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PEG-lipid micelles enable cholesterol efflux in Niemann-Pick Type C1 disease-based lysosomal storage disorder


2-Hydroxy-propyl-β-cyclodextrin (HPβCD), a cholesterol scavenger, is currently undergoing Phase 2b/3 clinical trial for treatment of Niemann Pick Type C-1 (NPC1), a fatal neurodegenerative disorder that stems from abnormal cholesterol accumulation in the endo/lysosomes. Unfortunately, the extremely high doses of HPβCD required to prevent progressive neurodegeneration exacerbates ototoxicity, pulmonary toxicity and autophagy-based cellular defects. We present unexpected evidence that a poly (ethylene glycol) (PEG)-lipid conjugate enables cholesterol clearance from endo/lysosomes of Npc1 mutant (Npc1−/−) cells. Herein, we show that distearyl-phosphatidylethanolamine-PEG (DSPE-PEG), which forms 12-nm micelles above the critical micelle concentration, accumulates heavily inside cholesterol-rich late endosomes in Npc1−/− cells. This potentially results in cholesterol solubilization and leakage from lysosomes. High-throughput screening revealed that DSPE-PEG, in combination with HPβCD, acts synergistically to efflux cholesterol without significantly aggravating autophagy defects. These well-known excipients can be used as admixtures to treat NPC1 disorder. Increasing PEG chain lengths from 350 Da-30 kDa in DSPE-PEG micelles, or increasing DSPE-PEG content in an array of liposomes packaged with HPβCD, improved cholesterol egress, while Pluronic block copolymers capable of micelle formation showed slight effects at high concentrations. We postulate that PEG-lipid based nanocarriers can serve as bioactive drug delivery systems for effective treatment of lysosomal storage disorders.


Niemann Pick Type C (NPC) is an inherited autosomal recessive lysosomal storage disorder that affects approximately 1:120,000 children globally and results in hepatomegaly, progressive neurodegeneration, and finally death1,2. There are no current treatments available for children suffering from this devastating rare genetic disease. 95% of NPC cases result from defects in the NPC1 protein, a large glycoprotein with 13-membrane-spanning domains that resides on the surface of late endosomes/lysosomes, with a sterol-sensing domain in the lumen that binds to cholesterol and enables egress to a cytoplasmic location3. NPC1 deficiency causes cholesterol accumulation that manifests as enlargement of late endosomes/lysosomes, ultimately leading to neurodegeneration, especially loss of Purkinje fibers in the cerebellum, which leads to ataxia and cognitive loss4,5. HPβCD is a Food and Drug Administration (FDA) approved hydrophilic small molecule excipient that has a hydrophobic pocket capable of binding and solubilizing cholesterol6. It is capable of the efflux and redistribution of cholesterol in mammalian cells7; however, it does not readily cross the blood brain barrier (only 0.2% reaches the brain on systemic administration). In preclinical studies, a direct brain injection of HPβCD into an NPC mouse model slowed the progression of neuronal loss and improved its survival8,9,10,11. Similar results were observed in a feline model of NPC disease, with an intra-cisternal administration used to decrease neurodegeneration and prolong survival12. More recently, an intrathecal cyclodextrin injection in a single NPC1 patient led to an increase in cholesterol redistribution in the central nervous system and improved vertical gaze palsy, a clinical indicator of NPC-linked neurodegeneration13. Based on these results, HPβCD has entered NIH initiated Phase 2b/3 clinical trial, and the FDA has granted orphan drug status to further accelerate use of HPβCD for treating NPC disease. An impediment to the clinical translation of HPβCD is the exorbitant amount of drug required to clear cholesterol in order to elicit a significant response. In a single example, a biweekly administered dose of 200 mg, with a total of 27 injections, applied by lumbar puncture to a child with NPC, slowed neurodegeneration but resulted in high-frequency hearing loss13. In the feline model, a subcutaneous injection of 8000 mg/kg was necessary to halt the loss of Purkinje neurons, but resulted in significant pulmonary toxicity12.

Liposomes are among the most advanced drug delivery systems for effective intracellular delivery, and thus an obvious carrier choice for delivery of HPβCD to remove intracellular cholesterol aggregates14,15,16. Liposomal drug delivery vectors have several advantages, including prolonged circulation times, the potential to incorporate multiple drugs with different mechanisms of action and solubility, and surface decoration with a variety of targeting ligands (e.g. transferrin) that can enable transport across the blood brain barrier14,17,18. Lipid nanoparticles (LNPs), a subset of liposomal vectors, have been very effective in the delivery of nucleic acids19,20. LNPs are shown to enter cells through endocytic portals and are selectively recycled through NPC1-positive late endosomes; the absence of NPC1 showed a 10–15-fold retention of LNPs inside cells which translated to improved nucleic acid delivery21. Hydrogenated soy phosphatidylcholine (HSPC) based liposomes that incorporate water-soluble small molecules in the core had a similar pattern of retention in the endo/lysosomal system of NPC1 deficient cells21. Based on these studies, we hypothesized that simple liposomal formulations would enhance site-specific delivery of HPβCD into the cholesterol rich endo/lysosomes in Npc1 deficient mouse embryonic fibroblasts (MEFs). We created a small set of two-component liposomes from HSPC and distearyl-phosphatidylethanolamine conjugated with polyethylene glycol (DSPE-PEG), a common PEG-lipid known to improve nanocarrier stability. Surprisingly, we found that increasing the molar ratio of DSPE-PEG in the liposomes improved HPβCD mediated cholesterol efflux, and ultimately deduced that DSPE-PEG on its own triggered cholesterol clearance. Most remarkably, we found that DSPE-PEG used in combination with HPβCD showed a substantial decline in the lysosomal cholesterol content in Npc1-deficient cells. These studies strongly suggest that a simple mixture of two well-characterized biocompatible excipients can have a significant impact in the treatment of NPC lysosomal storage disorder.


A filipin-based assay was used to visualize accumulation of cholesterol in Npc1−/− MEFs. Filipin interacts with cholesterol to form a complex that is fluorescent at 405 nm. This assay has been utilized as a clinical diagnostic test for NPC disease and allows for rapid identification of molecules capable of sequestering cholesterol from intracellular membranes22,23. Using this assay, we confirmed heavy accumulation of cholesterol in enlarged punctate structures inside Npc1−/− MEFs, relative to Npc1+/+ MEFs (Fig. 1A). To characterize these structures, we transfected both cell lines with Rab7-GFP, a late-endosome marker. Fluorescence microscopy revealed enlarged late-endosomes in Npc1−/− cells, with a clear demarcation of Rab7-GFP on the lysosomal surface. Filipin-stained cholesterol was observed within the lumen of Rab7-positive late-endosomes (Fig. 1B). In contrast, Npc1+/+ cells showed smaller Rab7-positive punctate structures, and the filipin stain appeared substantially lower and markedly more diffused in the cytoplasm (Fig. 1B), suggestive of normal cholesterol transport in these cells. These studies confirm abnormal accumulation of cholesterol in late endo/lysosomes of Npc1−/− MEF cells.

Figure 1: Npc1 deficiency leads to cholesterol accumulation in enlarged late endosomes/lysosomes.

(A) Filipin staining was performed to visualize subcellular cholesterol in Npc1−/− and Npc1+/+ MEFs. A high throughput microscope was used to compare subcellular cholesterol (psuedo colored red) in both cell types. Nucleus was stained using HCS nuclear mask deep red stain. (psuedo colored blue) (B) Npc1−/− and Npc1+/+ MEFs were transfected with to Rab-7 GFP (pseudo colored green) using a baculovirus. Cells were fixed 18 hours post transfection and stained with filipin (red). The cell outline is demarcated with dotted line; white arrow shows filipin and black arrow endosomal Rab7-GFP. All experiments were conducted in triplicates.

We further utilized filipin imaging to demonstrate the well-documented use of HPβCD to decrease intracellular cholesterol from endo/lysosomes in Npc1−/− cells, by cholesterol solubilization, which perhaps enables efflux from these intracellular depots. Npc1−/− cells show a marked decrease in filipin fluorescence with increasing concentration of HPβCD treatment, up to 10 mM (Fig. 2A). Quantitative analysis of filipin staining shows that a 0.5 mM HPβCD treatment for 24 hours reduced endosomal cholesterol by 50%. A 10 mM HPβCD treatment further decreased cholesterol levels in Npc1−/− cells (ca. 75–80%), which is comparable to the levels in Npc1+/+ MEFs (Fig. 2B). In addition, we used an amplex-red assay to quantify cholesterol in whole cell lysates. We confirm a dose-dependent decrease in the total cholesterol in Npc1−/− cells (Fig. 2C).

Figure 2: HPβCD removes cholesterol from Npc1−/− cells.

Npc1−/− MEFs were incubated with HPβCD (0–10 mM) for 24 hours. Cells were either fixed or lysed. (A) Fixed cells were imaged for filipin stain using high throughput imaging and representative images are show for 0.01, 0.1, 1 and 10 mM HPβCD treatments. (B) Filipin fluorescence per cell was quantified using Olympus scanR analysis software, and normalized to untreated cells. 48 images per treatment group were analyzed. (C) Cell lysates were analyzed for total cellular cholesterol using the amplex red assay and normalized by total protein content. Untreated Npc1+/+ MEFs are shown for comparison. Results were tested for statistical significance using one-way ANOVA with Tukey’s multiple comparison test. *P < 0.05, **P < 0.01, ***P < 0.001 and NS = not significant.

We initially set out to encapsulate HPβCD in the hydrophilic core of liposomes, formulated from HSPC and DSPE-PEG2k, in order to site-specifically deliver HPβCD into the endo/lysosomal system. DSPE-PEG2k is a known liposomal stabilizer, and we tested liposomes composed of different molar ratios of these two lipids in order to optimize the formulation. Liposomes were assembled by thin film rehydration in the presence of a concentrated HPβCD solution and dialyzed to remove free cyclodextrin. Liposomes were characterized for their size, shape, and encapsulation efficiency. We confirmed liposomal assembly using Transmission Electron Microscopy (TEM) imaging and measured their average hydrodynamic sizes using Dynamic light scattering (DLS). Both DLS and TEM showed that increasing PEG-lipid content decreased the size of the nanoparticles from 150 nm to 10–15 nm (Fig. S1A,B). However, in formulations containing both lipid components, DLS suggested the presence of a mixed population of liposomes and micelles. We measured the loading efficiency using LC/MS/MS and found a gradual decrease in encapsulation with increasing PEG-lipid, which may be due to the increasing hydrophobic microenvironment of the core along with the decreasing size of the carrier. Surprisingly, when testing these formulations on Npc1−/− cells, the nanocarriers with higher molar ratios DPSE-PEG2k were the most potent in terms of cholesterol clearance despite a relatively lower loading efficiency of HPβCD (Fig. S1C).

DSPE-PEG2k forms spherical micelles above the critical micelle concentration (CMC), of 1 μM. DLS of assembled micelles showed a consistent and uniform 12 nm hydrodynamic size and TEM imaging showed a 5 nm electron dense core (Fig. 3A). This data is consistent with published models of PEG-lipid micelles that self-assemble to form a core-shell structure, in which the DSPE tail aggregates into a hydrophobic core and PEG chains are exposed to the aqueous solvent (Fig. 3B). To our surprise, treatment with only DSPE-PEG2k micelles resulted in a dose-dependent decrease in cholesterol levels in Npc1−/− cells (Fig. 3C,D). Treatments as low as 1 μM DSPE-PEG2k led to 13% reduction in cholesterol, which, when increased to 10 μM, resulted in a ~40% reduction in cholesterol. The 40% reduction was the highest cholesterol egress achieved, even with concentrations up to 500 μM. This decrease was significant, since a 75–80% reduction of cholesterol in Npc1−/− cells reduced cholesterol to normal cellular levels (Fig. 2B,C). Both filipin and amplex red cholesterol assays show similar results, which strongly suggests that these materials are capable of reducing intracellular cholesterol deposits and enabling cholesterol efflux from the endo/lysosomal system.

Figure 3: DSPE-PEG2k reduces cellular cholesterol in Npc1−/− cells with a dose dependent response.

DSPE-PEG2k micelles were assembled by thin film rehydration method. (A) TEM images of micelles show electron dense cores that are approximately 5 nm. (B) Schematic diagram of assembled DSPE-PEG2k micelles has an electron dense hydrophobic core, with extended hydrophilic PEG head groups. (C) Npc1−/− cells were exposed to different concentrations of DSPE-PEG2k (0–500 μM), fixed and a dose dependent decrease in filipin fluorescence per cell was observed by high throuhgput screening. (D) Whole cell cholesterol (per mg protein), normalized to un-treated cells, also shows a dose dependent reduction in cholesterol when treated with DSPE-PEG2k. Results were tested for statistical significance using one-way ANOVA with Tukey’s multiple comparison test. *P < 0.05, **P < 0.01, ***P < 0.001 and NS = not significant.

DSPE-PEG2k is an essential component of LNPs that have been shown to preferentially accumulate in the late endosomes/lysosomes of Npc1−/− cells. Therefore, we hypothesized that DSPE-PEG2k actively accumulates in these cells and subsequently leads to solubilization of cholesterol. To test this hypothesis, we evaluated the uptake kinetics of carboxy-fluorescein (CF) labeled DSPE-PEG2k micelles at different time points and monitored their localization within filipin-positive late-endosomes using automated high-throughput imaging. The DSPE-PEG2k-CF was detected by cellular internalization after approximately 2 hours, and saturated the endo/lysosomal system within 24 hours; the relatively slow rate of uptake is suggestive of macropinocytosis (Fig. 4A,B). We utilized filipin to measure localization of DSPE-PEG2k-CF delivered to the cholesterol-rich late endosomes/lysosomes in Npc1−/− cells. At 2 hours, the labeled micelles show ~50% co-localization with filipin-stained cholesterol deposits (Fig. 4C) but within 4–6 hours ~60% of the labeled micelles reached filipin-positive endosomes and by 24 hours we observed an 80% co-localization with late endosomes/lysosomes (Fig. 4C). These studies clearly show a substantial delivery of DSPE-PEG2k-CF micelles into the cholesterol-laden endo/lysosomes of Npc1−/− cells. It is likely that DSPE-PEG interacts with large cholesterol deposits in the late endosomes, which leads to a degree of aggregate solubilization and potentially releases them from the lysosomal compartment. Interestingly, DSPE-PEG2k-CF did not show enhanced accumulation in wild-type cells (data not shown), suggestive of enhanced accumulation in late-endosomes due to recycling defects present in Npc1−/− cells as previously observed21.

Figure 4: Labeled DSPE-PEG2k is internalized and localized to filipin positive vesicles in Npc1−/− cells.

Carboxy-Fluorescein (CF) labeled DSPE-PEG2k assembled into micelles by thin film rehydration was exposed to cells at 10 μM concentration for different time points (2, 3, 4, 6, 24 hours), cells were washed, fixed and filipin stained. (A) High throughput imaging (16 images/well) was performed to monitor DSPE-PEG2k-CF uptake and co-localization with endosomal cholesterol. (B) Image-J software was utilized to measure DSPE-PEG2k-CF uptake and (C) Monitor co-localization by calculation of Pearson Coefficient. (n = 5). Results were tested for statistical significance using one-way ANOVA with Tukey’s multiple comparison test relative to untreated cells (B) or 24 hour treated cells (C). *P < 0.05, **P < 0.01, ***P < 0.001 and NS = not significant.

We set out to evaluate the synergy of combinatorial treatments with both DSPE-PEG and HPβCD to potentiate cholesterol removal. We created a matrix of treatment groups consisting of DSPE-PEG2k micelles (0.05–500 μM) and HPβCD ranging from 0.01 mM–10 mM. Npc1−/− cells were exposed to these treatments, in combination or alone, for 24 hours, prior to fixing, staining and imaging (Fig. 5A). Quantification of filipin fluorescence showed a decrease in cholesterol with individual treatments, and a synergistic effect when both treatments were administered together (Fig. 5B). We observed that a treatment of 0.05 mM HPβCD and 5 μM DSPE-PEG2k showed a 30% cholesterol clearance, which was further reduced to 50% with 0.05 mM HPβCD and 10 μM–100 μM DSPE-PEG2k treatment. This effect became more pronounced as the concentration of each component was increased. A 75% cholesterol reduction resulted from treatment of 0.25 mM of HPβCD combined with 10 μM DSPE-PEG2k, making cholesterol levels comparable to wild-type cells. It has been observed that a dose of 1 mM HPβCD in Npc1 mutant neuronal cultures or in plasma of human patients elicits a drug response that affects the disease phenotype8,24. We showed that 1 mM HPβCD reduces cholesterol by ~50%, but a comparable cholesterol reduction can be achieved with 10 μM DSPE and a 4-fold lower concentration of HPβCD (0.05 mM). We observed no toxicity at these concentrations, and only at an exceptionally high treatment combination i.e. 10 mM HPβCD and 500 μM DSPE-PEG2k, there was a dramatic reduction in total cell number (Fig. S2).

Figure 5: Combination treatment of PEG-lipid and HPBCD lead to synergistic clearance in Npc1−/− cells.

Npc1−/− MEFs cells were treated with DSPE-PEG2k micelles (0–500 μM) and HPβCD (0–10 mM). Cells were fixed and stained with filipin and nuclear mask. (A) Representative images of select treatments are shown and illustrate the synergistic cholesterol reduction of the two treatments. (B) Cells were quantitatively analyzed for filipin fluorescence per cell, and the dose dependent reduction of filipin fluorescence is shown normalized to untreated cells. Images per well were taken (n = 3, 16 images/well) and cells were quantified for total filipin fluorescence. The treatment with 500 μM DSPE-PEG2k and 10 mM HPβCD is toxic, and no cells are observed. Results were tested for statistical significance using one-way ANOVA with Tukey’s multiple comparison test. *P < 0.05, **P < 0.01, ***P < 0.001 and NS = not significant.

PEG-lipids are commercially available with various PEG chain lengths, and we tested a diverse set that included DSPE-PEG350, DSPE-PEG1k, DSPE-PEG2k, DSPE-PEG5k, DSPE-PEG10k, DSPE-PEG20k, and DSPE-PEG30k at 10 μM both with and without 0.1 mM HPβCD (Fig. 6A). DSPE (unconjugated), DSPE-PEG350 and DSPE-PEG1k treatments did not decrease cellular cholesterol. On the other hand, DSPE-PEG2k, DSPE-PEG5k, DSPE-PEG10k, DSPE-PEG20k, and DSPE-PEG30k showed cholesterol reduction where longer PEG chain lengths performed marginally better relative to shorter chain lengths. The co-treatment of low dose DSPE-PEGs with 0.1 mM HPβCD further reduced cellular cholesterol in most treatments. Interestingly, treatment with PEG2k or combination treatment of PEG2k and DSPE (unconjugated) showed increased cholesterol accumulation in Npc1−/− cells (Fig. 6A, S3). We observed that as the PEG chain length increases the size of the micelles also increase from 5 nm (DSPE-PEG350) to 24 nm (DSPE-PEG10–30k). Micelles with the hydrodynamic size of 16–24 nm, independent of PEG chain length, were capable of equivalent cholesterol efflux suggesting that this size range is important for access to lysosomal pathways (Fig. 6B). We further tested if other polymers with micelle forming capacity can cause cholesterol clearance. Pluronic block copolymers are composed of poly (ethylene oxide) (PEO) and poly(propylene oxide) (PPO) segments, that above CMC self assemble as micelles with hydrophobic PPO cores and hydrophilic PEO shell. These polymers have the ability to solubilize drugs for cellular internalization and have been used extensively to deliver various drugs25. Pluronic block copolymers interact with cholesterol subdomains within lipid rafts in cellular membranes and cause membrane fluidization26. We tested whether a set of block copolymers including L64, P84, P103 and F127 containing 30, 39.7, 59 and 65.2 number of respective PPO blocks would affect cholesterol efflux. We observed effects on cholesterol clearance with F127 at 1.5 mg/ml, which is an exceptionally high dose. The other polymers had showed toxicity at a high dose in Npc1−/− cells (Fig. S4).

Figure 6: PEG chain length in DSPE-PEG micelles affects cholesterol reduction in Npc1−/− cells.

(A) Npc1−/− MEFs were treated with DSPE-PEG micelles (10 μM) with increasing PEG chain length in the presence or absence of low dose HPβCD (0.1 mM). Cells were washed and stained for filipin. (A) Longer PEG chain lengths (>2,000 MW) show effective cholesterol reduction when treated with 10 μM. Micelle treatment with 0.1 mM HPBCD additionally reduces cholesterol when administered with DSPE-PEG micelles. (B) DLS was used to calculate average diameter of DSPE-PEG micelles, data is reported as distributed by number. Results were tested for statistical significance using one-way ANOVA with Tukey’s multiple comparison test. *P < 0.05, **P < 0.01, ***P < 0.001 and NS = not significant.

Autophagy, a catabolic process that directs cytosolic components towards the lysosomes for degradation, has been suggested to be dysregulated in lysosomal storage disorders27. It has been shown that Npc1−/− cells have a block in autophagic flux that leads to accumulation of toxic components within the cells28. We evaluated autophagic activity using Npc1−/− and Npc1+/+ MEFs that stably express a doxycycline-inducible firefly luciferase-p62 construct (p62-fluc). p62 acts as a marker for cellular cargo that is specifically degraded by autophagy. Therefore, higher luciferase expression corresponds to lower autophagic degradation. In Npc1+/+ MEFs there was a little if any retardation in the degradation of p62-fluc with increasing concentrations of DSPE-PEG without any significant effect on cell viability when treated for 24 hours and 48 hours (Fig. 7A,C). We then analyzed the effect on autophagy in Npc1−/− MEFs treated with DSPE-PEG. While, we did not observe a change in p62 degradation in 24 hours post treatment (Fig. 7B) a dose-dependent decrease in p62-fluc degradation was seen with DSPE-PEG treatment after 48 hours, without any substantial effect on cell viability (Fig. 7D). We treated Npc1−/− MEFs for 24 hours with a combination of 0.25 mM or 1 mM HPβCD and between 0.1 and 100 μM DSPE-PEG. We observed that the combinations at these doses did not substantially exacerbate autophagy (Fig. 7E,F). To further investigate the effect of DSPE-PEG and HPβCD treatment on the autophagic flux we used Npc1−/− and Npc1+/+ MEFs that stably express a tandem fluorescent-tagged LC3 reporter, TF LC3 (mRFP-EGFP-LC3). LC3 is a specific marker of autophagosomes since it is present on autophagosomal membrane from their formation until degradation in autolysosomes29. Coupling LC3 with mRFP and EGFP gives us the ability to distinguish between autophagosomes (mRFP+/EGFP+) and autolysosomes (mRFP+/EGFP) as EGFP is acid-labile and therefore its signal is quenched in autolysosomes. We noted an increased number of autophagosomes and decreased number of autolysosomes in the Npc1−/− MEFs compared to Npc1+/+ MEFs (Fig. 8A), suggestive of an impairment in autophagy in NPC1 disorder, as previously described28. A combination of 0.25 mM HPβCD and 10 μM DSPE-PEG, compared to 10 μM DSPE-PEG alone had no effect on the percentage of autophagosomes and autolysosomes (Fig. 8B). However, there was a decrease in the overall number of autophagosomes and autolysosomes (Fig. 8C) upon exposure of these admixtures, although this difference did not translate into defects of p62 clearance (Fig. 7), which suggests that this combination may have an effect on the dynamics of autophagic vesicles without exacerbating defects in autophagic cargo clearance. Overall, these studies indicate that low dose combination treatment with these molecules to enable cholesterol efflux, do not worsen the defects in autophagy prevalent in Npc1−/− cells.

Figure 7: DSPE-PEG treatment slightly reduces autophagic degradation in Npc1+/+ and Npc−/− MEFs

(A,C) p62-fluc.Npc1+/+ and, (B,D) p62-fluc. Npc−/− MEFs were induced to accumulate p62-fluc fusion protein with 1 μg/ml of Doxycycline for 24 hours. Doxycycline was washed from the cells and then they were treated with 0–100 μM DSPE-PEG2k for 24 (A and B upper panels) or 48 (C and D, upper panel) hours and autophagic degradation was measured using luciferase intensity. The cells were also analyzed for cell viability (lower panels). (E,F) Npc1−/− p62-fluc were also treated with a combination of HPβCD (0.25 mM or 1 mM, respectively) and DSPE-PEG (0–100 μM) for 24 hours after being induced for 24 hours with 1 μg/ml of Doxycycline. Results were tested for statistical significance using one-way ANOVA with Tukey’s multiple comparison test. *P < 0.05, **P < 0.01, ***P < 0.001 and NS = not significant.

Figure 8: The effect on autophagic flux by DSPE-PEG and HPβCD combination treatment.

TF.LC3.Npc1+/+ and TF.LC3.Npc1−/− MEFs were treated for 24 hours with 10 μM DSPE-PEG2k, 0.25 mM HPβCD or the combination of the two chemicals. Cells were then fixed, counterstained with DAPI and imaged at 100x magnification. (A) Representative images showing EGFP signal (far-left panel), mRFP signal (mid-left panel), merged EGFP and mRFP (mid-right panel) and colocalization of EGFP and mRFP (far-right panel). Scale bar = 20 μm. Images were quantified using ImageJ software. Quantification of microscope images showing the (B) number of autophagosomes and autolysosomes as a percentage or as (C) total number. Results were tested for statistical significance using two-tailed student’s t-test. *P < 0.05, **P < 0.01, ***P < 0.001 and NS = not significant.


PEG-conjugated lipids are used extensively in the field of drug delivery as excipients30. DSPE-PEGs are biocompatible, biodegradable and have been a component of several nanoparticle platforms for drug or nucleic acid delivery that are undergoing clinical trials30,31,32,33. The liposomal formulation Doxil contains DSPE-PEG as one of its constituents and has been clinically approved for use against ovarian cancer and AIDS related Kaposi sarcoma34. DSPE anchors PEG to the surface of these liposomes, which forms a protective hydrophilic coating that maintains stability of the nanoparticles. PEGylation of nanoparticles mitigates binding to serum proteins, which provides certain stealth effects, as nanoparticles evade recognition and opsonization by macrophages and prolongs circulation time17,35,36. Tuning PEG density at the surface of nanocarriers allows delivery across biological barriers, e.g. high PEG density assists in traversing mucosal barriers and can also enable widespread distribution in the CNS tissue once injected directly into the brain37,38. PEG-lipids are amphiphilic by nature and at low concentrations exist as single-coil unimers; above the CMC PEG-lipids form micelles with a core-shell morphology. The hydrophobic core can solubilize hydrophobic drugs, while the shell interacts with the aqueous serum environment39. The derivitization of PEG-lipids allows liposomal surface decoration of a repertoire of ligands for the purposes of tissue targeting. These conjugates have been even used to tether ligands on the surface of cells for ex vivo therapies40. DSPE-PEG micelles have been explored as carriers for diagnostic imaging agents, and have been safely injected into mice with a detected circulation concentration of greater than 1 mM, three orders of magnitude above the CMC41. These studies, to the best of our knowledge, for the first time reveal that DSPE-PEG can have the ability to preferentially accumulate inside the late endosomes of Npc1−/− cells and remove cholesterol from the endo/lysosomal system.

The NPC1 protein is a cholesterol efflux transporter that shunts cholesterol from the late endosomes to the endoplasmic reticulum42. Functional absence of NPC1 results in lipid accumulation in late endosomes/lysosomes. We observed cholesterol aggregates sequestered in the lumen of Rab7 positive late endosomes. Cholesterol aggregation results in cytotoxicity of neurons and hepatocytes due to their high sensitivity towards lipid accumulation5. Furthermore, the absence of NPC1 was shown to downregulate caveolae/lipid raft-mediated endocytosis while other entry pathways, such as macropinocytosis and clathrin-mediated endocytosis, remained intact43,44. Moreover, it was discovered that biodegradable nanoparticles that utilize caveolae/lipid-raft based micro-domains to enter cells fail to internalize and deliver DNA in Npc1−/− cells, while LNPs that enter cells using macropinocytosis show a high retention due to defects in their recycling in Npc1−/− cells that translate to effective siRNA delivery at very low doses21. Interestingly, this study shows similar retention of DSPE-PEG in late endosomes/lysosomes through a striking co-localization with filipin, which suggests that these nanocarriers possibly interact with cholesterol in the closed microenvironment of the late-endosomes and promote cholesterol solubilization. We speculate that within the DSPE-PEG construct, the DSPE serves to integrate into the cell membrane to enter cells and further interacts with the hydrophobic sterol aggregates promoting solubilization while the PEG chains interact with the hydrophilic glycocalyx that surrounds the lumen of the lysosomes45, enabling cholesterol efflux from these compartments. DSPE-PEG has been shown to stimulate cholesterol release from synthetic donor liposomes; perhaps such cholesterol release occurs in the multi-vesicular late endosome as well46. It is possible that the presence of DSPE-PEG triggers the formation of liposomal structures in situ that disassembles cholesterol/lipid aggregates, with the PEG chain lining the surface of the liposome to promote transfer across the lysosomal luminal membrane. PEGs exist in brush or mushroom conformations dependent on chain length, when assembled onto a nanocarrier surface47, and whether these conformations form within the confines of the endosomal microenvironment remains to be tested. It is also possible that among the different PEG-lipids, a particular size range may play an important role in targeting nanocarriers precisely to the endosomal compartment that requires cholesterol sequestration.

NPC is a devastating disease for which no treatment is available in the United States. There is a tremendous excitement among scientists for a solution for this disease as preclinical animal models and patients respond positively to HPβCD treatment. Yet, the relatively high dose required to achieve therapeutic response has been associated with hearing loss that occurs due to interaction of HPβCD with prestin, a protein located on outer-hair cells of the cochlea48. To overcome these issues of efficacy, new polymers such as Pluronic/β-cyclodextrin polyrotaxanes have been synthesized to release multiple cyclodextrin molecules in the reducing endosomal environment49,50,51. Unfortunately these new compounds will require extensive preclinical and clinical testing prior to translational development. HPβCD, at high doses, exacerbates autophagy defects; on the other hand, repeated administration of PEG has been associated with complement activation28,52 and perhaps by combining DSPE-PEG and HPβCD a synergistic response at low doses can promote cholesterol egress without causing toxicity. It has been observed in Npc1−/− cats that a 120 mg of intra-cisternal dose of HPβCD increased survival from 22 weeks to 76 weeks to 4 years12, and it is therefore, tempting to speculate that injecting admixtures of cyclodextrin with DSPE-PEG, directly into the brain will lower the dose necessary for survival and decrease the substantial side effects of HPβCD, otherwise observed in clinical and preclinical models of NPC disorder.

Liposomes with increasing amounts of PEG-lipids were developed for encapsulation and co-delivery of HPβCD, and we observed that the liposomal size decreased from roughly 100 nm to 10–20 nm as the PEG-lipid molar ratio increased. Nanoparticles transition from an aqueous core encapsulated in a lipid bilayer to a micelle with a hydrophobic core with increasing molar ratios of DSPE-PEG, thus decreasing the encapsulation efficiency of the hydrophilic drug. We observed that when treatments were normalized for HPβCD concentrations and constant lipid concentrations, the nanocarriers with higher DSPE-PEG content resulted in substantial cholesterol clearance, and DSPE-PEG micelles were the most potent. PEG-lipid micelles or liposomes with high amounts of DSPE-PEG might serve as bioactive drug delivery agents for treatment of NPC. We were further able to test whether other polymers have the ability to egress cholesterol. We tested a set of Pluronic block copolymers that have the capability to self-assemble as micelles. Pluronic micelles utilize clathrin-mediated endocytosis to access endo/lysosomes and modulate cholesterol fluidity to inhibit drug efflux transport, activate gene expression, and induce dose-dependent hyperlipidemia25,53. Among the materials tested, Pluronic F127 showed an effect at very high concentrations, suggesting that some of these surfactants might cause non-specific cholesterol clearance.

There are several new strategies for potential therapeutics against NPC disease that may require nanocarrier based drug delivery systems. Vironosotat, a histone deacetylase inhibitor (HDACi) has been shown to clear cholesterol in human patient fibroblasts carrying the NPC1I1061T mutation54,55. HDACi inhibitors enhance transcriptional activity; overexpression partially compensated for the NPC1I1061T mutation and acts as a chaperone to untangle mis-folded protein. HPβCD has recently been used to solubilize the hydrophobic vironosat, and when administered subcutaneously to NPC1I1061T mutant mice, substantially improved life span56. However, this formulation consists of high amounts of cyclodextrin and 5% DMSO, a toxic organic solvent that could limit clinical applicability56. Carbamazepine an autophagy inducer used to overcome the autophagy blockade57 and remove toxic cytosolic debris, will be an important ingredient in the formulation for treatment of NPC28. PEG-lipid micelles can entrap hydrophobic drugs, such as vironostat or carbamazepine in the core, and when formulated with cyclodextrin could result in a potent drug combination against NPC. As new variants of cyclodextrin that have different degree of substitutions are identified for improved efficacy and reduced ototoxicity in NPC disease, these agents can be replaced in the aforementioned drug cocktail58. Additionally genetic editing and gene delivery approaches have been used to correct mutated genes, including Npc1, which offers a precise treatment and potential cure for rare genetic disorders and can benefit from non-viral delivery technologies19,59. Finally, traversing the blood brain barrier is required for successful translation of this technology, and we anticipate modification of these nanocarriers with multivalent targeting ligands for brain delivery60. Potentially attaching new brain shuttle technologies that have shown to enhance brain penetration in different animal models, including non-human primates, or temporary opening of the blood- brain barrier will enable brain targeting61,62. This information serves as a blueprint to further develop PEG-lipid based bioactive nanocarriers with brain targeting capability that can exploit trafficking defects to site-specifically deliver drugs or their combinations for effective treatment of NPC. Taken together, nanocarriers can serve as a platform that can effectively deliver small molecules, genes and perhaps imaging agents for treatment and diagnosis of a wide variety of other rare lysosomal storage disorders.

Materials and Methods

Assembly of Liposomes or Micelles

Liposomes were formed using the thin film rehydration method. Briefly HSPC (Avanti Polar Lipids), DSPE-PEG2k (NOF America) or a combination, were dissolved in ethanol at 20 mM. To make thin films, 2 μMol of lipid was dried in 20 mL glass scintillation vial (approximately 1 in2) under vacuum and rehydrated by sonication for 20 mins at 40 °C in a bath sonicator. Liposomes were formed in 200 μL of 400 mM HPβCD (ACROS Organics) in PBS. Clean DSPE-PEG2k micelles were assembled in 200 μL Opti-MEM and cooled on ice until further use. Liposomes were washed twice in PBS to remove unencapsulated HPβCD using a centrifugal filter concentrator (Amicon Ultra−15 10 k MWCO) for 10 minutes at 17 k × G. Assembled micelles (without HPβCD) were diluted as necessary to be used in cell treatment studies. Additional lipid micelles, including DSPE, DSPE-PEG350, DSPE-PEG1k, DSPE-PEG5k or DSPE-PEG2k-CF (Avanti-Polar lipids) and DSPE-PEG10k, DSPE-PEG20k, DSPE-PEG30k, (Creative PEGWorks) were formed from lipid stocks stored in chloroform. Thin films (100 nmoles lipid) were formed as described above and hydrated in 100 μL Opti MEM to make 1 mM stock solutions. For PEG2k a 10 μM solution was made from powder rehydrated in Opti MEM, and diluted to desired concentrations. Pluronics P84 (Sigma Aldrich), L64, F127 and P103 (BASF SE) were diluted from stock solutions (150 mg/mL) in Opti MEM for cell treatments as described above.

Materials Analysis

Liposomes or micelles were confirmed using dynamic light scattering (Malvern Zetasizer) in PBS and average size is reported based on a number distribution. Transmission Electron Microscopy (TEM) was performed on an FEI Tecnai F-20 TEM operating at 200 kV. Samples of liposomes or micelles were prepared by drop casting onto a carbon coated copper grid (Ted Pella), and allowed to air dry. HPβCD was measured using an adapted LC-ESI-MS/MS method63. Briefly, washed liposomes were digested in methanol and subjected to high-performance liquid chromatography (HPLC)-tandem mass spectrometry using a 75 × 2 mm C18 3 μm particle LC column (Phenomenex Torrance, CA) coupled to a SCIEX 4000 QTRAP LC/MS/MS equipped with a electrospray ionization (ESI) source operating in the positive mode. The HPLC column temperature was kept at 40 °C. Analyte and internal standard (methyl-β-cyclodextrin) were resolved using a gradient method with solvents A (methanol at 0.1% formic acid) and B (100 mM ammonium formate) at a flow rate of 0.5 ml/min changed as follows: 5% to 95% B over 1 minute, held at 95% B for 1.5 minutes and equilibrated at 5% B for 2.5 minutes. The ESI ion source parameters were as follows: 48 V collision energy, 30 units curtain gas, 5000 V ion spray, 450 C temperature, 40 units gas 1 and 50.00 gas 2. Multiple reaction monitoring mass transitions scanned for 100 msec were m/z 1307 → 367.4 for methyl-β-cyclodextrin, and m/z 1385 → 383.4 and 1443 → 383.4 for HPβCD. HPβCD and internal standard had a retention time of approximately 1.7 minutes. Calibration curves for quantification were created using HPβCD standard across the concentration range 0.05–500 μg/ml with methyl-β-cyclodextrin at 25 μg/mL. The area ratio of analyte to internal standard was plotted against the nominal concentration for calibrators and a quadratic regression analysis was used to calculate the concentration in unknown samples.


Npc1−/− and Npc1+/+ immortalized mouse embryonic fibroblasts (MEFs) (kind gifts from the Langer Lab at MIT) were cultured in DMEM/10% FBS at 37 °C. Cells were plated into a 96 well plate (4 k cell/well with 100 μL media) and allowed to settle for 24 hours. Intracellular staining of cholesterol in these cells was performed using filipin staining of paraformaldehyde fixed cells. Cells were washed in PBS and 2 mM Glycine in PBS for 10 minutes, prior to staining with 0.05 mg/mL, filipin complex (Sigma Aldrich) in 10% FBS for 2 hours. Cells were then washed in PBS three times and stored in 100 μL PBS with 1x HCS NuclearMask Deep Red Stain (Life Technologies) at 4 °C for further analysis. Npc1−/− cells were treated with drug (HPβCD), PEG-lipid or a combination of drug with PEG-lipid, dissolved in Opti-MEM (Thermo Fisher). After a 24-hour incubation, media was removed, cells were washed in PBS and fixed in 4% paraformaldehyde at room temperature for 20 minutes, followed by filipin staining. Reduction of filipin staining from the lysosomal stores of Npc1−/− cells is referred as cholesterol efflux. For Rab7-GFP (marker of late endosomes) experiments, Npc1+/+ or Npc1−/− cells were each transfected with Rab7-GFP using a baculovirus (Bacmam 2.0) for 18 hours, fixed and filipin stained as described, and imaged. For uptake and localizationstudies,1,2-distearoyl-sn-glycero-3-phosphoethanolamine-N-[poly(ethylene glycol)-2000-N′-carboxyfluorescein] (Avanti Polar Lipids) (DSPE-PEG-CF) were assembled into micelles (described below) and incubated with cells for specified time points prior to fixing and filipin staining. High throughput imaging was performed using either an automated high-throughput fluorescence microscope (Olympus scanR) at 20X with at least 16 images/well were analyzed using the Olympus scanR analysis software. In select cases, EVOS FL Auto Cell imaging system (Invitrogen) 20X or 40X was utilized. All experiments were performed in triplicates and errors are reported as S.E.M.

Total cellular cholesterol from cell lysates

Amplex Red cholesterol assay (Amplex Red Cholesterol Assay Kit, ThermoFisher) was performed according to manufacturers instructions and used to quantify total cellular cholesterol from cell lysates, which was normalized to total protein content using the Bradford Assay. Briefly, after drug treatments, cells were washed with PBS and lysed with Cholesterol Mammalian Protein Extraction Reagent (ThermoFisher Cat # 78501). The cells were frozen for 10 mins at −80 °C and plates were thawed for 30 mins at 37 °C. The cell lysates were treated with Amplex red reagent (prepared using Manufacturers protocol) in presence of Halt Protease inhibitor (Halt™ Protease and Phosphatase Inhibitor Cocktail, EDTA-free (100X), ThermoFisher Cat # 78445). Cell lysates were incubates at room temperature for 1 hr and fluorescence (Ex/Em = 540/590) was measured using Tecan Microplate reader (Tecan). The cell lysates were treated with Bradford reagent (Pierce™ Coomassie (Bradford) Protein Assay Kit, (ThermoFisher) and their absorbance (595 nm) was measured. Standard curves were plotted using known concentrations of Cholesterol (Amplex Red assay) and Bovine Serum Albumin (Bradford) to interpolate cell lysates based data. All experiments were performed in triplicates and errors are reported as S.E.M.

Cloning and generation of stable cell lines

p62-Lucifearse expressing Npc1 stable cell lines

Npc1+/+ and Npc1−/− MEFs were transduced with a doxycycline inducible p62-firefly luciferase (p62-fluc) construct that also had a puromycin resistance gene were maintained in 1 μg/ml puromycin (Sigma-Aldrich P8833). Briefly, the doxycycline inducible pCW57.1 backbone was purchased from Addgene (41393). Gibson assembly was used to insert firefly luciferase (Fluc) and p62 into the pCW57.1 backbone. Fluc, p62 and pCW57.1 were PCR amplified using pfu polymerase (Life technologies) and Gibson assembly primers with 20 bp overhangs. PCR products were separated by agarose gel electrophoreses, and fragments excised and purified before use in DNA assembly reaction with the NEBuilder HiFi DNA Assembly kit (New England Biolabs) according to the manufacturer’s instructions. After the assembly, the reaction mix was transformed into NEB3040 NEB Stable Competent E. coli (New England Biolabs). After 24 h growth at 31 °C the plasmid was extracted using QIAprep Spin Miniprep Kit (Qiagen). The plasmid was sequenced to confirm correct insertion of Fluc-p62. To generate Npc1+/+ and Npc1−/− MEFs stably expressing doxycline inducible Fluc-p62, HEK293FT cells were transfected with Fluc-p62-pCW57.1 and the ViraPower Packaging Mix (Invitrogen) to produce lentivirus. Npc1+/+ and Npc1−/− MEFs were transduced with the obtained lentiviral stock followed by selection with 1 μg/ml puromycin.


Tandem Fluorescent LC3 expressing Npc1 stable cell lines

Npc1+/+ and Npc−/− MEFs were transduced with a tandem-fluorescent LC3 reporter (TF-LC3 (mRFP-EGFP-LC3)) which also contained a puromycin resistance gene. MEFs were selected with 1 μg/ml of puromycin. After 1 week of selection the cells were plated as single cells in a 96 well plate to generate monoclonal TF-LC3 lines. pLenti-Synapsin-hChR2(H134R)-EYFP-WPRE (purchased from Addgene (20945)) was digested with PacI and EcoRI enzymes. TF-LC3 and IRES-PURO were amplified using PCR with Q5 HighFidelity DNA Polymerase (NEB) using Gibson Assembly primers, which contained 15bp overhangs. Purified amplicons were mixed and assembled using Gibson Assembly Master Mix (NEB). The assembled DNA was transformed into NEB® 5-alpha Competent E. coli (NEB). DNA was amplified in E. coli and sequenced to check for correct insertion of the TF-LC3 and the puromycin resistance gene. Then plasmid DNA was transfected into 293T cells with lentiviral packaging plasmids (tat, rev, gag/pol and vsv-g). Lentiviral particles were collected after 24 hours and used to transduce Npc1+/+ and Npc−/− MEFs.


Luciferase Assay

First, the p62-fluc.Npc1+/+ and p62-fluc.Npc1−/− MEFs were plated into white 96 well plates (2 k cell/well with 100 μL media) and allowed to settle for 24 hours. Next, the MEFs were treated with 1 μg/ml doxycycline (Sigma-Aldrich 33429) for 24 hours before being washed off 3 times with PBS. Subsequently, the specified drug or a combination of drugs was dissolved in Opti-MEM (Thermo Fisher) and all of media was removed from cells and replaced with DSPE-PEG2k containing media and incubated for 24 hours. MEFs to be treated for 48 hours with the micelles were aspirated after 24 hours and fresh DSPE-PEG2k media was added for the final 24 hours. After 24 hours or 48 hours of drug treatment, MEFs were analyzed using ONE-Glo™ + Tox Luciferase Reporter and Cell Viability Assay (Promega) by following the manufacturer’s protocol.

TF.LC3 analysis

Analysis of autophagosome maturation using mRFP-EGFP-LC3 (TF-LC3) reporter was performed in the following way. TF-LC3.Npc1+/+ and TF-LC3.Npc−/− MEFs were plated onto 9 mm glass coverslips coated with 0.2% gelatin (Sigma) at a density of 25000 per coverslip. The following day the cells were treated with for 24 hours with 10 μM DSPE-PEG2k, 0.25 mM HPβCD or the combination of the two chemicals. After 24 hours the cells were washed with PBS and then fixed with 4% methanol free-paraformaldehyde (Thermo Fisher) for 15 minutes at room temperature. The formaldehyde was washed off twice with PBS and then the cells were quenched with 100 mM glycine (Sigma) for 10 minutes. Next, the cells were permeabilized with 0.5% Triton X-100 (Sigma) for 10 minutes. Subsequently, cells were washed twice with PBS and then counter stained with 1x DAPI for 5 minutes at room temperature. The DAPI was washed off twice with PBS and then the coverslips were mounted onto Prolong Diamond Anti-fade reagent (Life Technologies). Mounted slides were cured overnight and then imaged on a Carl Zeiss LSM 780 confocal microscope at 100x magnification. Images were processed using ImageJ software.

Additional Information

How to cite this article: Brown, A. et al. PEG-lipid micelles enable cholesterol efflux in Niemann-Pick Type C1 disease-based lysosomal storage disorder. Sci. Rep. 6, 31750; doi: 10.1038/srep31750 (2016).


  1. 1

    Carstea, E. D. et al. Niemann-Pick C1 Disease Gene: Homology to Mediators of Cholesterol Homeostasis. Science 277, 228–231 (1997).

    CAS  Article  Google Scholar 

  2. 2

    Vanier, M. T. Niemann-Pick disease type C. Orphanet J. Rare Dis. 5, 16 (2010).

    Article  Google Scholar 

  3. 3

    Ikonen, E. Cellular cholesterol trafficking and compartmentalization. Nat. Rev. Mol. Cell Biol. 9, 125–138 (2008).

    CAS  Article  Google Scholar 

  4. 4

    Ottinger, E. A. et al. Collaborative development of 2-hydroxypropyl-β-cyclodextrin for the treatment of Niemann-Pick type C1 disease. Curr. Top. Med. Chem. 14, 330–339 (2014).

    CAS  Article  Google Scholar 

  5. 5

    Walkley, S. U. & Suzuki, K. Consequences of NPC1 and NPC2 loss of function in mammalian neurons. Biochim. Biophys. Acta 1685, 48–62 (2004).

    CAS  Article  Google Scholar 

  6. 6

    Szente, L. & Szejtli, J. Highly soluble cyclodextrin derivatives: chemistry, properties, and trends in development. Adv. Drug Deliv. Rev. 36, 17–28 (1999).

    CAS  Article  Google Scholar 

  7. 7

    Kilsdonk, E. P. C. et al. Cellular Cholesterol Efflux Mediated by Cyclodextrins. J. Biol. Chem. 270, 17250–17256 (1995).

    CAS  Article  Google Scholar 

  8. 8

    Peake, K. B. & Vance, J. E. Normalization of Cholesterol Homeostasis by 2-Hydroxypropyl-β-cyclodextrin in Neurons and Glia from Niemann-Pick C1 (NPC1)-deficient Mice. J. Biol. Chem. 287, 9290–9298 (2012).

    CAS  Article  Google Scholar 

  9. 9

    Davidson, C. D. et al. Chronic Cyclodextrin Treatment of Murine Niemann-Pick C Disease Ameliorates Neuronal Cholesterol and Glycosphingolipid Storage and Disease Progression. PLoS One 4 (2009).

  10. 10

    Camargo, F. et al. Cyclodextrins in the treatment of a mouse model of Niemann-Pick C disease. Life Sci. 70, 131–142 (2001).

    CAS  Article  Google Scholar 

  11. 11

    Ramirez, C. M. et al. Weekly Cyclodextrin Administration Normalizes Cholesterol Metabolism in Nearly Every Organ of the Niemann-Pick Type C1 Mouse and Markedly Prolongs Life. Pediatr. Res. 68, 309–315 (2010).

    CAS  Article  Google Scholar 

  12. 12

    Vite, C. H. et al. Intracisternal cyclodextrin prevents cerebellar dysfunction and Purkinje cell death in feline Niemann-Pick type C1 disease. Sci. Transl. Med. 7, 276ra26 (2015).

    CAS  Article  Google Scholar 

  13. 13

    Maarup, T. J. et al. Intrathecal 2-hydroxypropyl-beta-cyclodextrin in a single patient with Niemann-Pick C1. Mol. Genet. Metab. 116, 75–79 (2015).

    CAS  Article  Google Scholar 

  14. 14

    Torchilin, V. P. Recent advances with liposomes as pharmaceutical carriers. Nat. Rev. Drug Discov. 4, 145–160 (2005).

    CAS  Article  Google Scholar 

  15. 15

    Szoka, F. & Papahadjopoulos, D. Procedure for preparation of liposomes with large internal aqueous space and high capture by reverse-phase evaporation. Proc. Natl. Acad. Sci. USA. 75, 4194–4198 (1978).

    CAS  ADS  Article  Google Scholar 

  16. 16

    Allen, T. M. & Cullis, P. R. Liposomal drug delivery systems: from concept to clinical applications. Adv. Drug Deliv. Rev. 65, 36–48 (2013).

    CAS  Article  Google Scholar 

  17. 17

    Klibanov, A. L., Maruyama, K., Torchilin, V. P. & Huang, L. Amphipathic polyethyleneglycols effectively prolong the circulation time of liposomes. FEBS Lett. 268, 235–237 (1990).

    CAS  Article  Google Scholar 

  18. 18

    Pardridge, W. M. Blood-brain barrier drug targeting: the future of brain drug development. Mol. Interv. 3, 90–105 (2003).

    CAS  Article  Google Scholar 

  19. 19

    Yin, H. et al. Non-viral vectors for gene-based therapy. Nat. Rev. Genet. 15, 541–555 (2014).

    CAS  Article  Google Scholar 

  20. 20

    Guo, X. & Huang, L. Recent advances in nonviral vectors for gene delivery. Acc. Chem. Res. 45, 971–979 (2012).

    CAS  Article  Google Scholar 

  21. 21

    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 

  22. 22

    Vanier, M. T. & Latour, P. Laboratory diagnosis of Niemann-Pick disease type C: the filipin staining test. Methods Cell Biol. 126, 357–375 (2015).

    Article  Google Scholar 

  23. 23

    Rujoi, M., Pipalia, N. H. & Maxfield, F. R. Cholesterol Pathways Affected by Small Molecules That Decrease Sterol Levels in Niemann-Pick Type C Mutant Cells. PLOS ONE 5, e12788 (2010).

    ADS  Article  Google Scholar 

  24. 24

    Tanaka, Y. et al. Influence of Npc1 genotype on the toxicity of hydroxypropyl-β-cyclodextrin, a potentially therapeutic agent, in Niemann–Pick Type C disease models. Mol. Genet. Metab. Rep. 1, 19–30 (2014).

    CAS  Article  Google Scholar 

  25. 25

    Kabanov, A. V., Batrakova, E. V. & Alakhov, V. Y. Pluronic® block copolymers as novel polymer therapeutics for drug and gene delivery. J. Controlled Release 82, 189–212 (2002).

    CAS  Article  Google Scholar 

  26. 26

    Batrakova, E. V. & Kabanov, A. V. Pluronic block copolymers: evolution of drug delivery concept from inert nanocarriers to biological response modifiers. J. Control. Release Off. J. Control. Release Soc. 130, 98–106 (2008).

    CAS  Article  Google Scholar 

  27. 27

    Lieberman, A. P. et al. Autophagy in lysosomal storage disorders. Autophagy 8, 719–730 (2012).

    CAS  Article  Google Scholar 

  28. 28

    Sarkar, S. et al. Impaired autophagy in the lipid-storage disorder Niemann-Pick type C1 disease. Cell Rep. 5, 1302–1315 (2013).

    CAS  Article  Google Scholar 

  29. 29

    Kimura, S., Noda, T. & Yoshimori, T. Dissection of the autophagosome maturation process by a novel reporter protein, tandem fluorescent-tagged LC3. Autophagy 3, 452–460 (2007).

    CAS  Article  Google Scholar 

  30. 30

    Che, J., Okeke, C. I., Hu, Z.-B. & Xu, J. DSPE-PEG: a distinctive component in drug delivery system. Curr. Pharm. Des. 21, 1598–1605 (2015).

    CAS  Article  Google Scholar 

  31. 31

    MacLachlan, I. & Cullis, P. Diffusible-PEG-lipid stabilized plasmid lipid particles. Adv. Genet. 53, 157–188 (2005).

    CAS  Article  Google Scholar 

  32. 32

    Dong, Y. et al. Lipopeptide nanoparticles for potent and selective siRNA delivery in rodents and nonhuman primates. Proc. Natl. Acad. Sci. USA. 111, 3955–3960 (2014).

    CAS  ADS  Article  Google Scholar 

  33. 33

    Kauffman, K. J., Webber, M. J. & Anderson, D. G. Materials for non-viral intracellular delivery of messenger RNA therapeutics. J. Control. Release Off. J. Control. Release Soc. doi: 10.1016/j.jconrel.2015.12.032 (2015).

  34. 34

    Gabizon, A. et al. Prolonged circulation time and enhanced accumulation in malignant exudates of doxorubicin encapsulated in polyethylene-glycol coated liposomes. Cancer Res. 54, 987–992 (1994).

    CAS  PubMed  Google Scholar 

  35. 35

    Immordino, M. L., Dosio, F. & Cattel, L. Stealth liposomes: review of the basic science, rationale, and clinical applications, existing and potential. Int. J. Nanomedicine 1, 297–315 (2006).

    CAS  Article  Google Scholar 

  36. 36

    Gref, R. et al. Biodegradable long-circulating polymeric nanospheres. Science 263, 1600–1603 (1994).

    CAS  ADS  Article  Google Scholar 

  37. 37

    Suk, J. S., Xu, Q., Kim, N., Hanes, J. & Ensign, L. M. PEGylation as a strategy for improving nanoparticle-based drug and gene delivery. Adv. Drug Deliv. Rev. 99, 28–51 (2016).

    CAS  Article  Google Scholar 

  38. 38

    Nance, E. A. et al. A dense poly(ethylene glycol) coating improves penetration of large polymeric nanoparticles within brain tissue. Sci. Transl. Med. 4, 149ra119 (2012).

    Article  Google Scholar 

  39. 39

    Gill, K. K., Kaddoumi, A. & Nazzal, S. PEG-lipid micelles as drug carriers: physiochemical attributes, formulation principles and biological implication. J. Drug Target. 23, 222–231 (2015).

    CAS  Article  Google Scholar 

  40. 40

    Takafuji, Y. et al. Factors influencing the surface modification of mesenchymal stem cells with fluorescein-pegylated lipids. Biol. Pharm. Bull. 36, 1731–1738 (2013).

    CAS  Article  Google Scholar 

  41. 41

    Beilvert, A. et al. A tyrosine PEG-micelle magnetic resonance contrast agent for the detection of lipid rich areas in atherosclerotic plaque. Magn. Reson. Med. Off. J. Soc. Magn. Reson. Med. Soc. Magn. Reson. Med. 62, 1195–1201 (2009).

    CAS  Article  Google Scholar 

  42. 42

    Pfisterer, S. G., Peränen, J. & Ikonen, E. LDL-cholesterol transport to the endoplasmic reticulum: current concepts. Curr. Opin. Lipidol. 27, 282–287 (2016).

    CAS  Article  Google Scholar 

  43. 43

    Rappaport, J., Manthe, R. L., Solomon, M., Garnacho, C. & Muro, S. A Comparative Study on the Alterations of Endocytic Pathways in Multiple Lysosomal Storage Disorders. Mol. Pharm. doi: 10.1021/acs.molpharmaceut.5b00542 (2016).

  44. 44

    Eltoukhy, A. A., Sahay, G., Cunningham, J. M. & Anderson, D. G. Niemann-Pick C1 affects the gene delivery efficacy of degradable polymeric nanoparticles. ACS Nano 8, 7905–7913 (2014).

    CAS  Article  Google Scholar 

  45. 45

    Li, J., Deffieu, M. S., Lee, P. L., Saha, P. & Pfeffer, S. R. Glycosylation inhibition reduces cholesterol accumulation in NPC1 protein-deficient cells. Proc. Natl. Acad. Sci. USA. 112, 14876–14881 (2015).

    CAS  ADS  Article  Google Scholar 

  46. 46

    Janout, V., Daly, T. A., Cline, L. L., Kulp, L. J. & Regen, S. L. Stimulated release of cholesterol from liposomal membranes by a PEGylated phospholipid. Bioconjug. Chem. 23, 336–339 (2012).

    CAS  Article  Google Scholar 

  47. 47

    Perry, J. L. et al. PEGylated PRINT Nanoparticles: The Impact of PEG Density on Protein Binding, Macrophage Association, Biodistribution, and Pharmacokinetics. Nano Lett. 12, 5304–5310 (2012).

    CAS  ADS  Article  Google Scholar 

  48. 48

    Takahashi, S. et al. Susceptibility of outer hair cells to cholesterol chelator 2-hydroxypropyl-β-cyclodextrine is prestin-dependent. Sci. Rep. 6, 21973 (2016).

    CAS  ADS  Article  Google Scholar 

  49. 49

    Mondjinou, Y. A. et al. Synthesis of 2-hydroxypropyl-β-cyclodextrin/pluronic-based polyrotaxanes via heterogeneous reaction as potential Niemann-Pick type C therapeutics. Biomacromolecules 14, 4189–4197 (2013).

    CAS  Article  Google Scholar 

  50. 50

    Tamura, A. & Yui, N. Lysosomal-specific cholesterol reduction by biocleavable polyrotaxanes for ameliorating Niemann-Pick type C disease. Sci. Rep. 4, 4356 (2014).

    ADS  Article  Google Scholar 

  51. 51

    Tamura, A. & Yui, N. β-Cyclodextrin-threaded biocleavable polyrotaxanes ameliorate impaired autophagic flux in Niemann-Pick type C disease. J. Biol. Chem. 290, 9442–9454 (2015).

    CAS  Article  Google Scholar 

  52. 52

    Chanan-Khan, A. et al. Complement activation following first exposure to pegylated liposomal doxorubicin (Doxil®): possible role in hypersensitivity reactions. Ann. Oncol. 14, 1430–1437 (2003).

    CAS  Article  Google Scholar 

  53. 53

    Batrakova, E. V. & Kabanov, A. V. Pluronic block copolymers: evolution of drug delivery concept from inert nanocarriers to biological response modifiers. J. Control. Release Off. J. Control. Release Soc. 130, 98–106 (2008).

    CAS  Article  Google Scholar 

  54. 54

    Pipalia, N. H. et al. Histone deacetylase inhibitor treatment dramatically reduces cholesterol accumulation in Niemann-Pick type C1 mutant human fibroblasts. Proc. Natl. Acad. Sci. USA. 108, 5620–5625 (2011).

    CAS  ADS  Article  Google Scholar 

  55. 55

    Helquist, P., Maxfield, F. R., Wiech, N. L. & Wiest, O. Treatment of Niemann–Pick Type C Disease by Histone Deacetylase Inhibitors. Neurotherapeutics 10, 688–697 (2013).

    CAS  Article  Google Scholar 

  56. 56

    Alam, M. S., Getz, M. & Haldar, K. Chronic administration of an HDAC inhibitor treats both neurological and systemic Niemann-Pick type C disease in a mouse model. Sci. Transl. Med. 8, 326ra23 (2016).

    Article  Google Scholar 

  57. 57

    Sarkar, S., Maetzel, D., Korolchuk, V. I. & Jaenisch, R. Restarting stalled autophagy a potential therapeutic approach for the lipid storage disorder, Niemann-Pick type C1 disease. Autophagy 10, 1137–1140 (2014).

    CAS  Article  Google Scholar 

  58. 58

    Davidson, C. D. et al. Efficacy and ototoxicity of different cyclodextrins in Niemann-Pick C disease. Ann. Clin. Transl. Neurol. 3, 366–380 (2016).

    CAS  Article  Google Scholar 

  59. 59

    Maetzel, D. et al. Genetic and Chemical Correction of Cholesterol Accumulation and Impaired Autophagy in Hepatic and Neural Cells Derived from Niemann-Pick Type C Patient-Specific iPS Cells. Stem Cell Rep. 2, 866–880 (2014).

    CAS  Article  Google Scholar 

  60. 60

    Wiley, D. T., Webster, P., Gale, A. & Davis, M. E. Transcytosis and brain uptake of transferrin-containing nanoparticles by tuning avidity to transferrin receptor. Proc. Natl. Acad. Sci. USA. 110, 8662–8667 (2013).

    CAS  ADS  Article  Google Scholar 

  61. 61

    Yu, Y. J. et al. Therapeutic bispecific antibodies cross the blood-brain barrier in nonhuman primates. Sci. Transl. Med. 6, 261ra154–261ra154 (2014).

    Article  Google Scholar 

  62. 62

    Kroll, R. A. & Neuwelt, E. A. Outwitting the Blood-Brain Barrier for Therapeutic Purposes: Osmotic Opening and Other Means: Neurosurgery 42, 1083–1099 (1998).

  63. 63

    Jiang, H. et al. Development and validation of sensitive LC-MS/MS assays for quantification of HP-β-CD in human plasma and CSF. J. Lipid Res. 55, 1537–1548 (2014).

    CAS  Article  Google Scholar 

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This project was supported through OSU College of Pharmacy startup funding (G.S. and C.S.), OSU Venture Development Funds (G.S.). AACP New Investigator Award (G.S.), Birmingham Fellowship (S.S.) and Wellcome Trust Seed Award (S.S.). S.S. is also a Former Fellow at Hughes Hall, University of Cambridge, UK. We will like to thank Kelsey Kubiak for technical assistance and Dr. Andrea Debarber at OHSU for her assistance with the LC/MS/MS analysis and Dr. Adam Alani for access to Malvern Zetasizer, and the Portland State University Center for Electron Microscopy and Nanofabrication for access to electron microscopes. We thank Dr. Peter Lobel for providing Npc1 MEFs, Dr. T. Yoshimori and Addgene for mRFP-GFP-LC3 construct. G.S. will like to thank College of Pharmacy for Dean’s funding for collaborative research with Oregon Translation Research And Development Institute (OTRADI). G.S., C.S. and L.H. thank the Murdock foundation for supporting the high throughput screening facility at Collaborative Life Science Building at OHSU.

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G.S. conceived the idea. A.B. performed all experiments except autophagy based assays and reported the data with S.P., A.L., A.D. A.E., L.H., A.B. and F.W. conducted high-throughput screens. S.S., V.K., C.W., M.O. and E.G.O. generated Npc1+/+ and Npc1−/− cells with p62-Luc and TF-LC3 and conducted autophagy assays with DSPE-PEG2k and cyclodextrin provided by the Sahay Lab (A.B.). G.S. and C.S. directed research on the cholesterol assays. G.S. and S.S. directed research on the autophagy based assay. G.S, S.S., C.W. and A.B. analyzed results. All authors provided feedback on the research. G.S. managed the overall project and wrote the paper.

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Correspondence to Gaurav Sahay.

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Competing interests

G.S., A.B. and C.S. have filed invention disclosure under OSU disc. no. 15–43 for nanoparticle based formulations for NPC disorder. Remaining authors declare no other competing financial interests.

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Brown, A., Patel, S., Ward, C. et al. PEG-lipid micelles enable cholesterol efflux in Niemann-Pick Type C1 disease-based lysosomal storage disorder. Sci Rep 6, 31750 (2016).

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