The application of nanotechnology in biological research is beginning to have a major impact leading to the development of new types of tools for human health. One focus of nanobiotechnology is the development of nanoparticle-based formulations for use in drug or gene delivery systems. However most of the nano probes currently in use have varying levels of toxicity in cells or whole organisms and therefore are not suitable for in vivo application or long-term use. Here we test the potential of a novel silica based nanoparticle (organically modified silica, ORMOSIL) in living neurons within a whole organism. We show that feeding ORMOSIL nanoparticles to Drosophila has no effect on viability. ORMOSIL nanoparticles penetrate into living brains, neuronal cell bodies and axonal projections. In the neuronal cell body, nanoparticles are present in the cytoplasm, but not in the nucleus. Strikingly, incorporation of ORMOSIL nanoparticles into the brain did not induce aberrant neuronal death or interfered with normal neuronal processes. Our results in Drosophila indicate that these novel silica based nanoparticles are biocompatible and not toxic to whole organisms, and has potential for the development of long-term applications.
Citation: Barandeh F, Nguyen P-L, Kumar R, Iacobucci GJ, Kuznicki ML, Kosterman A, et al. (2012) Organically Modified Silica Nanoparticles Are Biocompatible and Can Be Targeted to Neurons In Vivo. PLoS ONE 7(1): e29424. https://doi.org/10.1371/journal.pone.0029424
Editor: Brian D. McCabe, Columbia University, United States of America
Received: February 3, 2011; Accepted: November 28, 2011; Published: January 3, 2012
Copyright: © 2012 Barandeh et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This work is supported by funds from the State University of New York at Buffalo and from John R. Oishei Foundation to SG. GJI and MK were funded by a fellowship from the Center for Undergraduate Research and Creative Activities (CURCA) from State University of New York (SUNY) at Buffalo. An award from the Julian Park Publication Fund (College of Arts and Sciences, SUNY at Buffalo) helped defray publication costs for this manuscript. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
The use of nanotechnology in biomedical research is expected to have a major impact on human welfare, due to the development of new types of diagnostic and therapeutic tools. However, the same properties that make nanoparticles so attractive for development in nanomedicine could also prove deleterious when nanoparticles interact with cells within a living organism. Indeed, there are a number of nano probes (quantum dots (QDs) , upconverting nanophosphors , and luminophore-containing nanoparticulate carriers such as liposomes , polymersomes  ceramic , , or polymeric  nanoparticles), which claim to be efficient theranostic tools for in vivo imaging and also have potential for use in therapeutic applications. However, many of these nano probes have long-term toxicity issues that dilute their efficiency for long-term use in vivo.
Recently, interest has generated in the use of new silica-based nanoparticles for imaging. Silica-based nanomaterials such as sol-gel, colloidal, mesoporous and organically modified silica (ORMOSIL) nanoparticles, have shown promising potential in biotechnological applications such as nanoprobes for actively targeted optical imaging , . These inert, optically transparent materials can be conjugated with any desired fluorophore (visible or NIR), leading to the generation of robust, fluorescent nanoparticles , . Furthermore, these nanoparticles are porous and have tunable pore size, so they can be incorporated with bioactive molecules such as enzymes, genetic materials, and chemotherapeutic drugs. They can also be tagged with a peptide for a specific biological function , , thus allowing targeting to specific cell types or tissues. In addition, the chemistry of silica provides the opportunity for a variety of surface functionalities (hydroxyl/amino/thiol/carboxyl groups, , ), which can be used to attach biotargeting molecules. Previously ORMOSIL nanoparticles conjugated with fluorophores and targeting ligands have been used in optical imaging of tumor cells in vitro , . These particles have also been tested for potential use in photodynamic therapy, and as targeted optical probes for imaging of pancreatic cancer cells in in vitro experiments , , . However, to date the biocompatibility, bio distribution and toxicity of ORMOSIL has not been tested in living organisms.
Drosophila melanogaster is an ideal model system to rapidly test novel nanoparticles that have potential therapeutic applicability for human diseases. The Drosophila genome is highly conserved when compared to higher organisms. Many homologous genes encoding proteins that cause human diseases have been identified . Many human neuronal disease models such as Alzheimer's disease, Huntington's disease and Parkinson's disease have also been developed in the fly . Furthermore, cellular and developmental mechanisms are extensively conserved between flies and humans. Thus studies on the uptake of new therapeutic agents and their lethality in Drosophila can be well correlated to mammalian systems. The developmental and behavioral aspects of Drosophila are also documented, thus making the fly an informative and adaptable model to investigate a wide variety of toxicological endpoints relevant to human biology. Recently, a number of powerful assay methods have been developed in Drosophila to test developmental and behavioral toxicology of potential therapeutic agents. Results from these tests have been used to prioritize further testing in rodents, and some of these agents have later been translated into human clinical trails , , .
Here we report the in vivo characterization of a novel silica based nanoparticle, ORMOSIL in Drosophila. We provide evidence that these nanoparticles are biocompatible and can be effectively used in living organisms for a long period of time. We show that these nanoparticles are not toxic to the developing organism and do not disrupt any major cellular functions. ORMOSIL nanoparticles readily incorporate into living neuronal cells. Incorporation of ORMOSIL does not activate aberrant neuronal death pathways, nor does it affect the long distance transport pathway (axonal transport), which is essential for the growth, maintenance and survival of all neurons. Taken together, our results suggest that ORMOSIL nanoparticles can be safely used in living neuronal tissues and in living organisms with minimal effects on normal cellular functions. This is the first study that thoroughly investigates the biocompatibility of this class of nanoparticles throughout an organism's development and in neuronal cells, which is an important consideration for these particles to be eventually translated into use in humans.
Physiochemical properties of ORMOSIL nanoparticles
To test the biocompatibility, bio distribution, and the eventual fate of ORMOSIL nanoparticles in vivo following systemic delivery, we used fluorescently conjugated ORMOSIL. We use both unconjugated and conjugated (receptor and peptide-conjugated) rhodamine-ORMOSIL nanoparticles (RORM). The synthesis of the RORM nanoparticles was adapted from our previous work with minor modifications , [ 26] and the nanoparticles were characterized by various methods as described in figure 1. Figure 1, shows the basic properties of RORM including its absorption and emission spectra. RORM emits at a typical emission band for rhodamine, which is λmax 600 nm (Figure 1A). The size distribution profile as measured by dynamic light scattering (DLS) method (Figure 1B) and transmission electron microscopy (TEM, Figure 1C) indicate that the diameter of RORM particles are on average 20 nm, much smaller than the average diameter of synaptic vesicles, which are on average about 40 nm . For receptor-conjugated RORM, we use the transferrin receptor (TfR, TfR-RORM). Transferrin bound TfR receptor is transported into the cell by endocytosis in a vesicle  and is the major route of cellular iron uptake. This cellular uptake pathway is currently being exploited for site-specific delivery of anticancer drugs and therapeutic genes into proliferating malignant cells . For peptide-conjugated RORM (peptide-RORM), we used 15aa of the C-terminus of the amyloid precursor protein (APP). APP transports a subclass of vesicles in the anterograde direction down the axon . Both conjugation strategies involved the use of simple Ethyl-3-(3-dimethylaminopropyl) carbodiimide (EDCI) chemistry using the functional amine groups present on the surface of RORM and carboxyl group of APP. Recent work has shown that 15aa of the C-terminus of APP is sufficient for APP to bind to the anterograde molecular motor for axonal transport . Both TfR-RORM and peptide-RORM particles have similar diameters as unconjugated RORM, and these particles resemble the size of biological vesicles. As a control for fluorescence and to see the applicability of ORMOSIL nanoparticles with different fluorophores, we tested cy5 conjugated ORMOSIL (cy5ORM, Figure S1, Table 1) and observe similar effects as RORM (see below). In addition, although in many of our experiments (Table 1) we have used cy5ORM we have focused on RORM as the main formulation.
(A) The absorption and emission spectra for rhodamine-ORMOSIL (RORM) particles. The typical emission band of rhodamine is λmax 600 nm. (B) The ORMOSIL nanoparticle size distribution profile as measured by the dynamic light scattering (DLS) method indicates that the diameter of ORMOSIL nanoparticles are on average 20 nm. (C) A transmission electron microscope (TEM) image of ORMOSIL nanoparticles. Bar = 100 nm.
Drosophila development is not affected by ORMOSIL particles
To test the biocompatibility of ORMOSIL in a living organism, we used Drosophila as a model system. Because of its rapid life cycle and relatively low maintenance costs, Drosophila provides us with an ideal system to test initial toxicological effects and obtain dosage information for potential new therapeutic agents. We evaluated the effects of ORMOSIL throughout the life cycle of the fly (Figure 2A). Unlike vertebrate model systems, Drosophila is very amenable to rapid analysis since its life cycle is short ,  and thus effects on an organisms' entire development can be quickly analyzed. Briefly, at room temperature (25°C), 1st instar larvae hatch within 24 hours after fertilization. Hatched larvae undergo three larval stages, each stage lasting about a day. After the 3rd larval stage, metamorphosis and pupation occur, and after 4–5 days of pupation adult flies eclose. Adult flies typically live for over 100 days, which also allows studies on aging to be easily performed.
(A) The Drosophila melanogaster developmental cycle and ORMOSIL feeding scheme. At room temperature (25°C) larvae hatch from embryos and undergo three larval stages (1st, 2nd and 3rd instar) each lasting approximately 1 day. After the 3rd instar larval stage larvae begin to pupate. Pupation lasts for 4 days. Once adult flies eclose they can live for over 100 days. Embryos were collected and placed in food vials containing different forms of ORMOSIL, buffer or water. Larvae hatch from embryos and immediately begin feeding. All feedings were done until 3rd instar larvae pupated. The red line depicts the extent of oral administration of ORMOSIL during Drosophila development. The dashed red line depicts the duration of ORMOSIL exposure. Adult flies that eclosed from each feeding condition were collected and placed in new food vials containing the same food that they fed on as larvae. The adult flies continued to feed on different forms of ORMOSIL, buffer or water from the day they eclosed (red arrows). We quantified the survival of adult flies for 33 days (D), while we monitored the survival of adult flies for over 100 days. Note that Drosophila was continuously fed ORMOSIL for a total of 39 to 139 days while they were exposed to ORMOSIL for a total of 43 to 143 days. (B) Oral administration of ORMOSIL nanoparticles has no affect on the survival of Drosophila. The survival of larvae fed on different forms of ORMOSIL was quantified to evaluate survival of pupae and adults. Feedings on buffer (1XPBT) and water were done as controls. All larvae were allowed to develop into pupae and adults, and the total numbers of pupae and adults were counted, normalized and graphed as percentage of survival (Y-axis). No significant difference is seen in the survival of pupae (green) and adults (orange) between the different forms of ORMOSIL, buffer or water fed conditions. (C) Oral administration of ORMOSIL has no affect on the developmental time of when adult flies eclose from pupae. No significant difference is seen in the total number of adult flies that eclosed from RORM, Peptide-RORM and TfR-RORM (1 mg/ml) or buffer (1XPBT) fed larvae on 3 different days. On each day the total number of flies were counted, normalized and graphed as percentage of number of flies eclosing vs day 1, 2 or 3. (D) Oral administration of ORMOSIL nanoparticles has no affect on the survival of adult flies. The number of adult flies in each food vial was counted on day 0, 18, 25 and 33. The total number of flies in each vial was normalized to 100 and the survival of adult flies was graphed as a survival curve. Y axis represents the percentage of adults that survived. On day 0 flies were collected, counted and transfered to new food vials. On day 18 flies in each of the vials were again counted. No significant difference in survival was seen in adult flies fed on RORM, Peptide-RORM, TfR-RORM (1 mg/ml) or buffer. Similarly, on day 25 and 33 flies were again counted and no significant difference in the rate of survival of adults fed on RORM, Peptide-RORM, TfR-RORM or buffer was seen. Note that these flies fed on ORMOSIL or buffer for a total of 39 days (6 days as larvae+33 days as adults), while they were exposed to ORMOSIL or buffer for a total of 43 days (6 days as larvae+33 days as adults+4 days exposed as pupape).
To test the toxicity of ORMOSIL in a whole organism we fed RORM (and cy5ORM, data not shown) to Drosophila larvae that had just hatched and we continued to feed ORMOSIL through the developmental cycle of the fly (Figure 2A, red, a total of 39 feeding days and a total of 43 days of exposure). To date no other animal study has fed nanoparticles or followed their survival for such a long duration of time and through an organisms' entire life cycle.
For our feeding experiments, equal numbers of embryos were placed in food-containing vials. We used three different forms of ORMOSIL particles, unconjugated RORM and two forms of conjugated-RORM (TfR-RORM and peptide-RORM). We used Instant Medium (Carolina Biological), which is a commonly used food for Drosophila in the form of dry flakes to mix all ORMOSIL formulations (at concentrations of 0.2, 0.4 and 1 mg/ml) for all feedings. As controls, food was also mixed with the buffer used to dilute ORMOSIL, (1× phosphate buffered saline with 0.1% triton (1XPBT)) and water. In each food vial containing the different ORMOSIL formulations (three forms of RORM each at concentrations of 0.2, 0.4 and 1 mg/ml), buffer, or water, larvae were allowed to hatch and were allowed to grow until the larvae pupated (6 days). During the three larval stages, larvae actively gorged and only fed on food containing nanoparticles, buffer or water. During the larval stages, larvae were assayed to determine if feeding on nanoparticles caused locomotion defects. We failed to observe any crawling or locomotion defects for larvae fed on the three forms of ORMOSIL, and these larvae were comparable to control conditions (buffer and water fed larvae, data not shown, Table 1). Larval viability changes were also assessed and no significant difference in the survival of larvae fed on ORMOSIL was seen compared to buffer or water fed conditions (data not shown, Table 1). Thus our observations indicate that feeding on ORMOSIL had no affect on the behavior or on the viability of larvae (Table 1). Further, unconjugated and conjugated RORM fed larvae were undistinguishable from each other.
To test the affect of ORMOSIL on pupal development, we counted the number of pupae that pupated from ORMOSIL, buffer and water fed larvae (see methods). Larvae were allowed to pupate in the same food vials that they fed on as larvae and the pupae were counted. No effect was seen in the number of larvae that pupated between ORMOSIL, buffer or water fed conditions (Figure 2B, Table 1). Figure 2B depicts the normalized percentage of pupae for all feeding conditions from three different feeding experiments. Further, no abnormality was seen in pupation of ORMOSIL fed larvae compared to buffer or water fed larvae. Note that since larvae were allowed to pupate in the same food vials as they fed on, pupae were still exposed to the same food conditions (4 days of exposure as pupae).
To determine ORMOSIL effects on survival to adulthood, flies were collected as they eclosed and were placed in new food vials containing food laced with the corresponding nanoparticle (form and dose), buffer or water and examined (see methods). We failed to see any abnormality in flies that survived to adults between ORMOSIL, buffer or water fed conditions (Figure 2B). No significant difference in the percentage of flies that eclosed from pupae for the different feeding conditions were observed (Figure 2B, Table 1). In addition, there was no abnormality in the developmental time of when adults emerged from pupae, with almost all adults emerging on the 3rd day for all feeding conditions (Figure 2C). Thus unconjugated or conjugated RORM appear to be benign and show good biocompatibility during the entire life cycle of the fly (10 days).
We continued to test the biocompatibility of ORMOSIL during adulthood by evaluating adult flies. To test this, the flies that eclosed from larvae fed on ORMOSIL or control conditions (buffer and water) were counted and placed in new food vials containing the corresponding food source (day 0) and the survival of adult flies were monitored for a total of 33 days. Note that during these 33 days adult flies were feeding on the same food source that they fed on as larvae. On day 18, 25, and 33, we counted the number of flies that had died in each vial and plotted the percentage of survival on a survival plot (Figure 2D, see methods). During these 33 days no difference was seen in the survival of adult flies feeding on ORMOSIL or buffer (Figure 2D, blue, Table 1). Furthermore, we also failed to see any behavioral defects. Adult flies were evaluated for flying defects and for the bang sensitive phenotype, a characteristic phenoytpe that depicts problems in synapse transmission. Typically flies that show a bang sensitive phenotype become paralyzed after the flies are given a mechanical shock such as a bang of the vial on a bench/table , . We failed to observe any of these problems in flies fed on ORMOSIL and their behavior was undistinguishable from buffer or water fed flies (data not shown, Table 1). We continued to follow these flies as they aged for over three months (approx 100 days) and found no difference in their survival or in their behavior, regardless of the feeding regime (data not shown). In our studies Drosophila was continuously fed ORMOSIL for a total of 39 to 139 days while they were exposed to these particles for a total of 43 to 143 days. Thus continuous feeding of ORMOSIL (unconjugated or conjugated) in Drosophila did not affect the behavior or the survival of adult flies.
The short-term survival of dissected larvae is not affected by ORMOSIL nanoparticles
To further evaluate the toxicity of ORMOSIL nanoparticles, we applied ORMOSIL to dissected living larvae and evaluated their survival. We routinely use this larval dissection procedure in our laboratory to study the larval nervous system  and dissected larvae can survive under physiological conditions (in dissection buffer) for at least 180 minutes. Under physiological conditions larvae were treated with ORMOSIL for 10 minutes immediately after dissection. The same three doses of RORM (0.2, 0.4 and 1 mg/ml) that we used for our feeding experiments were used for larval treatment. RORM-treated larvae were then washed with dissection buffer and immediately evaluated. We found that application of RORM directly to dissected larvae did not cause any adverse effects to the dissected living larvae. Similarly application of cy5ORM or conjugated RORM (peptide-RORM or TfR- RORM) also did not show any adverse effects (data not shown). Thus the survival of all ORMOSIL treated larvae (unconjugated or conjugated) was comparable to buffer treated larvae (Figure 3).
Dissected living larvae were treated with RORM (1 mg/ml and 0.2 mg/ml are shown) or buffer and larval survival was quantified by evaluating the twitching phenotype. We assigned “survival” values or survival points according to the extent of twitching observed when the larva was stimulated with a forceps. As described in the text, the more the larva twitched, the higher the “survival” value, indicating that the dissected larva was alive , , . The extent of twitching was recorded every 15 minutes for a total of 60 minutes. No significant difference was seen between the survival of ORMOSIL treated or buffer treated dissected living larvae.
We quantified the survival of dissected living larvae by evaluating the twitching phenotype. We assigned a “survival” value according to the extent of twitching observed when the larva was stimulated with a forceps. The twitching phenotype or the twitch tension is a commonly used phenotype in Drosophila larvae and evaluates nerve-stimulated contractions of larval body-wall muscles , , . The more the larva twitched or contracted, the higher the “survival” value, indicating that the dissected larva is alive. Using this quantification method we found no obvious difference in the survival of larvae between the three different doses of ORMOSILor buffer treated larvae (Figure 3). The steady decline in twitching that we observed for all conditions can be attributed to a decline in the proper physiological conditions because the dissection buffer was not replaced every 20–30 minutes . Taken together our observations indicate that application of ORMOSIL does not affect the short-term survival of dissected living larvae.
ORMOSIL nanoparticles incorporate into living larval and adult neuronal tissues
For a nanoparticle to be successful as a therapeutic tool for neuronal diseases in humans, it must effectively and specifically incorporate into living neuronal tissues and must not cause any adverse effects to living neuronal cells or tissue. To test this, we first evaluated ORMOSIL incorporation into the Drosophila larval neuronal tissues. The Drosophila larval nervous system is a powerful and a well-characterized model system. The central and peripheral nervous systems are remarkably similar in function and in morphology to vertebrates. The larval nervous system is highly organized with the brain at the anterior near the head of the larva (Figure 4A). Segmental nerves extend from the cell bodies in the brain along the length of the larva and these nerves end at the nerve terminals at the distal ends of the larva. Segmental nerves contain bundles of both motor and sensory neurons and are much like the sciatic nerve or the brain stem of mammals.
(A) A diagram depicting the larval nervous system. The brain is at the anterior. Segmental nerves that originate at the brain extend along the length of the larvae and form synapses or nerve terminals at their ends. Segmental nerves contain bundles of motor and sensory axons, with have their cell bodies located in the brain. (B) Buffer treated larval brain. A representative fluorescence image from a buffer treated larval brain. No fluorescence is observed using the 568 nm filter. Images were taken using the 10× objective. Bar = 10 µm. (C) ORMOSIL is observed within the larval nervous system. A representative low magnification (20×) light microscopy image of a larval brain (dashed outline) and segmental nerves show incorporation of RORM particles (arrows). ORMOSIL is observed within the brain (outlined, arrows) and the nerves (arrows). Images were obtained using the 568 nm filter to visualize RORM. Bar = 10 µm. (D) ORMOSIL is observed within the cell bodies of the larval brain. A representative high-magnification fluorescence image using the 100× objective from the ventral ganglion region of an ORMOSIL treated larval brain shows that RORM is incorporated into the cytoplasm of the neuronal cell bodies (arrows). Note that the cell body nuclei are devoid of RORM and that the fluorescence signal is in a discrete pattern within the cell body (arrows). Bar = 5 µm. (E) Unconjugated ORMOSIL is observed within the larval segmental nerve. A representative high magnification fluorescence image using the 100× objective from a segmental nerve (outlined) show that RORM is incorporated into the larval segmental nerve (arrows). RORM is observed throughout the nerve as bright puncta (arrows). The fluorescence signal we observe can be attributed to accumulated ORMOSIL. Bar = 5 µm (F, G) Conjugated ORMOSIL is observed within the larval segmental nerve. A representative high magnification fluorescence image using the 100× objective from a segmental nerve (outlined) show that conjugated ORMOSIL (Peptide-RORM, F, and TfR-RORM, G) are incorporated into the larval segmental nerves (arrows). Bar = 5 µm.
To determine if ORMOSIL can penetrate and integrate into live larval neuronal tissues, we incubated dissected living larvae with unconjugated and conjugated ORMOSIL (0.2, 0.4 and 1 mg/ml). Larvae were dissected to expose the larval nervous system and incubated in ORMOSIL for 10 minutes. Dissected living larvae were washed in dissection buffer and immediately observed using a confocal microscope under 568 nm fluorescence to visualize ORMOSIL integration into larval neuronal tissues. From our survival experiments we know that ORMOSIL-treated larvae were alive and can survive to over 60 minutes, so our observations were conducted within a 30 min time frame. Unconjugated and conjugated RORM were found in the larval brain and in the larval segmental nerves (Figure 4). Similarly we also found cy5ORM in the larval brain and larval segmental nerves (Figure S2). The fluorescence we observe was specific to ORMOSIL and was not the result of autofluorescence since buffer or water treated larvae did not show any fluorescence in any of the larval neuronal tissues (Figure 4B and data not shown). In addition, while single nanoparticles are below the resolution of the fluroscence microscope, the fluroscence signal we do observe can be attributed to the accumulations of ORMOSIL nanoparticles at single points. High magnification images taken using a 100× objective indicate that RORM (or cy5ORM) was present within the cytoplasm of the neuronal cell bodies of the larval brain (arrows, Figure 4D, Figure S2A). Further, RORM (or cy5ORM) appears to be present in specific cellular compartments and the cell body nuclei appear to be devoid of particles (Figure 4D, Figure S2A). Indeed, in larval cell bodies, some ORMOSIL puncta (Figure S3B, red) colocalized with golgi puncta (Figure S3A, green, merged Figure S3C, arrows). Similar cell body staining was observed for both conjugated forms of RORM (data not shown). In larval segmental nerves, RORM (or cy5ORM) was present as puncta along the length of the segmental nerves (Figure 4E, Figure S2B arrows). These puncta may represent small aggregates of ORMOSIL that have accumulated during the 10 min period of nanoparticle incubation. Similarly, Peptide-RORM and TfR- RORM puncta were also observed in larval segmental nerves (Figure 4F,G arrows). From these observations we can conclude that ORMOSIL can readily incorporate into living larval neuronal tissues perhaps into discrete cellular compartments as suggested previously , .
We also tested ORMOSIL incorporation in living primary neuronal cultures. Primary neuronal cultures were generated from wild type larval brains and allowed to grow for 4 days, when relatively long neuronal projections could be seen. On the fourth day, cultures were incubated with nanoparticles at the three doses (0.2, 0.4 and 1 mg/ml) for 10 minutes. Cultures were washed to remove any unincorporated particles and immediately imaged. Similar to our observations in larval brains, accumulations of RORM were seen in the cell body and in the neuritis of primary neuronal cultures (Figure 5A, arrows). DAPI staining indicates that the cell body nuclei were also devoid of RORM particles (Figure 5FGH). Control cultures treated with buffer did not show any fluorescence (Figure 5E). To evaluate if RORM incorporation caused toxicity to the primary neuronal cultures, and to determine the retention of ORMOSIL in neurons, RORM treated cultures were allowed to grow for 3 more days (for a total of 7 days) and imaged. RORM could still be observed 3 days after the initial nanoparticle treatment, in both the cell bodies (Figure 5B, insert) and in the neurites (Figure 5B). The fluroscence intensity was comparable to the initial intensity of RORM observed 3 days before (compare Figure 5A to 5B). In addition, these neuronal cultures were healthy and the neuritis had grown much longer (about 2 to 3 times longer) during the 3 additional days (Figure 5B). TfR or peptide- RORM treatment (Figure 5C, D) also showed a similar biodistribition and was comparable to unconjugated-RORM treated primary neuronal cultures. The pattern of unconjugated, TfR or peptide-RORM uptake by these neuronal cells appear to be consistent with previous observations in different cancer cell lines , , , , . To further evaluate how ORMOSIL incorporation affected the growth of neurons in culture, we compared and quantified growth by quantifying the changes in the size of the cell body and the changes in the length of neuronal projections for 120 hours (5 days) after RORM treatment (Figure 5IJ). No statistically significant difference in the growth of either the cell body size or the length of neuronal projections was observed between non-treated cultures (syntaptotagmin-GFP, SYNT-GFP expressing cultures) and RORM treated cultures (treated with either unconjugated-RORM (cell body, p = 0.728, neuritis, p = 0.698 N = 10–12) or peptide-RORM (cell body, p = 0.737, neuritis, p = 0.861, N = 8–10) during 120 hours after RORM treatment. In addition no difference in growth was seen in cultures treated with either unconjugated-RORM or peptide-RORM (cell body, p = 0.915, neuritis, p = 0.914, N = 10). Together, these observations suggest that ORMOSIL treatment or incorporation into neurons does not interfere with the normal growth of neurons. Further, ORMOSIL particles are retained within living neurons without any aberrant toxicity.
(A) Unconjugated ORMOSIL is observed in 4 day old primary neuronal cultures. 4 day old primary neuronal cultures generated from larval brains were incubated with RORM. Cultures were imaged using the 568 nm filter. RORM is observed within the cytoplasm of the cell body in a discrete pattern and within neuritis (arrows). Images were taken using the 100× objective. Bar = 5 µm. (B) Unconjugated ORMOSIL is also observed 3 days after ORMOSIL treatment. To determine how ORMOSIL affected the growth of cultures, ORMOSIL treated cultures were allowed to grow and again imaged after 3 days of ORMOSIL treatment. These cultures were now 7 days old. These treated cultures showed growth with very long neuronal projections compared to day 4. RORM was still observed within the cell bodies (insert) and the neuritis (arrows,). Note that the fluorescence intensity at day 7 was similar to the intensity observed at day 4. Images were taken using the 100× objective. Bar = 5 µm. (C) Receptor-conjugated ORMOSIL is observed in 4 day old primary neuronal cultures. 4 day old primary neuronal cultures generated from larval brains were incubated with transferrin receptor conjugated ORMOSIL (TfR-RORM). TfR-RORM can be observed within the cell body and within the neuritis. Images were taken using the 100× objective. No significant different in the distribution of ORMOSIL was seen between RORM and TfR-RORM treated cultures. Bar = 5 µm. (D) Peptide -conjugated ORMOSIL is observed in 4 day old primary neuronal cultures. 4 day old primary neuronal cultures generated from larval brains were incubated with peptide-conjugated ORMOSIL (Peptide-RORM). Peptide-RORM can be observed within the cell body and within the neuritis. Images were taken using the 100× objective. No significant different in the distribution of ORMOSIL was seen between RORM and peptide-RORM treated cultures. Bar = 5 µm. (E) Untreated control cultures. Control 4 day old cultures treated with buffer do not show fluorescence using the 568 nm filter. Images were taken using the 100× objective. Bar = 5 µm. (F, G, H) ORMOSIL is absent from the cell body nucleus. 4 day old primary neuronal cultures were incubated with RORM (F, red). Incubated cultures were fixed and stained with DAPI to localize the nuclei (G, blue). A representative merged image (H) indicates that ORMOSIL is absent from the cell body nucleus. Note that ORMOSIL is present in a discrete pattern within the cell body cytoplasm. Images were taken using the 100× objective. Bar = 5 µm. (I) Quantification of cell body growth after ORMOSIL treatment. Graphs depict cell body growth for 120 hours (5 days) after ORMOSIL treatment. For untreated cultures, cultures expressing synaptotagmin-EGFP (SYNT-EGFP) was used. The effect of treatment was evaluated for unconjugated ORMOSIL (ORMOSIL) and for peptide-conjugated ORMOSIL (pep-ORMOSIL). For each time point 8–12 cells from three different experiments were analyzed. The average diameter and standard error was calculated and the average cell body diameter in microns was plotted against time in hours. No statistically significant difference was seen between ORMOSIL treated (unconjugated or peptide-conjugated) and cultures expressing SYNT-EGFP. (J) Quantification of neurite growth after ORMOSIL treatment. Graphs depict neurite growth for 120 hours (5 days) after ORMOSIL treatment. For each time point 8–12 cell from three different experiments were analyzed. The average projection length in micron was plotted against time in hours. The standard error was calculated and plotted. No statistically significant difference was seen in neurite growth between ORMOSIL treated (unconjugated or peptide-conjugated) and cultures expressing SYNT-EGFP.
We also evaluated ORMOSIL-fed larvae to determine if these nanoparticles could incorporate into larval neuronal tissues by feeding. We failed to see ORMOSIL within the larval brain (data not shown). However, ORMOSIL was present in many other larval tissues including the larval gut (Figure S1C), malpighian tubes (Figure S1C), trachea (Figure S1B) and skin (cutical, Figure S1B), indicating that these particles can incorporate into larval tissues by feeding. It is possible that ORMOSIL incorporation into neuronal tissues require longer exposure times. In this context, we evaluated adult brains after approx 12–15 days of ORMOSIL exposure. In these adults ORMOSIL was continuously provided by feeding; from the time they hatched into larvae until the time the adults were dissected. Consistent with our hypothesis, we observe unconjugated and conjugated ORMOSIL in dissected adult brains (RORM, Figure 6AB, TfR and peptide-RORM, Figure 6CD), while no fluorescence is observed in brains from control adults (buffer or water fed, compare Figure 6A to 6E). High magnification (100×) images show that ORMOSIL was present in clusters or aggregates within the CNS of the adult brain (Figure 6BCD). These observations were consistent for all 6 adult brains that were imaged (from 3 different feeding experiments). We also noted that the ORMOSIL puncta were consistently in the same region of the brain. These observations suggest that ORMOSIL can be directed into adult neuronal tissues by feeding.
(A) Unconjugated ORMOSIL is observed in adult fly brains. A representative fluorescence image of an adult brain from a fly that was fed on RORM from the time it was a larvae was dissected and observed using the 568 nm filter. RORM aggregates are observed within the adult brain. Images were taken using the 10× objective. The boxed region is enlarged in B. Bar = 10 µm. (B) Unconjugated ORMOSIL aggregates are observed as puncta within adult fly brains. A high magnification (using the 100× objective) image of the boxed region from A. RORM aggregates (arrows) are seen as puncta within the adult brain. Interestingly, in all 6 adult brains imaged showed similar puncta of ORMOSIL. Bar = 5 µm. (C) Peptide conjugated ORMOSIL aggregates are observed as puncta within adult fly brains. A representative high magnification image shows peptide-RORM puncta within the adult brain (arrows). Bar = 5 µm. (D) Receptor conjugated ORMOSIL aggregates are observed as puncta within adult fly brains. A representative high magnification image shows TfR-RORM puncta within the adult brain (arrows). Bar = 5 µm. (E) No fluorescence is observed in buffer fed adult fly brains. A representative image from a buffer (1XPBT) fed adult fly brain imaged using the 568 nm filter. Note that there is no fluorescence in these brains. Images were taken using the 10× objective. Bar = 10 µm.
ORMOSIL nanoparticle incorporation does not activate aberrant neuronal cell death pathways or interfere with normal neuronal processes
If these nanoparticles are to be used to develop effective therapeutic tools for human diseases, these particles by themselves should not cause any adverse affects to the target tissue. In this context, we evaluated if ORMOSIL incorporation caused any adverse effects to the normal cellular processes within neurons, such as cell viability and axonal transport. To test this, first, larvae were dissected, treated with ORMOSIL (unconjugated, peptide or TfR-conjugated), fixed and analyzed using the TUNEL assay to evaluate if incorporation of ORMOSIL into neuronal cells activated aberrant neuronal cell death pathways. During cell death, the DNA within the nucleus becomes fragmented and the presence of nicked DNA can be identified by terminal deoxynucleotidyl transferase, an enzyme that catalyzes the addition of dUTPs which can be fluorescently assayed using the TUNEL assay. Thus the presence of fluorescence within nuclei indicates cell death (Figure 7A). We found that ORMOSIL incorporation into larval cell bodies failed to cause aberrant neuronal death. No TUNEL-positive nuclei were observed in RORM treated larval brains (compare Figure 7B to Figure 7A), although ORMOSIL is observed within the cell bodies (arrows, Figure 7C). Similar observations were seen with conjugated RORM treated larval brains (data not shown). We further evaluated neuronal cell death in ORMOSIL fed adult brains. Although ORMOSIL puncta were observed in adult brains, there were no TUNEL positive nuclei, indicating that ORMOSIL incorporation by feeding did not trigger abnormal neuronal cell death in adult ORMOSIL-fed brains (unconjugated and conjugated RORM, data not shown). Thus ORMOSIL incorporation failed to trigger aberrant neuronal cell death pathways.
(A, B, C) ORMOSIL nanoparticle incorporation does not induce aberrant neuronal cell death pathways in the cell bodies of the larval brain. A control brain incubated with DNAse and treated with the TUNEL assay shows TUNEL positive cells (A, arrows). A representative fluorescence image from a larval brain (outlined) incubated with RORM was assayed for neuronal cell death using the TUNEL assay. Using the 488 nm filter, no fluorescence was observed in the larval brain indicating that there were no nuclei showing neuronal cell death (B) in contrast to A. However, RORM was present within the larval brain (using the 568 nm filter, arrows). Note that ORMOSIL is seen as puncta (C). Images were taken using the 40× objective. Bar = 20 µm. (D, E, F, G) ORMOSIL incorporation does not affect the axonal transport pathway. A representative image of larval segmental nerves from a dissected RORM treated larvae does not show axonal blockages using the synaptic vesicle antibody, CSP (E). Note that ORMOSIL aggregates can be seen in these larval segmental nerves (arrows, D). F shows the merged image. In contrast, larval segmental nerves from an axonal transport mutant (dynein mutant, DLC) show axonal blockages (arrows, G). Images were taken using the 40× objective. Bar = 20 µm.
Secondly, to determine if ORMOSIL incorporation interfered with normal cellular processes within the axon we evaluated the axonal transport pathway using antibodies against the synaptic vesicle marker, cystein string protein (CSP). Within axons, essential components are transported from the cell body, the site where many proteins are synthesized, to the synapse where these components are utilized. This process known as axonal transport is essential for the growth, maintenance and survival of all neurons. Recently, perturbations in this pathway have been implicated in many human neuronal diseases , . Previously, we found that segmental nerves from larvae that contain a mutation for a protein involved in axonal transport (i.e., a mutation in the gene encoding the motor protein dynein light chain, DLC) showed bright clusters of CSP accumulations that we call axonal blockages ,  (Figure 7G, arrows), in contrast to wild type larval segmental nerves that show smooth CSP staining , . These blockages are packed with many types of identifiable axonal cargo, namely mitochondria, vesicles, large multi-vesicular bodies, and large prelysosomal vacuoles, which interferes with the normal transport of components within the axon . Thus we hypothesized that if ORMOSIL incorporation interfered with the transport of components within the axon then we should observe axonal transport defects similar to these blockages. In contrast to larvae carrying an axonal transport mutation (Figure 7G), ORMOSIL nanoparticle containing larval segmental nerves were smoothly stained (compare Figure 7E to 7G), indicating that the presence of ORMOSIL in larval nerves (Figure 7D arrows) does not cause aberrant axonal transport defects and does not affect the distribution of CSP vesicles. Observations were similar in unconjugated and conjugated forms of RORM treated larvae (Figure 7 and data not shown). Thus ORMOSIL incorporation does not affect the axonal transport pathway.
We further investigated if ORMOSIL incorporation affected the in vivo transport dynamics of vesicles within larval axons in whole-mount larvae. Larvae expressing a GFP tagged vesicle protein (synaptotagmin-EGFP, SYNT-EGFP) were dissected and treated with ORMOSIL particles (unconjugated or conjugated) at doses 0.2, 0.4 or 1 mg/ml. Simultaneous observations using dual view imaging, a beam splitter and split view software showed the movement of the GFP-tagged synaptotagmin vesicles (Figure 8AC) within larval axons, together with ORMOSIL (Figure 8BD, data not shown). The movement dynamics of GFP-tagged synaptotagmin vesicles was not altered by the incorporation of ORMOSIL (both unconjugated and conjugated) at these doses, and was comparable to the movement dynamics of GFP-tagged synaptotagmin vesicles in untreated larvae . Similar observations were also seen in primary neuronal cultures generated from larval brains expressing SYNT-GFP treated with ORMOSIL (unconjugated and conjugated, data not shown). Thus our observations indicate that ORMOSIL incorporation at the concentrations we used does not interfere with the movement of synaptic vesicles in vivo, an essential pathway for neuronal integrity and survival.
(A, B) In vivo imaging suggests that ORMOSIL incorporation does not affect the movement of GFP-tagged synaptotagmin vesicles within living dissected ORMOSIL treated larvae. Single frames from a representative movie containing both GFP-tagged synaptotagmin vesicles (SYNT-GFP, A) and RORM (B) simultaneously imaged show the movement of SYNT-GFP vesicles within a larval segmental nerve incubated with ORMOSIL. Note that the SYNT vesicle shows movement in each frame (arrow). (B) Note that ORMOSIL is also observed within the same larval segmental nerve (arrow). Note that ORMOSIL does not dramatically change in each frame (arrow). A 1 min movie is depicted. Movies were taken using the 100× objective. Bar = 10 µm. (C,D) Kymographs show that ORMOSIL treatment does not affect the movement of GFP-tagged synaptotagmin vesicles. Kymographs from the above movies show that the movement dynamics of SYNT-GFP vesicles are not affected in RORM treated larvae. The movement of a SYNT-GFP vesicle is seen moving from the left to the right (arrow, C), while a slight shift is seen for ORMOSIL (arrow, D).
For any nanoparticle to be useful as a therapeutic delivery system, it must first pass three basic criteria; it should not be toxic to the organism, it should effectively incorporate into the specific tissue type that the treatment targets and it must not interfere with the normal functions of that tissue type. Our study demonstrates that a novel silica based particle named ORMOSIL successfully passes all three of these tests and could have enormous potential for the development of a therapeutic system for living neurons within whole organisms.
Until now, only viral carriers have been successfully used in treatment strategies in animal models of disease and injury , , but safety concerns relating to the toxicity and immunogenicity of viral vectors remain a challenge to clinical translation . Non-viral delivery vehicles such as ORMOSIL have the potential to avoid the safety issues inherent in viral delivery, but lack of knowledge about their behavior in neuronal tissues and how these particles affect normal cellular processes within a whole organism has so far limited their use. Our study tested the behavior of both unconjugated and receptor or peptide conjugated ORMOSIL in whole living organisms, throughout development, and in living neuronal cells. We found that these novel particles are biocompatible, are not cytotoxic and incorporate into neuronal tissues. Thus these particles have great potential to be effectively translated for used in neuronal therapeutic applications.
Unlike other nanoparticles, these nanoparticles have several physiochemical properties that facilitate their use in many biomedical applications . They are easily synthesized in a cost-efficient manner, have excellent storage stability and are resistant to contamination. They are optically transparent and are excellent optical probes following encapsulation or conjugation of flurophores because nano-incorporation protects flurophores from photobleaching and prevents interaction with the biological environment . They have also been extensively used as probes for imaging in in vitro experiments . Further, the porus surface of ORMOSIL allows co-incorporation of other diagnostic probes for recognition of molecules for target-specific delivery without changing its size , .
Previous studies using ORMOSIL nanoparticles in a pancreatic cancer cell culture system showed no indication of cytotoxicity and good uptake of these particles was observed using confocal microscopy , . Further, fluorescence anisotropy experiments demonstrated that the flurophores were still coupled to the particles. Robust uptake was also detected with ORMOSIL particles conjugated with various biotargeting molecules with no cytotoxicity. Although studies using systemic injection in mice have been performed, these studies failed to assess the long-term toxicity of ORMOSIL to the animal or to the animal's tissues , . Thus we chose Drosophila as a model organism to test toxicological effects and to obtain dosage information because the fly has a rapid life cycle and the maintenance costs are relatively low. Our observations in a whole organism indicate that ORMOSIL is not toxic to developing Drosophila. Oral administration of ORMOSIL by feeding to Drosophila, (through its development) failed to show any developmental defects or induced lethality. Phenotypically and behaviorally larvae and adults continuously fed on ORMOSIL were undistinguishable from those fed on water or buffer. Further more, our feeding experiments used doses of ORMOSIL that were much higher than what has previously been used in intravenous experiments in mice , . We also failed to see any behavioral defects or any abnormalities to the adult lifespan in flies that were continuiously fed ORMOSIL. Importantly, different nanoparticle formulations with different fluorescent tags and different biotargeting tags showed very similar behaviors, uptake patterns and distributions inside living animals and living neuronal cells. Thus these novel particles appear to be good candidates for the development of therapeutics in a whole organism. Further, our study is the first to test the biocompatibility of a nanoparticle through the development of an organism and through long-term administration. A recent invertebrate study in C. elegans examined the effects of a different kind of nanoparticle in adults, but failed to determine its effects through the developmental cycle of C. elegans .
Recently the biodistribution of ORMOSILwas tested by systemic injection in mice . In these studies 2.0 mg per kg of body weight of ORMOSILwas injected into the tail vein and the incooperation of particles were followed in different tissues. Almost 75% of the injected dose was observed in the liver, spleen and skin, whereas the lung, kidney and the heart accounted for less than 5% of the injected dose. However, no particles were seen in neuronal tissues. Although our feeding experiments also show ORMOSIL in the gut and skin, in contrast, we found ORMOSIL incorporation in the adult brain, indicating that continuous ingestion of ORMOSIL for an extended period of time can lead to the incorporation of these particles into the adult fly brain. Although further study is needed to elucidate the exact mechanism of incorporation, our observations propose that single ORMOSIL particles may penetrate the Drosophila blood-brain barrier  and form ORMOSIL aggregates. Since penetration of the blood-brain barrier is an important requirement for an effective therapeutic particle further study is needed to evaluate the exact mechanism.
Our observations also indicate that ORMOSIL is an attractive new particle for the development of therapies specifically targeted to neuronal tissues. Previous studies have proposed that silica based nanoparticles can be readily taken up by the cell as individual entities mostly by phagocytosis or receptor mediated uptake followed by accumulation in specific cellular compartments , . We also found that ORMOSIL particles can readily incorporate into the cytoplasm of the neuronal cell bodies and to larval axonal projections or neuritis. The puncta of fluorescence we observe (Figure 4E, 6B) can be attributed to the fluorescence from ORMOSIL particles, which entered the cells as individual entities and accumulated. Incorporation also appears to be to a specific cellular compartment (Figure S3) and ORMOSIL was absent from the neuronal cell body nuclei (Figure 5). Importantly, since both unconjugated and peptide or receptor conjugated ORMOSIL was seen in cell bodies and neuritis, conjugation of ORMOSIL does not appear to change the localization of ORMOSIL within the neuronal cell, although the mechanism of uptake may be different for unconjugated (by phagacytosis) and receptor/peptide conjugated (receptor mediated) ORMOSIL , . Further study will be needed to elucidate this proposal.
We also observe that the presence of ORMOSIL within neurons did not activate aberrant neuronal cell death pathways or interfere with normal neuronal processes such as axonal transport. Incorporation of ORMOSIL did not induce neuronal cell death. Further, incorporation of ORMOSIL into living larval axons or neuritis did not affect the movement dynamics of synaptic vesicles. Thus while ORMOSIL can affectively incorporate into neurons these particles do not appear to interfere with normal neuronal processes, two important requirements for an effective therapeutic particle.
In conclusion, our study demonstrates that ORMOSIL nanoparticles have great promise for the development of therapeutic applications for human neuronal disease for long-term use within whole organisms. Its non-toxic characteristic and its ability to readily incorporate into living neuronal tissues together with its porous surface that allows incorporation of specific molecules for targeting, make ORMOSIL nanoparticles the next generation of particles that can be effectively used to develop targeted therapeutic treatments to specific areas of the brain or to specific populations of neurons. Development of such treatment strategies have great potential in minimize global deleterious affects while maximizing beneficial affects, which is a problem in many of the current treatment strategies that are used for many human neuronal diseases.
Materials and Methods
Synthesis of ORMOSIL nanoparticles
ORMOSIL nanoparticles with covalently incorporated fluorophores, rhodamine or cy5, were synthesized in the non-polar core of an oil-in-water microemulsion, as per our earlier report but with a slight modification . Briefly, 0.2 g of surfactant AOT and 300 µl of n-butanol and 100 µl of DMSO were dissolved in 10 ml HPLC grade water by magnetic stirring. To this microemulsion system, 100 µl of 1 mg/ml of rhodmaine-silane precursor (rhodamine NHS ester, conjugated to aminopropyltriethoxy silane) in DMSO was added and stirred, followed by an addition of 100 µl of neat VTES. The reaction mixture was stirred for another hour and polymerization reaction was started by the addition of 10 µl of amino-propyltriethoxysilane. The final reaction mixture was allowed to stir overnight. The mixture was then dialyzed against distilled water for 48 h at room temperature, using a cellulose membrane with a cut-off size of 12–14 kD. Following dialysis, the nanoparticles were sterile filtered and stored at 4°C for future use. Using the oil-in-water microemulsion method RORM was conjugated with the bioactive molecules transferrin (Sigma-Aldrich, ) and the 15 aa peptide (G-Y-E-N-P-T-Y-K-F-F-E-Q-M-Q-N, Celtek peptide, ). As described previously , 1 mL of stock solution of -COOH-terminated RORM nanoparticles was mixed with 25 µl of 0.1 M EDC solution and gently stirred for 30 min. Next, 5 µl of 5 mg/mL of transferrin or 5 µl of 5 mg/ml of peptide was added into this mixture, and the mixture was incubated at room temperature for 2 h to allow the proteins to covalently bond to the COOH group of the ORMOSIL nanoparticles. The conjugation was confirmed by agarose gel electrophoresis by measuring the ζ-potential values of the resulting nanoparticles .
Drosophila feeding experiments
Wild type Drosophila cages were used to collect embryos for ORMOSIL (unconjugated or receptor or peptide conjugated) feeding experiments. Eggs were collected on egg laying apple plates for 12 hours at room temperature. Using a brush the eggs were collected into a fine sieve, washed and placed in a microcentrifuge tube in a suspension of water. 200 µl of egg/water solution was placed in each vial that contained dry food (Instant Medium, Carolina Biological, which is a commonly used food for Drosophila), mixed with the three different doses of ORMOSIL (0.2, 0.4 and 1 mg/ml), 1X PBT (Phosphate Buffered Saline (PBS) containing triton X-100) buffer or water. 1 mg/ml ORMOSIL were diluted to 0.2 and 0.4 mg/ml using 1X PBT buffer. Similar procedures were previously used in a chemical screen that tested 500 small molecular compounds to identify chemical modifiers of axonal blockages (Gunawardena unpublished). In this screen we found that feedings using concentrations of 1 mg/ml of modifier compound was very toxic to developing Drosophila (Gunawardena unpublished). Thus we determined that concentrations of 1 mg/ml and below were ideal for nanoparticle feeding experiments in Drosophila.
Vials containing food laced with the different forms of ORMOSIL, buffer or water were kept in the dark in a humid chamber and the larval, pupae and adult development was observed at room temperature (25°C). At each developmental stage of the Drosophila life cycle, larvae, pupae and adults were counted. The larvae were counted as the larvae crawled up the vial. The pupae were counted as the larvae pupated. As adults eclosed from pupae they were counted and placed in a new vial that contained the corresponding concentration of ORMOSIL, buffer or water. The survival of adults was assayed for over 100 days.
To assay for ORMOSIL incorporation, ORMOSIL fed whole 3rd instar larvae were mounted on a slide and imaged under a Nikon TE 2000 fluorescent microscope. For visualization of RORM/cy5ORM the 568/680 nm filter was used to observe rhodamine distribution within the larva (Figure S1BC). As controls buffer fed and water fed larvae were also imaged. These larvae did now show any fluorescence in the 568 nm/680 nm filter (Figure S1DE and data not shown). For each condition over 10 larvae were imaged. Visualization was also done using the 488 nm filter. Images were also taken in phase contrast to visualize the whole larvae (Figure S1A).
Quantification of survival of larvae, pupae and adults
To quantify the survival of ORMOSIL and control fed larvae we counted and labeled larvae using a colored pen. Each day new larvae were counted and recorded were recorded for each experimental condition. As the larvae pupated each pupae was counted and labeled using a different colored pen to determine the survival of pupae. Each day new pupae were counted and the total numbers of pupae were recorded for each condition. Further, as adults emerged they were collected, counted and placed in new vials containing food laced with the appropriate feeding condition. This day was recorded as Day 0. More than 100 flies from 3 experiments were pooled for quantification and graphing. For each feeding condition the total numbers of pupae and adults were normalized and graphed as percent survival (Figure 2B). Once adults started eclosing the numbers of adult flies eclosing on 3 constisutive days were counted and normalized to determine if there was a delay in development between the different feeding conditions (Figure 2C). To generate the survival curve the number of dead adults were counted on day 18, 25 and 33. These numbers were subtracted from the total number of flies on day 0 and normalized and plotted as percent survival (Figure 2D). Note that survival of adult flies was counted for a total of 33 days, although vials were evaluated for over 100 days. Student T-test was used to determine statistically significant differences between the feeding conditions. Graphs were plotted using an EXCEL spreadsheet.
Larval dissections and adult brain dissections
Larvae were dissected as described previously in 1× dissection buffer, under physiological conditions , . Usually during dissections, the buffer is replaced every 20–30 minutes to keep the physiological conditions constant and under these conditions dissected larvae survive for over 180 minutes. However, since we were evaluating the effect of ORMOSIL on dissected larval survival, the buffer was not changed. Under these modified conditions the dissected larvae survived for more than 60 minutes. ORMOSIL or dissection buffer was added to living dissected larvae and incubated for 10 minutes at room temperature in the dark. After treatment the living dissected larvae were washed with dissection buffer and mounted for immediate observation using a Nikon TE 2000 fluorescent microscope using the 568 nm filter or a Leica TCS SP2 AOBS spectral confocal microscope (Leica Microsystems Semiconductor GmbH, Wetzler, Germany) using the krypton/argon laser. Images were obtained using a 100× or 63× objective.
The survival of dissected living larvae incubated with ORMOSIL or dissection buffer was quantified using “survival points”. “Survival points” were assigned according to the extent of twitching observed when the larva was stimulated with a forceps , , . The higher the survival value the more the larva twitched, indicating that the larva was alive. The lower the survival value the less the larva twitched and was more likely to be dying. The twitching phenotype or the twitch tension is a commonly used phenotype in Drosophila larvae and evaluates nerve-stimulated contractions of larval body-wall muscles , , . For each condition the survival of 10 treated larvae was followed for 60 minutes. The extent of twitching for each larva was recorded every 15 minutes for a total of 60 minutes. Graphs were plotted using an EXCEL worksheet, with the Y axis depicting the larval survival and the x axis depicting the time in minutes (Figure 3).
Adult flies fed on ORMOSIL or control conditions were aged for 10 days and their brains were dissected using 1× dissection buffer. 6 dissected brains for each feeding condition were immediately mounted and imaged using the 568 nm filter to image for ORMOSIL incorporation using a 20× and 40× objective.
Immunohistochemistry, TUNEL assay and Confocal Imaging
Dissected larvae were treated with ORMOSIL, buffer or water as described above and fixed in 4% formaldehyde. Immunohistochemistry was performed as previously described in , , . Briefly, fixed larvae were washed in 1XPBT and incubated overnight with antibodies against CSP (cysteine string protein, a synaptic vesicle protein, Developmental Studies Hybridoma Bank), to assay for axonal blockages at a dilution of 1∶10. The primary antibody were incubated overnight at 4°C. The secondary antibody Alexa 488 anti-mouse (Invitrogen) was used at a concentration of 1∶200 since ORMOSILwas imaged using the 568 nm filter. The secondary antibody was incubated for one hour at room temperature in the dark. After washing with 1XPBT, larvae were mounted on slides using vectorshield mounting medium for confocal microscopy using a Leica TCS SP2 AOBS spectral confocal microscope (Leica Microsystems Semiconductor GmbH, Wetzler, Germany). Images were taken using a 63× oil immersion objective using the krypton/argon laser to image the synaptic protein CSP in 488 nm and ORMOSIL in 568 nm.
To evaluate cell death, the TUNEL assay (Roche) was performed as previously described in , . Larval brains were dissected in 1× dissection buffer and incubated in ORMOSIL similar to what was done in larval dissections. Larval brains were fixed using 4% formaldehyde and the TUNEL assay was performed as per manufactures instructions. Negative (no substrate) and positive (DNAse digestion of larval brains, Figure 7A) were done as controls to test the sensitivity of the assay. Larval brains were mounted using vectorshield mounting medium and imaged using the confocal microscope using the krypton/argon laser to assay for cell death in 488 nm and ORMOSIL incorporation in 568 nm. Images were taken using the 63× oil immersion objective and the Leica TCS SP2 AOBS spectral confocal microscope.
In vivo imaging of GFP-tagged vesicles and ORMOSIL in dissected living larval segmental nerves
GFP-expressing larvae were generated by crossing males that carried the transgene synaptotagmine-EGFP (UAS-SYNT-EGFP) to female virgins that carried the transgene APPL-GAL4 as described in , . In the progeny the activator GAL4 binds to the GAL4 binding sites of UAS-SYNT-EGFP thus expressing the synaptotagmin-EGFP vesicle protein. GAL4 expression is controlled by a neuronal specific promoter (APPL) thus SYNT-EGFP expression only occurs in neuronal tissues. Synaptotagmin is a vesicle protein. GFP expressing larvae are dissected and incubated with ORMOSIL as described above. After ORMOSIL incubation (10 minutes), ORMOSIL was washed using dissection buffer. These dissected larvae are immediately imaged using the 100× oil immersion objective. Using the beam splitter and split view software simultaneous movies are obtained for GFP (488 nm filter) and RORM (568 nm filter), using the Nikon TE 2000 fluorescent microscope. Simultaneous movies of GFP vesicles and ORMOSIL particles containing 100 frames were taken at 150 msec as previously done , . Kymographs of each movie are generated using MetaMorph software.
ORMOSIL treatment in primary neuronal cultures and quantification of neuronal growth
Primary neuronal cultures were generated from wild type 3rd instar larval brains as previously described . Briefly, larval brains are dissected, washed with ethanol and incubated in a Liberase enzyme solution (17 ul liberase solution and 1 mL of Ranaldini's Saline) for 1 hour at 29 degrees. The enzyme is replace by medium and the medium is replace three times. After the last replacement with medium, the neurons are resuspended with a pipette to break the cells. The suspension of cells is pipetted onto culture dishes containing glass coverslip bottoms and incubated at 29 degrees. Cultures are flooded with flooding medium (S10-I medium and 20E hormone). The cultures are allowed to grow for 4 days at 29 degrees. On the 4th day, the flooding medium is replaced with the flooding medium containing different forms of ORMOSIL (0.2 mg/ml, 0.4 mg/ml and 1 mg/ml) or buffer for 10 minutes at 29 degrees. After 10 minutes the cultures are washed with flooding medium and immediately imaged using the Nikon TE 2000 fluorescent microscope, the 100× oil immersion objective and the 568 nm filter. After imaging the cultures are allowed to grow for another 3 days at 29 degrees. These cultures (7 days old) are again imaged to evaluate the growth of these cultures 3 days after ORMOSIL incorporation. The growth in ORMOSIL treated cultures is evaluated by comparing the lengths of neuritis in ORMOSIL treated cultures to non-treated cultures. Both ORMOSIL treated and non-treated cultures showed 2–3 times longer neuritis at 7 days than 4 days. 4 day old cultures were also treated with Transferrin and peptide-conjugated ORMOSIL as described above.
To quantifying neuronal cell growth in cultures the diameter of the cell body and neurite length were measured. For neurite length the longest projection was used. Quantification was done in untreated cultures expressing SYNT-EGFP and in cultures treated with unconjugated and peptide conjugated ORMOSIL. All measurements were taken in MetaMorph using the multi-line tracing tool. To measure the cell body diameter, a linear line was traced through the cell body end to end. In the case of asymmetrical cell bodies, two lines were used perpendicular to each other and averaged to get the diameter. To measure the neurite length, one line was traced along the length of the longest neurite. Any cells lacking visible neurites were omitted from the analysis. Measurements were obtained from 8 to 12 individual cells and averaged. Data was plotted on an Excel worksheet and the standard error and p values were calculated.
ORMOSIL conjugated with Cy5 also penetrates into larval cell bodies and larval segmental nerves. (A) Cy5ORM treated larvae show ORMOSIL in larval cell bodies (arrows), similar to figure 4D. Note that the cell body nuclei are devoid of ORMOSIL. Bar = 5 µm. (B) A representative high magnification fluorescence image from a segmental nerve (outlined) shows that cy5ORM is also incorporated into the larval segmental nerve (arrows). cy5ORM is observed throughout the nerve as bright puncta (arrows). The fluorescence signal we observe can be attributed to accumulated ORMOSIL. Bar = 5 µm.
ORMOSIL nanoparticles incorporate into living larval tissues. (A) A composite phase contrast image of a living larva. The head is at the anterior end while the tail is at the posterior end. These images of whole larvae were constructed by putting together several images taken using the 10× objective. (B) A composite fluorescence image of an ORMOSIL fed living larva imaged for RORM using the 568 nm filter. ORMOSIL nanoparticles can be observed within the skin (cuticle) and trachea (anterior posterior lines). Bar = 100 µm. (C) A composite fluorescence image of an ORMOSIL fed living larva imaged for RORM. Note that ORMOSIL nanoparticles are observed as puncta and are present in the guts and malpighian tubes. (D) A composite fluorescence image of a control, buffer (1XPBT) fed living larva imaged using the 568 nm filter. Note that no distinct fluorescence is observed. (E) A composite fluorescence image of a control, water fed living larva imaged using the 568 nm filter. No obvious fluorescence is observed. The guts show some auto fluorescence, but note that the staining pattern is different from what is seen in C and B.
ORMOSIL is present within specific cellular compartments. (A) A representative image showing cell bodies from ORMOSIL treated larval brains stained with the golgi marker gp120 (green). (B) ORMOSIL can be observed in red. Note that some ORMOSIL puncta and golgi puncta colocalize (arrows in merged image, C) indicating that ORMOSIL is present within discret compartments within the cell body and is not at the cell surface. Bar = 5 µm.
We thank Hasan Hasanov for troubleshooting initial larval lethality experiments, Dr Restifo for assistance with the primary neuronal culture protocol, Drs Slaughter and Hollingsworth for helpful comments, Kate Kowalski for editorial assistance and Dr Karunaratne for constant support. We also thank to our anonymous reviewers for their comments and suggestions. We dedicate this work to the memory of Herschel Gunawardena and Tom Gehrels.
Conceived and designed the experiments: FB PLN RK GJI MLK AK EJB PNP SG. Performed the experiments: FB PLN RK GJI MLK AK. Analyzed the data: FB PLN GJI AK SG. Wrote the paper: RK EJB SG.
- 1. Kim S, Lim YT, Soltesz EG, De Grand AM, Lee J, et al. (2004) Near-infrared fluorescent type II quantum dots for sentinel lymph node mapping. Nat Biotechnol 22: 93.S. KimYT LimEG SolteszAM De GrandJ. Lee2004Near-infrared fluorescent type II quantum dots for sentinel lymph node mapping.Nat Biotechnol2293
- 2. Nyk M, Kumar R, Ohulchanskyy TY, Bergey EJ, Prasad PN (2008) High contrast in vitro and in vivo photoluminescence bioimaging using near infrared to near infrared up-conversion in Tm3+ and Yb3+ doped fluoride nanophosphors. Nano Lett 8: 3834.M. NykR. KumarTY OhulchanskyyEJ BergeyPN Prasad2008High contrast in vitro and in vivo photoluminescence bioimaging using near infrared to near infrared up-conversion in Tm3+ and Yb3+ doped fluoride nanophosphors.Nano Lett83834
- 3. Deissler V, Ruger R, Frank W, Fahr A, Kaiser WA, et al. (2008) Fluorescent liposomes as contrast agents for in vivo optical imaging of edemas in mice. Small 4: 1240.V. DeisslerR. RugerW. FrankA. FahrWA Kaiser2008Fluorescent liposomes as contrast agents for in vivo optical imaging of edemas in mice.Small41240
- 4. Ghoroghchian PP, Frail PR, Susumu K, Blessington D, Brannan AK, et al. (2005) Near-infrared-emissive polymersomes: self-assembled soft matter for in vivo optical imaging. Proc Natl Acad Sci USA 102: 2922.PP GhoroghchianPR FrailK. SusumuD. BlessingtonAK Brannan2005Near-infrared-emissive polymersomes: self-assembled soft matter for in vivo optical imaging.Proc Natl Acad Sci USA1022922
- 5. Altinoglu EI, Russin TJ, Kaiser JM, Barth BM, Eklund PC, et al. (2008) Near-infrared emitting fluorophore-doped calcium phosphate nanoparticles for in vivo imaging of human breast cancer. ACS Nano 2: 2075.EI AltinogluTJ RussinJM KaiserBM BarthPC Eklund2008Near-infrared emitting fluorophore-doped calcium phosphate nanoparticles for in vivo imaging of human breast cancer.ACS Nano22075
- 6. Josephson L, Kircher MF, Mahmood U, Tang Y, Weissleder R (2002) Near-infrared fluorescent nanoparticles as combined MR/optical imaging probes. Bioconjugate Chem 13: 554.L. JosephsonMF KircherU. MahmoodY. TangR. Weissleder2002Near-infrared fluorescent nanoparticles as combined MR/optical imaging probes.Bioconjugate Chem13554
- 7. Park JH, von Maltzahn G, Ruoslahti E, Bhatia SN, Sailor MJ (2008) Micellar hybrid nanoparticles for simultaneous magnetofluorescent imaging and drug delivery. Angew Chem Int Ed 47: 7284.JH ParkG. von MaltzahnE. RuoslahtiSN BhatiaMJ Sailor2008Micellar hybrid nanoparticles for simultaneous magnetofluorescent imaging and drug delivery.Angew Chem Int Ed477284
- 8. Kumar R, Roy I, Ohulchanskyy TY, Goswami LN, Bonoiu AC, et al. (2008) Covalently dye-linked, surface-controlled, and bioconjugated organically modified silica nanoparticles as targeted probes for optical imaging. ACS Nano 2: 449.R. KumarI. RoyTY OhulchanskyyLN GoswamiAC Bonoiu2008Covalently dye-linked, surface-controlled, and bioconjugated organically modified silica nanoparticles as targeted probes for optical imaging.ACS Nano2449
- 9. Slowing II, Wu CW, Vivero-Escoto JL, Lin VS (2009) Mesoporous silica nanoparticles for reducing hemolytic activity towards mammalian red blood cells. Small 5: 57–62.II SlowingCW WuJL Vivero-EscotoVS Lin2009Mesoporous silica nanoparticles for reducing hemolytic activity towards mammalian red blood cells.Small55762
- 10. Ow H, Larson DR, Srivastava M, Baird BA, Webb WW, et al. (2005) Bright and stable core-shell fluorescent silica nanoparticles. Nano Lett 5: 113.H. OwDR LarsonM. SrivastavaBA BairdWW Webb2005Bright and stable core-shell fluorescent silica nanoparticles.Nano Lett5113
- 11. Zhao X, Hilliard LR, Mechery SJ, Wang Y, Bagwe RP, et al. (2004) A rapid bioassay for single bacterial cell quantitation using bioconjugated nanoparticles. Proc Natl Acad Sci USA 101: 15027.X. ZhaoLR HilliardSJ MecheryY. WangRP Bagwe2004A rapid bioassay for single bacterial cell quantitation using bioconjugated nanoparticles.Proc Natl Acad Sci USA10115027
- 12. Sharma RK, Das S, Maitra A (2004) Surface modified ormosil nanoparticles. J Colloid Interface Sci 277: 342–6.RK SharmaS. DasA. Maitra2004Surface modified ormosil nanoparticles.J Colloid Interface Sci2773426
- 13. Qian J, Li X, Wei M, Gao X, Xu Z, et al. (2008) Bio-molecule-conjugated fluorescent organically modified silica nanoparticles as optical probes for cancer cell imaging. Opt Express 16: 19568–78.J. QianX. LiM. WeiX. GaoZ. Xu2008Bio-molecule-conjugated fluorescent organically modified silica nanoparticles as optical probes for cancer cell imaging.Opt Express161956878
- 14. Walcarius A, Ganesan V (2006) Ion-exchange properties and electrochemical characterization of quaternary ammonium-functionalized silica microspheres obtained by the surfactant template route. Langmuir 22: 469–77.A. WalcariusV. Ganesan2006Ion-exchange properties and electrochemical characterization of quaternary ammonium-functionalized silica microspheres obtained by the surfactant template route.Langmuir2246977
- 15. Han L, Sakamoto Y, Che S, Terasaki O (2009) Insight into the defects of cage-type silica mesoporous crystals with Fd3m symmetry: TEM observations and a new proposal of “polyhedron packing” for the crystals. Chemistry 15: 2818–25.L. HanY. SakamotoS. CheO. Terasaki2009Insight into the defects of cage-type silica mesoporous crystals with Fd3m symmetry: TEM observations and a new proposal of “polyhedron packing” for the crystals.Chemistry15281825
- 16. Santra S, Liesenfeld B, Dutta D, Chatel D, Batich CD, et al. (2005) Folate conjugated fluorescent silica nanoparticles for labeling neoplastic cells. J Nanosci Nanotechnol 5: 899–904.S. SantraB. LiesenfeldD. DuttaD. ChatelCD Batich2005Folate conjugated fluorescent silica nanoparticles for labeling neoplastic cells.J Nanosci Nanotechnol5899904
- 17. Santra S, Yang H, Dutta D, Stanley JT, Holloway PH, et al. (2004) TAT conjugated, FITC doped silica nanoparticles for bioimaging applications. Chem Commun (Camb) 24: 2810–1.S. SantraH. YangD. DuttaJT StanleyPH Holloway2004TAT conjugated, FITC doped silica nanoparticles for bioimaging applications.Chem Commun (Camb)2428101
- 18. Bharali DJ, Klejbor I, Stachowiak EK, Dutta P, Roy I, et al. (2005) Organically modified silica nanoparticles: a nonviral vector for in vivo gene delivery and expression in the brain. Proc Natl Acad Sci U S A 102: 11539–44.DJ BharaliI. KlejborEK StachowiakP. DuttaI. Roy2005Organically modified silica nanoparticles: a nonviral vector for in vivo gene delivery and expression in the brain.Proc Natl Acad Sci U S A1021153944
- 19. Roy I, Ohulchanskyy TY, Pudavar HE, Bergey EJ, Oseroff AR, et al. (2003) Ceramic-based nanoparticles entrapping water-insoluble photosensitizing anticancer drugs: a novel drug-carrier system for photodynamic therapy. J Am Chem Soc 125: 7860–5.I. RoyTY OhulchanskyyHE PudavarEJ BergeyAR Oseroff2003Ceramic-based nanoparticles entrapping water-insoluble photosensitizing anticancer drugs: a novel drug-carrier system for photodynamic therapy.J Am Chem Soc12578605
- 20. Kim S, Ohulchanskyy TY, Pudavar HE, Pandey RK, Prasad PN (2007) Organically modified silica nanoparticles co-encapsulating photosensitizing drug and aggregation-enhanced two-photon absorbing fluorescent dye aggregates for two-photon photodynamic therapy. J Am Chem Soc 129: 2669–75.S. KimTY OhulchanskyyHE PudavarRK PandeyPN Prasad2007Organically modified silica nanoparticles co-encapsulating photosensitizing drug and aggregation-enhanced two-photon absorbing fluorescent dye aggregates for two-photon photodynamic therapy.J Am Chem Soc129266975
- 21. Adams MD, Celniker SE, Holt RA, Evans CA, Gocayne JD, et al. (2000) The genome sequence of Drosophila melanogaster. Science 287: 2185–95.MD AdamsSE CelnikerRA HoltCA EvansJD Gocayne2000The genome sequence of Drosophila melanogaster.Science287218595
- 22. Lessing D, Bonini NM (2009) Maintaining the brain: insight into human neurodegeneration from Drosophila melanogaster mutants. Nat Rev Genet 10: 359–70.D. LessingNM Bonini2009Maintaining the brain: insight into human neurodegeneration from Drosophila melanogaster mutants.Nat Rev Genet1035970
- 23. Affleck JG, Walker VK (2008) A role for Drosophila in understanding drug-induced cytotoxicity and teratogenesis. Cytotechnology 57: 1–9.JG AffleckVK Walker2008A role for Drosophila in understanding drug-induced cytotoxicity and teratogenesis.Cytotechnology5719
- 24. Nichols CD (2006) Drosophila melanogaster neurobiology, neuropharmacology, and how the fly can inform central nervous system drug discovery. Pharmacol Ther 112: 677–700.CD Nichols2006Drosophila melanogaster neurobiology, neuropharmacology, and how the fly can inform central nervous system drug discovery.Pharmacol Ther112677700
- 25. Rand MD (2010) Drosophotoxicology: the growing potential for Drosophila in neurotoxicology. Neurotoxicol Teratol 32: 74–83.MD Rand2010Drosophotoxicology: the growing potential for Drosophila in neurotoxicology.Neurotoxicol Teratol327483
- 26. Kumar R, Roy I, Ohulchanskky TY, Vathy LA, Bergey EJ, et al. (2010) In vivo biodistribution and clearance studies using multimodal organically modified silica nanoparticles. ACS Nano 4: 699–708.R. KumarI. RoyTY OhulchanskkyLA VathyEJ Bergey2010In vivo biodistribution and clearance studies using multimodal organically modified silica nanoparticles.ACS Nano4699708
- 27. Qu L, Akbergenova Y, Hu Y, Schikorski T (2009) Evolutionary conservation of vertebrate blood-brain barrier chemoprotective mechanisms in Drosophila. J Comparative Neurology 514: 343–352.L. QuY. AkbergenovaY. HuT. Schikorski2009Evolutionary conservation of vertebrate blood-brain barrier chemoprotective mechanisms in Drosophila.J Comparative Neurology514343352
- 28. de Jong G, van Dijk JP, van Eijk HG (1990) The biology of transferrin. Clin Chim Acta 190: 1–46.G. de JongJP van DijkHG van Eijk1990The biology of transferrin.Clin Chim Acta190146
- 29. Qian ZM, Li AN, Sun H, Ho K (2002) Targeted Drug Delivery via the Transferrin Receptor- Mediated Endocytosis Pathway. Pharmacol Rev 54: 561–587.ZM QianAN LiH. SunK. Ho2002Targeted Drug Delivery via the Transferrin Receptor- Mediated Endocytosis Pathway.Pharmacol Rev54561587
- 30. Gunawardena S, Goldstein LS (2001) Disruption of axonal transport and neuronal viability by amyloid precursor protein mutations in Drosophila. Neuron 32: 389–401.S. GunawardenaLS Goldstein2001Disruption of axonal transport and neuronal viability by amyloid precursor protein mutations in Drosophila.Neuron32389401
- 31. Satpute-Krishnan P, Degiorgis JA, Conley MP, Jang M, Bearer EL (2006) A peptide zipcode sufficient for anterograde transport within amyloid precursor protein. Proc Natl Acad Sci U S A 103: 16532–7.P. Satpute-KrishnanJA DegiorgisMP ConleyM. JangEL Bearer2006A peptide zipcode sufficient for anterograde transport within amyloid precursor protein.Proc Natl Acad Sci U S A103165327
- 32. Ashburner M, Thompson JN (1978) The laboratory culture of Drosophila. In: Ashburner M, Wright TRF, editors. The Genetics and Biology of Drosophila, vol. 2a. London: Academic Press. pp. 1–109.M. AshburnerJN Thompson1978The laboratory culture of Drosophila.M. AshburnerTRF WrightThe Genetics and Biology of Drosophila, vol. 2aLondonAcademic Press1109
- 33. Ashburner M, Golic KG, Hawley RS (2005) Drosophila: a laboratory handbook. Second edition xxviii + 1408.M. AshburnerKG GolicRS Hawley2005Drosophila: a laboratory handbook.Second editionxxviii + 1408
- 34. Pavlidis P, Tanouye MA (1995) Seizures and failures in the giant fiber pathway of Drosophila bang-sensitive paralytic mutants. J Neurosci 8: 5810–9.P. PavlidisMA Tanouye1995Seizures and failures in the giant fiber pathway of Drosophila bang-sensitive paralytic mutants.J Neurosci858109
- 35. Lee J, Wu CF (2002) Electroconvulsive seizure behavior in Drosophila: analysis of the physiological repertoire underlying a stereotyped action pattern in bang-sensitive mutants. J Neurosci 22: 11065–79.J. LeeCF Wu2002Electroconvulsive seizure behavior in Drosophila: analysis of the physiological repertoire underlying a stereotyped action pattern in bang-sensitive mutants.J Neurosci221106579
- 36. Fye S, Dolma K, Kang MJ, Gunawardena S (2010) Visualization of larval segmental nerves in 3rd instar Drosophila larval preparations. J Vis Exp 43: 2128.S. FyeK. DolmaMJ KangS. Gunawardena2010Visualization of larval segmental nerves in 3rd instar Drosophila larval preparations.J Vis Exp432128
- 37. Hewes RS, Snowdeal EC 3rd, Saitoe M, Taghert PH (1998) Functional redundancy of FMRFamide-related peptides at the Drosophila larval neuromuscular junction. J Neurosci 18: 7138–51.RS HewesEC Snowdeal 3rdM. SaitoePH Taghert1998Functional redundancy of FMRFamide-related peptides at the Drosophila larval neuromuscular junction.J Neurosci18713851
- 38. Meeusen T, Mertens I, Clynen E, Baggerman G, Nichols R, et al. (2002) Identification in Drosophila melanogaster of the invertebrate G protein-coupled FMRFamide receptor. Proc Natl Acad Sci U S A 99: 15363–8.T. MeeusenI. MertensE. ClynenG. BaggermanR. Nichols2002Identification in Drosophila melanogaster of the invertebrate G protein-coupled FMRFamide receptor.Proc Natl Acad Sci U S A99153638
- 39. Pereanu W, Spindler S, Im E, Buu N, Hartenstein V (2007) The emergence of patterned movement during late embryogenesis of Drosophila. Dev Neurobiol 67: 1669–85.W. PereanuS. SpindlerE. ImN. BuuV. Hartenstein2007The emergence of patterned movement during late embryogenesis of Drosophila.Dev Neurobiol67166985
- 40. Kuznicki ML, Gunawardena S (2010) In vivo visualization of synaptic vesicles within Drosophila larval segmental axons. J Vis Exp 44: 2151.ML KuznickiS. Gunawardena2010In vivo visualization of synaptic vesicles within Drosophila larval segmental axons.J Vis Exp442151
- 41. Ohulchanskyy TY, Roy I, Goswami LN, Chen Y, Bergey EJ, et al. (2007) Organically modified silica nanoparticles with covalently incorporated photosensitizer for photodynamic therapy of cancer. Nano Lett 7: 2835–42.TY OhulchanskyyI. RoyLN GoswamiY. ChenEJ Bergey2007Organically modified silica nanoparticles with covalently incorporated photosensitizer for photodynamic therapy of cancer.Nano Lett7283542
- 42. Gunawardena S, Goldstein LS (2005) Polyglutamine diseases and transport problems: deadly traffic jams on neuronal highways. Arch Neurol 62: 46–51.S. GunawardenaLS Goldstein2005Polyglutamine diseases and transport problems: deadly traffic jams on neuronal highways.Arch Neurol624651
- 43. Gunawardena S, Goldstein LS (2004) Cargo-carrying motor vehicles on the neuronal highway: transport pathways and neurodegenerative disease. J Neurobiol 58: 258–71.S. GunawardenaLS Goldstein2004Cargo-carrying motor vehicles on the neuronal highway: transport pathways and neurodegenerative disease.J Neurobiol5825871
- 44. Gunawardena S, Her LS, Brusch RG, Laymon RA, Niesman IR, et al. (2003) Disruption of axonal transport by loss of huntingtin or expression of pathogenic polyQ proteins in Drosophila. Neuron 40: 25–40.S. GunawardenaLS HerRG BruschRA LaymonIR Niesman2003Disruption of axonal transport by loss of huntingtin or expression of pathogenic polyQ proteins in Drosophila.Neuron402540
- 45. Hurd DD, Saxton WM (1996) Kinesin mutations cause motor neuron disease phenotypes by disrupting fast axonal transport in Drosophila. Genetics 144: 1075–85.DD HurdWM Saxton1996Kinesin mutations cause motor neuron disease phenotypes by disrupting fast axonal transport in Drosophila.Genetics144107585
- 46. Pluskota A, Horzowski E, Bossinger O, von Mikecz A (2009) In Caenorhabditis elegans nanoparticle-bio-interactions become transparent: silica-nanoparticles induce reproductive senescence. PLoS One 4: e6622.A. PluskotaE. HorzowskiO. BossingerA. von Mikecz2009In Caenorhabditis elegans nanoparticle-bio-interactions become transparent: silica-nanoparticles induce reproductive senescence.PLoS One4e6622
- 47. Kaspar BK, Lladó J, Sherkat N, Rothstein JD, Gage FH (2003) Retrograde viral delivery of IGF-1 prolongs survival in a mouse ALS model. Science 301: 839–42.BK KasparJ. LladóN. SherkatJD RothsteinFH Gage2003Retrograde viral delivery of IGF-1 prolongs survival in a mouse ALS model.Science30183942
- 48. Kells AP, Fong DM, Dragunow M, During MJ, Young D, et al. (2004) AAV-mediated gene delivery of BDNF or GDNF is neuroprotective in a model of Huntington disease. Mol Ther 9: 682–8.AP KellsDM FongM. DragunowMJ DuringD. Young2004AAV-mediated gene delivery of BDNF or GDNF is neuroprotective in a model of Huntington disease.Mol Ther96828
- 49. Hsich G, Sena-Esteves M, Breakefield XO (2002) Critical issues in gene therapy for neurologic disease. Hum Gene Ther 13: 579–604.G. HsichM. Sena-EstevesXO Breakefield2002Critical issues in gene therapy for neurologic disease.Hum Gene Ther13579604
- 50. Mayer F, Mayer N, Chinn L, Pinsonneault RL, Kroetz D, et al. (2009) Evolutionary conservation of vertebrate blood-brain barrier chemoprotective mechanisms in Drosophila. J Neurosci 29: 3538–50.F. MayerN. MayerL. ChinnRL PinsonneaultD. Kroetz2009Evolutionary conservation of vertebrate blood-brain barrier chemoprotective mechanisms in Drosophila.J Neurosci29353850
- 51. Kraft R, Levine RB, Restifo LL (1998) The steroid hormone 20-hydroxyecdysone enhances neurite growth of Drosophila mushroom body neurons isolated during metamorphosis. J Neurosci 18: 8886–99.R. KraftRB LevineLL Restifo1998The steroid hormone 20-hydroxyecdysone enhances neurite growth of Drosophila mushroom body neurons isolated during metamorphosis.J Neurosci18888699