Open access peer-reviewed chapter

Electrically Mediated Gene Delivery : Basic and Translational Concepts

By J. Teissie

Submitted: May 5th 2012Reviewed: October 31st 2012Published: February 13th 2013

DOI: 10.5772/54780

Downloaded: 1153

1. Introduction

Naked plasmid (pDNA) electrotransfer is an approach for gene transfer that is very efficient for in vitro studies since its introduction in 1982. It was extended for a use in vivo in a perspective for clinical gene therapy.

This chapter is a review on the state of the art. The molecular processes bringing the pDNA transfer and expression will be described. A critical view of the barriers preventing an efficient level of expression is given. This gives the tools to design the relevant protocols for the use on animals and the potential clinical trials.

Delivery of naked plasmids (pDNA) in tissue to obtain gene expression was facing the limit of a poor level of expression [1]. But the clinical advantage was that it was a safe approach for the patient. Improvement of the delivery and the resulting expression was known to be obtained at the cellular level by applying electric field pulses to the cell-pDNA mixture [2]. It was shown that this boost in expression could be obtained on tissues [3]. During the last 15 years, many developments in this approach have been performed and Electrotransfection is now considered as a perspective for gene therapies [4-9]. A Phase I clinical trial using gene therapy by electrically mediated delivery has been performed ( identifier NCT00323206)[10]. More recent data showed that the delivery and expression can be obtained on very sensitive organs [11-13]. Electropulsation mediated gene delivery appears now to be one of the effective contributors for the success of gene therapy

2. Basic processes

2.1. Electropermeabilization

Biological membrane cohesion is known for almost 40 years to be affected by external electric field pulses [14]. A transient and reversible membrane permeabilization (Electropermeabilization) results from a controlled application of electric pulses to cells [15]. This can be induced not only in vitro but on living tissues as well. The key feature is that the structural transition is obtained only when the external field is larger than a critical value. A physical targeting of the effect is therefore present in tissues. This improves the safety of the approach as only a limited volume of the tissue is affected. This metastable membrane structural organization remains poorly understood. New properties are brought to the cell plasma membrane that, besides being permeabilized, becomes fusogenic and allows exogenous proteins to be inserted in it. Electropermeabilization is used to introduce a large variety of molecules into many different cells in vitro [16, 17]. The molecular transports, that result, are either due to an electrophoretic drift or/and to a concentration driven diffusion [18, 19]. The practical use for drug delivery remains rather empirical but results from more than 20 years of trials. Clinical applications of the method are now routinely used in many oncology centers (more than 100 in Europe only) as results from the EU funded Cliniporator and ESOPE programs. A local anti-tumoral drug delivery to patients (electrochemotherapy) results from the direct application of electric pulses to the patient [20-27]. In Europe, the treatment has been approved and patients can be reimbursed,

2.2. Electrotransfection

The most frequent application of electric field induced membrane permeabilization is the transfer and expression of gene into mammalian cells. Plasmid DNA (pDNA) can be transferred and expressed in mammalian cells when electropermeabilization is triggered [2]. This a complex process that involves not only the transport of pDNA into the cytoplasm, but also depends on subsequent cellular processes [27]. The transfer of naked DNA plasmid and the expression of the gene of interest are enhanced by electropulsation into different tissues, including the skeletal muscle [28, 29], liver [3,30], skin [31, 32], lungs [33] and tumors [34, 35]. The transfection efficiency of this physical method in vivo must still be improved compared to the viral vectors. But it is obtained with naked pDNA avoiding the biological risks associated to the viral methods. Furthermore there is no theoretical restriction on the size of the pDNA to transfer. As a result, due to its easiness to perform, to the very fast expression after electric pulse delivery, reproducibility, limited costs (of the technology and logistics) and safety, gene electrotransfer is an attractive technology of gene therapy for clinical application. This is well illustrated by the increasing number of reviews covering the pre-clinical developments of the approach [4-9, 36].

As mentioned above, one of main limits of the widespread use of electropermeabilization is that very few is known on the biophysical mechanisms supporting the reorganization of the cell membrane (pore, electropore, defects?). The molecular target of the field effect remains unclear [15]. The other main limit in gene electrotransfer is that the transport is not only across the plasma membrane but must target the nucleus volume.

The present review focuses on the processes supporting gene electrotransfer in vitro and their implications for the clinical applications. The events occurring before, during, after pulse application leading to gene electrotransfer will be described. Theoretical considerations about membrane structures involved in the plasmid uptake will be described in a (very) critical manner as very few direct experimental data are available.

3. Theories of DNA plasmid electroentry

Although the first pioneering report on gene electrotransfer in cells was published 30 years ago by E. Neumann, the molecular basis behind the process of gene electrotransfer is still highly debated.

3.1. The sliding model

Most theories are based on the DNA sliding model [37]. Several steps are predicted: entry, electrophoretic translocation as long as the field was present, diffusion after the pulse delivery. An interesting simulation with predictive conclusions has just been published [38]. The DNA translocation was through a putative “electropore” assuming that the DNA was double stranded but linear (i.e open) meaning that the length was 2.4 μm. Indeed the sliding model needs the DNA to be linear to allow the “binding” of one end to the “electropore” entry. Experimental results just showed that the closed form was more effective for expression [39]. One speculative hypothesis in the simulation was that it always assumed that the binding step (entry) of the DNA to the “electropore” was present before the simulation started. De Gennes predicted that it was a very limiting step in the process (a crucial moment) when a chain end faces the electropore and enters it against the strong friction coefficient against the “pore” sides. A black box remains the “electropore”.

3.2. The electropore

The major hypothesis in the sliding model is that “pores” must be present. Krassowska’s model supports the simplest mechanism, in which plasmid enters the 5 nm thick membrane through stable electropores (up to 20 nm in diameter)[40, 41]. The electrically induced defects result from the field associated membrane potential changes. It predicts a post-pulse growth of “macropores” on the sub-second time scale fairly consistent with experimental evidence on pure lipid vesicles [42]. This model predicts “electropores” large enough to permit the plasmid uptake (under a linear form). These “electropores” are supposed to remain open for the entire duration of electrotransfer providing adequate time for the plasmid to enter the cell [43]. Indeed in Lin’s simulation [38], they may remain present on a much longer duration than the pulse as a diffusion might follow a partial electrotransfer.

This model remains very attractive in spite of the existence of many experimental contradictions. Indeed, until now, no study made it possible to visualize these membrane pores. This validation appears impossible [27]. Moreover, the resealing time of pores appears to be shorter in this lipidic model than in experiments on cells (e.g. seconds rather than minutes) [44-47]. The conclusion is that pDNA transport across the membrane is always very fast. To date, theoretical models could predict stable pores of only a few nanometers in radius; larger pores are unstable while they are needed for the sliding pDNA transfer [48, 49]. These models are confirmed by some experiments, in which high-voltage pulses a few microseconds long are used that are supposed to have created a large number of very small pores (radii of about 1 nm, i.e. the size of a few phospholipids cluster) [50]. To reconcile these results with the experimental evidence of plasmid translocation after electropulsation, some researchers postulated that plasmid entry into cells relies on the plasmid/membrane interactions, which may be facilitated by a coalescence of many small, 1 nm defects [51-54, 43]. The slow transport of DNA across the electropermeabilized membrane reflects a highly interactive electrotransfer, where many small lipid defects coalesced into large DNA-lipids assemblies where the transmembrane transport occurs [55].

3.3. Electrophoresis across the micellar structures

Other data report that gene electrotransfer through lipid bilayer could be mediated by transient complexes between plasmid and specific lipids in the edges of elongated, electropercolated hydrophilic membrane associated micellar structures [56]. The plasmid association with a lipid bilayer results in a facilitated transport of small ions. A locally conductive plasmid/lipid interaction zone is induced where parts of the plasmid may be inserted in the bilayer. Plasmid is transiently inserted in, and then electrophoretically pulled through the permeabilized zones onto the other membrane side [57]. With such a model, in the case of mammalian cells, the resting potential difference should be the driving force for plasmid translocation after the pulse induced insertion. The external field is only used to electrophoretically accumulate the pDNA on the cell surface. This has not been checked yet.

3.4. An electrophoretic transfer

Previous works suggested that electric pulses induce the membrane permeabilization, then plasmid molecules are concentrated near the membrane surface and pushed through by electrophoretic forces [58-60, 54]. The plasmid may interact with electropermeabilized membrane by three possible ways: (a) the plasmid coil is aligned in an electric field, and at the appropriate pulse polarity it moves toward the permeabilized membrane. Transfer is dependent on electrophoretic forces and is complete at the end of the pulse. Post pulse cell treatment should not affect the efficiency of transfer.

If the electrophoretic forces are the only driving forces of the plasmid transfer into the cell, similar transfection efficiencies should be obtained for equal E.T values (i.e. E, field strength and T, pulse duration). This is not supported by the experiments [61] When the E.N.T value is constant, transfection rate depends preferentially on T [52]. Therefore, the electrophoretic migration cannot be the only driving force of the plasmid transfer into the cells but clearly supports the formation of aggregates. Trypsin treatment of cells at 10 min post electrotransfection stripped off membrane-bound pDNA and resulted in a significant reduction in transfection, indicating that the time period for complete cellular uptake of pDNA (between 10 and 40 min) far exceeded the lifetime of electric field-induced transient pores (10 msec) in the cell membrane [62]. In addition, in the case of CHO cells, plasmid remains accessible to DNAase I in the minute, which follows the end of electropulsation. This shows that the plasmid transfer inside the cell occurs after the electropulsation [17].

3.5. In silico electrotransfer

A molecular dynamic approach gives a mechanism, in which plasmids do not translocate across the membrane during the electropulsation [63]. The DNA/lipid system simulation was undertaken starting from a well-equilibrated 12bp-DNA duplex placed near a model POPC bilayer. The perturbation of the system under a 1.0 V.nm−1 transverse electric field (i.e. a transmembrane voltage of 5 V !) is followed during 2 ns. Under this high electric field, the DNA duplex diffuses towards the interior of the bilayer only after the creation of a pore beneath it, and within the same timescale, it remains at the interfacial region when no pore is present. Diffusion of the strand toward the interior of the membrane leads to a DNA/lipid complex in which the lipid head groups encapsulate the strand. The dipole carried by the zwitterionic phosphatidylcholine groups of the lipids is known to be efficient for neutralizing the charges carried by the DNA [64]. Such interactions between the plasmid and the lipids contribute to the effective screening of DNA charges and therefore to the stabilization of the complex. One should not forget that electropulsation-mediated gene delivery concerns much larger supercoiled plasmids than the 12 bp construct considered in the MD simulation.

3.6. Endocytosis

Most methods for chemically mediated gene transfer described the transport as an endocytotic complex formation between the DNA vesicles and the cell surface. Several studies investigated if this can occur in electrotransfection. Treatment of cells with three endocytic inhibitors (chlorpromazine, genistein, dynasore) yielded substantial and statistically significant reductions in the electrotransfection mediated expression [62]. These findings suggest that electrotransfection depends on endocytosis of membrane-bound pDNA. [65]. Colocalization studies with endocytotic markers under a microscope showed that pDNA is internalized with concomitant clathrin- and caveolin/raft-mediated endocytosis [66]. But this cannot explain how the pDNA is released from the endocytic vesicles and why free PDNA was observed in the cytoplasm a few minutes after the pulse delivery [67]. A direct assay of the formation of endocytic vesicles brought the conclusion that endocytosis was not stimulated by applying electric pulses with intensities above the threshold value for gene electrotransfer. The conclusion was that electro-endocytosis is not a crucial mechanism for gene electrotransfer [68].

3.7. The multistep model

PDNA electrotransfer was observed at the single cell level by digitized high resolution fluorescence microscopy [67]. The introduction of DNA only occurs in the part of the membrane facing the cathode and requires a number of consecutive steps: electrophoretic migration of DNA towards the cell, DNA insertion into the membrane, translocation across the membrane, migration of DNA towards the nucleus and, finally, transfer of DNA across the nuclear envelope. Only localized parts of the cell membrane brought to the permeabilized state are competent for transfer. The transport of plasmid follows an “anchoring step”, connecting the plasmid to the permeabilized membrane, that takes place during the pulse. During the first pulsation, plasmids are electrophoretically drifted and interact with a limited number of sites on the membrane. These sites become highly conductive and attract the field lines giving an electrophoretic local accumulation [69]. PDNAs form a limited number of aggregates on the cell surface. Their sizes increase during the pulses or with successive pulses but not their number [70]. Transfer of membrane bound plasmids is certainly a complex process, that is not occurring during but after the pulse delivery. Two classes of DNA/membrane interactions result from the pulse: (i) a metastable DNA/membrane complex from which the DNA can leave and return to external medium and (ii) a stable DNA/membrane. Only DNA belonging to the second class may be effective for transmembrane transport and the resulting gene expression [71]. Nevertheless this model shows that the plasmid is stabilized in the millisecond following the pulse in the membrane core after electropulsation (in agreement with the overall experimentally observed process of DNA translocation).

4. The cytoplasmic transfer

Transfer from the membrane to the nucleus is mediated by the cell (cytoskeleton with molecular motors?). The final step should take place through the nuclear pore complex [72-74]. No direct biophysical method to alter the nuclear envelope or pore has been reported (yet). But imaging methods [75, 76] support the occurrence of a direct effect of the field on organelles [77].

For non-viral gene delivery to be successful, plasmids must move through the cytoplasm to the nucleus in order to be transcribed. 2 steps are therefore present involving 2 classes of barriers. The cytoskeletal meshwork prevents pDNA (larger than 1 kb) movement in the cytoplasm. Actin patches colocalizing with the DNA at the plasma membrane were observed several minutes after pulse delivery with characteristics similar to those of the DNA aggregates, that are formed during the early stages of electrotransfection [78]. The microtubule network is required for directed plasmid trafficking to the nucleus [79]. Microtubule–DNA interactions can be enhanced due to sequence specificity with promoters containing binding sites for cyclic AMP response-element binding protein (CREB), such as the cytomegalovirus immediate early promoter (CMViep). Insertion of cytoplasmic adapter proteins transcription factors (TFs) binding sites within plasmids permits cytoplasmic trafficking of plasmids and an effective expression.

NLS sequences can help for the transfer inside the nucleus. In non-dividing cells, the nuclear envelope is an especially problematic hurdle to gene transfer. A successful approach is in modifying plasmid (pDNA) vectors to enhance nuclear import through the Nuclear Pore Complex [80]. Proteomics tools have been used to study DNA nuclear entry telling that Transcription factor-binding sites promote DNA nuclear translocation and Cell-specific transcription factors drive cell-specific DNA nuclear entry [81]. NLS peptides or nuclear proteins complexed with plasmids may enhance DNA nuclear translocation.

5. PDNA under electrotransfection conditions

5.1. Complexities in the determination of pDNA size evaluation

The size of the plasmid can be a significant modulator of the efficiency of transfer. The sliding model assumed that the pDNA was linear. This is not relevant of the experiments where a closed form was used in almost all reported cases. The gyration volume appears more appropriated. It is known that this diameter is highly sensitive to the compaction factors that are present. A tightly packed form is found in viral capsids. During the last 20 years, biotechnologists have been playing with chemical additives to obtain more compact forms. Indeed adding NaCl and/or MgCl2 is affecting the diameters. In [82] the authors wrote: “conformational and thermodynamic properties of supercoiled DNA depend strongly on ionic conditions. The effective double-helix diameter increases from 3 to 15 nm as the salt concentration is reduced from 1.00 to 0.01 M.”. It was later observed with pUC18 (2686 bp), in dilute aqueous solution at salt concentrations between 0 and 1.5 M Na+ in 10 mM Tris, that the superhelix diameter from the simulated conformations decreased from 18.0 +/- 1.5 nm at 10 mM to 9.4 +/- 1.5 nm at 100 mM salt concentration[83]. This value did not significantly change to lower values at higher Na+ concentration. And in [84] upon addition of 0.122 M NaCl, the radius of gyration (RG) decreased substantially, which indicates that p30 delta adopts a more compact structure. When 4 mM Mg2+ was added to native supercoiled p30 delta in 0.1 M NaCl, Rg decreased.

Using Polymethacrylate monoliths,[85], size evaluations are described on a model plasmid, consisting of 4.9 kbp, Under physiological conditions, a 45 nm radius was evaluated. But the pore size distributions in these samples (see below) are broad: as such, the changes in the median pore diameter measured by mercury intrusion porosimetry reflect general shifts in the position of the pore distribution envelope, rather than the position of a well-defined, sharp peak [86](in [87] it was found for covalently closed supercoiled ColE1-plasmid DNA in 0.2 M NaCl, 0.002 M NaPO4 pH 7.0,0.002 M EDTA, a gyration radius about 100 nm but with EDTA meaning with no divalent ions but in 0.2 M NaCl. Finally, in [88] for pGem1a plasmids (3730 base pairs) in the relaxed circular (nicked) and supercoiled forms, RG = 90 +/- 3 nm,, and RG = 82 +/- 2.5 nm were obtained.

As a conclusion, a large distribution of gyration radii is described in the literature but, they are all larger that the compact form reported by Krassowska and that she used to predict the need of “electropores” of about 10 nm for DNA translocation during the pulse. Even larger sizes are requested with linearized form, that are known to be effective for expression after their electrotransfer [39]. For a closed form (highly effective for expression after the electrotransfer), in a condensed form under physiological conditions (Na> 20 mM, MgCl2 about 1 mM), the diameter of the structures supporting a free transmembrane transfer needs to be at least 100 nm.

Simulations give shapes of supercoiled closed form of PDNA (7 kb) [89]

As NaCl concentration decreases, the superhelix becomes less regular and more compact. In the presence of just 10 mM MgCl2, supercoiled DNA adopts essentially the same set of conformations as in moderate to high concentrations of NaCl.

The size of a supercoiled plasmid is difficult to access. As shown in [89], the bulk size is large. This explains why many reports are giving data around 100 nm. But in fact, it is not a sphere (a coil) but a rather elongated thread-like shape that is more relevant. The DNA topology is described quantitatively by the twist of double helix and by the number of times the helix crosses over on itself (plectoneme). Plectonemic structures are typically formed by bacterial plasmids. Then in one direction we got a cross section close to the 20 nm used by Krassowska. A larger value is indeed observed under the low salt (Mg free) solution [90, 91].

The final conclusion is that the general conformation of pDNA used for electrotransfection is “complex” and do not support the model used for the sliding model. The lack of knowledge on the theoretical processes supporting the transmembrane transport brings the need of a rather empirical approach in the optimization of the technology for gene therapy.[92].

5.2. Smaller plasmids are more effective

The basic protocols are using Naked plasmid DNA under a Double strand closed form. No advantage is brought by preparing the linear form by restriction enzymes digestion.

As size controls the efficiency of transfer, minicircle forms (MC) are more efficient [93]. Minicircle DNA lacks the bacterial backbone sequence consisting of an antibiotic resistance gene, an origin of replication, and inflammatory sequences intrinsic to bacterial DNA that represent a potential risk for safe clinical application and reduce gene transfer rates as well as transgene expression. Expression following electrotransfer is improved with MC constructs over full-length plasmid (same promoter, same coding cassette) with different reporter genes. This great efficiency of MC was correlated to more efficient vector uptake by cells. Nevertheless, one should keep in mind that huge pDNA have been transferred and that decreasing the size of the plasmid is just bringing improvement but is not needed [94].

5.3. Field effect on pDNA conformation

Under electrotransfection protocols, besides the ionic content of the buffer that can be easily adjusted under in vitro protocols (but remains poorly controlled for gene therapy)[95], a critical parameter is present. An electric field is present that may affect the conformation of the pDNA.

Concerning DNA in electric fields, conflicting observations and predictions are present in the literature. Low DC field do not greatly perturb the conformation of large DNA. In [96], it is reported that larger fields give rise to chain orientation and stretching. This is in agreement with a simulation [97]. In fact, at high concentrations, strong intermolecular aggregation was observed even under 100V/cm [98, 99]. This can be considered as an explanation for the formation of the stable spots that we observed as an early stage in the multistep process.

6. Physical controls in optimizing the protocols

6.1. Electrical pulse parameters

Cell electropermeabilization must occur and an efficient electrophoretic accumulation of pDNA must be applied. This means that the field strength must be larger than a critical value (permeabilizing threshold at the level of the target in the tissue). Again the advantage of a targeted effect in tissues is present. But a modulation of transfer in this well defined volume by the cumulated pulse duration is present[100, 101].

The pulse duration can be short (0.1 ms) but longer pulses are more efficient as they are associated to a longer and therefore more efficient electrophoresis of the pDNA [102, 104]. The electrical parameters must be chosen to preserve the cell viability.

A double pulse method (a short high voltage pulse followed after a short delay by a long low voltage one)(HV LV) was therefore described [105]. The electrophoretic drift can be delayed from the permeabilizing pulse. This protocol is better to preserve the viability.

A destructive Joule effect can be present bringing limits in the parameters of the protocol. Intra pulse delay choice in a train of pulses can help to reduce this damaging effect by allowing a inter-pulse cooling of the pulsed sample.

6.2. Electrodes

Getting an optimized field distribution of the field intensities at the level of the target in the tissue is controlled by the geometry of the electrodes [106].

Most trials are performed by using needle electrodes that are penetrating inside the target tissues. Many designs have been reported (number of needles, diameters, distances, number, depth of penetration (see [107]). One major concern with these systems (that allow a deep penetration of the field) is the damaging effects of the electrodes (not only due to the perforation of the tissue but linked to the local effects at the electrode surface (local heating [108], electrochemical reactions [109]). Contact electrodes appear less destructive as the skin to electrodes contact is due to a conductive gel [110] but the field penetration remains rather limited

7. Cellular responses and controls

7.1. Reactive Oxygen Species (ROS)

Cellular responses are present under electrotransfection. The field induced membrane reorganization is a stress for the molecular assembly. A defense mechanism is present as shown by the generation of reactive oxygen species at the surface of the permeabilized cell [111-113]. ROS are highly destructive for DNA and reduce the number of copies that remains intact and therefore effective for expression. Protective effects are brought by the addition of anti-oxydants as long as they are not interfering with the transport.[114, 115]. There is a need to find biocompatible additive to reduce the ROS generation. Co-block polymers appear as a promising pathway.It was shown that postshock poloxamer administration reduced tissue inflammation and damage in comparison with dextran-treated or control tissues [116].

7.2. Extracellular matrix (ECM)

Uniform DNA distribution in tumors is a prerequisite step for an homogeneous transfection efficiency in solid tumors. This is of course valid for other target tissues (skin, muscles). The interstitial space is a rate limiting physiological barrier to non-viral gene delivery. External pulsed electric fields have been proposed to increase DNA transport in the interstitium, thereby improving non-viral gene delivery. The characteristic electromobility behavior, under most electrotransfection pulsing conditions, consisted of three distinct phases: stretching, reptation, and relaxation. Electromobility depended strongly on the field magnitude, pulse duration, but a decisive role is played by the pore size of the fibrous matrix (the extracellular matrix in tumors) through which the DNA migrated [117, 118]. The intratumoral field, which determines the efficiency of electric field-mediated gene delivery, can differ significantly from the applied field at the surface of the tumor.[119]. This local field is under the control of the geometry of the electrodes as described above. The field strengths in tumor tissues were significantly lower (down to 50%) than the applied field due to the multicellular organization. But when the external field was uniform (plate parallel electrodes) the electric fields in the center region of tumors were macroscopically uniform on ex Vivo slices.

Indeed tumor histological properties strongly affected transfection efficiency. Soft tumors with larger spherical cells, low proteoglycan and collagen content, and low cell density are more effectively transfected than rigid tumors with high proteoglycan and collagen content, small spindle-shaped cells and high cell density [120].

Electrotransfection in tissue can be improved by modulation of the extracellular matrix, using collagenase and/or hyaluronidase in tumors [121] as well as in muscles, a major target organ for DNA vaccination, a great topic for gene therapy [122].

8. Conclusion

Even if our knowledge on the molecular mechanisms governing the transfer of pDNA due to the delivery of pulsed electric field remains limited, it gives recommandations for an optimal choice of the protocols.

Pulse generators should provide the largest flexibility in the choice of the electrical parameters (voltage, duration, delay, number, current intensity, sharpness of the pulse onset) and offer an internal monitoring of the delivered pulse. Very few products on the market meet these specifications.

The local field on the tissue target is a complex function of the choice of the electrodes and on the electrical changes of the tissue due to the electrical treatment. This last parameter is highly dynamic and takes place during the pulse delivery. This remains under technical investigations by using simulations in electrical engineering [123, 124]. This time dependence of the electrical properties of the pulse tissue is an important parameter for the proper choice of the sequence of electrical pulses that must be delivered [125].

But clearly the biotechnological contributions cannot be neglected. Optimization in the plasmid constructs is strongly needed. The use of minicircles is promising to get a better transfer. But a key problem remains the design of the promoter that is shown to be an active partner in the cytoplasmic traffic to the nuclear volume.


The work was supported by grants from the seventh framework programme OncomiR (# 201102) and from the region Midi-Pyrénées (#11052700). The author wants to thank Dr JM Escoffre for many discussions.

© 2013 The Author(s). Licensee IntechOpen. This chapter is distributed under the terms of the Creative Commons Attribution 3.0 License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

How to cite and reference

Link to this chapter Copy to clipboard

Cite this chapter Copy to clipboard

J. Teissie (February 13th 2013). Electrically Mediated Gene Delivery : Basic and Translational Concepts, Novel Gene Therapy Approaches, Ming Wei and David Good, IntechOpen, DOI: 10.5772/54780. Available from:

chapter statistics

1153total chapter downloads

More statistics for editors and authors

Login to your personal dashboard for more detailed statistics on your publications.

Access personal reporting

Related Content

This Book

Next chapter

Solid Lipid Nanoparticles: Tuneable Anti-Cancer Gene/Drug Delivery Systems

By Tranum Kaur and Roderick Slavcev

Related Book

First chapter

The DNA-Damage Response to Ionizing Radiation in Human Lymphocytes

By Maddalena Mognato, Mauro Grifalconi, Sabrina Canova, Cristina Girardi and Lucia Celotti

We are IntechOpen, the world's leading publisher of Open Access books. Built by scientists, for scientists. Our readership spans scientists, professors, researchers, librarians, and students, as well as business professionals. We share our knowledge and peer-reveiwed research papers with libraries, scientific and engineering societies, and also work with corporate R&D departments and government entities.

More About Us