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In vitrocorrection of cystic fibrosis epithelial cell lines by small fragment homologous replacement (SFHR) technique

  • Federica Sangiuolo1,
  • Emanuela Bruscia1, 2,
  • Annalucia Serafino3,
  • Anna Maria Nardone4,
  • Emanuela Bonifazi1,
  • Monica Lais1,
  • Dieter C Gruenert2 and
  • Giuseppe Novelli1Email author
BMC Medical Genetics20023:8

DOI: 10.1186/1471-2350-3-8

Received: 29 April 2002

Accepted: 23 September 2002

Published: 23 September 2002

Abstract

Background

SFHR (small fragment homologous replacement)-mediated targeting is a process that has been used to correct specific mutations in mammalian cells. This process involves both chemical and cellular factors that are not yet defined. To evaluate potential of this technique for gene therapy it is necessary to characterize gene transfer efficacy in terms of the transfection vehicle, the genetic target, and the cellular processing of the DNA and DNA-vehicle complex.

Methods

In this study, small fragments of genomic cystic fibrosis (CF) transmembrane conductance regulator (CFTR) DNA, that comprise the wild-type and ΔF508 sequences, were transfected into immortalized CF and normal airway epithelial cells, respectively. Homologous replacement was evaluated using PCR and sequence-based analyses of cellular DNA and RNA. Individual stages of cationic lipid-facilitated SFHR in cultured cell lines were also examined using transmission electron microscopy (TEM).

Results

We demonstrated that the lipid/DNA (+/-) ratio influences the mode of entry into the cell and therefore affects the efficacy of SFHR-mediated gene targeting. Lipid/DNA complexes with more negative ratios entered the cell via a plasma membrane fusion pathway. Transfer of the DNA that relies on an endocytic pathway appeared more effective at mediating SFHR. In addition, it was also clear that there is a correlation between the specific cell line transfected and the optimal lipid/DNA ratio.

Conclusions

These studies provide new insights into factors that underlie SFHR-mediated gene targeting efficacy and into the parameters that can be modulated for its optimization.

Keywords

gene therapy cystic fibrosis transmembrane conductance regulator (CFTR) gene targeting transmission electron microscopy (TEM) transfection

Background

Homologous replacement is a technology that can be used to modify specific genes within chromosomal DNA [16]. The potential of this type of strategy has obvious implications for maintaining genomic integrity and cell-specific expression. The direct conversion of mutant genomic sequences to a wild-type genotype, restoring the normal phenotype, has clear advantages over therapeutic cDNA. By preserving the integrity of the targeted gene, the relationship between the coding sequences and regulatory elements remains intact. Consequently, cell-specific expression is not altered. Small fragment homologous replacement (SFHR) involves the introduction of small fragments (~500-bp) of DNA into cells. After entering the cells, the fragment pairs with its genomic homologue and replaces the endogenous sequence with the exogenous fragment through an, as yet, undefined mechanism [1, 2, 6].

SFHR has already been successfully used to correct ΔF508 mutation in the cystic fibrosis (CF) transmembrane conductance regulator (CFTR) gene [1, 2, 710]. The ΔF508 is the most common mutation associated with CF [11, 12] and demonstration of its correction has significant therapeutic implications. The studies showed that SFHR-mediated replacement of mutant or wild-type genomic sequences after the introduction of small DNA fragment (491/488 nt) into cultured epithelial cells [7, 10]. In some studies, the fragment, also carried a silent mutation that introduced a unique XhoI restriction site that could be used as a secondary marker of SFHR-mediated correction [7, 8].

Recent in vivo studies have also indicated that SFHR could be used to modify endogenous mouse CFTR in the lung and in the intestine [9]. Not only was it possible to demonstrate SFHR-mediated modification of the DNA, but there was also a clear indication that the cells expressing CFTR were modified [9]. However, there has been no detailed SFHR optimization analysis as it relates to the behaviour of the DNA during and after SFHR uptake, the intracellular distribution of the DNA, and long-term stability of SFHR using non-viral vehicles. In this study, different parameters that influence SFHR in human epithelial cells were evaluated to determine whether SFHR could be an effective strategy for gene therapy. These include the type of transfected cells, DNA fragment to lipid ratio (+/-, respectively) and the time of harvest after initiation of transfection (incubation time). Different DNA transfection conditions were evaluated with respect to their ability to modulate SFHR-mediated correction.

SFHR-mediated replacement at the appropriate genomic locus and expression of the exogenous sequences was assayed using polymerase chain reaction (PCR) amplification, restriction fragment length polymorphic (RFLP) analysis and DNA sequencing. The intracellular fate of transfected gold-labelled DNA fragments was monitored by transmission electron microscopy (TEM). The results presented here provide insight into the mechanisms underlying SFHR-mediated correction of the most common CF mutation, the ΔF508.

Methods

Cell cultures

Studies were carried out in CF tracheobronchial cells transformed with an origin of replication defective simian virus 40 (SV40) containing plasmid (pSVori-) [1315]. The cell line, CFBE41o-, is homozygous for the ΔF508 mutation (ΔF508/ΔF508). A wild-type airway epithelial cell line 16HBE14o-, also transformed with the pSVori- plasmid was used as representative of the normal cells [1416]. Cells were grown in Eagle's Minimal Essential Medium (MEM) supplemented with 10% fetal bovine serum (FBS) and antibiotics under humidified conditions at 37°C in 5% CO2. Stock cultures were grown in T75 flasks coated with an extracellular matrix of collagen/fibronectin/bovine serum albumin and subculture by trypsinization as described previously [17].

Synthesis of DNA fragments

DNA fragments, 491-bp and 488-bp, that comprised exon 10 as well as the 3' and 5' flanking intron regions of the wild-type (wt) and mutant (ΔF508) CFTR gene respectively, were generated by PCR as previously described [7, 8, 10]. Fragments were column purified (Qiagen) and ethanol precipitated for subsequent use.

Preparation of lipid/fragment complexes

DNA-cationic lipid complexes were generated using the GENEPORTER (Gene Therapy Systems, San Diego, USA) liposome. The complexes were made at different charge ratios (+/-), by increasing the concentration of the double stranded DNA fragments and mixing with a constant quantity of LIPID (22.5 μl) according to manufacturer's specifications. The mixture was then incubated at room temperature for 45 min and diluted to a final volume of 2 ml with serum-free MEM. DNA without lipid was used as the control in all experiments.

Transfection protocol

Approximately 2.5 × 106 cells were seeded in T75 flask 24 h before treatment. Cells were incubated with lipoplexes for 5 h in serum free medium at 37°C. After the initial 5 h incubation, cell cultures were supplemented with medium containing a final 10% FBS concentration. Cells were harvested by trypsinization following removal of the culture medium and washing twice with cold Phosphate Buffered Saline (PBS).

DNA analysis

Genomic DNA from transfected cells was initially PCR amplified with primers (CF1B/CF6) located outside the region of homology defined by the 491/488 bp transfection fragment (Fig. 1A). These primers localize the amplification to genomic DNA and inhibit amplification of free fragment. A secondary amplification was carried out with primers CF1B and ΔF2 with the primary amplification product as template. Primer ΔF2 is located inside the region of homology. A schematic representation of primer localization is depicted in Fig 1A. The product from the secondary PCR amplification was extracted from agarose gel (Millipore Ultrafree-DA, Bedford MA USA) and then subjected to a final round of radioactive PCR amplification with primers (ΔF1/ΔF2). These PCR products were sized by polyacrylamide gel electrophoresis (Storm 860, Molecular Dynamics, Little Chalfout, UK). The gel was exposed autoradiographically and then analyzed densitometricly to compare the relative intensity of the two bands (97 and 94 bp). These two bands correspond to the wild-type and mutant sequence, respectively. Oligonucleotide sequences are reported in Table I.
Figure 1

Localisation of primer pairs used for DNA (A) and RNA (B) analysis protocols. ΔF508 position is showed. PCR products length is of 771/768-bp, 373/370-bp and 97/94-bp for CF1B/CF6, CF1B/ΔF2 and ΔF1/ΔF2 oligonucleotide pairs respectively.

Table 1

PCR primers for SFHR DNA and RNA analysis

Primer

Sequence

Location

CF1B (S)

5'-CCTTCTCTGTGAACCTCTATCA-3'

Intron 9

CF6 (A)

5'-CCACATATCACTATATGCATGC-3'

Intron 10

CF17 (S)

5'-GAGGGATTTGGGGAATTATTTG-3'

Intron 9

CF22 (A)

5'-CTTGCTAAAGAAATTCTTGCTC-3'

Intron 11

ΔF1 (S)

5'-TCCTGGATTATGCCTGGCACC-3'

Exon 10

ΔF2 (A)

5'-GGCATGCTTTGATGACGCTTC-3'

Exon 10

Primer sequences are reported from ref. [7]

RNA analysis

Total RNA was extracted by using RNeasy Mini kit (Qiagen, Germany). Reverse Transcriptase PCR (RT-PCR) amplification of total RNA was carried out using Superscipt™ II RNAse H- Reverse Transcriptase (Gibco BRL Life Technologies, Gaithersburg, USA) to generate first strand cDNA. The cDNA was initially amplified with primers external from the homology region (CF17/CF22) and then with primers (CF17/ΔF2) (Fig. 1B). The PCR product from this secondary amplification was extracted from the agarose gel as above and subjected to a final round of PCR amplification with primers (ΔF1/ΔF2). The amplicons were sized and analysed by densitometric analysis. Results are presented as the standard error of the mean. Oligonucleotide sequences are reported in Table I.

Transmission electron microscopy analysis (TEM) of gold-labelled DNA fragments

DNA fragments were gold-labelled with photoactive biotin (Pierce, Illinois, USA), and Auroprobe EM streptavidin G10 (Amersham, United Kingdom), as previously described [13]. The CFBE41o- and 16HBE14o- cells were transfected with different amounts of labelled DNA/ lipid complex at varying charge ratios and analyzed at different times of transfection. Gold-labelled fragments (not complexed with lipid) were also transfected as controls. Cells were fixed for 1 hour at 4°C with 2.5% glutheraldheyde in 0.1 M Millonig's phosphate buffer (MPB) containing 2% sucrose. Samples were then post-fixed for 1 hour at 4°C with 1% OsO4 in MPB, dehydrated in ascending ethanol concentrations and embedded in Spurr epoxy resin (Agar Scientific LTD, Stanted, Essex, UK). Ultrathin sections were stained with uranyl acetate and lead citrate and observed under a Philips CM12 transmission electron microscope (Philips, Philips Electronics, NV).

Results

Correction efficiency as function of lipid to DNA charge ratio (+/-): DNA analysis

The lipid/DNA ratios, based on charge ratio, were optimized using gel electrophoresis [1820]. Complete neutralization of the negative DNA charge was achieved at a lipid to DNA charge ratio (+/-) of 2.2/1. A number of different lipid/DNA ratios were used to transfect (ΔF508/ΔF508) CFBE41o- cells with wild-type 491 bp fragment. Fig. 2A shows allele-specific PCR analysis as a function varying the lipid/DNA ratio. A faint 97-bp amplification product, corresponding to the wild-type allele was evident at the highest lipid/DNA ratio. A more intense wild-type specific band was detectable up to 2.2+/1- ratio. The autoradiographic signal of the 97-bp band increased in intensity as the amount of DNA fragment in the lipid/DNA complex increased. Consequently, the overall charge of the lipid/DNA complex became less positive. However, when the charge of the complex was neutral, i.e. 1+/1-, the wild-type was not detectable. Densitometric analysis indicates that the relative signal of the wild-type band was maximal at a lipid /DNA charge ratio of 6+/1- (Fig. 2B). Thus, it appears the optimal Gene Porter/DNA fragment charge ratio of 6+/1- for SFHR-mediated replacement of ΔF508-CFTR in CFBE41o- cells.
Figure 2

DNA analysis performed on CFBE41o- transfected cells harvested 120 hrs after transfection. (A) PCR analysis of wild-type (WT) and ΔF508 alleles as a function of lipid to DNA charge ratios in CFBE41o- cells. Replacement was indicated by the presence of the WT-allele for lipid/DNA ratios ranging from 42+/1- to 1+/1- corresponding to lanes from 1 to 7. DNA from untrasfected cells was amplified in lane 8 as negative control; (B) Densitometric analysis revealed that the maximum correction efficiency is reached with a ratio of lipid/DNA 6+/1-. No correction was observed at 1+/1- ratio.

SFHR-mediated gene modification was further characterised in wild-type cells (16HBE14o-) transfected with the ΔF508-CFTR DNA fragment (488-bp) in a lipid complex as described above. The subsequent PCR and radiographic analysis of the wild-type and ΔF508-CFTR alleles is presented in Fig. 3. A faint 94-bp, ΔF508-specific, amplification product could be detected at lipid/DNA charge ratio of 4.2+/1-. However, the 94-bp band with the greatest relative intensity was observed at a lipid/DNA ratio of 2.2+/1-. Densitometric analysis indicated that the amount of wild-type and ΔF508 product were equivalent (Fig. 3B). This result was supported by allele specific reverse-dot blot analysis of CFTR exon 10 (data not shown).
Figure 3

Analysis of DNA from 16HBE14o- transfected cells. (A) PCR analysis of wild-type (WT) and ΔF508 alleles as a function of lipid to DNA charge ratios in 16HBE14o- cells transfected with the ΔF508 DNA fragment. Replacement was indicated by the presence of the ΔF-allele after transfection at lipid to DNA ratios ranging from 42+/1- to 1+/1- (lanes from 1 to 7). DNA from untrasfected cells was amplified in lane 8 as negative control; (B) Densitometric analysis revealed that the maximum correction efficiency is reached with a lipid/DNA ratio of 2.2+/1-. With this cell line no correction was observed at ratios of 42+/1-, 12+/1-, 6+/1-and 1+/1-.

Correction efficiency as function of lipid to DNA charge ratio (+/-): RNA analysis

CFBE41o- cells showed expression of the normal allele in a pattern similar to that observed for the relative DNA levels of the wild-type allele (Fig. 4A). However, the SFHR-modified wild-type allele is expressed at the levels much lower than the endogenous mutant allele (ΔF508), as shown by densitometric analysis revealing that the maximum correction efficiency in CFBE41o- is reached with a lipid/DNA ratio of 6+/1- (Fig. 4B).
Figure 4

Analysis of RNA from CFBE41o- (A, B) and 16HBE14o- (C, D) transfected cells at different lipid/DNA ratios and harvested 120 hrs after transfection. Lanes 1-7 correspond to lipid/DNA charge ratios ranging from 42+/1- to 1+/1-. Lane 8 is RNA analysis of untransfected cells (A, C). The expression of the recombinant allele was detected in lanes 1 to 6 in (A) and in lane 6 only in (C). Densitometric analysis revealed that the maximum correction efficiency in CFBE41o- is reached with a lipid/DNA ratio of 6+/1- (B), whereas in 16HBE14o- recombinant allele is expressed only at 2.2/1 charge ratio (+/-) as reported in (D).

Similar results were obtained for the 16HBE14o- cells transfected with the ΔF508 DNA fragment (Fig. 4C). Transcription of the ΔF508 mutant allele was only detectable at a lipid/DNA ratio of 2.2+/1- (Fig. 4C/D), corresponding to the maximum correction efficiency observable in genomic DNA (Fig. 3A/B).

Analysis of targeted replacement at different times after transfection with small DNA fragments

The stability of the SFHR-mediated exchange after exposure to the lipoplexes was evaluated to determine the effective detectability of SFHR-mediated homologous replacement as a function of time. Cells were transfected at the optimal lipid/DNA charge ratio for each cell line (6+/1- and 2.2+/1- for CFBE41o- and 16HBE14o-, respectively) and harvested at 24 h, 48 h, 72 h, 96 h and 120 h after termination of the lipoplex incubation. Analysis of the DNA from transfected CFBE41o- cells indicates the greatest degree of SFHR-mediated replacement 24 h after transfection (Fig. 5A). SFHR-mediated homologous replacement continued to be detectable up to 11 days post transfection in CFBE41o- cell (data not shown). No apparent signal was detected when cells were harvested at 16, 21, and 30 days following transfection (data not shown). It has to be noted that the intensity values between densitometric analysis results in fig 2B (lane 3) and fig. 5B (lane 5) are different. The experiments were repeatead twice and the results come out from arithmetic mean. These results could be explained by the polyploid status of the cell line used for transfections. Thus, the fragment can recombine in more CFTR loci. The highest level of SFHR-mediated exchange in 16HBE14o- cells was observed at 48 h and then again at 120 h post transfection (Fig. 5B).
Figure 5

Analysis of DNA from CFBE41o- (A) and 16HBE14o- (C) transfected cells at optimal lipid/DNA charge ratio (6+/1- and 2.2+/1- respectively) and harvested at 24 h (lane1), 48 h (lane2), 72 h (lane 3), 96 h (lane 4) and 120 h (lane 5) after transfection. Lane 6 corresponds to untransfected cells. Densitometric analysis revealed that the maximum correction efficiency in CFBE41o- is reached at 24 h after transfection (B), while in 16HBE14o- at 48 h and again at 120 h after transfection (D).

TEM analysis of lipoplex-cell interactions

The intracellular route that the DNA fragments take to traffic to the cell nucleus was monitored using TEM and lipid/gold-labelled DNA complexes at different charge ratios (+/-). Cells were fixed and observed at different times after the start of transfection ranging from 5 h to 96 h (Fig. 6,7,8,9). In cells treated at the optimal lipid/DNA charge ratio complexes (6+/1-), an endocytotic-like pattern of internalization was observed (Fig. 6B,6C). Nevertheless, DNA/lipid complexes were never observed in coated pits, suggesting that the internalization of the complexes was not achieved through receptor-mediated endocytosis (Fig 6B,6C).
Figure 6

Transmission EM of CFBE41o- cells transfected at the optimal lipid/DNA ratio (6+/1-) and fixed 5 h after the start of transfection. (A) gold-labelled DNA complex; (B) labelled complexes interacting with cell membrane; (C) a detail of B at higher magnification. ee: early endosome. Arrows indicate endocytosis of the lipid/DNA complex. Bars: 200 nm.

Figure 7

Transmission EM of CFBE41o- cells transfected at the optimal lipid/DNA ratio (6+/1-) and fixed 72 h after the start of transfection. (A)-(C) large membrane-bound vesicles containing aggregates of labelled complexes in the perinuclear region of transfected cells. Destabilization of an early endosome (D), late endosome (E) and membrane-bound vesicles (F and G) by lipid/DNA complexes; (G) a higher magnification of (F). Arrows indicate a part of the aggregated complexes extruded into the cytoplasm and not surrounded by an endosome or a large vesicle membrane. ee: early endosome; g: Golgi apparatus; le: late endosome; mbv: membrane-bound vesicle; ly: lysosome; n: nucleus. Bars: (A)-(C): 1 μm; (D)-(G)): 200 nm.

Figure 8

Transmission EM of CFBE41o- cells transfected at the (6+/1-) lipid/DNA ratio and fixed 96 h after the start of transfection. (A)-(C) Large vesicles filled with labelled complexes in the cytoplasm of a transfected cell; (C) a higher magnification of (B). Arrows indicate a fusion site between a large vesicle and a lysosome. (D)-(F) labelled membranous body and lysosome in the cytoplasm of a transfected cell; (F) a higher magnification of a membranous body, in which the lipid/DNA complexes appeared partially degraded. ly: lysosome; mb: membranous body; mbv: membrane-bound vesicles. Bars: (A)-(E): 300 nm; (F): 100 nm.

Figure 9

Transmission EM of CFBE41o- cells transfected at a lipid/DNA ratio having no transfection activity (1+/1-). Cells were fixed at 5 h (A and B) and at 72 h (C and E) after the start of transfection. (A) and (B) show labelled complexes adhering to the cellular membrane; (B) is a higher magnification of (A). Arrows indicate sites at the plasma membrane that appear to be destabilised by the adhering complex. (C)-(E) show a labelled lysosome in a transfected cell; (E) is at high magnification. In (E) the lipid/DNA complexes, adhering to the lysosome membrane, appear to be free within the cytoplasm (arrowhead). ly: lysosome. Bars: (A), (C), (D), (E): 300 nm; (B): 100 nm.

The complexes appeared as structures around gold-labelled DNA (Fig. 6A). Some endosomes containing the complexes were near the cell surface suggesting that these were early endosomes (Fig. 6C). With an increase in the time of exposure to the transfection complexes, the endosomes appeared to move towards the perinuclear region. Late endosomes fused together to generate large membrane-bound vesicles containing aggregates of labelled complexes (Fig 7A,7B,7C). As shown in Fig. 7D,7E,7F,7G the DNA lipid complexes seemed to destabilize both endosomes and large membrane-bound vesicles. It should be noted that the destabilization site along the progression of the endosome to large vesicle seemed to be preferentially near the Golgi apparatus and the vesicular compartment of endoplasmic reticulum (Fig 7F,7G). These observations suggest that the DNA-liposomes complexes might be released into the cytoplasm by destabilizing either the endosome and large vesicle membrane and that the endoplasmic reticulum may be involved in the transport of free DNA towards the nucleus. Occasionally, gold labelled electron-dense material, apparently not bound to liposome structures, was observed near the ER and near the nuclear pores (data not shown). Free gold labelling was never observed in the nucleus. This may be due to the fact that, because of the size of the DNA fragments, not all the DNA was gold labeled. Consequently, our inability to observe free gold labeled DNA in the nucleus might reflect that very little DNA (gold labeled and unlabeled) escaped from the endosome and that the sensitivity of electron microscopy is not high enough to detect it. Alternatively, it is possible that, during the delivery of the DNA fragments from the complexes, some of the gold labelling was removed. At 96 hrs after the start of transfection, very large vesicles filled with gold-labelled complexes were observed (Fig 8A,8B,8C). Furthermore, large membranous bodies showing a regular lamellar pattern, similar to those described previously [21], were frequently observed (Fig 8D,8E). Of note is that the multilamellar packed structure of complexes that was still visible in the large cytoplasmic vesicles (Fig 8C), whereas in the large membranous bodies and apparent lysosomes the liposome complexes were not distinguishable (Fig 8E,8F). One possible explanation for this observation is that continued cellular exposure to the liposomes/DNA complexes results in their accumulation in large cytoplasmic vesicles. When the complexes in these vesicles exceed a critical concentration, the vesicles could neither fuse with lysosomes (Fig. 8C) and result in degradation of the complexes inside the large membranous bodies.

TEM analysis of cells treated with lipid/ DNA ratios that showed no SFHR-mediated modification showed labelled complexes adhering to the cytoplasmic membrane of a small number of cells (Fig. 9A). These complexes were never observed inside endosomes. Furthermore, in some cases the adherent complexes seemed to destabilize, the cell membrane (arrows in Fig. 9B). Both observations suggest that these lipid/DNA complexes penetrated the cell by a fusion mechanism. At these charge ratios, gold labelling was observed almost exclusively around and inside lysosomes (Fig. 9C,9D), and labelled complexes were never observed in late endosomes or large vesicles. These observations suggest that when lipid/DNA complexes enter the cell via a fusion mechanism, they are immediately digested by lysosomes. Thus, the entry of lipid/DNA complexes via an endocytic mechanism seems to be a requirement for the release of the DNA from the lipoplexes and transport into the nucleus. Controls were monitored in which labelled fragments, not complexed with lipid, were transfected for testing labelling toxicity. No fragments were seen inside cells (data not shown).

Discussion

SFHR-mediated gene targeting has been used to correct a specific CFTR mutation, in the 3-bp ΔF508 deletion [7, 10]. Recently, this strategy was successfully employed to correct a nonsense mutation in the dystrophin (dys) locus of the mdx mouse both in vitro and in vivo[22]. Previous studies have also shown that DNA fragments can be delivered to the lung by lipid vehicles. In this study, SFHR-mediated correction was detected up to seven days at mRNA level within lung and lower airways, suggesting its therapeutic potential within this organ [9].

These previous studies results suggest that SFHR has therapeutic potential for treatment of inherited disorders. However, to enhance this therapeutic potential, transfection conditions need to be optimized. This can, in part, be achieved by analysis of the cellular and molecular mechanisms that underlie transport of the therapeutic fragments to the nucleus. One of the necessary conditions to achieve therapeutically relevant SFHR-repair efficiencies is a careful optimization of delivery methodologies to overcome both extracellular and intracellular barriers that preclude the nuclear localization of the small fragments.

In fact, a major hurdle of gene therapy is the limited nuclear uptake of intact therapeutic DNA that inhibits its full performance [21].

The lipid/DNA ratio appears to be an important factor influencing the success of transfection [18, 23, 24]. The results of the studies presented here indicate that the lipid/DNA charge ratios for optimal SFHR-mediated modification are cell line dependent. A molar charge ratio of 2.2 (+)/1(-) and 6 (+)/1(-) for the wild-type (16HBE14o-) and the mutant (CFBE41o-) cell lines, respectively, was found to be optimal for SFHR when assessed by PCR. When the amount of lipid was held constant and the amount of DNA was increased, a more negatively charged lipid/DNA complex was formed. While increasing the amount of DNA in the lipoplexes, SFHR-mediated modification was observed to progressively decrease until it was undetectable (up to 30 μg of fragment). These findings indicate that the amount of DNA is not rate limiting in itself, but rather that the reduction in positive charge caused by an increase in DNA within the lipoplexes, impacts SFHR-mediated modification. This effect on SFHR was clearly cell line dependent and appears to be associated with the transport of the DNA to the nucleus. Alternatively, it can not be ruled out that the increased amount of DNA in negatively charge lipid/DNA complexes might competitively inhibit the enzymatic processes that leads to DNA uptake and/or SFHR. If the enzymatic pathways are saturated with DNA fragments they might not be as effective at mediating exchange. This will require further analysis in a future study.

Knowledge of the internalization mechanism and intracellular fate of lipoplexes is a prerequisite for the further development of efficient SFHR-based gene repair protocols. TEM analysis demonstrated that the lipoplexes enter cells via different mechanisms that depend on the lipid/DNA charge ratio. At a more negative charge ratio, lipoplexes enter into cells via a fusion pathway. Complexes that enter the cell via fusion with the plasma membrane appear not to enter the nucleus to mediate SFHR as is implied by the apparent lack of correction detected by molecular analysis. These results are consistent with previous work investigating the role of helper lipid in the assembly [18] and destabilization [23] of lipoplexes, and in the finding that lipid can inhibit SFHR-mediated modification of mutant plasmids after transient transfection [24].

The TEM analysis also demonstrated that lipoplexes with the appropriate charge could be taken up in endosomes within 5 h after initiation of transfection and become associated with the nucleus within 72 h. This endocytic uptake mechanism for the lipoplex appears to be distinct from that involving fusion with the plasma membrane, but also dependent on the lipoplex charge. As the lipoplex molar charge ratio becomes more positively charged, the lipoplexes appear to enter the cells via an endocytic pathway. It is this pathway that appears to be more effective at transferring DNA to the nucleus and mediating SFHR. Therefore, strategies that enhance endosome disruption might further improve delivery to the nucleus and thus potentiate SFHR-mediated modification. These include incorporation of synthetic virus-derived "fusogen" into the lipid complex [25, 26], the introduction of membrane destabilizing peptides into DNA/poly-lysine conjugates [27], transfection in the presence of inactivated adenovirus [28, 29] as well as treatment of the cells with agents that enhance endosome lysis such as chloroquine and glycerol [3032].

SFHR-mediated DNA modification was detected within the population of transfected cells for at least 120 hours post-transfection. Analysis of the transfected CFBE41o- cells showed the 3-bp insertion at 11 days post-transfection. However, at 30 days, the insertion was no longer apparent. Recent studies in which the mixed population of transfected cells was sorted into isogenic cell lines have indicated that subpopulations of corrected cells exist within the larger population, albeit at a frequency that is detectable by allele-specific PCR [33]. Thus, it does appear that SFHR-mediated modification of CFBE41o- cells is stable over time, but the proportion of corrected cell is reduced, leading to dilution of the signal because of the passing of time.

Conclusions

These studies demonstrate that the efficacy of lipid assisted SFHR-mediated modification appears to be cell line-dependent. Different charge ratios were optimal for SFHR-mediated targeting when comparing CFBE41o- cells to 16HBE14o- cells. This suggests that, as yet undefined, intracellular factors influence lipid-facilitated SFHR-mediated modification. The data are also consistent with previous observations that the efficiency of cationic lipid-mediated transfection varies with different cell types [18, 34, 35]. This issue will be particularly relevant to the selection of the delivery vehicles for SFHR in vitro and in vivo[9, 22].

While recent studies demonstrated that SFHR delivery can be achieved in vivo in the mouse lung [9] and muscle [22], there are still questions that need to be answered before SFHR can be applied therapeutically. Although it is difficult to extrapolate conditions and optimal delivery vehicle formulations from in vitro experiments to in vivo, these studies on human airway epithelial cell lines provide insights into therapeutic application of SFHR in human airways. In the context of a reliable assay system these cell systems, can be useful for elucidating those conditions that will optimize SFHR in the airways [18, 24].

Declarations

Acknowledgements

This work was supported by Ministero della Sanità and Regione Lazio Fondo Sanitario Nazionale per la Prevenzione e la Cura della Fibrosi Cistica (Legge 23 dicembre 1993, n.548), NIDDK 46002, 47766, CFF, CFRI and PACFI.

Authors’ Affiliations

(1)
Department of Biopathology, Human Genetics Unit, Tor Vergata University of Rome
(2)
Department of Medicine, Human Molecular Genetics Unit, University of Vermont
(3)
Institute of Experimental Medicine, CNR
(4)
Azienda Ospedaliera Universitaria Policlinico Tor Vergata

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  36. Pre-publication history

    1. The pre-publication history for this paper can be accessed here:http://www.biomedcentral.com/1471-2350/3/8/prepub

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