Diolistic labeling of neuronal cultures and intact tissue using a hand-held gene gun

Diolistic labeling is a highly efficient method for introducing dyes into cells using biolistic techniques. The use of lipophilic carbocyanine dyes, combined with particle-mediated biolistic delivery using a hand-held gene gun, allows non-toxic labeling of multiple cells in both living and fixed tissue. The technique is rapid (labeled cells can be visualized in minutes) and technically undemanding. Here, we provide a detailed protocol for diolistic labeling of cultured human embryonic kidney 293 cells and whole brain using a hand-held gene gun. There are four major steps: (i) coating gold microcarriers with one or more dyes; (ii) transferring the microcarriers into a cartridge to make a bullet; (iii) preparation of cells or intact tissue; and (iv) firing the microcarriers into cells or tissue. The method can be readily adapted to other cell types and tissues. This protocol can be completed in less than 1 h.     

Transient gene expression in HEK293 and vero cells immobilised on microcarriers

The upscale of transient gene expression (TGE) gained popularity over the last decade as it drastically shortens timelines for the production of recombinant proteins. Bottlenecks of the method turned out to be media composition and media exchange, which is usually required as conditioned medium drastically reduces the transfection efficiency. Media exchanges are typically done by centrifugation, which limits upscale, is prone to contamination or is a high cost factor when continuous centrifuges are used. In this work HEK/EBNA cells were grown and transfected on microcarriers. Cell immobilisation allows easy media exchange after sedimentation. The transfection method was optimised regarding polyethylenimine (PEI) concentration, optimal DNA:PEI ratio, type of PEI, incubation time and polyplex formation time. In addition to HEK, Vero cells were also transfected using the same protocol. The method was established in spinner flasks and scaled up to a 1.5 litre stirred tank reactor. Transfection efficiencies of up to 33% with pCEP4 and 98% with pMAX were reached. Additionally immobilisation on microcarriers was used to retain the cells during cultivation, thus allowing media replacement and prolonging cultivation time from one to two weeks with continuous expression of the recombinant protein.     

Highly efficient transfection of mammalian cells by electric field pulses. Application to large volumes of cell culture by using a flow system.

We have transfected mammalian cells with plasmid DNA by application of electric pulses. Chinese hamster ovary cells were chosen as a model in order to study and to optimize the transfection protocol. A plasmid carrying the gene coding for beta-galactosidase activity was used to determine transient expression of the electrotransferred activity at the cell level. Optimum transient expression for cells in suspension was obtained by application of 10 square wave pulses of 5-ms duration and 0.6-kV/cm intensity. Under the best conditions, transfection frequencies as high as 50-60% could be obtained and appeared to be highly dependent on the age of the cell culture. The method was applicable to plated cells growing in a petri dish or on microcarriers. The possibility of extension of the technique to large volumes of cells is presented. A flow system, composed of a peristaltic pump connected to the electropulser chamber, allowed large volumes of cells to be treated with flow rates in the order of several milliliters/minute. Transfection frequencies for the large volumes were 25% for cells in suspension and 35% for cells on microcarriers. These results open new perspectives in large-scale transfection technology of cells however they are grown.     

In vivo single-cell electroporation for transfer of DNA and macromolecules

Single-cell electroporation allows transfection of plasmid DNA or macromolecules into individual living cells using modified patch electrodes and common electrophysiological equipment. This protocol is optimized for rapid in vivo electroporation of Xenopus laevis tadpole brains with DNA, dextrans, morpholinos and combinations thereof. Experienced users can electroporate roughly 40 tadpoles per hour. The technique can be adapted for use with other charged transfer materials and in other systems and tissues where cells can be targeted with a micropipette. Under visual guidance, an electrode filled with transfer material is placed in a cell body-rich area of the tadpole brain and a train of voltage pulses applied, which electroporates a nearby cell. We show examples of successfully electroporated single cells, instances of common problems and troubleshooting suggestions. Single-cell electroporation is an affordable method to fluorescently label and genetically manipulate individual cells. This powerful technique enables observation of single cells in an otherwise normal environment.     

A rapid method to monitor DNA precipitation onto microcarriers before particle bombardment

The binding or precipitation of DNA onto gold or tungsten microcarriers represents one of the most crucial steps for gene transfer via the particle bombardment process. We have developed a simple and rapid method to monitor DNA precipitation onto microcarriers before delivery to intact cells or tissues. Binding of DNA constructs to different microcarriers was evaluated with relative fluorescence values using a dedicated fluorometer. Significantly greater precipitation was detected using gold vs. tungsten microcarriers. Addition of glycerol resulted in a 46% increase in precipitation. A 42% difference in precipitation was observed using two different brands of polyproplyene tubes. Fluorescence values dropped 10–50% 3 hr after initial precipitation. Fluorescence values were correlated with the number of transient GUS transformants of rice (Oryza sativa, L.) cells. Precipitation with PEG gave higher fluorescent values and GUS transformants than a similar method without PEG. Results from these experiments indicate that fluorescence measurements are an effective and rapid method to monitor DNA precipitation for particle bombardment experiments.Communicated by C. Quiros     

Highly Efficient Transfection of Human THP-1 Macrophages by Nucleofection

Macrophages, as key players of the innate immune response, are at the focus of research dealing with tissue homeostasis or various pathologies. Transfection with siRNA and plasmid DNA is an efficient tool for studying their function, but transfection of macrophages is not a trivial matter. Although many different approaches for transfection of eukaryotic cells are available, only few allow reliable and efficient transfection of macrophages, but reduced cell vitality and severely altered cell behavior like diminished capability for differentiation or polarization are frequently observed. Therefore a transfection protocol is required that is capable of transferring siRNA and plasmid DNA into macrophages without causing serious side-effects thus allowing the investigation of the effect of the siRNA or plasmid in the context of normal cell behavior. The protocol presented here provides a method for reliably and efficiently transfecting human THP-1 macrophages and monocytes with high cell vitality, high transfection efficiency, and minimal effects on cell behavior. This approach is based on Nucleofection and the protocol has been optimized to maintain maximum capability for cell activation after transfection. The protocol is adequate for adherent cells after detachment as well as cells in suspension, and can be used for small to medium sample numbers. Thus, the method presented is useful for investigating gene regulatory effects during macrophage differentiation and polarization. Apart from presenting results characterizing macrophages transfected according to this protocol in comparison to an alternative chemical method, the impact of cell culture medium selection after transfection on cell behavior is also discussed. The presented data indicate the importance of validating the selection for different experimental settings.     

Gene printer: laser-scanning targeted transfection of cultured cardiac neonatal rat cells

Heterogeneous gene expression in cardiac cells and tissues which requires targeted delivery of foreign DNA into selected cells or regions is needed for the development of novel therapies. Several techniques have been employed for targeted transfection, such as direct microinjection into cells or targeted electroporation. However, these techniques have limited bandwidth or spatial resolution of transfection. We aimed to develop a method for transfection of cardiac cells by means of laser-assisted optoporation using a standard confocal microscope. This technique allows for the transfection of selected cell types in the presence of other cell types as long as they are distinguishable with a microscope. This technique can work as a “gene printer” creating arbitrarily shaped areas of transfected cells.     

Generation of magnetic nonviral gene transfer agents and magnetofection in vitro

This protocol details how to design and conduct experiments to deliver nucleic acids to adherent and suspension cell cultures in vitro by magnetic force-assisted transfection using self-assembled complexes of nucleic acids and cationic lipids or polymers (nonviral gene vectors), which are associated with magnetic (nano) particles. These magnetic complexes are sedimented onto the surface of the cells to be transfected within minutes by the application of a magnetic gradient field. As the diffusion barrier to nucleic acid delivery is overcome, the full vector dose is targeted to the cell surface and transfection is synchronized. In this manner, the transfection process is accelerated and transfection efficiencies can be improved up to several 1,000-fold compared with transfections carried out with nonmagnetic gene vectors. This protocol describes how to accomplish the following stages: synthesis of magnetic nanoparticles for magnetofection; testing the association of DNA with the magnetic components of the transfection complex; preparation of magnetic lipoplexes and polyplexes; magnetofection; and data processing. The synthesis and characterization of magnetic nanoparticles can be accomplished within 3-5 d. Cell culture and transfection is then estimated to take 3 d. Transfected gene expression analysis, cell viability assays and calibration will probably take a few hours. This protocol can be used for cells that are difficult to transfect, such as primary cells, and may also be applied to viral nucleic acid delivery. With only minor alterations, this protocol can also be useful for magnetic cell labeling for cell tracking studies and, as it is, will be useful for screening vector compositions and novel magnetic nanoparticle preparations for optimized transfection efficiency in any cell type.     

Isolation of circular yeast artificial chromosomes for synthetic biology and functional genomics studies

Circular yeast artificial chromosomes (YACs) provide significant advantages for cloning and manipulating large segments of genomic DNA in Saccharomyces cerevisiae. However, it has been difficult to exploit these advantages, because circular YACs are difficult to isolate and purify. Here we describe a method for purification of large circular YACs that is more reliable compared with previously described protocols. This method has been used to purify YACs up to 600 kb in size. The purified YAC DNA is suitable for restriction enzyme digestion, DNA sequencing and functional studies. For example, YACs carrying full-size genes can be purified from yeast and used for transfection into mammalian cells or for the construction of a synthetic genome that can be used to produce a synthetic cell. This method for isolating high-quality YAC DNA in microgram quantities should be valuable for functional and synthetic genomic studies. The entire protocol takes ～3 d to complete.     

An improved method for routine preparation of intact artificial chromosome DNA (340-1000 kb) for transfection into human cells

The transfer of high molecular weight (HMW) DNA into mammalian cells is an important strategy for assessing human gene expression and chromosome structure and function. However, using current methods, it is difficult to dependably prepare intact HMW DNA because of the susceptibility of the DNA to degradation and physical shearing. Here we describe a strategy whereby intact artificial chromosome DNA (as large as 1 Mb) can be routinely prepared from yeast. Strict adherence to this protocol has resulted in: (i) >90% of liquid DNA preparations containing largely intact DNA; (ii) transfection efficiencies for the development of stable human clonal cell lines ranging from 5 x 10(-7) to 8.8 x 10(-5); and (iii) the presence of markers from both YAC arms in 30-42% of the human fibrosarcoma cell HT1080 clones and 100% of the CF lung epithelial cell lines IB3-1 and CFT1 clones, suggesting that the HMW DNA is potentially intact in a substantial proportion of clones. Using this protocol for DNA preparation, successful transfection of functional 1 Mb human artificial chromosome DNA into human cells has also been achieved. This methodology should prove useful to those interested in using HMW human DNA for gene expression and functional analysis or for linear artificial chromosome construction, since integrity is absolutely critical for the success of these studies.     

Enhancement and optimization of plasmid expression in femtosecond optical transfection

Cell transfection using femtosecond lasers is gaining importance for its proven ability to achieve selective transfection in a sterile and relatively non‐invasive manner. However, the net efficiency of this technique is limited due to a number of factors that ultimately makes it difficult to be used as a viable and widely used technique. We report here a method to achieve significant enhancement in the efficiency of femtosecond optical transfection. The transfection procedure is modified by incorporating a suitable synthetic peptide containing nuclear localization and DNA binding sequences, assisting DNA import into the nucleus. We achieved a 3‐fold enhancement in the transfection efficiency for adherent Chinese Hamster Ovary (CHO‐K1) cells with this modified protocol. Further, in the presence of this biochemical reagent, we were able to reduce the required plasmid concentration by ～70% without compromising the transfection efficiency. Also, we report for the first time the successful photo‐transfection of recently trypsinised cells with significantly high transfection efficiency when transfected with modified plasmid. This paves the way for the development of high throughput microfluidic optical transfection devices. (© 2011 WILEY‐VCH Verlag GmbH & Co. KGaA, Weinheim)     

Transfecting human neural stem cells with the Amaxa Nucleofector

Transfection of primary mammalian neural cells, such as human neural stem/precursor cells (hNSPCs), with commonly used cationic lipid transfection reagents has often resulted in poor cell viability and low transfection efficiency. Other mechanical methods of introducing a gene of interest, such as a "gene gun" or microinjection, are also limited by poor cell viability and low numbers of transfected cells. The strategy of using viral constructs to introduce an exogenous gene into primary cells has been constrained by both the amount of time and labor required to create viral vectors and potential safety concerns. We describe here a step-by-step protocol for transfecting hNSPCs using Amaxa's Nucleofector device and technology with electrical current parameters and buffer solutions specifically optimized for transfecting neural stem cells. Using this protocol, we have achieved initial transfection efficiencies of ~35% and ~70% after stable transfection. The protocol entails combining a high number of hNSPCs with the DNA to be transfected in the appropriate buffer followed by electroporation with the Nucleofector device.     

A simple and rapid nonviral approach to efficiently transfect primary tissue-derived cells using polyethylenimine

This protocol outlines steps for optimizing the transfection of adherent primary mammalian cells using the readily available off-the-shelf cationic polymer, 25-kDa branched polyethylenimine (bPEI25). Transfection efficiency of cationic polymers varies among cell lines and is highly dependent on the conditions and environment in which complexes are formed. Factors requiring optimization include the salt concentration, volume, incubation time, mixing order and ratio of polymer to DNA. In this transfection protocol, complexes are prepared in 30 min, with analysis 24 h later; thus, experiments can be completed in 2 d. In this protocol, as an example, we describe the parameters we have optimized for the transfection of bone marrow stromal cells and normal human foreskin fibroblasts. By using this protocol, we have obtained transfection efficiencies comparable to lipofection. An appropriately optimized protocol enhances the utility of cationic polymers in transfecting mammalian cells, thereby providing an effective alternative to expensive commercial reagents.     

High efficiency,Site-specific Transfection of Adherent Cells with siRNA Using Microelectrode Arrays (MEA)

The discovery of RNAi pathway in eukaryotes and the subsequent development of RNAi agents, such as siRNA and shRNA, have achieved a potent method for silencing specific genes^1-8 for functional genomics and therapeutics. A major challenge involved in RNAi based studies is the delivery of RNAi agents to targeted cells. Traditional non-viral delivery techniques, such as bulk electroporation and chemical transfection methods often lack the necessary spatial control over delivery and afford poor transfection efficiencies^9-12. Recent advances in chemical transfection methods such as cationic lipids, cationic polymers and nanoparticles have resulted in highly enhanced transfection efficiencies¹³. However, these techniques still fail to offer precise spatial control over delivery that can immensely benefit miniaturized high-throughput technologies, single cell studies and investigation of cell-cell interactions. Recent technological advances in gene delivery have enabled high-throughput transfection of adherent cells^14-23, a majority of which use microscale electroporation. Microscale electroporation offers precise spatio-temporal control over delivery (up to single cells) and has been shown to achieve high efficiencies^{19, 24-26}. Additionally, electroporation based approaches do not require a prolonged period of incubation (typically 4 hours) with siRNA and DNA complexes as necessary in chemical based transfection methods and lead to direct entry of naked siRNA and DNA molecules into the cell cytoplasm. As a consequence gene expression can be achieved as early as six hours after transfection²⁷. Our lab has previously demonstrated the use of microelectrode arrays (MEA) for site-specific transfection in adherent mammalian cell cultures^17-19. In the MEA based approach, delivery of genetic payload is achieved via localized micro-scale electroporation of cells. An application of electric pulse to selected electrodes generates local electric field that leads to electroporation of cells present in the region of the stimulated electrodes. The independent control of the micro-electrodes provides spatial and temporal control over transfection and also enables multiple transfection based experiments to be performed on the same culture increasing the experimental throughput and reducing culture-to-culture variability. Here we describe the experimental setup and the protocol for targeted transfection of adherent HeLa cells with a fluorescently tagged scrambled sequence siRNA using electroporation. The same protocol can also be used for transfection of plasmid vectors. Additionally, the protocol described here can be easily extended to a variety of mammalian cell lines with minor modifications. Commercial availability of MEAs with both pre-defined and custom electrode patterns make this technique accessible to most research labs with basic cell culture equipment.     

Selection of microcarrier diameter for the cultivation of mammalian cells on microcarriers

The kinetics of mammalian cell growth in a microcarrier culture are affected by the distribution of cells on microcarriers. It has been shown previously that a critical cell number per microcarrier is required for the growth of FS-4 cells on microcarriers. It is advantageous to alter the cell distribution on microcarriers to allow for a larger fraction of microcarriers to acquire enough cells to initiate normal growth. This can be achieved by selecting the diameter of the microcarriers employed. It has also been shown previously that the critical cell number could be reduced by choosing a better culture medium to support low density growth. However, even if all cells inoculated into a culture are capable of growing to confluence, it is still necessary to select the microcarrier diameter ration ally to improve the growth kinetics. The method of selecting the microcarrier diameter is discussed. By employing a improved medium as well as using microcarriers of selected diameter, the multiplication ratio was in creased to 15- to 16-fold for FS-4 cells, as opposed to 3- to 4-fold typically obtained in a batch culture.     

Electroporation optimization to deliver plasmid DNA into dental follicle cells

Electroporation is a simple and versatile approach for DNA transfer but needs to be optimized for specific cells. We conducted square wave electroporation experiments for rat dental follicle cells under various conditions. These experiments indicated that the optimal electroporation electric field strength was 375 V/cm, and that plasmid concentrations greater than 0.18 μg/μL were required to achieve high transfection efficiency. BSA or fetal bovine serum in the pulsing buffer significantly improved cell survival and increased the number of transfected cells. The optimal pulsing duration was in the range of 45–120 ms at 375 V/cm. This electroporation protocol can be used to deliver DNA into dental follicle cells to study the roles of candidate genes in regulating tooth eruption. This is the first report showing the transfection of dental follicle cells using electroporation. The parameters determined in this study are likely to be applied to transfection of other fibroblast cells.     

High level transient expression of a chloramphenicol acetyl transferase gene by DEAE-dextran mediated DNA transfection coupled with a dimethyl sulfoxide or glycerol shock treatment.

Using a plasmid containing the bacterial chloramphenicol acetyl transferase gene, we have assayed for transient expression of DNA introduced into mouse L cells by a variety of transfection conditions. High efficiency uptake and expression of this foreign DNA have been achieved by modifying the DEAE dextran mediated transfection procedure of McCutchan and Pagano (1) to include a shock with either dimethyl sulfoxide or glycerol. Inclusion of the shock step can increase expression of the transfected gene a surprising approximately 50 fold. With plasmid constructs that do not replicate after transfection, we can readily detect CAT activity in an overnight autoradiographic exposure from less than 0.1% of an extract from a 60 mm dish of transfected cells. We have determined the amounts of DNA, the amount and time course of DEAE-dextran and dimethyl sulfoxide treatments, the effects of additional DNA, and the time after transfection which yield maximal expression. Overall, this transfection protocol using DEAE-dextran coupled to a shock treatment is simple, straightforward, and gives consistently high levels of expression of the input DNA.