to alter gene expression in host cells and suppress innate immune responses in mice .
Here we show that larval and adult stage B. malayi secrete prodigious quantities of extracellular vesicles in vitro whose size and morphology are consistent with exosomes. These exosome-like extracellular vesicles (ELVs) contain small RNA species, including specific miRNA and are enriched in miRNA that are identical to host miRNAs with known immunomodulatory roles [31–34]. The protein cargo of the vesicles is relatively scant but includes bioactive proteins, proteins with putative RNA binding properties and proteins commonly associated with exosomes . The parasite ELVs are internalized by host macrophages and elicit a classically activated phenotype in these cells. The demonstration that filarial nematodes secrete exosomal RNA and proteins that potentially function at the host-parasite interface is significant. Defining this parasite effector toolkit exposes an array of new molecules that may be exploited in novel LF control strategies.
Results and Discussion
Infective-stage B. malayi release exosome-like vesicles
In order to ascertain whether exosomes are released by B. malayi, extracellular vesicles were isolated from parasites incubated in culture media using a filtration and ultracentrifugation protocol. We focused our initial discovery efforts on larval and adult stage parasites. L3, adult male, and adult female B. malayi were incubated in vitro for 24 hour periods under standard culture conditions, and purified vesicle preparations were evaluated with electron microscopy (EM). Infectious stage L3 parasites in culture release abundant 50–120 nm microvesicles consistent with the classical “deflated ball” morphology of mammalian and non-mammalian exosomes reported in the literature  (Fig 1A & 1B). We refer to these as exosome-like vesicles (ELVs) throughout this manuscript, in recognition that they cannot be unequivocally designated as exosomes, rather than another class of extracellular vesicles, because their biogenesis has not been determined. Preparations from adult stage B. malayi were more heterogenous and dilute, not allowing for the definitive categorization of putative exosome-like vesicles (Fig 1C). This, despite the fact a much higher mass of total parasite tissue was used for adult preparations as compared to larval preparations. These data suggest ELV release to be a predominantly larval phenomenon in B. malayi, a working hypothesis supported by analysis of RNA associated with the vesicles. We therefore chose to focus our subsequent experiments on L3 stage parasites. A compelling overall hypothesis for the function of B. malayi ELVs is that they mediate the secretion and trafficking to host cells of effector molecules that facilitate parasitism and the observation that ELV secretion occurs primarily in those parasite stages that infect the host and establish parasitemia is consistent with this narrative.
TEM images of L3 (A and B) and adult female (C) ELV preparations are shown. L3 vesicles take on a distinct morphology often reported in the literature. Adult isolations are more heterogenous and may require further optimization to achieve uniform vesicle preparation. White arrows show canonical L3 ELVs (B) and putative adult ELVs (C). This provides evidence for the release of exosome-like vesicles in the human-infective L3 stage of the parasite and much of the rest of the work we report is focused on vesicles derived from this larval stage.
Time course profile of exosome-like vesicle release from infectious stage B. malayi
To more accurately resolve the dynamics of ELV release in L3 B. malayi, we used a nanoparticle tracking analysis (NTA) system to measure vesicle output in a 72 hr in vitro time course. Media was collected from 300 worms after three successive 24 hr incubation periods, vesicles were purified by ultracentrifugation as before and individual vesicle preparations were analyzed via NanoSight LM10 as shown in Fig 2 (sample recording: S1 Video). Day 1 (0–24 hr in culture) preparations reveal a prolific ELV release rate (> 9,000 ELVs/parasite/min) with a very narrow size distribution centered at ∼90 nm. Day 2 (24–48 hr in culture) preparations show an essentially equivalent rate of release, but a stark broadening of the size distribution. Day 3 (48–72 hr in culture) preparations are associated with significantly lower levels of release (<4,000 ELVs/parasite/min) and an even wider multimodal size distribution. These data suggest an overall time-dependent decay in vesicle rate of release and size specificity, which correlates to decreased L3 viability in vitro. The release of considerable quantities of precisely-sized ELVs in viable worms (Days 1–2) is followed by the release of smaller quantities of a broader size range of particles that potentially include larger membrane vesicles and apoptotic blebs (Days 2–3). This suggests an active and regulated mechanism of ELV release in healthy and viable L3 stage parasites, as opposed to a passive mode of noisy cellular deterioration.
Profile of ELVs isolated from culture media incubated with 300 L3 parasites for successive 24 hr incubations. The size distribution of L3-derived ELVs from Day 1 (left), Day 2 (center) and Day 3 (right) incubations are shown (mean ± SD). Calculated vesicle release rates are provided in tabular format. ELV rate of release and size specificity decay in a time-dependent manner in vitro. * re-scaled based on dilution for comparison to 0–24 hour (1:20) dilution.
The protein cargo of Brugia exosome-like vesicles
The protein content of B. malayi ELVs was determined using nanoscale liquid chromatography coupled to tandem mass spectrometry (nano LC/MS/MS). A total of 32 proteins each containing at least two unique peptides were identified using MASCOT (Table 1). Specific proteins identified within the pellet included characteristic markers of exosomes including Hsp70, elongation factor-1α, elongation factor-2, actin, and Rab-1. In addition, over 80% of the proteins identified are orthologous to proteins identified in mammalian exosome proteomes, strongly suggesting that these vesicles are exosome-like in nature and supporting our ELV designation here. Interestingly, this set of vesicle-specific proteins is entirely distinct from the proteins previously identified in pre- and post-molt L3 secretions .
UniProt-GOA and quickGO were used to sort proteins into functional groups based on assigned gene ontology (GO) terms [38, 39], as shown in Fig 3. Based on GO annotations, 20% of the proteins identified are involved in binding of bioactive molecules including nucleic acids and other proteins, 16% function in the transport of various ions and proteins and 14% are ribosomal proteins. In addition, a large fraction of proteins identified (21%) appear to be involved in various metabolic processes including hydrolase and transferase activities while the remaining 29% comprises proteins with translational, cytoskeletal and other functions.
GO functional annotation of 32 proteins identified in ELVs isolated from B. malayi L3 stage parasites.
Included in the list of Brugia ELV proteins are potential effector molecules. Bm-CPL-1 is a cathepsin L-like cysteine protease robustly expressed across the B. malayi life cycle . Upregulation of Bm-cpl-1 expression coincides with transition between life cycle stages and an important role in the modulation of parasite molting has been confirmed [41–43]. This is the first demonstration that B. malayi secretes CPL-1 although other cathepsin-like cysteine proteases have been identified in the B. malayi secretome [14, 37] and a cathepsin L-like molecule is secreted by intra-mammalian stage Haemonchus contortus . The exogenous function of exosomal Bm-CPL-1 is not clear but evidence points to some manipulation of the host-parasite interface. In a previous study, we suppressed Bm-cpl-1 expression using in vivo RNAi during the mosquito life stages . Loss-of-function reduced prevalence of infection in mosquitoes by nearly 40%, suggesting Bm-CPL-1 is important for establishing or maintaining parasitemia. In flatworms, an immunomodulatory role for secreted cathepsin L-like proteases is better established ; in Fasciola infection cathepsin L contributes to the permissive polarized Th2 > Th1 host response.
The proteomic profiles of parasitic helminth exosomes are broad in range; for example, over 350 proteins were identified in the putative exosomes secreted by Heligmosomoides polygyrus  whilst 45 and 79 proteins were identified in exosome-like vesicles from Echinostoma caproni and Fasciola hepatica, respectively . The B. malayi L3 stage profile identified here is relatively scant but consistent with this broad distribution. It may be that this is a stage-specific observation and ELV secreted by other B. malayi life stages display a more complex and abundant protein cargo tailored to distinct functional demands. Reflecting the small RNA component of these ELVs (see later sections), it may also be that larval stage Brugia ELVs are primarily vehicles for protected RNA secretion. Replication of the experiments conducted here might add depth to the MS data set and identify further ELV-associated proteins.
B. malayi ELVs contain small RNA including miRNAs with potential host targets
We probed larval and adult microvesicle preparations for the presence of small RNA species. Exosomes have been found to contain both non-coding RNAs (ncRNAs) and messenger RNAs (mRNAs) in a diverse range of species and cell types. Of particular interest to us was the potential presence of small non-coding RNAs, including microRNAs (miRNAs), that could potentially mediate parasite-parasite communication or modulate host gene expression. Small RNA species were preferentially isolated from putative ELV-containing pellets and examined with an Agilent Bioanalyzer. The microvesicle fractions of L3 B. malayi (24 hr incubations of 300 worms) revealed an abundance of small RNA species in the 25–200 nt range (Fig 4). Much less RNA was detected from incubations of adult male and female B. malayi (24 hr incubations of 30 adult worms), despite the much higher mass of tissue in adult stage culture media. This lack of correlation between total parasite tissue material and RNA yield, coupled to the differential quality of larval and adult microvesicle preparations as evaluated by EM, further indicates that ELV release is primarily a characteristic of larval-stage parasites and perhaps more biologically relevant to early parasite infection.
Bioanalyzer data are shown for RNAs isolated from L3, adult male, and adult female Brugia preparations. L3 ELVs contain significant amounts of small RNAs in the 25–200 nt range (25 and 200 nt reference peaks labeled), while adult male and female vesicle preparations yield fewer RNAs. Vesicle fractions were prepared from 300 L3 and 30 adults in 24 hr culture incubations. Despite the much higher total tissue amounts used in adult culture, we detect much higher levels of small RNAs in L3-derived ELVs.
To more fully investigate the nucleic acid contents of these newly discovered vesicles, we carried out RNA-Seq with both L3 ELV and tissue-derived small RNAs. Reads generated by Illumina sequencing were processed and used to seed an miRNA discovery and abundance estimation pipeline using miRDeep2  (read statistics and raw miRNA abundances can be found in S1 Table). To compare ELV and cellular RNA abundance, miRNA expression was normalized to the total miRNA read count within each sample. miRNA discovery and profiling was augmented with data from previously discovered miRNAs in closely related nematode species to help overcome gaps in the B. malayi draft genome assembly (see Methods). Fig 5A compares normalized miRNA expression between ELV and tissue for the 20 most abundant miRNAs in each sample. Although there is considerable conservation in relative miRNAs abundances, there are some notable observations and exceptions.
(A) Comparative abundance of miRNAs in L3 ELV and tissue-derived samples. miRNA discovery and abundance estimation was carried out using the mirDeep2 pipeline. The 20 miRNAs with highest expression in each sample were retained for comparison and abundance was normalized with respect to total miRNA-mapping reads within each sample. Normalized read count is plotted on a log scale for ELV and tissue miRNAs to provide a relative ordering of fractional abundance. Bma-let-7 only appears in the highly expressed subset, and a number of miRNAs with perfect mature sequence identity to host homologs are highlighted (outer blue circle). (B) Sequence conservation between B. malayi ELV-origin miRNAs and the host ( H. sapiens ) miRNA complement. Reduced heat map showing one-to-one homology between a given B. malayi miRNA and its nearest matching human counterpart in terms of percent identity. Bma-let-7, bma-miR-1, bma-miR-9, bma-miR-92, and bma-miR-100b (white asterisks) share 100% identity with a host miRNA, while bma-miR-34 shows high identity with a host miRNA (21/23 nucleotides). This B. malayi miRNA subset (shown in blue) contains potential modulators of host gene expression. (C) Sequence conservation between B. malayi ELV-origin miRNA seed sites and host ( H. sapiens ) miRNA seed sites. miRNAs sharing perfectly conserved seed sites, defined here as nucleotides 2–8 of the mature miRNA, are marked (blue circles).
Bma-let-7 is significantly enriched in L3 ELVs as compared to L3 tissue, where it does not appear among the 20 most abundant miRNAs. Bma-let-7, along with four other B. malayi mature miRNAs found in ELVs (bma-miR-1, bma-miR-9, bma-miR-92, and bma-miR-100b), share perfect sequence identity with host (Homo sapiens) mature miRNAs, as shown in Fig 5B. Additionally, bma-miR-34 shares near perfect sequence identity with its H. sapiens homolog. 11 B. malayi miRNAs also share common seed sites with H. sapiens miRNAs (Fig 5C). Brugia ELV miRNA sequences were more broadly clustered by putative seed site and aligned to miRNAs from the soil-transmitted parasitic nematode Ascaris suum, the free living model nematode Caenorhabditis elegans, and mammalian host species H. sapiens and Mus musculus (Fig 6 and S1 Fig). In all cases, Brugia ELV miRNAs that share common seed sites with host miRNAs have one-to-one A. suum orthologs. In some cases, parasite miRNAs are better conserved in mammalian hosts than in C. elegans (e.g., bma-miR-9, bma-miR-993, and bma-miR-100b/c).
miRNAs from B. malayi, A. suum, C. elegans, H. sapiens, and M. musculus were grouped by seed site sequence identity (nucleotides 2–8) for multiple sequence alignments. Alignments are shown for bma-let-7, bma-miR-9 and bma-miR-993. bma-let-7 is shown as an example of a Brugia ELV miRNA that exhibits both seed site and full length sequence conservation extending to other parasitic and free-living nematodes, as well as to mammalian host species. bma-miR-9 and bma-miR-993 are presented as examples where conserved parasite miRNAs have clear host homologs, yet lack one-to-one C. elegans orthologs. The complete set of alignments can be found in S1 Fig.
We examined the complement of the most abundant Brugia ELV-associated miRNAs with respect to very recent investigations of miRNAs released by other parasitic nematode species and found circulating in host biofluids [26, 48–50]. Common markers include let-7, lin-4, miR-34, miR-71, miR-92, and miR-100c (Fig 7A and 7B). While all members of this subset share seed site sequence identity with mammalian host miRNAs, lin-4, miR-34, miR-71, and miR-100c are sufficiently diverged from host miRNAs over their full length mature miRNA sequence and can potentially serve as biomarkers of filarial infection. Additionally, we compared the complements of the 20 most abundant Brugia ELV and H. polygyrus exosomal  miRNAs, identifying six miRNAs shared between these vesicles and a large number of miRNAs unique to each species (Fig 7C).
(A & B) Comparison of the 20 most abundant B. malayi ELV miRNAs with the complements of miRNAs found circulating in the serum and plasma of definitive and model mammal hosts burdened with filarial infection (Litomosoides sigmodontis , Dirofilaria immitis , Loa loa , Onchocerca volvulus [48, 50], and Onchocerca ochengi ). The D. immitis miRNAs in (A) are restricted to the 20 most abundant miRNAs, and the O. volvulus miRNAs in (B) represent the combination of two non-overlapping sets arising from separate reports. (C) Comparison of the 20 most abundant miRNAs identified in B. malayi ELVs and H. polygyrus exosomes. These analyses reveal sets of common markers and a number of miRNAs unique to each species.
Enrichment of bma-let-7 and the high fractional presence of other parasite miRNAs sharing perfect or high homology to host miRNAs, leads us to speculate about a potential ELV-mediated mechanism by which parasite RNAs can be used to efficiently direct aspects of gene expression in host cells. Targets of endogenous let-7 family miRNAs in vertebrates include oncogenes, as well as genes involved in proliferation, apoptosis, and innate immunity [51–53]. Let-7 is intricately involved in macrophage polarization and responses to pathogen challenge [31, 33, 54], and the altering of host let-7 expression therefore represents a potentially advantageous point of intervention for an invading parasite. Live pathogens down-regulate the expression of let-7 family miRNAs, and let-7 miRNAs act on toll-like receptors (e.g. TLR4) that directly mediate macrophage responses [54–56]. Clearly, there is an important association between macrophage response to pathogens and let-7 expression. Our observation that B. malayi secrete let-7 and other potential modulators of host gene expression identifies a mechanism by which this host immune response might be manipulated. Supporting this hypothesis, let-7 and other miRNAs with host conservation have been identified in immunomodulatory H. polygyrus adult stage exosomes . To fully dissect this hypothesis, a broad investigation of the interaction of ELV miRNAs and host immune cells in vivo is needed.
Brugia ELVs are internalized by host macrophages
Macrophages are critical mediators of the early immune response to invasive Brugia parasites . To test the hypothesis that secreted Brugia ELVs interact with host macrophages, we used fluorescent lipophilic dyes to visualize the interaction between J774A.1 murine macrophages and ELVs. This cell line was chosen because it is commercially available, can be cultured readily and because it recapitulates the biology of primary macrophages and dendritic cells . ELVs were labeled with PKH67, a green fluorescent dye, and incubated with J774A.1 labeled with PKH26, a red fluorescent dye. Confocal microscopy revealed efficient internalization of the ELVs by this macrophage cell line (Fig 8). Internalization was observed diffusely throughout the cell cytoplasm with focus around membrane-rich puncta associated with the surface of the macrophages (Fig 8B). This pattern of internalization is consistent with other studies describing a phagocytic route of vesicle internalization [58, 59]. Macrophages were counterstained with DAPI to determine the efficiency of cell labeling and ELV uptake. PKH26-labeling of J774A.1 was very efficient and all cells were visualized although intensity of labeling was variable (Fig 8D). Approximately 40–50% of macrophages internalized labeled ELVs to some degree (Fig 8E) with approximately 10% of macrophages internalizing ELVs at markedly higher levels (Fig 8E). There was no correlation between strong PKH 26-labelling of macrophages and vesicle uptake indicating internalization is not a factor of receptiveness to labeling.
(A and D) J774A.1 macrophages were labeled with PKH26 (red) and counterstained with DAPI (blue) to visualize nuclei. (B and E) B. malayi L3 stage ELVs were purified from a 24 hr parasite culture and labeled with PKH67 (green). 3 × 105 J774A.1 were co-incubated with approximately 3 × 107 labeled ELVs for 6 hrs at 37°C and washed repeatedly to remove unbound ELVs. Vesicles internalized by macrophages appear diffusely throughout cytoplasm and focused in discrete puncta associated with the cell membrane. (C and F) Merged images showing internalization of parasite ELVs. All images were acquired using a using a Leica TCS SP5 X Confocal/multiphoton microscope system with 20X (A-C) or 60X (D-F) objectives. Scale bars: 10 μm (A-C) and 25 μm (D-F).
Brugia ELVs elicit a classically activated phenotype in host macrophages
Macrophage activation is dichotomous; classically activated macrophages (CAMΦ) are elicited by LPS or IFN-γ and have a generally pro-inflammatory phenotype whereas alternatively activated macrophages (AAMΦ), driven by IL-4 and IL-13, appear immunosuppressive or anti-inflammatory. Helminth infection is typically associated with the AAMΦ pathway although both CAMΦ and AAMΦ are involved in the immune response to, and immunopathology caused by, Brugia infection. Experiments demonstrate different Brugia preparations can generate both CAMΦ and AAMΦ activation phenotypes; dead and moribund worms and worm lysates produce CAMΦ  but live worms and complete excretory/secretory (ES) preparations drive AAMΦ [61–63]. To test the hypothesis that ELVs activate host macrophages, J774A.1 were treated with purified ELV preparations and their cytokine/chemokine responses monitored. J774A.1 were treated for 48 hrs with approximately 4 × 108 L3 stage vesicles, purified from in vitro culture medium by ultracentrifugation. The macrophage response was assayed using the Milliplex MAP Mouse Cytokine/Chemokine kit (EDM Millipore) interfaced with a Bio-Plex System (Bio-Rad) utilizing Luminex xMAP technology, a platform capable of simultaneously identifying and quantifying 32 cytokines/chemokines. Vesicle treatment effectively activated J774A.1 macrophages with significant increases in G-CSF, MCP-1, IL-6 and MIP-2 levels compared to control macrophages treated with naïve RPMI 1640 culture media, (p ≤ 0.001)(Fig 9A). Smaller increases in LIX, RANTES and TNF-α were also noted. Healthy, viable L3 stage parasites produced an almost identical response (Fig 9A), the only difference being a modest but significant enhancement of G-CSF stimulation by the viable parasites (p < 0.001), suggesting that the dominant parasite immunogen(s) are found in the vesicle pellet. Finally, parasite culture media from which the ELVs had been removed by centrifugation did not produce this response, nor did live schistosomes (S. mansoni cercaria) or their secreted vesicles (S2 Fig) suggesting the Brugia-associated activation is specific to this parasite and not a general response to helminths or their secreted vesicles.
(A) J774A.1 (5 × 105) were treated with approximately 4 × 108 purified L3 stage ELVs, live L3 stage parasites (10 worms) or naïve culture media (control) and supernatents collected after 48 hr. The presence of 32 cytokines/chemokines was simultaneously assayed using the Milliplex MAP Mouse Cytokine/Chemokine kit (EDM Millipore) interfaced with a Bio-Plex System (Bio-Rad) utilizing Luminex xMAP technology (Luminex). The quantification of identified cytokines is presented. The cytokine profile generated by ELV treatment is consistent with a classically activated phenotype. (B) Cytokine response to ELV treatment is compared to LPS (200 ng/mL). The close correlation of responses indicates ELV treatment generates a classically activated phenotype. (C) J774A.1 (5 × 105) were treated with high dose LPS (200 ng/mL), low dose LPS (0.003 ng/mL), ELV or naïve culture media (control) for 24 hr, supernatant collected and assayed for G-CSF using a Mouse G-CSF Quantikine ELISA kit (R&D Systems). The absence of response to low dose LPS suggests the classically activated response is not due to LPS-like contamination.
The activation profile observed would be considered more indicative of a CAMΦ response than AAMΦ; to confirm the response was CAMΦ-like, we compared it to the response elicited by LPS (200 ng/mL). The only significant differences were that ELV treatment stimulated G-CSF and IL-6 less effectively (p < 0.001) and stimulated MCP-1 more effectively (p < 0.001) than LPS (Fig 9B). The overall conservation of response, however, indicates these ELVs generate a CAMΦ phenotype. Since Wolbachia, the endosymbiont present in filarial nematodes, lack LPS biosynthetic capacity it seemed unlikely our CAMΦ-like response was driven by LPS-like contamination but to rule this out, endotoxin levels in our vesicle preparation were determined commercially (Lonza, Walkersville, MD). LPS-like activity was present (0.003 ng/mL) but at a concentration several orders of magnitude lower than the minimum dose required to stimulate J774A.1 macrophages . As expected, treatment of macrophages with this low LPS dose was insufficient for activation (Fig 9C) indicating that the CAMΦ response we observe is not due to an LPS-like component in our preparation.
Since the stimulation of an AAMΦ phenotype by live Brugia and ES preparations thereof in vivo and in vitro has been well established [61–63] it might be expected that Brugia ELV preparations also stimulate a AAMΦ phenotype, especially since complete Brugia ES preparations are likely to include ELVs similar to those examined here, albeit at reduced concentrations. We observed a response consistent with a CAMΦ phenotype, however, although without the acute elevation in IL-β and TNF-α production others have seen in response to LPS . One interpretation is that the CAMΦ > AAMΦ phenotype may be a somewhat artificial function of the homogenous J774A.1 monoculture used here as other studies describing a AAMΦ phenotype often use PBMC or other heterogeneous primary cell types. It would be instructive to monitor the responses of such mixed cell populations to the ELV preparation. Additionally, although the murine model is regarded as valuable for illuminating both how parasites establish themselves and the early host immune response, J774A.1 may not be optimal for studying this particular Brugia-host interaction and optimization with other murine or human cells may be required. Another interpretation, however, is that the purified ELVs examined here should be considered a distinct and specific fraction of the highly complex immunogenic facade presented by filarial parasites and may elicit a genuine CAMΦ phenotype when examined in isolation. Supporting this interpretation, exosomes isolated from other biological systems effectively generate a CAMΦ phenotype [59, 65, 66]. A key mediator of this pro-inflammatory response is Hsp70 , which was identified in our ELV proteomic profile. In summary, irrespective of the polarity of macrophage activation phenotype, our results unequivocally identify secreted ELVs as distinct parasite-derived structures capable of activating the host immune system.
A picture is emerging that parasitic helminths secrete functional exosome-like vesicles. The protein and small RNA cargo of these vesicles have putative effector functions at the host-parasite interface and potentially serve to create conditions favorable to the establishment or maintenance of infection. The identification of these cell-to-cell effector structures is exciting and prompts further investigation of their functional relevance. In particular, it will be important to describe the roles of individual miRNAs and proteins contained within the ELVs, to identify the host molecular targets being manipulated in vivo, and reveal any conserved or stage-specific effectors secreted across the parasite life cycle. Another intriguing question is whether or not there is any specificity or selectivity in host cells or tissues targeted and if so, what molecular mechanisms underscore this specificity. Addressing such questions will illuminate the fundamental interactions that occur between parasite and host, and may open previously unexploited opportunities for parasite control and diagnostics.
Materials and Methods
Aedes aegypti (Black eyed Liverpool strain, LVP), previously selected for susceptibility to infection with Brugia malayi , were maintained in controlled conditions (27°C ± 1°C and 75% ± 5% relative humidity) with a 16:8 photoperiod. Adult mosquitoes were fed a diet of 10% sucrose. Approximately 4,000 and 2,600 mosquitos were used for proteomics and RNA sequencing, respectively.
Establishing Brugia malayi infection
For proteomics and transcriptomics, B. malayi microfilaria (mf) infected cat blood was obtained from the University of Georgia NIH/NIAID Filariasis Research Reagent Resource Center (FR3). Blood containing the parasites was diluted with defibrinated sheep’s blood (Hemostat Laboratories, CA, USA) to achieve a concentration of 80–100 mf per 20μL. To establish infection, 3- to 5-day-old Ae. Aegypti (LVP) were allowed to feed for one hour on a glass membrane feeder. Mosquitoes were sucrose-starved for 24 hrs prior to blood feeding and those that did not take a blood meal were removed. Infected mosquitoes were maintained in the above described conditions for 13–15 days post infection (dpi) to allow development of parasites.
Brugia malayi maintenance and collection of vesicle-containing media
In exploratory studies, larval (300 L3) and adult (30 male or 30 female) B. malayi were procured from the FR3. On arrival, parasites were cultured in 50 mL RPMI 1640 (Sigma-Aldrich, St. Louis, MO) at 37°C (5% CO2). Cell culture media was collected and replaced at 24 hr intervals for up to 72 hrs to collect secreted ELVs. For downstream sequencing and proteomics, B. malayi (13–15 dpi) were locally collected using methods described by FR3. Briefly, infected mosquitoes were immobilized by cooling to 4°C for 15 minutes. Immobilized mosquitoes were crushed in a mortar containing 5 ml of chilled Hanks’ balanced salt solution (HBSS, pH 7.0) containing pen-strep (0.4 units penicillin/ml, 0.4 mcg streptomycin/ml). Mosquitoes were then rinsed onto a 150 mesh sieve contained in a deep well plastic petri dish and washed 3–4 times using fresh chilled HBSS + pen-strep. Sieves were then placed into petri dishes containing warm (40°C) HBSS + pen-strep to allow infective larvae to migrate out. Sieves were transferred to new deep well petri dishes containing fresh warm HBSS every 30 minutes. Collected parasites were washed twice with warm HBSS + pen-strep, placed into 25 mL RPMI 1640 containing pen-strep (0.4 units penicillin/ml, 0.4 mcg streptomycin/ml) and held at 37°C, 5% CO2 for 24 hrs to collect secreted ELVs.
Exosome-like vesicle purification
Differential centrifugation was used to isolate ELVs from 25 or 50 mL aliquots of Brugia culture media. Aliquots were collected from 24 hr incubations of larval or adult worms in culture media. Lower speed centrifugation and filtration steps were used to remove contaminating cells (300 × g, 10 mins) and cellular debris (10,000 × g, 15 mins). The resulting supernatants underwent filtration through 0.22 μm filters and ultracentrifugation at 105,000 × g for 90 mins to pellet ELVs. Pellets were then washed with cold phosphate-buffered saline (PBS) and a final spin was carried out at 105,000 × g for 90 mins. Supernatants were discarded and pellets were resuspended in small volumes (30–250 uL) of PBS for imaging, sequencing, and proteomics, and RPMI for immunological assays. Samples were kept on ice and centrifugation steps were carried out at 4°C. Resuspended ELVs were stored at −80°C.
Electron microscopy and nanoparticle tracking analysis
Small aliquots of ELV suspension (3 μl) were applied to carbon coated 200 mesh copper grids and negatively stained with 2% uranyl acetate. Images were taken using a JEOL 2100 scanning and transmission electron microscope (Japan Electron Optics Laboratories, Akishima, Japan) at the Microscopy and NanoImaging Facility (Iowa State University). Nanoparticle tracking analysis was carried out with the NanoSight LM10 (NanoSight Ltd., Amesbury, UK) to ascertain the size and frequency distribution of individual vesicle preparations, assayed in triplicate. The Brownian motion of particles in solution is related back to particle sizes and numbers, allowing better statistical resolution of vesicle size and concentration .
LC-MS/MS and proteomic analysis
Protein was isolated from purified exosome-like vesicles for proteomic analysis (System Biosciences). Briefly, samples were modified with 10% SDS to a final concentration of 2% SDS, heated at 100°C for 15 minutes and clarified by centrifugation. Protein concentration was determined using a Qubit fluorometry assay (Invitrogen). 15 μg of material was processed by SDS-PAGE using a 10% Bis-Tris homogeneous gel and the MES buffer system. In-gel digestion with trypsin was done at 37°C for 4 hrs using a ProGest robot (DigiLab, Marlborough, MA). The digested sample was analyzed by nano LC-MS/MS analysis using a Waters NanoAcquity HPLC system interfaced to a ThermoFisher Q Exactive. Data were searched against a copy of the B. malayi UniProt database (taxon ID: 6278) using a locally running copy of MASCOT (Matrix Science Ltd., London, UK). The search was restricted using the following parameters; maximum missed cleavages = 2, fixed modifications = carbamidomethyl (C), variable modifications = Oxidation (M), Acetyl (N-term), Pyro-Glu (N-term Q) and Deamidation (N, Q), a peptide mass tolerance of 10 ppm, and a fragment mass tolerance of 0.02 Da. Mascot DAT files were parsed into the Scaffold software for validation, filtering and to create a nonredundant list per sample. Data were filtered using a minimum protein value of 90%, a minimum peptide value of 50% (Prophet scores) and requiring at least two unique peptides per protein.
RNA isolation and sequencing
For detection of RNA species in ELV preparations, small RNAs were preferentially isolated from vesicle-containing pellets using the miRCURY RNA Isolation Kit (Exiqon, Vedbaek, Denmark) and RNA samples were examined with an Agilent 2100 Bioanalyzer using the RNA 6000 Nano Kit. For small RNA sequencing (RNA-Seq), total RNA was isolated from ELVs released by ∼5,000 L3s over a 24 hr incubation period using the Total RNA and Protein Isolation Kit (Invitrogen, Carlsbad, CA). In parallel, total RNA was isolated from whole worm tissue using a TRIzol (Invitrogen) protocol, where a 6 hr precipitation step was carried out at -80°C to improve small RNA recovery. RNA NGS libraries were constructed using modified Illumina adapter methods using SBI’s XRNA Sample Preparation Kit (System Biosciences, Mountain View, CA) and indexed with separate bar codes for multiplex sequencing on an Illumina MiSeq v3 instrument using a 2 × 75 bp paired end run setting.
miRNA discovery and abundance estimation
Raw reads were trimmed to remove adapter sequences, filtered by quality score, and de-multiplexed using the FASTX-Toolkit  (sequencing data are deposited with the NCBI SRA under project number PRJNA285132). The miRDeep2 pipeline was used to map short RNA reads (>15 nt) to the B. malayi genome for miRNA discovery, and to estimate and normalize miRNA abundances with respect to total miRNA read count. Nematode precursor and mature miRNA sequences deposited into miRBase  were used in the pipeline, including known B. pahangi, Caenorhabditis elegans, Ascaris suum, Haemonchus contortus, and Strongyloides ratti miRNAs. Non-mapped reads were ranked by abundance, filtered for homology against known miRNAs in the phylum Nematoda using BLASTn , and incorporated for final quantification of abundance with the miRDeep quantifier script, allowing for capture of miRNAs that did not map to the B. malayi assembly due to sequencing gaps. The ggplot2 package  of the statistical programming language R was used to organize and visualize comparisons between vesicular and tissue RNA samples.
J774A.1 murine macrophages (ATCC, Manassas, VA) were maintained in complete tissue culture medium (Dulbecco’s modified Eagle’s medium, 25 mM HEPES, pH 7.4 supplemented with 2 mM L-glutamine, 100 U/mL penicillin, 100 μg/mL streptomycin, 0.05 μM 2-mercaptoethanol, and 10% heat-inactivated fetal bovine serum) at 37°C and 5% CO2. 24 hrs prior to assays, 400 μL cells were plated in standard 24-well plates at a density of 5 × 105 cells/well.
Vesicle labeling and uptake
Exosome-like vesicles were purified from a 24 hr culture of 300 Brugia malayi L3 parasites as described above and labeled with the green fluorescent dye, PKH67 (Sigma-Aldrich, St Louis, MO,USA), according to the manufacturer’s instructions. ELVs were incubated with PKH67 for 5 min at room temperature and the reaction terminated by addition of 1% BSA in PBS. RPMI 1640 media was added, mixed and centrifuged at 105,000 × g for 1 hr to separate ELV-bound PKH67 from excess PKH67. Labeled ELV were washed again then resuspended in an appropriate volume of complete tissue culture medium (Dulbecco’s modified Eagles medium, 25 mM HEPES, pH 7.4 supplemented with 2 mM L-glutamine, 100 U/mL penicillin, 100 μg/mL streptomycin, 0.05 μM 2-mercaptoethanol and 10% heat-inactivated fetal bovine serum).
J774A.1 were labeled with red fluorescent lipophilic dye, PKH26 (Sigma-Aldrich, St Louis, MO), according to the manufacturer’s instructions. Macrophages were incubated with PKH26 for 5 min at room temperature and the reaction terminated by addition of 1% BSA. To remove excess unbound dye, samples were centrifuged at 400 × g for 10 minutes at room temperature and the supernatant discarded. Centrifugation was repeated three more times using 10 ml of complete media to ensure full removal of unbound dye and the cells were re-suspended in 1 mL of complete medium. Approximately 3 × 105 labeled cells were plated onto sterile coverslips and incubated overnight at 37°C/5% CO2. Labeled ELV suspension (approximately 3 × 107 per coverslip) was added to labeled J774A.1 and incubated for 6 hrs. Cells were washed 5 times with ice-cold PBS to remove excess labeled ELVs, the cells fixed in 4% paraformaldehyde (Sigma-Aldrich), washed and counterstained with DAPI before mounting and storage at 4°C. Preparations were visualized using a Leica TCS SP5 X Confocal/multiphoton microscope system (Leica Microsystems Inc., Buffalo Grove, IL).
Detection of macrophage modulation by Luminex assay
Triplicate wells of adhered J774A.1 were treated with approximately 4 × 108 purified L3 stage ELVs. The ELVs were purified by ultracentrifugation as previously described, resuspended in RPMI 1640 medium (Gibco/Life Technologies, Carlsbad, CA) and quantified by nanoparticle tracking analysis. Other treatments were similar volumes of vesicle depleted L3 culture medium (supernatant created following pelleting of ELV fraction from spent parasite culture medium), live B. malayi L3 parasites (10 worms/well), lipopolysaccharide (LPS; final concentration 200 ng/mL)(Sigma-Aldrich, St. Louis, MO), naïve RPMI 1640 culture medium and various combinations of these conditions. Supernatants from these cell cultures (400 μL/well) were collected 24 or 48 hrs post-treatment and centrifuged briefly (2,000 × g for 10 min) to remove non-adhered cells and cell debris before being analyzed for the presence of cytokines/chemokines. The Milliplex MAP Mouse Cytokine/Chemokine kit (EDM Millipore, Billerica, MA) interfaced with a Bio-Plex System (Bio-Rad, Hercules, CA) utilizing Luminex xMAP technology (Luminex, Austin, TX) allowed the simultaneous identification and quantification of the following analytes in the cell culture supernatant: Eotaxin, G-CSF, GM-CSF, IFNγ, IL-1α, M-CSF, IL-1β, IL-2, IL-3, IL-4, IL-5, IL-6, IL-7, IL-10, IL-12(p40), IL-13, IL-15, IL-17, IP-10, MIP-2, KC, LIF, LIX, MCP-1, MIP-1α, MIP-1β, MIG, RANTES, TNFα, IL-12(p70), VEGF, IL-9. Briefly, experimental samples, background, standards and controls were added to a 96-well plate and combined with equal volumes of pre-mixed, antibody coated magnetic beads; the plate was sealed and incubated overnight at 4°C. Following washing, 25 μL of detection antibody was added and the plate incubated for one hour at room temperature with shaking. Streptavidin-Phycoerythrin (25 μL) was added to each well and the plate incubated for a further hour at room temperature before washing. Finally, 150 μL assay buffer was added to all wells and fluorescence immediately recorded. Median fluorescent intensity data were analyzed as recommended using a five-parameter logistic curve-fitting method for calculating cytokine/chemokine concentration.
Triplicate wells of adhered J774A.1 cells, prepared as described above, were treated with LPS (final concentration 200 ng/mL or 0.003 ng/mL), approximately 4 × 108 purified L3 stage ELVs as described above, or RPMI 1640 as negative control. Cell culture supernatants were collected 24 hrs after treatment, cleared via centrifugation as described previously and assayed for G-CSF using a Mouse G-CSF Quantikine ELISA kit (R&D Systems, Minneapolis, MN). Standard curves were generated using Prism 6 software (GraphPad Software, San Diego, CA) and sample G-CSF concentrations determined by regression analysis.
For analysis of Luminex data, Tukey’s test was used to compare overall treatments while multiple t-tests, incorporating the Holm-Sidak method to correct for multiple comparisons, were used to compare individual chemokines/cytokines following treatments. t-tests were used to compare treatment groups following ELISA analysis. All statistical analyses were performed using Prism 6 for Mac (Graphpad).
S1 Video. Brugia malayi L3 ELVs recorded via NanoSight.
S1 Table. Small RNA-Seq miRNA abundances and read statistics.
S1 Fig. Brugia malayi ELV miRNA sequence homology to nematode and mammalian host miRNAs.
miRNAs are grouped by putative seed site and aligned.
S2 Fig. Macrophage activation is a specific function of Brugia ELVs.
(A) J774A.1 macrophages (5 × 105) were treated with approximately 4 × 108 purified L3 stage ELVs, an equivalent volume of culture media supernatant from which ELVs had been depleted by centrifugation (SN Treated) or naïve culture media (control). The presence of 32 cytokines/chemokines was simultaneously assayed using the Milliplex MAP Mouse Cytokine/Chemokine kit (EDM Millipore) interfaced with a Bio-Plex System (Bio-Rad) utilizing Luminex xMAP technology (Luminex). The quantification of identified cytokines is presented. ELV treatment, but not the ELV depleted culture media, generates a classically activated phenotype. (B) J774A.1 macrophages were treated with approximately 4 × 108 ELVs collected from a culture of Schistosoma mansoni invasive stage schistosomules as described for Brugia (Sm ELV), live S. mansoni schistosomules (300 per well; Sm) and naïve RPMI 1640 culture media (control). Macrophages were not activated by either schistosome preparation.
The authors would like to thank Marie Bockenstedt, Mary J. Long, and Dr. Douglas E. Jones for helpful discussions and technical guidance relating to the luminex experiments. The authors would also like to acknowledge parasite materials provided by Erica Burkman and the NIH-NIAID Filariasis Research Reagent Resource Center (FR3). The authors thank Michael Nazarchyk and Brendan Dunphy for technical assistance with mosquito infections and mosquito maintenance, and Morgan Pearson for assistance with vesicle isolation.
Conceived and designed the experiments: MZ LMF LCB MJK ARM. Performed the experiments: MZ LMF HH PNA. Analyzed the data: MZ LMF TAD LCB MJK. Contributed reagents/materials/analysis tools: ARM. Wrote the paper: MZ LMF LCB MJK.
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