Skip to main content

Thank you for visiting You are using a browser version with limited support for CSS. To obtain the best experience, we recommend you use a more up to date browser (or turn off compatibility mode in Internet Explorer). In the meantime, to ensure continued support, we are displaying the site without styles and JavaScript.

Targeted delivery of lysosomal enzymes to the endocytic compartment in human cells using engineered extracellular vesicles


Targeted delivery of lysosomal enzymes to the endocytic compartment of human cells represents a transformative technology for treating a large family of lysosomal storage diseases (LSDs). Gaucher disease is one of the most common types of LSDs caused by mutations to the lysosomal β-glucocerebrosidase (GBA). Here, we describe a genetic strategy to produce engineered exosomes loaded with GBA in two different spatial configurations for targeted delivery to the endocytic compartment of recipient cells. By fusing human GBA to an exosome-anchoring protein: vesicular stomatitis virus glycoprotein (VSVG), we demonstrate that the chimeric proteins were successfully integrated into exosomes which were secreted as extracellular vesicles (EVs) by producer cells. Isolation and molecular characterization of EVs confirmed that the fusion proteins were loaded onto exosomes without altering their surface markers, particle size or distribution. Further, enzyme-loaded exosomes/EVs added to cultured medium were taken up by recipient cells. Further, the endocytosed exosomes/EVs targeted to endocytic compartments exhibited a significant increase in GBA activity. Together, we have developed a novel method for targeting and delivery of lysosomal enzymes to their natural location: the endocytic compartment of recipient cells. Since exosomes/EVs have an intrinsic ability to cross the blood-brain-barrier, our technology may provide a new approach to treat severe types of LSDs, including Gaucher disease with neurological complications.


Lysosomal storage diseases (LSDs) are a group of over 50 inherited metabolic disorders that have a devastating effect and impose a heavy burden on both the patient and the health care system1,2,3. Although many of these disorders are rare, the combined incidence is high with an estimation of 1 in 7,000~8,000 live births4. LSDs are heterogeneous; each one is caused by a defect to a different lysosomal enzyme. The loss of these enzymatic activities leads to accumulation of undegraded substrates, which can be toxic to cells and result in multiple organ damage5. The clinical signs and symptoms include facial dimorphism, hepatosplenomegaly, ocular impairment, skeletal and cardiovascular involvement, as well as hematological abnormalities. Moreover, two-thirds of patients with LSDs manifest distinct neurological symptoms, ranging from progressive neurodegeneration to severe cognitive impairment as well as epilepsies, behavioral abnormalities and/or psychiatric disorders6.

Current options for treating hereditary LSDs are limited. They include specific enzyme replacement therapy (ERT) with recombinant human enzymes or a handful of supportive measures7,8,9. ERT was first used to replace defective enzymes for Gaucher’s patients in the 1990s10,11. Subsequently, this approach became the standard of care and has extended to other LSDs including Fabry disease, Pompe disease, mucopolysaccharidosis, metachromatic leukodystrophy, and acid lipase deficiency12,13,14,15,16. Although ERT is effective in reversing the visceral and hematologic manifestations associated with the mild form of the disease, critical limitations have emerged, including insufficient reversal of the pathology in tissues such as muscle, bone, cartilage, heart and lung17. Importantly, ERT has little effect on cases with severe neurological complications, putatively due to difficulty crossing the blood-brain barrier8,18. Although there are some promising outcomes recently to increase enzyme delivery to the brain, these methods tend to be more invasive and require additional improvements19,20. One solution to the current drawbacks of protein therapy to Gaucher treatment is to develop delivery systems that can both reach and penetrate barriered tissues, such as the brain. Ideally, these systems would deliver functional enzymes to their native action sites, namely the endocytic compartments of diseased cells.

EVs are cell-derived nano-vesicles that play an important role in mediating cell-to-cell communication21,22,23. These vesicles have been shown to shuttle a large number of macromolecules, including proteins, enzymes, nucleic acid and lipids to various tissues and organs24,25. Due to their intrinsic tissue-penetrating ability, EVs represent a more desirable delivery tool over other existing technologies such as liposomes, synthetic polymers and gold nanoparticles26,27. In fact, engineered EVs, particularly exosomes (the subpopulation of EVs derived from multiple vesicular bodies), have been shown to deliver RNA therapeutics or other drugs to both brain tissues and deep-seated cancer cells28,29,30,31. Recently, we have developed a decoy exosome system that functions as a biological sponge to antagonize tumor-necrosis factor alpha32. In this previous study, we tested the hypothesis that engineered EVs or exosomes and related biologics can function as an effective extracellular sponge binding to inflammatory agents in the extracellular space. In exploiting EVs for targeted delivery of bioactive enzymes to an intracellular site for the treatment of human diseases33, one abstract reported the preliminary work on the potential use of opto-genetically engineered exosomes and β-glucocerebrosidase (GBA) for the treatment of Gaucher disease34

Human β-glucocerebrosidase (GBA) is an important well-characterized lysosomal enzyme that localizes within the endocytic compartment of human cells. Defective forms of GBA are responsible for Gaucher disease and previous studies have shown that the introduction of functional GBA can effectively reverse disease symptoms35,36.

Here, we describe a de novo method to load GBA onto exosomes by developing a genetic fusion protein using an exosome targeting transmembrane protein, VSVG. These GBA-loaded exosomes can be isolated in a pure form from conditioned medium. The isolated exosomes/EVs are added to the medium of targeted recipient cells, where they effectively deliver bioactive GBA to their endocytic compartments.



Reagents were obtained from the following commercial sources: recombinant human glucosylceramidase/GBA protein (R&D Systems/Bio-Techne; Minneapolis MN); 4-methylumbelliferyl-beta-D-glucopyranoside, sodium cholate, glycine, citric acid, DTT, and NaOH (Sigma Aldrich; St. Louis, MO); Human embryonic kidney cell line HEK293 (Alstem; Richmond, CA); Human glioblastoma cell line U87 (ATCC; Manassas, VA); Human hepatocellular carcinoma cells, HepG2 (ATCC; Manassas, VA); Lipofectamine2000 (Thermo Fisher Scientific; Waltham, MA); FuGENE6 (Promega; Madison, WI); Dulbecco’s Modified Eagle Medium (DMEM), fetal bovine serum (FBS), UltraCULTURE (Lonza; Allgendale, NJ); LysoTracker Red DND-99, CellLight Early Endosomes-RFP/Late Endosome-RFP BacMam 2.0, polyclonal TurboGFP primary antibody, goat anti-rabbit horseradish peroxidase conjugated secondary antibody (Invitrogen; Carlsbad, CA); Dot-blot antibody arrays, ExoQuick-TC exosome precipitation solution (SBI; Palo Alto, CA); Prestained protein markers and precast 4~12% SDS-PAGE (GenScript; Piscataway, NJ); Hoechst 33342 and Pierce ECL Western Blotting Substrate (ThermoFisher Scientific; Fremont, CA).

Vector design and construction

The mammalian vector expressing the VSVG-GFP fusion gene was constructed as previously described [28]. The full-length coding sequence of human GBA (XM_006711270) was purchased from Genscript (Piscataway, NJ). The partial GBA coding sequence was inserted into two locations of the VSVG-GFP vector, yielding two construct designs, GBA-VSVG-GFP and VSVG-GFP-GBA, depending on whether GBA were appended at the N- or C- terminus of the VSVG-GFP vector respectively. The final constructs were verified by double-stranded DNA sequencing (GenScript; Piscataway, NJ); their encoded chimeric proteins were annotated and provided (Supplementary Sequences).

Cell culture and transfection

Human cells (HEK293, U87 and HepG2) were cultured in high glucose Dulbecco’s Modified Eagle Medium (DMEM) supplemented with 10% FBS, 2 mM glutamine and 100 U/mL penicillin/streptomycin (Gibco; Manassas, VA). Cells were maintained at 37 °C and 5% CO2. Cells were transiently transfected using either Lipofectamine 2000 transfection reagents. Typically, 1.5~2 μg of plasmid DNA was used to transfect cells (40~60% confluency) in each well of a 6-well plate. After 24~48 hours, over 80% of cells were effectively transfected.

Nuclear and lysosomal staining

Cultured cells on glass bottom dishes were incubated with a PBS-diluted Hoechst 33352 stain (1:1000 dilution) for 10 minutes at 37 °C. The Hoechst solution was removed and cells were washed with PBS before imaging via confocal microscopy to show nuclear staining (blue). Similarly, cells were stained with a dilution of 75 nM LysoTracker Red DNA-99 in cultured medium and incubated at 37 °C for 30 minutes. The LysoTracker solution was then replaced with either fresh culture medium or PBS before imaging via confocal microscopy to show lysosomal staining (red).

Extracellular vesicle preparation

A combination of centrifugation, ultrafiltration and precipitation was used to prepare EVs/exosomes as described37. Briefly, HEK293 cells cultured in 10% FBS supplemented complete medium were switched to serum-free UltraCULTURE for 48 hours. The conditioned medium was then collected, centrifuged at 1500xg for 10 min and filtered through a 0.2 µm syringe filter to remove cell debris and large extracellular vesicles ( > 200 nm in diameter). Finally, EV-containing medium was mixed with the ExoQuick-TC solution (1:4 dilutions) and incubated overnight at 4 °C. The precipitate was then collected by centrifugation at 3,000xg for 90 min at 4 °C. The EV pellet was resuspended in PBS and stored at −20 °C.

Nanoparticle tracking analysis (NTA)

EVs isolated from modified producer cells were subjected to nanoparticle tracking analysis (NTA) using a NanoSight LM10 instrument (Malvern Instruments Ltd; Malven, UK) with a 405 nm and 60 mV laser source as previously described [31]. Typically, 1 ml of a diluted exosome preparation was used for the laser light scattering study. The instrument rendered 3 recordings per sample at 60 seconds each; NTA software was then used to determine the size distribution of exosomes.

Western blot and dot-blot analysis

Whole cell lysates (WCLs) were prepared from either control or transiently transfected HEK293 cells38. 30–150 μg of proteins from either exosome or WCLs were loaded on a precast gradient gel (4~12%) and blotted on a polyvinylidenedifluoride membrane. The membrane was blocked for 1 hour at room temperature before overnight incubation at 4 °C with anti-rabbit Turbo-GFP antibody (1:2000) and subsequently with horseradish peroxidase conjugated goat anti-rabbit secondary antibody (1:4000) for 1 hour at room temperature. The membrane was visualized with Pierce ECL Western Blotting Substrate on ImageQuant LAS 500 imager (GE Healthcare Life Sciences; Issaquah, WA).

A dot-blot kit from SBI (Palo Alto, CA) was used to identify target proteins as described39,40. Each blot contained 12 pre-printed spots and featured 8 antibodies against exosomal markers including CD63, CD81, ALIX, FLOT1, ICAM1, EpCam, ANXAS and TSG101, as well as a negative control, cytosolic GM130 to identify any cellular contamination. 100~200 μg of exosomal proteins were used in each assay according to the immuno-binding and detection protocol described in the user manual.

Enzyme assays

GBA activity was determined fluorometrically using 4-methy-lumbelliferyl-beta-D-glucopyranodide (NBD-Glu) as a substrate40,41. For each assay, the NBD-Glu solution was freshly prepared and positive controls (recombinant human GBA) was included. Typically, the enzymatic reaction was carried out in a volume of 50 µl, using either 150 µg (WCLs) or 50 µg (exosomes), in a pH 6 solution containing 50 mM sodium citrate, 25 mM sodium cholate and 5 mM DTT. The reaction was incubated for 30 min at 37 °C and stopped by adding 50 µl of stop solution (0.5 M glycine, 0.3 NaOH, pH 10). The fluorescent signal at a wavelength of 365 nm excitation and 445 nm emission was recorded using a TECAN infinite M200PRO plate reader.

Fluorescence-activated cell sorting (FACS) analysis

Equal amounts of exosomes were chemically stained using a green fluorescent dye, Exo-Glow (SBI, Palo Alto, CA) according to the manufacturer’s instructions. 0.3 µg/μl of stained exosomes were added into cultured media of HEK293 cells to allow for cellular uptake during 48 hour incubation periods. The cells were then washed, trypsinized and re-washed using PBS. The corresponding cells were then subjected to FACS analysis using channels to detect GFP fluorescence42.

Fluorescence and confocal microscopy

For live cell experiments, cultured cells were imaged using an Olympus fluorescence microscope (Waltham, MA), or a Leica TCS SP8 confocal microscope (Buffalo Grove, IL). Images were taken at indicated time-points using the same exposure conditions within the group for comparison. To show the intracellular localization of the fluorescent fusion proteins, both fluorescence and phase/TLD images were overlaid using the Leica Las X imaging software.

Data collection, analysis and statistics

The student’s t-test was used to determine statistical significance of our studies, with P values < 0.05 being considered significant. All values were expressed as mean ± standard deviation.


System design and exosome loading strategy of lysosomal enzyme GBA

We have previously developed a method that enables protein loading onto exosomal targeting and anchoring protein, VSVG42. Using a genetic fusion approach, it is possible to utilize intracellular targeting and anchoring of a protein payload to the exosomal compartments of human cells. In this study, this approach was used to load the lysosomal enzyme GBA onto exosomes by fusing GBA with VSVG-GFP (Fig. 1a). The coding sequence of mature human GBA was inserted in one of two locations, creating two distinct fusion genes, whose expression was controlled by a CMV promoter (Fig. 1a). To ensure fusion proteins were anchored to the exosomal membrane with the correct spatial topography, we left the signal peptide (SP) sequence and the transmembrane helix of VSVG fully intact in all constructs. The first fusion gene (Upper, Fig. 1a) was expected to produce a protein chimera with GBA at the N-terminus of the VSVG-GFP, while the second (Lower, Fig. 1a) should create a chimera with GBA at the C-terminus after the GFP. When incorporated in exosomes, the first chimera should display the GBA enzyme on the outer surface of exosome, while in the second chimera, GBA would localize within the lumen of the exosomes (Fig. 1b). We fused a fluorescent GFP to all constructs, which allowed us to observe and quantify molecular trafficking of the gene product in human cell cultures. Compared to earlier studies on exosome-engineering, we can identify several innovations: the loading of functional GBA enzymes with defined geometry on the exosome surface and the integration of a sensitive probe for high-resolution imaging of distributions of the engineered exosomes in live cells28,42,43.

Figure 1

Design of GBA fusion proteins for exosome targeting and anchoring. (a) Schematic illustration of expression cassettes for two GBA fusion genes. CMV: cytomegalovirus promoter; SP: signal peptide coding sequences, where the red arrows indicate the cleavage site of the SP; PolyA: polyadenylation signaling. (b) GBA-loaded exosome illustration. The red arrow heads indicate different localization of GBA enzymes on exosomes according to the topology of VSVG on the lipid bilayer. The mature GBA is situated on the outer surface of exosome when GBA is fused at the N-terminus of VSVG, while GBA is situated within the lumen of the exosome when tagged at the C-terminus of VSVG.

Loading bioactive GBA onto exosomes in living human cells

First, we investigated the subcellular localization of GBA fused to the VSVG scaffold and imaged the GFP to visualize its intracellular trafficking to exosomes in live HEK293 cells. The cells were transfected with genetic constructs as detailed in the Methods section and imaged via confocal fluorescence microscopy for up to 3 days to assess GFP expression patterns and intracellular localization. Analysis of these images showed that within 24-hours of post-transfection with the GBA-VSVG-GFP construct, GFP fusion proteins (green, arrow) localized to puncta (Fig. 2,a1). The cytosolic localization of these intracellular fluorescent proteins was evident in an overlay of fluorescence and phase contrast images (Fig. 2,a4). This finding was consistent with the localization of the fusion protein to endocytic structures. Similar results were obtained when cells were transfected with VSVG-GFP-GBA (Fig. 2,a13–16). Together these data indicated that the protein chimeras including the GBA appendages were efficiently expressed and properly directed to exosomes in transfected cells.

Figure 2

Molecular trafficking of GBA-fusion proteins in genetically modified HEK293 cells. HEK293 cells were transfected with either GBA-VSVG-GFP alone (a) or co-transfected with either endosomal marker CD63-RFP (b) or XPACK-RFP (c) for 72 hours. Confocal images of live cells expressing GBA-VSVG-GFP (a1; green, arrow) and with Hoechst nuclear stain (a2, blue) and their overlay (a4) are shown. GBA-VSVG-GFP (green; b5, c9) is co-expressed with either CD63-RFP (b6) or XPACK-RFP (c10) as shown by their co-localization in overlay images (b8, c12). Parallel experiments were performed using VSVG-GFP-GBA, and similar results were obtained showing the expression of VSVG-GFP-GBA (d13–16) and co-expression with either CD63-RFP (e17–20) or XPACK-RFP (f21–24). Scale bar represents 10 µm. Arrows indicate subcellular locations of fusion protein. Nu: nucleus.

We next investigated whether these displayed fluorescent VSVG fusion proteins were correctly integrated into pre-exosomal compartments during biogenesis. For this purpose, HEK293 cells were co-transfected with one of the GBA-VSVG-GFP constructs and one of two validated exosomal markers, namely CD63-RFP or XPACK-RFP. Confocal images of transfected cells were recorded for 72 hours after co-transfection. The results revealed extensive overlap of green and red fluorescence signals of GBA-VSVG-GFP co-transfected with either CD63-RFP (Fig. 2b5–8) or XPACK-RFP (Fig. 2c9–12). We obtained similar results in cells expressing VSVG-GFP-GBA and either CD63-RFP (Fig. 2e17–20) or XPACK-RFP (Fig. 2f21–24). Together, our data strongly indicate that both GBA protein chimeras successfully targeted and incorporated themselves onto exosomes before their release to extracellular environments.

Post-translational modification of GBA such as glycosylation is an important step in the production of a functional enzyme44,45.To assess whether our expressed enzymes were active post-exosomal loading, transfected cells were cultured in serum free media and modified exosome were isolated as described. GBA activity was then measured from isolated exosomes. Whole cell lysates (WCL) were prepared from the transfected cells as detailed in the Methods section. As shown in Fig. 3b, the relative GBA activities in the WCL drastically increased by 7.1- and 8.4-fold for GBA-VSVG-GFP and VSVG-GFP-GBA respectively, compared to a mock control (P < 0.001). As expected, the GBA activities in isolated exosomes also increased by 4.0- and 4.2-fold compared to those mock controls for GBA-VSVG-GFP and VSVG-GFP-GBA respectively (Fig. 3c, P < 0.001).

Figure 3

Enzyme assay protocol and GBA activities in whole cell lysates and exosomes. (a)Workflow of preparation of whole cell extracts and exosomes for a GBA enzyme assay following transfection of HEK293 cells with either GBA-VSVG-GFP, VSVG-GFP-GBA, or control (unmodified plasmid) for 24 hours. At the end of transfection, cells were collected and both the whole cell lysates and exosomes were prepared for a GBA enzyme assay. The relative GBA activity in whole cell extracts (b) and in exosomes (c) is shown. All values are expressed as mean ± standard deviation (n = 3). ***p < 0.001 significant vs control, using a student-t test.

In summary, our data support that VSVG serves as a molecular scaffold that can both target and load their appended GBA and GFP components to exosomes in HEK293 cells. The readily detectable GFP signal in transfected cells suggests that the loading of both GBA and GFP is robust. Moreover, the drastically increased levels of GBA activity demonstrate that the enzyme payloads in both transfected producer cells and modified exosomes remain active.

Characterization of engineered EVs

We next characterized isolated EVs to assess whether the gene-product modifications affected their physical or biochemical properties. HEK293 cells were cultured and transfected with either construct for 72 hours, before WCL and EVs preparation as described earlier. First, we verified the size and particle distribution of the modified EVs were consistent with those of native (control) EVs, using a NanoSight NS80 system. As shown in Fig. 4, the peak size of 62–64 nm of exosomes modified by either GBA-VSVG-GFP (middle panel) or VSVG-GFP-GBA (right panel) did not differ from that measured in native (control) EVs (left panel).

Figure 4

Characterization of engineered exosomes. HEK293 cells were transfected with either GBA-VSVG-GFP, or VSVG-GFP-GBA, or mock control (control plasmid) for 72 hours, and exosomes were prepared and subjected to nanoparticle-tracking analysis (a), a dot-blot array analysis (b), confocal images (c) and Western blot analysis. (d) As shown in (a), there is no difference of particle size and distribution between these exosomes from control cells a GBA-VSVG-GFP or VSVG-GFP-GBA transfected cells. Dot-blot array analysis of 9 exosomal markers also showed similar expression pattern of engineered exosomes from cells transfected with GBA-VSVG-GFP (b; upper panel) vs. non-modified control (b; lower panel). (c) Confocal images of GBA-VSVG-GFP and VSVG-GFP-GBA modified exosomes. Western blot analysis showed the expression of GBA-VSVG-GFP and VSVG-GFP-GBA fusion proteins in transfected cell lysates or exosomes, compared with background levels of that in a mock control. (d) Arrows indicates the predicted size of the trimeric (GBA + VSVG + GFP) fusions (~140 kDa), and possibly differently post-translational modification or partially de-gradated bands (~113 kDa).

To further confirm that the purified product consisted of exosomes rather than other EVs, we performed an immune dot-blot analysis on isolated exosomes using a panel of 9 anti-exosomal antibodies following the manufacturer’s protocol. The blot revealed positive stains for 7 out of 8 exosome markers including FLOT1, ICAM1, CD81, CD63, EpCam, ANX5, and TSG101 for GBA-VSVG-GFP modified exosomes (Fig. 4b, Upper Panel) as well as native (control) (Fig. 4b, Lower Panel). The control cytosolic marker (GM130) was negative on both dot-blots, an indication of high purity of our exosome preparations. The same dot-blot but with different exposure times (Fig. S1) can be found in the Supplementary Information.

Next, we investigated whether our isolated EVs, exosomes, were properly loaded with the genetically encoded chimeric proteins. As shown in Fig. 4c, confocal fluorescence images of purified exosomes presented strong GFP expression for both GBA-VSVG-GFP and VSVG-GFP-GBA modified exosomes, indicating that the chimeras were appropriately targeted and anchored to exosomes. To further demonstrate that the full-length chimeras were properly expressed in transfected cells and integrated into secreted exosomes, we performed Western-blot analysis on both WCL and modified exosomes. Using an anti-TurboGFP antibody, we identified a ~140 kDa band was apparent in both GBA-VSVG-GFP and VSVG-GFP-GBA transfected cells but not in mock control samples (Fig. 4d), suggesting specific expression of the full-length chimeras in isolated exosomes and transfected producer cells. An uncropped immune-blot (Fig. S2) can be found in the Supplementary Information. Additionally, we notice some smaller positive bands (such as ~113 kDa) in both WCL and exosome samples, which may have resulted from differential post-translational modifications or partial degradations during sample preparation or exosome loading.

Together, these data demonstrate that our chimeras were properly expressed and integrated into EVs, most likely exosomes. These exosomes were then were released into conditioned medium and isolated with other EVs, after which they still retained their activity.

Targeted delivery of GBA to the endocytic compartment of recipient cells

Next, we investigated the intracellular delivery of GBA via engineered exosomes to human recipient cells using a combination of confocal monitoring and enzymatic assays. We first performed confocal imaging on HEK293 cells to track the distributions of these GBA chimeras after internalization. We observed cellular uptake in a concentration and time-dependent manner. The uptake was initially noticeable after 3~6 hours and became attenuated and plateaued after 24 hours (Levy D et al. unpublished data). Exosomes were presumed to enter cells via receptor-mediated endocytosis through surface protein interactions (Fig. 5a)46. Because VSVG ligand binds strongly to the VLDL-receptor, which appears on the surface of all human cell types, it was expected that VSVG-modified exosomes could effectively enter recipient cells, ultimately targeting their endocytic compartments46. In the case of GBA-VSVG-GFP modified exosomes, GBA enzymes would situate on the outer surface of exosomes, thus allowing for degradation of their substrates within the endosomal lumen. We further hypothesized that in the case of VSVG-GFP-GBA, the enclosed GBA enzyme would be released after the integration of modified exosomes into late endosomes (Fig. 5a). To determine the subcellular locations of modified exosomes post-uptake by recipient cells, we first added the either GBA-VSVG-GFP or VSVG-GFP-GBA loaded exosomes into the culture medium of HEK293 cells. We monitored the cellular up-take processes up to 72 hours using fluorescence microscopy. The punctated GFP-fluorescence signal within recipient cells was visible as early as 6 hours after uptake, with increasing intensity for 48 hours and persisted at least72 hours. Confocal images of cellular uptake of modified GBA-VSVG-GFP (Fig. 5,b1–4) and VSVG-GFP-GBA (Fig. 5,b5–8) endosomes recorded at 48 hours clearly identified punctated distributions of fluorescent label in the cytosol, which would be consistent with endocytic compartmentalization post-uptake. This cellular uptake was also observed in two additional human cell types, including human glioblastoma cell line U87 (Fig. S3a in Supplementary Information) and human hepatoma cell line HepG2 (Fig. S3b in Supplementary Information). To further verify whether these puncta were truly endocytic components, we carried out a co-localization assay using known markers for either early endosome, late endosomes or lysosomes. We identified endosomes by transfecting HEK293 cells with either early (RAB5a-RFP) or late endosome (RAB7a-RFP) markers before adding GBA-VSVG-GFP loaded exosomes into culture medium for cellular uptake. Confocal images revealed significant co-localization (yellow) of uptake exosomes (green) with red endosomal markers of early endosomes (Fig. 5c1–5) and late endosomes (Fig. 5c6–10). In a separate study, we first added GBA-VSVG-GFP loaded exosomes (green) to HEK293 cells to allow for cellular uptake for 24 hours before staining the cells with LysoTracker Red DND-99 to indicate lysosomal compartments. Analysis of these images showed that the engineered exosomes colocalized with lysosomal marker probe (Fig. 5c11–15). This finding supports our view that the internalized exosomes ultimately migrate to lysosomes. Together, these results demonstrate that our genetically modified exosomes were able to target endocytic compartments after entering recipient cells.

Figure 5

Delivery of GBA enzyme into endocytic compartments of recipient cells. (a) Schematic illustration of cellular uptake and lysosomal release of engineered GBA via the endocytosis process. (b) Parental HEK293 cells were treated with either GBA-VSVG-GFP (b1–4) or VSVG-GFP-GBA (b5–8) loaded exosomes in a glass bottom culture dish. 48 hours post-treatment, fluorescent, Hoechst stained, and PMT-Trans images were taken and overlaid (b1 and b8). In a set of separate experiments, GBA-VSVG-GFP or VSVG-GFP-GBA loaded exosomes were used to treat HEK293 cells that were either transfected with RFP-labeled early/late endosome reporters, Rab5a-RFP and Rab7a-RFP (c1–10) or stained with a red fluorescent-dye specific to lysosomes (c11–15). Arrows indicate early/late endosomes, or lysosomal structures. Scale bar 10 μm.

Next, we quantified the effectiveness of engineered exosomes to enter recipient cells by using FACS analysis. Following transfection of the cells with our engineered chimeras, we isolated exosomes expressing either the GBA-VSVG-GFP or VSVG-GFP-GBA and further labeled these preparations with a green fluorescent dye to enhance the sensitivity of FACS detection. We introduced the fluorescent dye-labeled exosomes to cultured HEK293 cells for 48 hours and conducted FACS to evaluate exosome uptake. When compared to unlabeled control exosomes, the uptake rates of both GBA-VSVG-GFP and VSVG-GFP-GBA were similar and equal to the control values of 73~75%. Overall, the uptake into HEK293 cells showed a 50-fold increase in fluorescent intensity over the unlabeled control (Fig. 6a). Thus, FACS data independently confirmed that our GBA-loaded exosomes are effective in gaining entry to recipient cells.

Figure 6

Intracellular delivery of bioactive GBA into living HEK293 cells. (a) Parental HEK293 cells were treated with either GBA-VSVG-GFP or VSVG-GFP-GBA modified exosomes for 48 hours before being subjected to FACS analysis. Right shifts in fluorescent signals for both GBA-VSVG-GFP (red line) and VSVG-GFP-GBA (green line) were observed as compared to control cells treated with unlabeled exosomes (black line). (b) HEK293 cells were treated with either isolated engineered exosomes or unmodified control exosomes for 48 hours, then washed and lysed. Equal amounts of proteins from the whole cell extracts were subjected to GBA enzymatic assays as described in the Materials and Methods. Values were expressed as mean ± standard deviation from 3 independent experiments (n = 11). *p < 0.05, **p < 0.01 significant vs control using a student-t test.

Next, we tested whether GBA remained enzymatically active after internalization in recipient cells. We conducted an enzyme assay to quantify the levels of GBA activity in engineered exosomes post-cellular uptake and compared these results to an unmodified control group. Equal amounts of GBA-VSVG-GFP, VSVG-GFP-GBA and unmodified control exosomes were added to HEK293 cells for 48 hours. Subsequently, GBA activities from the WCL and the resultant activities normalized to the control group (set as 100%). As shown in Fig. 6b, both the GBA-VSVG-GFP and VSVG-GFP-GBA modified exosomes exerted significantly greater GBA activity by ~45% (P < 0.05) and ~40% (P < 0.01) respectively, compared to the unmodified control. Thus, our data indicate that the genetically modified exosomes taken up by recipient cells display functionally active GBA.

In summary, the methods we have described to load GBA on the outer surface and inner lumen of exosomes produces functional enzymes that are properly directed to endocytic compartments within recipient cells. The highly efficient delivery and internalization of our modified exosomes was shown to significantly enhance GBA activity within these cells.


We have developed a genetic method to produce engineered exosomes that deliver functional lysosomal enzymes to the endocytic compartments of recipient cells. Unlike other nanoparticle-based carriers, exosomes are produced in human cells and exhibit intrinsic and specific mechanisms to enter the cytosol of living cells both in vitro and in vivo. Consequently, engineered exosomes hold promise in delivering protein payloads to targeted cells that are deep-seated in brain tissue28. Using this method, we effectively demonstrated that our engineered exosomes successfully delivered GBA, an enzyme associated with LSD, to human cells, where they target endocytic compartments. Our method may provide an alternative and more effective treatment option to manage LSDs, the largest family of human metabolic diseases. That includes Gaucher disease, which has been linked to neurological complications.

Over the past decade, there have been significant advances in engineering exosomes as drug delivery vehicles. The ability to use exosomes to deliver therapeutic cargo, including siRNA, mRNA, proteins, and small molecule drugs presents new opportunities for targeted delivery to treat various human diseases including cancer, inflammation, and hereditary diseases such as LSDs47,48,49,50,51. While loading and delivery of biologically active lysosomal enzymes onto exosomes has been hypothesized, we are unaware of any demonstration of the feasibility or effectiveness of this approach. Lysosomal enzymes have a natural address (targeting lysosomes instead of exosomes). Moreover the activities of lysosomal enzymes require specific post-translational modifications, including glycosylation44,45. Consequently, the delivery of these enzymes to cell models of LSDs requires the development of a robust exosome-targeting scaffold that projects the enzyme with the correct geometry and allows for post-translational modifications during exosome biogenesis. To achieve this goal, we employed the single transmembrane protein, VSVG, which we have previously shown to be efficiently expressed in human cells. VSVG serves as a scaffold amenable to load proteins onto exosomes in a predefined manner by genetic fusion42. VSVG has a number of advantages for exosome targeting compared to other exosome-targeting scaffolds, including tetraspanins (CD9, CD63, and CD81), lipid anchoring peptide (C1C2 domain of lactacherin) and lysosome membrane protein (Lamp2B)37,43,51,52. First, VSVG integrates into exosomal membranes providing a stable anchoring mechanism for their fused-enzyme cargo. Thus, VSVG is not conceptually different from lysosome proteins and lipid anchors, neither of which is sufficiently stable nor can they be specifically targeted. Second, VSVG is a single transmembrane protein with a well-defined domain structure and membrane topology, composed of an ectodomain, a transmembrane helix, and a small luminal peptide42. This linear structure streamlines the design of geometrically-defined fusion proteins that may be directed to the outer surface or inside the lumen of the exosome. We note other scaffolds often lack this flexibility. For example, tetraspanins and C1C2 restrict their cargo loading to either the inside or the outside of the exosomal membrane37,52, while Lamp2B requires additional glycosylation to maintain the stability of its protein cargo53. Third, VSVG has a programmable ectodomain that can be easily swapped with cell-specific peptides or nanobodies, therefore permitting advanced engineering for additional benefits such as specific cell type targeting, or purification42.

Post-translational modification of GBA such as glycosylation is an important step in the production of a functional enzyme44,45. Glycosylation occurs co-translationally and is needed for the stability and lysosomal targeting, therefore endogenous activities in lysosomes41,54,55,56. However, our engineered GBA-fusion proteins still go through normal translation, the intrinsic enzyme activities may not be severely affected as evidenced by readily detected increased GBA activities in our transfected cells and EVs. It remains unknown if our GBA-fusion proteins are subjected to differentially co-translational glycosylations as compared to native GBA.

Another unique feature of this study is the genetic design used to produce modified exosomes. The exosomes present functional GBA enzymes in two different spatial conformations (either the outer or inner surface of exosome membrane), and the scaffold is capable of accommodating a reporter protein (GFP). GFP is especially useful in the observation of intracellular trafficking and uptake of purified exosomes in recipient cells. Interestingly, the two different placements of GBA enzyme lead to similar results. However, the two methods may have distinct advantages and potential limitations. The surface display approach may allow to load many copies of the enzyme to the exosome membrane surface, which may also increase the chance of enzymatic degradation during delivery. Placing enzymes within the lumen of the exosome could provide increased protection and potentially elicit fewer off-target interactions, as the therapeutic enzyme would not be able to interact with external molecules, including proteases. Nevertheless, we did not observe a significant difference between these two GBA configurations, suggesting both approaches are effective. Further confirmation of GBA-loaded EVs using either patients-derived GBA mutant fibroblast cells or in vitro GBA mutant cells as functional relevance is critical for further development. Additionally, studies using animal models are needed to determine which composition would result in the most effective therapeutic benefit.

While our exosome surface display is promising for treating Gaucher disease, there may be some in vivo limitations such as immunological responses to this biologics, which needs further studies using animal models.


We have developed a genetic approach to produce enzyme-loaded EVs/exosomes for the targeted delivery of GBA enzyme to human cells. Through fusion with VSVG, the enzyme payloads are strongly enriched in EVs/exosomes, which are delivered to the endocytic compartments (early/late endosomes and lysosomes) of recipient cells. Our proof-of-concept work establishes the engineering methodology of EVs/exosomes for targeted delivery of bioactive lysosomal enzymes for a potential treatment strategy of Gaucher disease, especially for those with severe forms of the disease associated with neurological complications.


  1. 1.

    Parenti, G., Andria, G. & Ballabio, A. Lysosomal storage diseases: from pathophysiology to therapy. Annu Rev Med 66, 471–486 (2015).

  2. 2.

    Futerman, A. H. & van Meer, G. The cell biology of lysosomal storage disorders. Nat Rev Mol Cell Biol 5, 554–565 (2004).

    CAS  Article  Google Scholar 

  3. 3.

    Beck, M. New therapeutic options for lysosomal storage disorders: enzyme replacement, small molecules and gene therapy. Hum Genet 121, 1–22 (2007).

    CAS  Article  Google Scholar 

  4. 4.

    Parenti, G., Pignata, C., Vajro, P. & Salerno, M. New strategies for the treatment of lysosomal storage diseases (review). Int J Mol Med 31, 11–20 (2013).

  5. 5.

    Ballabio, A. & Gieselmann, V. Lysosomal disorders: from storage to cellular damage. Biochim Biophys Acta 1793, 684–696 (2009).

    CAS  Article  Google Scholar 

  6. 6.

    Aharon-Peretz, J., Rosenbaum, H. & Gershoni-Baruch, R. Mutations in the glucocerebrosidase gene and Parkinson’s disease in Ashkenazi Jews. N Engl J Med 351, 1972–1977 (2004).

    CAS  Article  Google Scholar 

  7. 7.

    Lachmann, R. H. Enzyme replacement therapy for lysosomal storage diseases. Curr Opin Pediatr 23, 588–593 (2011). 

    CAS  Article  Google Scholar 

  8. 8.

    Wraith, J. E. Limitations of enzyme replacement therapy: current and future. J Inherit Metab Dis 29, 442–447 (2006).

    CAS  Article  Google Scholar 

  9. 9.

    Wyatt, K. et al. The effectiveness and cost-effectiveness of enzyme and substrate replacement therapies: a longitudinal cohort study of people with lysosomal storage disorders. Health Technol Assess 16, 1–543 (2012).

  10. 10.

    Barton, N. W. et al. Replacement therapy for inherited enzyme deficiency–macrophage-targeted glucocerebrosidase for Gaucher’s disease. N Engl J Med 324, 1464–1470 (1991).

    CAS  Article  Google Scholar 

  11. 11.

    Barton, N. W., Furbish, F. S., Murray, G. J., Garfield, M. & Brady, R. O. Therapeutic response to intravenous infusions of glucocerebrosidase in a patient with Gaucher disease. Proc Natl Acad Sci USA 87, 1913–1916 (1990).

    ADS  CAS  Article  Google Scholar 

  12. 12.

    Kakkis, E. D. et al. Enzyme-replacement therapy in mucopolysaccharidosis I. N Engl J Med 344, 182–188 (2001).

    CAS  Article  Google Scholar 

  13. 13.

    Eng, C. M. et al. Safety and efficacy of recombinant human alpha-galactosidase A replacement therapy in Fabry’s disease. N Engl J Med 345, 9–16 (2001).

    CAS  Article  Google Scholar 

  14. 14.

    Schiffmann, R. et al. Enzyme replacement therapy in Fabry disease: a randomized controlled trial. JAMA 285, 2743–2749 (2001).

    CAS  Article  Google Scholar 

  15. 15.

    Van den Hout, H. et al. Recombinant human alpha-glucosidase from rabbit milk in Pompe patients. Lancet 356, 397–398 (2000).

    Article  Google Scholar 

  16. 16.

    Harmatz, P. et al. Enzyme replacement therapy for mucopolysaccharidosis VI: a phase 3, randomized, double-blind, placebo-controlled, multinational study of recombinant human N-acetylgalactosamine 4-sulfatase (recombinant human arylsulfatase B or rhASB) and follow-on, open-label extension study. J Pediatr 148, 533–539 (2006).

    CAS  Article  Google Scholar 

  17. 17.

    Brady, R. O. Enzyme replacement for lysosomal diseases. Annu Rev Med 57, 283–296 (2006).

    CAS  Article  Google Scholar 

  18. 18.

    Altarescu, G. et al. The efficacy of enzyme replacement therapy in patients with chronic neuronopathic Gaucher’s disease. J Pediatr 138, 539–547 (2001).

    CAS  Article  Google Scholar 

  19. 19.

    Scarpa, M. et al. Treatment of brain disease in the mucopolysaccharidoses. Mol Genet Metab 122S, 25–34 (2017).

    CAS  Article  Google Scholar 

  20. 20.

    Bellettato, C. M. & Scarpa, M. Possible strategies to cross the blood-brain barrier. Ital J Pediatr 44, 131 (2018).

  21. 21.

    Mittelbrunn, M. & Sanchez-Madrid, F. Intercellular communication: diverse structures for exchange of genetic information. Nat Rev Mol Cell Biol 13, 328–335 (2012).

    CAS  Article  Google Scholar 

  22. 22.

    Thery, C. Exosomes: secreted vesicles and intercellular communications. F1000 Biol Rep 3, 15 (2011).

  23. 23.

    Record, M., Carayon, K., Poirot, M. & Silvente-Poirot, S. Exosomes as new vesicular lipid transporters involved in cell-cell communication and various pathophysiologies. Biochim Biophys Acta 1841, 108–120 (2014).

  24. 24.

    Choi, D. S., Kim, D. K., Kim, Y. K. & Gho, Y. S. Proteomics, transcriptomics and lipidomics of exosomes and ectosomes. Proteomics 13, 1554–1571 (2013).

  25. 25.

    EL Andaloussi, S., Mager, I., Breakefield, X. O. & Wood, M. J. Extracellular vesicles: biology and emerging therapeutic opportunities. Nat Rev Drug Discov 12, 347–357 (2013).

  26. 26.

    Kumari, A., Yadav, S. K. & Yadav, S. C. Biodegradable polymeric nanoparticles based drug delivery systems. Colloids Surf B Biointerfaces 75, 1–18 (2009).

    Article  Google Scholar 

  27. 27.

    Sahay, G. et al. Efficiency of siRNA delivery by lipid nanoparticles is limited by endocytic recycling. Nat Biotechnol 31, 653–658 (2013).

    CAS  Article  Google Scholar 

  28. 28.

    Alvarez-Erviti, L. et al. Delivery of siRNA to the mouse brain by systemic injection of targeted exosomes. Nat Biotechnol 29, 341–345 (2011).

    CAS  Article  Google Scholar 

  29. 29.

    Kamerkar, S. et al. Exosomes facilitate therapeutic targeting of oncogenic KRAS in pancreatic cancer. Nature 546, 498–503 (2017).

    ADS  CAS  Article  Google Scholar 

  30. 30.

    Guo, S. et al. Intranasal Delivery of Mesenchymal Stem Cell Derived Exosomes Loaded with Phosphatase and Tensin Homolog siRNA Repairs Complete Spinal Cord Injury. ACS Nano (2019).

  31. 31.

    Gorabi, A. M. et al. The Therapeutic Potential of Mesenchymal Stem Cell-Derived Exosomes in Treatment of Neurodegenerative Diseases. Mol Neurobiol (2019).

  32. 32.

    Duong, N. C. et al. exosomes as a novel biologic reagent to antognize inflammation. International Journal of Nanomedicine 14, 3413–3425 (2019).

    CAS  Article  Google Scholar 

  33. 33.

    Kim, I. K., Kim, S. H., Choi, S. M., Youn, B. S. & Kim, H. S. Extracellular Vesicles as Drug Delivery Vehicles for Rheumatoid Arthritis. Curr Stem Cell Res Ther 11, 329–342 (2016). 

  34. 34.

    Choi, K., Choi, H., Yim, N., Ryu, S. W. & Choi, C. Exosome-based delivery of glucocerebrosidase lysosomal enzyme for treatment of Gaucher disease. Molecular Genetics and Metabolism. 123, S31–S32 (2017).

    Article  Google Scholar 

  35. 35.

    Hruska, K. S., LaMarca, M. E., Scott, C. R. & Sidransky, E. Gaucher disease: mutation and polymorphism spectrum in the glucocerebrosidase gene (GBA). Hum Mutat 29, 567–583 (2008).

    CAS  Article  Google Scholar 

  36. 36.

    Grabowski, G. A. Phenotype, diagnosis, and treatment of Gaucher’s disease. Lancet 372, 1263–1271 (2008).

    CAS  Article  Google Scholar 

  37. 37.

    Stickney, Z., Losacco, J., McDevitt, S., Zhang, Z. & Lu, B. Development of exosome surface display technology in living human cells. Biochem Biophys Res Commun 472, 53–59 (2016).

    CAS  Article  Google Scholar 

  38. 38.

    Hampf, M. & Gossen, M. A protocol for combined Photinus and Renilla luciferase quantification compatible with protein assays. Anal Biochem 356, 94–99 (2006).

    CAS  Article  Google Scholar 

  39. 39.

    Peterson, M. F., Otoc, N., Sethi, J. K., Gupta, A. & Antes, T. J. Integrated systems for exosome investigation. Methods 87, 31–45 (2015).

  40. 40.

    Mazzulli, J. R. et al. Gaucher disease glucocerebrosidase and alpha-synuclein form a bidirectional pathogenic loop in synucleinopathies. Cell 146, 37–52 (2011).

  41. 41.

    Yun, S. P. et al. alpha-Synuclein accumulation and GBA deficiency due to L444P GBA mutation contributes to MPTP-induced parkinsonism. Mol Neurodegener 13, 1 (2018).

  42. 42.

    Meyer, C. et al. Pseudotyping exosomes for enhanced protein delivery in mammalian cells. Int J Nanomedicine 12, 3153–3170 (2017).

    CAS  Article  Google Scholar 

  43. 43.

    Wang, J. H. et al. Anti-HER2 scFv-Directed Extracellular Vesicle-Mediated mRNA-Based Gene Delivery Inhibits Growth of HER2-Positive Human Breast Tumor Xenografts by Prodrug Activation. Mol Cancer Ther 17, 1133–1142 (2018).

    CAS  Article  Google Scholar 

  44. 44.

    Erickson, A. H., Ginns, E. I. & Barranger, J. A. Biosynthesis of the lysosomal enzyme glucocerebrosidase. J Biol Chem 260, 14319–14324 (1985).

    CAS  PubMed  Google Scholar 

  45. 45.

    Berg-Fussman, A., Grace, M. E., Ioannou, Y. & Grabowski, G. A. Human acid beta-glucosidase. N-glycosylation site occupancy and the effect of glycosylation on enzymatic activity. J Biol Chem 268, 14861–14866 (1993).

    CAS  PubMed  Google Scholar 

  46. 46.

    McKelvey, K. J., Powell, K. L., Ashton, A. W., Morris, J. M. & McCracken, S. A. Exosomes: Mechanisms of Uptake. J Circ Biomark 4, 7 (2015).

    Article  Google Scholar 

  47. 47.

    Ha, D., Yang, N. & Nadithe, V. Exosomes as therapeutic drug carriers and delivery vehicles across biological membranes: current perspectives and future challenges. Acta Pharm Sin B 6, 287–296 (2016).

  48. 48.

    Sterzenbach, U. et al. Engineered Exosomes as Vehicles for Biologically Active Proteins. Mol Ther 25, 1269–1278 (2017).

    CAS  Article  Google Scholar 

  49. 49.

    Shahabipour, F., Banach, M. & Sahebkar, A. Exosomes as nanocarriers for siRNA delivery: paradigms and challenges. Arch Med Sci 12, 1324–1326 (2016).

  50. 50.

    Riazifar, M., Pone, E.J., Lotvall, J. & Zhao, W. Stem Cell Extracellular Vesicles: Extended Messages of Regeneration. Annu Rev Pharmacol Toxicol 57, 125–154 (2017).

  51. 51.

    Yim, N. et al. Exosome engineering for efficient intracellular delivery of soluble proteins using optically reversible protein-protein interaction module. Nat Commun 7, 12277 (2016).

    ADS  CAS  Article  Google Scholar 

  52. 52.

    Antes, T. J. et al. Targeting extracellular vesicles to injured tissue using membrane cloaking and surface display. J Nanobiotechnology 16, 61 (2018).

  53. 53.

    Hung, M. E. & Leonard, J. N. Stabilization of exosome-targeting peptides via engineered glycosylation. J Biol Chem 290, 8166–8172 (2015).

  54. 54.

    Grace, M. E., Newman, K. M., Scheinker, V., Berg-Fussman, A. & Grabowski, G. A. Analysis of human acid beta-glucosidase by site-directed mutagenesis and heterologous expression. J Biol Chem 269, 2283–2291 (1994).

    CAS  PubMed  Google Scholar 

  55. 55.

    Smith, L., Mullin, S. & Schapira, A. H. V. Insights into the structural biology of Gaucher disease. Exp Neurol 298, 180–190 (2017).

  56. 56.

    Reczek, D. et al. LIMP-2 is a receptor for lysosomal mannose-6-phosphate-independent targeting of beta-glucocerebrosidase. Cell 131, 770–783 (2007).

    CAS  Article  Google Scholar 

Download references


The authors would like to thank Dr. Yan Jiang for help in editing the manuscript. We also would like to thank Mr. Kyle Asano for performing FACS and data analysis. The work was supported by internal grants of Santa Clara University.

Author information




B.L. developed the hypothesis, design, experimental approach, performed experiments, analyzed data, coordinated the project and wrote the manuscript. M.D., D.L. and A.B. conducted the experiments and revised the manuscript. G.M. helped to interpret data and revised the manuscript to add new content and perspectives. All authors read and approved the final manuscript.

Corresponding author

Correspondence to Biao Lu.

Ethics declarations

Competing interests

Santa Clara University has filed patents (pending) related to work presented in this manuscript.

Additional information

Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary information

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Do, M.A., Levy, D., Brown, A. et al. Targeted delivery of lysosomal enzymes to the endocytic compartment in human cells using engineered extracellular vesicles. Sci Rep 9, 17274 (2019).

Download citation

Further reading


By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.


Quick links