Multifunctional, lipopolyplex formulations comprising a mixture of cationic liposomes and cationic, receptor-targeting peptides have potential use in gene therapy applications. Lipopolyplex formulations described here are typically far more efficient transfection agents than binary lipoplex or polyplex formulations. It has been shown previously that the peptide component mediates both DNA packaging and targeting of the nanoparticle while in this report we investigate the contribution of the lipid component. We hypothesised that the lipid components synergise with the peptides in the transfection process by promoting endosomal escape after lipid bilayer fusion. Lipopolyplexes were prepared with cationic liposomes comprising DOTAP with either neutral lipid DOPE or DOPC. DOPE promotes fusogenic, inverted hexagonal lipid structures while DOPC promotes more stable laminar structures. Lipopolyplexes containing DOPE showed substantially higher transfection efficiency than those formulated with DOPC, both in vitro and in vivo. DOPE-containing lipopolyplexes showed rapid endosomal trafficking and nuclear accumulation of DNA while DOPC-containing formulations remained within the late endo-lysosomal compartments. These findings are consistent with previous finding for the role of DOPE in lipoplexes and support the hypothesis regarding the function of the lipid components in lipopolyplexes. These findings will help to inform future lipopolyplex design, strategies and clinical development processes.
Synthetic, non-viral vectors offer advantages over viral vectors for in vivo gene therapy in that they are less immunogenic, have fewer packaging constraints and are safer1,2. Cationic lipoplexes and polyplexes predominate in the non-viral vector field but increasingly lipopolyplex formulations, which are combinations of lipids with peptides or polymers, are being explored as appreciation develops of their wider range of functionalities and higher transfection efficiencies3,4,5,6,7,8,9,10,11. Further detailed functional and structural studies are required to understand the properties of lipopolyplexes, how to formulate components and to develop improved formulations.
We are developing a lipopolyplex formulation termed a Receptor Targeted Nanocomplex (RTN), which is a mixture of cationic, receptor-targeting peptides and cationic liposomes with plasmid DNA (pDNA)12,13,14,15,16,17. The lipid and peptide components of RTNs feature modular design elements that enable their functionality to be dissected at the molecular level13. We have shown previously that the peptide mediates DNA packaging and receptor targeting and so the focus of this study was to investigate the function of the lipids and how they contribute to the transfection efficiency of RTN lipopolyplexes. Endosomolysis is a major obstacle to transfection with peptide-DNA formulations and so we hypothesised that addition of the liposome to the peptide might enhance transfection by promoting fusion with the endosomal membrane, leading to improved cytoplasmic release of the DNA13,18. The neutral lipid DOPE in cationic lipoplex formulations enables higher transfection efficiencies as the conical structure of this lipid promotes the formation of inverted hexagonal structures that rapidly fuse with the endosomal lipid bilayer, independent of charge, thus enabling cytoplasmic release of the DNA. Substitution of DOPE for DOPC, a neutral lipid that favour more stable lamellar structures, greatly reduces lipoplex transfection efficiency18,19,20,21,22.
In this study, we aimed to explore whether the lipid components of the RTN lipopolyplex played a similar role in endosomal membrane fusion to that of lipoplexes and whether this contributed to their improved transfection efficiency. RTN formulations were therefore formulated with peptides mixed with cationic liposomes at the same charge density, containing either the fusogenic neutral lipid DOPE, or the non-fusogenic, neutral lipid DOPC. We hypothesised that if charge density of the liposome component was the more important factor then substituting the neutral lipid component would not affect transfection efficiency whereas if fusogenic properties were more important, the DOPE formulations would be superior to the DOPC formulations. The biophysical properties, transfection efficiencies and intracellular trafficking properties of each were investigated and compared to relate structural differences to functionality. Finally, in vivo transfection efficiencies of RTNs containing DOPE or DOPC were compared to assess the relevance of in vitro studies to in vivo applications.
This study will enable us to understand in more detail how such formulations function and to develop them further for gene therapy applications.
The lipids (Supplementary Fig. 1) 1,2-dioleoyl-3-trimethylammonium-propane (DOTAP), 1,2-dioleoyl-sn-glycero-sn-3-phosphatidylcholine (DOPC), 1,2-dioleoyl-sn-glycero-3-phosphatidyl-ethanolamine (DOPE) and Rhodamine-DOPE were purchased from Avanti Polar Lipids (Birmingham, Alabama, USA). The peptide sequences K16GACSERSMNFCG (K16E) and K16GACYGLPHKFCG (K16Y) were purchased from China Peptides (Shanghai, China) and dissolved to 10 mg/mL in DNase/RNase free water (Invitrogen, Paisley, UK). The plasmid pCI-Luc comprised the luciferase gene of pGL3 (Invitrogen, Paisley, UK) subcloned into the eukaryotic expression vector pCI (Promega, Southampton, UK).
Liposome, lipoplex and lipopolyplex formulation
The liposomes LC1, LC2 and LC3 comprised formulations of DOTAP: and DOPC weight ratios of 0.5:1, 1:1 and 3:1 respectively (DOTAP:DOPC). The homologous DOTAP/DOPE liposomes LE1, LE2 and LE3 comprised a mixture of DOTAP and DOPE at weigh ratios of 0.5:1, 1:1 and 3:1 respectively. Liposomes were prepared by mixing the component lipids dissolved in chloroform to a final volume of 200 μL, followed by rotary evaporation in a Buchi Rotavapor (Oldham, UK) under a partial vacuum to produce a thin lipid film. Lipids were then rehydrated with 1 ml of distilled water whilst rotating overnight and then sonicated in a XB3 Ultrasonic Bath (Grant Instruments, Cambridge, UK) until clear to make the liposome solution at 1 mg/ml.
Lipoplexes (LD) were then formed by mixing the cationic liposomes with pDNA at a weight ratio of 4:1 lipid (L):DNA (D), in distilled water or OptiMEM (Invitrogen, Paisley, UK) with DNA at a final concentration of 1 μg per 100 μl. LD mixtures were then incubated for 30 min at room temperature to stabilise before use. Lipid (L):Peptide (P):DNA (D) formulations were prepared by mixing the different liposomes with peptide in the order L:P:D at weight ratios of 0.5:4:1, 0.75:4:1, 1:4:1 and 2:4:1.
Hydrodynamic size and zeta potential measurements
The hydrodynamic size and zeta potential of the liposomes (5 μg lipid per ml), LD and LPD nanocomplexes (both at 2 μg/ml with respect to plasmid DNA) in distilled water were determined by dynamic light scattering (DLS) and laser Doppler velocimetry, respectively, using a Malvern Nano ZS (Malvern Instruments, Malvern, UK). The z-average data are reported with Polydispersity Index (PDI) values of less than 0.3 accepted as representing a monodisperse population of particles. The overall charge (zeta potential) that the nanocomplex acquires in water while attracted by the oppositely charged electrode was measured and reported as strength field unit (mV).
Negative staining transmission electron microscopy (TEM)
A 5 μl aliquot of LPD nanocomplexes was applied onto a 300-mesh copper grid coated with a Formvar/carbon support film (Agar Scientific, Essex, UK) then, after a few seconds, dried by blotting with filter paper. The sample was then negatively stained with 1% uranyl acetate for a few seconds, before blotting with filter paper and air dried. Imaging was carried out with a Philips CM120 BioTwin Transmission Electron Microscope and operated at an accelerating voltage of 120 kV.
Cell culture and luciferase transfection
The human bronchial epithelial cell line 16HBE14o- (D. Gruenert, San Francisco) was maintained in Eagle's Minimal Essential Medium (MEM; Sigma-Aldrich, Dorset, UK) supplemented with 10% (v/v) foetal bovine serum (FBS), 100 U/mL penicillin, 100 mg/mL streptomycin and 2 mmol/l L-glutamine. The murine neuroblastoma cell line Neuro-2A (ATCC, Manassas, VA, USA) was cultured in Dulbecco's Modified Eagle Medium (DMEM), 1% (v/v) non-essential amino acids, 1 mM sodium pyruvate and 10% (v/v) FBS (Invitrogen, Paisley, UK). Both cell lines were incubated at 37°C in a humidified atmosphere with 5% CO2. For transfections, cells were seeded into 96-well plates at 2.5 × 104 cells per well then LD or LPD nanocomplexes in OptiMEM added to each well containing 250 ng of plasmid DNA in 200 μl in replicates of six. Plates were centrifuged at 483 × g for 5 min to promote sedimentation of the nanocomplexes and incubated for a further 24 h. Cells were then lysed with Reporter Lysis Buffer and a chemiluminescence assay was performed to measure luciferase activity (Promega, Southampton, UK). Protein concentration in the lysate was determined using a Bio-Rad protein assay (Hemel Hempstead, UK) then luciferase activity expressed as relative light units (RLU) per milligram of protein.
Fluorescently-labelled LPD formulations were prepared with LC2 or LE2 liposomes containing Rhodamine-DOPE at 0.5% of total lipid while 50% of the pCI-Luc was labelled with Cy5 dye using the Universal Linkage System Nucleic Acid Labelling Kit (Kreatech Diagnostics, Amsterdam, Netherlands). 15 × 104 16HBE14o- cells were seeded onto glass coverslips in 6-well plates and incubated for 24 h at 37°C in a humidified atmosphere with 5% CO2. Fluorescently-labelled nanocomplexes LC2PD-0.75 and LE2PD-0.75 (Table 1) were added to the cells (1.5 μg DNA/well), the plates were centrifuged at 483 × g for 5 min and then incubated for 6 h or 22 h. The cells were then fixed with 4% paraformaldehyde, permeabilised with 0.1% Triton in phosphate-buffered saline, blocked with 3% bovine serum albumin (BSA) and stained for 2 h at room temperature with anti-Lysosomal-associated membrane protein 1 (LAMP-1) primary antibody (1:250 dilution in 1% BSA; product number H4A3, Abcam, Cambridge, UK), washed with phosphate-buffered saline and then incubated for 1 h at room temperature with Alexafluor 488 goat anti-mouse secondary antibody (1:1000 dilution in 1% BSA, Invitrogen, Paisley, UK) and DAPI (0.1 mg mL−1, Sigma-Aldrich, Poole, UK). The cells were washed and sealed in mounting media (Invitrogen, Paisley, UK) before visualising with a 63 × oil immersion objective (N.A. 1.4) under a Carl Zeiss LSM710 laser scanning microscope system (Carl Zeiss, Jena, Germany).
In vivo delivery and luciferase assay on lung tissues
Female CD1 mice were purchased from Charles River (Margate, UK). All procedures were approved by UCL animal care policies and were carried out under Home Office Licenses issued in accordance with the United Kingdom Animals (Scientific Procedures) Act 1986 (UK). LC1PD and LE1PD complexes were prepared at a weight ratio of L:P:D of 0.75:4:1 essentially as described previously15 at a final pDNA concentration of 0.33 mg/ml. 4-week old female CD1 mice were instilled oropharyngeally with nanocomplexes in 55 μl water containing 18.15 μg of pCI-Luc, with untreated mice used as controls (n = 3). 24 h following instillation, the mice were culled and their lungs extracted and snap frozen. Lungs were defrosted on ice, submerged in reporter gene assay lysis buffer (Roche, Basel, Switzerland), homogenized with a Precellys24 tissue homogenizer (Stretton Scientific, Stretton, Derbyshire, UK) and then centrifuged at 14,170 × g for 10 min at 4°C. The supernatant was removed and centrifuged for a further 10 min at 4°C then used in luciferase assays. Results were expressed as relative luminescence units per milligram of protein (RLU/mg).
Data are shown as mean ± standard deviation (S.D.). Statistical analysis was performed by unpaired t-test using GraphPad Prism Statistics software version 5.01 (GraphPad Software, Inc, La Jolla, CA, USA). A difference was considered statistically significant when P < 0.05.
The morphology of the representative samples
Biophysical analysis by transmission electron microscopy (TEM) (Fig. 1) and dynamic light scattering analysis (Table 1) showed that LC1PD-0.75 formulations formed spherical particles of 78 ± 0.6 nm (PDI < 0.3) and a zeta potential of 36.6 ± 1.8 mV with a tendency to agglomerate (Fig. 1A). LE1PD-0.75 formulations, in which DOPE replaced DOPC, formed mostly spheres (Fig. 1B) of a similar size 85.5 ± 0.6 nm (PDI < 0.3) but much higher zeta potential at +62.5 mV than LC1PD-0.75. On the other hand, LC3PD-0.75 and LE3PD-0.75 both formed mostly spheres of both similar size about 74 nm (PDIs < 0.3) and zeta potential at +42 and +39 mV respectively. Both also formed some rod-like structures in addition to sphere at about 10 nm wide and 40 nm long (Fig. 1C, D). Increasing the DOTAP content in the formulations LC1PD-0.75 (78 nm) to LC2PD-0.75 (68 nm) to LC3PD-0.75 (74 nm) produced no pattern in size changes but for the homologous DOPE formulations size decreased from 86 nm to 74 nm.
Luciferase transfection of LD and LPD nanocomplexes
The transfection efficiency of LC1-3D complexes (4:1 L:D weight ratios) improved with decreasing ΦDOPC in both 16HBE14o- and Neuro-2A cells (Supplementary Fig. 1), while there was no consistent trend when varying ΦDOPE for the transfection efficiency of LE1-3D lipoplexes. This pattern of results was consistent with previously reported transfection data with DOPC and DOPE-containing lipoplexes19,20.
The transfection efficiency of LEPD was significantly higher than that of LCPD nanocomplexes at the same weight ratio of liposome to pDNA (Fig. 2A–C). The transfection efficiencies of LCPD lipopolyplexes increased with decreasing ΦDOPC (Fig. 2D) while there was no consistent trend seen with decreasing ΦDOPE (Fig. 2E).
Cy-5-labelled pDNA (green) and Rhodamine-labelled liposome (red) were used to monitor the trafficking of LPD inside 16HBE14o- cells. Subcellular localisation of the vector components was assessed in relation to the late endosomal-lysosomal compartment marker (LAMP-1, magenta) and DAPI- stained nuclei (blue). At 6h, LC2PD-0.75 accumulated in perinuclear lysosomes (yellow dots representing colocalised Cy5-DNA and rhodamine-lipids) (Fig. 3A) and even after 22 h, most pDNA still resided in the late endosomes/lysosomes with very little free pDNA found in the cytoplasm or the nucleus (Fig. 3B). In contrast, free pDNA from LE2PD-0.75 complexes was found in the cytoplasm and nucleus as early as 6 h (Fig. 3C) which further increased by 22 h (Fig. 3D).
Luciferase assay of lung extracts
Finally we determined whether the in vitro results translated to an in vivo application by delivery to the airways of murine lungs. Twenty-four hours after administration, luciferase assays were performed on lung extracts of mice treated with either LC1PD-0.75 or LE1PD-0.75 nanocomplexes. These formulations were selected as they exemplified the effects of the neutral lipids on transfection efficiency in vitro. The luciferase expression from LE1PD-0.75 was five-fold higher than LC1PD-0.75 (Fig. 4) while the same formulations transfecting 16HBE14o- cells confirmed that LE1PD-0.75 was again significantly better than the LC1PD-0.75 nanocomplexes (Supplementary Figure 2).
We are developing formulations of lipids with peptides and DNA which self-assemble into nanoparticles electrostatically on mixing at optimised ratios of components13,14,15,16,17. The transfection efficiency of these lipopolyplexes is substantially higher than either the lipoplex or polyplex containing the same liposomes or peptides and so we aim to clarify the mechanism of synergy of the lipid and peptide components. We hypothesised that, while the peptide mediates packaging and targeting15,16,21 lipid components of lipopolyplexes may aid in endosomal disruption and the trafficking of the nucleic acid into the cytoplasm and therefore reasoned that strongly fusogenic lipids, such as DOPE, should display higher transfection efficiencies in lipopolyplexes than DOPC that promotes more stable laminar lipid bilayer structures.
Biophysical analysis revealed that lipopolyplex formulations containing DOPE and DOPC lipids in variable proportions, were of a consistent size and charge with only marginal affects of alterations to the lipid composition of each formulation. TEM images showed that there were no significant differences in lipopolyplex morphology with a mixture of spheres and rods observed in most cases of similar sizes. Despite only minor differences in biophysical properties, transfection results of LCPD and LEPD lipopolyplexes revealed that at higher weight fractions of neutral lipids (i.e., those containing LE1 and LC1) the transfection efficiency of LEPD formulations was significantly higher than that of LCPDs. As the weight fraction of neutral lipids decreased and the liposome charge density increased, the relative transfection efficiency of LCPDs was enhanced although even with lipids at the highest charge density, i.e., LE3 and LC3, the transfection efficiency of LEPD formulations remained approximately twice that of LCPD formulations. These same trends were also observed with LED and LCD lipoplex transfections, with LCD transfection efficiencies increasing significantly with higher charge density while the LED formulations showed no consistent trend in relation to charge density. The transfection enhancement of LD and LPD complexes containing DOPE rather than DOPC indicates the importance of the inverted hexagonal structure of the DOPE lipid in enabling endosomal membrane fusion and release of DNA compared to the lamellar DOPC structure. Cellular trafficking studies confirmed that the DOPC-containing cationic liposomes showed limited ability to escape from the endosome leading to lower transfection efficiencies of lipopolyplexes.
Finally, we investigated whether DOPE can improve the transfection efficiency of the RTN lipopolyplex in vivo by delivery to murine lungs (Fig. 4). LE1PD-0.75 yielded luciferase reporter gene expression levels five times higher than that of LC1PD-0.75 formulations. Thus we have shown that the advantages of DOPE for in vitro transfections in lipopolyplexes translated to an in vivo system. This result contrasted with a previous comparative study of DOPE-containing lipopolyplexes where the formulation was administered systemically and poor transfection efficiency was observed. However, this difference was due to serum interactions with lipopolyplexes neutralising DOPE activity before actually entering cells22.
We have shown that the fusogenic properties of DOPE, as in lipoplex formulations, are essential for the transfection function of lipopolyplex formulations but we have shown additionally that this property can be combined with the targeting and packaging properties of the peptide component to produce a significant enhancement of transfection efficiency compared to the lipoplex alone. The cationic lipid is important for the stability of the liposome component and its electrostatic association with DNA in formulating the lipopolyplex but probably does not contribute to membrane interactions in the cellular transfection pathway. These findings will be important in designing improved lipopolyplex formulations.
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Z. Du was financially supported by National Natural Science Foundation of China (Grant No. 30901881) and the Ministry of Science and Technology of China (No. 2011DFA30790), M. Munye was supported by a studentship from Great Ormond Street Hospital Children's Charity, A. Tagalakis was supported by a grant from EPSRC (EP/G061866/1) and Association for International Cancer Research (AICR), M. Manunta was supported by a grant from the Wellcome Trust (WT094348MA). SH is the recipient of a Research Leadership funding award from Great Ormond Street Hospital Children's Charity (V1298).
SH is consultant to and holds equity in, Nanogenic Solutions Ltd, a company set up to commercially develop transfection agents for genetic therapies.
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Du, Z., Munye, M., Tagalakis, A. et al. The Role of the Helper Lipid on the DNA Transfection Efficiency of Lipopolyplex Formulations. Sci Rep 4, 7107 (2014). https://doi.org/10.1038/srep07107