The identification of mRNAs in distal projections of model organisms has led to the discovery of multiple proteins that are locally synthesized for functional roles such as axon guidance, injury signaling and regeneration. The extent to which local protein synthesis is conserved in human neurons is unknown. Here we used compartmentalized microfluidic chambers to characterize the transcriptome of distal projections of human embryonic stem cells differentiated using a protocol which enriched for glutamatergic neurons (hESC-neurons). Using gene expression analysis, we identified mRNAs proportionally enriched in these projections, representing a functionally unique local transcriptome as compared to the human neuronal transcriptome inclusive of somata. Further, we found that the most abundant mRNAs within these hESC-neuron projections were functionally similar to the axonal transcriptome of rat cortical neurons. We confirmed the presence of two well characterized axonal mRNAs in model organisms, β-actin and GAP43, within hESC-neuron projections using multiplexed single molecule RNA-FISH. Additionally, we report the novel finding that oxytocin mRNA localized to these human projections and confirmed its localization using RNA-FISH. This new evaluation of mRNA within human projections provides an important resource for studying local mRNA translation and has the potential to reveal both conserved and unique translation dependent mechanisms.
Local translation within the axons and dendrites of neurons is involved in multiple neuronal functions, including axon maintenance, guidance, synaptogenesis, post- and presynaptic plasticity and response to injury1,2,3,4,5. Specific mRNAs implicated in these functions, distal from somata, have been experimentally identified in Aplysia sensory neurites, rodent peripheral and central neurons, and multiple other model systems2, 6,7,8,9,10. In axons and synapses, local translation may be critical for spatially restricted and rapid responses to extracellular signals such as glutamate, brain derived neurotrophic factor, neurotrophin-3 and netrin-18, 11,12,13,14.
Comparing axonal transcriptomes of various neuronal subtypes has the potential to highlight conserved roles of intra-axonal translation and reveal unique functions and targets within each neuron type. Direct evaluation of primary human neurons is severely restricted due to the limited ability to obtain tissue or culture isolated neurons. Human stem cell derived neurons are a biologically relevant and tractable in vitro system and protocols have been developed to differentiate stem cells into specific neuronal subtypes, such as motor, striatal, dopaminergic and glutamatergic neurons15,16,17,18,19,20. Here we sought to identify the transcriptome of the distal projections of human embryonic stem cell derived neurons enriched for glutamatergic lineage20, 21 and compare this transcriptome to axonal transcriptomes from rodent model systems.
Differentiation of human embryonic stem cell derived neurons in microfluidic chambers
To identify transcripts within human projections we first modified an existing microfluidic chamber design for compartmentalizing and harvesting pure axons, originally developed for murine neurons22. To optimize the growth of hESC-neurons, which have an increased nutrient demand compared to primary rodent neurons, we increased the height of the fluidically isolated compartments to provide a greater volume of media surrounding the cells. In these microfluidic chambers, neurons were seeded in the “somatic” compartment and stochastic process growth resulted in processes passing through the 450 µm long microgrooves to the “axonal” compartment (Fig. 1A). Similar chamber designs have been used to characterize the axonal transcriptome of primary rat cortical neurons and mouse motoneurons23, 24.
Differentiation of hESC-neurons began in traditional tissue culture dishes on days in vitro (DIV) 0 (Fig. 1A) according to an established protocol to enrich for functionally matured glutamatergic neurons that produce action potentials after approximately 6 weeks of differentiation20, 21. On DIV24 neural progenitor cells were transferred to our custom microfluidic chambers and matured to hESC-neurons over the next 30 day (>7 weeks in culture total). As early as DIV39 long neurites could be seen in the microgrooves. Microtubule-associated protein 2 (MAP2) and neuron-specific class III β-tubulin (β-tubulin III, βtub) staining, markers for cell bodies/dendrites and neurons inclusive of axons, respectively, suggest that the majority of neurites entering the axonal compartment are axon-like (Fig. 1B). β-tubulin III staining revealed extensive neurite growth within the axonal compartment at DIV58 (Fig. 1C) as well as healthy growth cones (Fig. 1D). After five weeks in culture, some clustering of somata occurred, as is common in long term cultures of hESC-neurons. Cells demonstrated neuron arborization as revealed by MAP2 staining (Fig. 1E). After DIV49 >90% of cells within the microfluidic chamber differentiated into neurons; 198 of 209 of DAPI-labeled nuclei were positive for MAP2 and/or β-tubulin III. The remaining cells had neurites but stained positive for the neural precursor marker Nestin (3.8%, 19 cells of 501 nuclei) or the astrocytic marker glial fibrillary acidic protein (GFAP, 3.7%, 27 cells of 724 nuclei). The enriched glutamatergic identity of these hESC-neurons was substantiated by staining for vesicular glutamate transporter 1 (VGLUT1), a marker of glutamatergic lineage (Fig. 1F). Approximately 38% of all cells were VGLUT1 positive (128 cells of 333 nuclei) and approximately 2.3% were GABAergic, as determined by glutamate decarboxylase (GAD67) immunostaining (12 cells of 516 nuclei). This differentiation efficiency and neuron subtype enrichment were consistent with published hESC-neuron differentiation protocols25.
To further evaluate the composition of neurites extending into the axonal compartment, we tested whether a modified rabies virus which infects neurons via axonally localized receptors and encodes a fluorescent protein would infect neurons when applied exclusively to the distal neurites within the axonal compartment. Rabies virus infection requires endocytosis and retrograde transport of viral particles following attachment to one of three axonal receptors: nicotinic acetylcholine receptor, neuronal cell adhesion molecule or p75 neurotrophin receptor26. A modified rabies virus incapable of trans-synaptic transmission and carrying the mCherry gene27 was exclusively added to the axonal compartment of hESC-neuron cultures for 2 hours. Once infected, fluorescent protein expression can be detected throughout the cell, including the axons and dendrites, within 48 hours. Live DIC and fluorescent imaging was performed to visualize the fine processes and fluorescent protein expression throughout the hESC-neurons cultured within the microfluidic chamber (Fig. 1G). Our data show that distal projections of hESC-neurons contain axonally-localized receptors sufficient for rabies viral infection.
Differential gene expression between distal projections and neurons derived from hESCs
On DIV58, after more than 8 weeks in culture, we harvested total RNA from hESC-neurons and isolated neurites within the somatic and axonal compartments of microfluidic chambers (referred to as “neuron” and “projection” samples, respectively). The neuron sample included somata, dendrite- and axon-like projections. The projection samples were stringently scrutinized by light microscopy to ensure no somata were present in the axonal compartment. The amount of RNA harvested from the axonal compartment of an individual microfluidic chamber was below detection limits, therefore one round of linear cDNA amplification was performed on a fixed volume of RNA and a fixed mass of neuronal RNA. As a control reaction 10 pg of neuronal RNA was subjected to linear amplification in parallel. The amount of cDNA generated in this reaction suggested that the RNA yield within the axonal compartment was approximately 2 pg/µL (data not shown). Equivalent amounts of cDNA from all samples was processed for microarray expression profiling, including the 10 pg neuronal sample. Potential chamber-to-chamber variability as well as possible variation in sample collection led us to evaluate the specificity and robustness of our expression profiling. Box-and-whiskers plot of the raw probe cell intensity (log2) by sample shows similarity between the dynamic range of replicates (t-test, p = 0.40) (Fig. 2A). Pearson’s correlation analysis demonstrated a high degree of correlation between replicates (correlation r-value >0.8) (Fig. 2B). This replicability suggests little variation in the differentiation efficiency between chambers. The 10 pg neuronal sample expression profile more closely resembled the neuronal samples than the axonal samples (data not shown), showing that the linear amplification step broadly preserved the gene expression profile of the low concentration samples.
The identity of transcripts within the axonal compartment that have disproportionally high expression may reveal functions reliant on local translation. We evaluated the proportionally enriched fraction of mRNAs within our axonal dataset by DAVID Gene Functional Classification28, 29. For comparison we also evaluated the proportionally depleted mRNAs within the axonal dataset. Figure 2C is a scatterplot of expression levels highlighting these fractions and Fig. 2D is a pie chart depicting the proportion of probe sets within these two fractions. DAVID Gene Functional Classification of these genes revealed functional categories which were assigned an enrichment score (Fig. 2E,F). This enrichment score measures and weighs the ratio of transcripts that fall into a given functional category. The proportionally enriched mRNAs within hESC-neuron projections were classified as “secreted” and “extracellular” proteins, “DNA sequence-specific binding” proteins, “neurofilament” proteins and “voltage-gated” and “cation” channels (Fig. 2E). This analysis suggests that translation of proteins within these classes may have a more prominent role within the specialized distal subcellular compartment than within the soma. The proportionally depleted mRNAs were associated with the terms “intracellular” and “nuclear” proteins and proteins that function in RNA splicing, protein degradation and maintaining genome organization and integrity (Fig. 2F), functions representative of the identity of this dataset inclusive of somata and dendrites. Taken together these data suggest that enriched transcripts within the distal projections of hESC-neurons have the capacity to support a repertoire of functions autonomously from the cell body.
Abundant transcripts within distal projections of hESC-neurons functionally resemble axonal transcripts localized to rat cortical neurons
Many of the mRNAs highly abundant within the long projections of hESC-neurons were not enriched relative to neuronal samples, yet may perform important biological functions that depend on local translation. For example, β-actin (ACTB) is not enriched in our dataset (expression in ‘projections’: 6.74; expression in ‘neurons’: 6.86; fold change −1.09) nor in the axonal transcriptome of rat cortical neurons, yet local translation of β-actin in neurites and axons is well-established14, 30. To assess the degree of functional similarity between the abundant transcripts within hESC-neuron long projections and comparable primary rodent glutamatergic neurons we first created a subset of our expression data containing the microarray probe sets with the highest average signal intensity in our projection samples, those above the 90th percentile (expression value ≥6.48), representing the highest expressed transcripts (Fig. 3A) (3696 transcripts). We compared this subset of highly expressed transcripts by DAVID Gene Functional Classification with a published dataset of mRNAs reliably localized to axons of primary embryonic rat cortical neurons grown in similar microfluidic chambers23. Transcripts encoding proteins involved in translation and ribosomal proteins were significantly over-represented in the resulting transcriptomes from both species as well as proteins of the mitochondrial “respiratory chain” and cytoskeletal proteins (“Neurofilament” in hESC-neurons and “Microtubule” and “Cell projection” in rat cortical neurons, Fig. 3B,C). Unique to the hESC-neuron were transcripts encoding “Extracellular” proteins. Post hoc evaluation of this threshold revealed that it excluded known abundant dendritic transcripts, such as ARC, CAMK2A and AMPA receptor subunits and included the well characterized axonal transcript GAP43 (>98th percentile) and ACTB (>93rd percentile); thus, suggesting that our ‘projection’ samples contain mostly axon-like projections. Overall, these data suggest that the axonal transcriptomes of hESC-neurons and primary rat cortical neurons are broadly similar, despite differences in species of origin and neuron derivation.
RNA-FISH verification of specific mRNAs within hESC-neuron distal projections
To validate our microarray results, we chose to verify the presence of known axonally localized mRNA transcripts and a novel distally localized mRNA identified in our expression data using fluorescence in situ hybridization (FISH). The transcripts selected for visualization were β-actin (ACTB), growth associated protein 43 (GAP43) and oxytocin (OXT). ACTB and GAP43 mRNA are well characterized within rodent axons and are locally translated31. We identified OXT mRNA as a potentially unique transcript present in these human axons, which is below detection in rodent cortical axons23. The presence and function of OXT mRNA within distal projections has not been investigated to our knowledge. Our FISH results confirmed the presence of ACTB, GAP43, and OXT transcripts within the long projections of hESC-neurons (Fig. 4A,C). RNA-FISH probes were omitted for negative control axons (Fig. 4B) and no fluorescence puncta were detected in these samples. Due to the short length of the oxytocin mRNA (548 nt) and homology with vasopressin mRNA (AVP) our custom OXT RNA-FISH probe set pool (Affymetrix) contained 7 branched DNA sequences instead of the customary 20 sequences, which may explain the smaller size of these fluorescent puncta. Together, these data validate our microarray data and demonstrate that these human distal projections contain mRNAs found in axons of model organisms, yet also have mRNAs that may be uniquely localized to human axons.
Subcellular compartments distal from the cell body, such as axons, were once thought to be devoid of mRNA and ribosomes but are proving to contain transcripts encoding thousands of proteins and the machinery for translation32, 33. Functionally, intra-axonal translation is necessary for growth cone guidance, axon maintenance, injury response and may be involved in presynaptic plasticity. Specific locally translated mRNAs involved in these cellular events have been identified6, 7, 9, 14, 30, 34,35,36,37,38,39,40,41,42,43. Discovery of axonally translated proteins in hESC-neurons has the potential to expand and deepen our knowledge of the role of local translation. While this study focuses on the proportionally enriched fraction and the abundant transcripts within distal projections local translation of moderate to low abundance axonal transcripts may also be functionally relevant.
Functional classification of differentially enriched mRNAs revealed that local, distal translation of transcription factors (Fig. 2D, “Sequence-specific DNA binding”) is likely a common mechanism by which distal events trigger a transcriptional response following transport of the protein to the nucleus. Axonal translation of the transcription factors ATF4 and STAT3 are induced following injury in CNS and PNS neurons, respectively39, 41. Retrograde transport of these proteins to the soma may mediate the transcriptional response to axon injury. Alternatively, some annotated transcription factors could have transcription-independent roles. For example, axonally synthesized β-catenin, a Wnt signal transducer, functions at the presynapse as a scaffold protein9, 39, 41, 44. The highly enriched category of “secreted” protein transcripts suggests a significant demand on distal projections to dynamically modulate the extracellular environment, likely as part of axon guidance, synaptogenesis and even synaptic plasticity. Differential expression of the proportionally enriched and proportionally depleted fractions may be the cumulative result of differential trafficking of RNA to distal subcellular compartments as well as differential mRNA stability. Messenger RNA stability can be regulated by multiple mechanisms, including microRNAs and nonsense mediated decay. MicroRNA mediated mRNA regulation is documented in axons45, 46. Nonsense mediated decay (NMD) components are present in axons and growth cones and in vivo disruption of NMD in mouse commissural neurons alters axon guidance. Spatiotemporal cues developmentally regulate NMD of Robo3.2 mRNA in the axons of these neurons40.
Our comparison of the most abundant distal mRNAs within hESC-neurons with that of axons of primary embryonic rat cortical neurons revealed functional similarities, specifically in mRNAs encoding proteins required for translation, ribosomal proteins and nuclear-encoded mitochondrial proteins necessary for ATP production (Fig. 3B and C). These axon enriched categories have been described in the adult rat neuropil, adult and embryonic rat DRGs, embryonic mouse DRGs, embryonic mouse motoneurons and mouse retinal ganglion cells10, 24, 47,48,49. Axonal translation of nuclear encoded mitochondrial respiratory chain proteins has been described previously50, 51. We speculate that it is more efficient to replenish critical mitochondrial proteins via de novo and in situ translation than for the neuron to support a continual cycle of soma to axon mitochondrial protein transport. The conservation of ribosomal protein transcripts in axons suggest that either the protein components of the ribosome have a shorter half-life than the RNA components or local translation of ribosomal proteins is a mechanism to dynamically regulate distal ribosomes and translation. There are over 100 human ribosomal proteins but only a few are characterized as constitutive ribosome components and the function of many of these proteins are unknown. It is interesting to speculate that the unique repertoire of ribosomal proteins associated with rRNA could confer target mRNA specificity. Ribosomes containing Ribosomal Protein L38 have been shown to preferentially interact with and translate the mRNA of Hox genes in mouse52. With the large number of ribosomal proteins it is possible that this is a common, under characterized, mechanism of translational regulation. Additionally, ribosomal proteins may mediate differential ribosome localization by regulating ribosome interaction with transmembrane proteins of organelles, such as the axonal endoplasmic reticulum, or growth factor receptors, such as the netrin-1 receptor Deleted in Colorectal Cancer (DCC)53.
We confirmed the presence of three specific mRNAs, ACTB, GAP43 and OXT, within hESC-neuron axons using multiplexed RNA-FISH. Axonal localization of ACTB and GAP43 appears to be conserved between rodents and humans suggesting that local synthesis of these proteins may also be conserved. Oxytocin mRNA within the axonal compartment and intra-axonal translation of oxytocin may be unique to human neurons.
The time course and identifying characteristics of human neuron polarization has not been rigorously investigated so researchers must apply what is known about neuron polarization from other species. Our immunofluorescent evaluation of the neurites within the microgrooves and the axonal compartment demonstrated that they were β-tubulin III positive and MAP2 negative; these are canonical features of properly polarized axons of embryonic and adult neurons from all model species. Further, a modified rabies virus delivered to the isolated axonal compartment was able to infect the hESC-neurons and the GO functional categories were similar between this hESC-neuron axonal transcriptome and the rat cortical axon transcriptome23.
Neurons derived from in vitro differentiated pluripotent stem cells are generally accepted as resembling fetal neurons54. While the differentiation and maturation protocol we used has generated neurons capable of action potentials as early as DIV4221, a characteristic of functionally mature neurons, these cells are not “aged” to a point of resembling adult neurons. RNA-mediated mechanisms have been implicated in both neurodegenerative and neurodevelopmental models, making “young” and “aged” neurons beneficial model systems. Researchers are working to generate appropriately aged stem cell derived neurons to model age-related neuronal function55.
In the future, the ability to generate patient derived induced pluripotent stem cells and differentiate these cells to neurons within axon isolating microfluidic chambers will facilitate studying axon function in complex genetic diseases such as schizophrenia and autism spectrum disorders. CRISPR-mediated engineered stem cells, such as targeted deletion of RNA binding proteins associated with neurological diseases, applied to our system would provide further insight into the role of local translation in human neurons. As the techniques and algorithms necessary to quantitatively evaluate single cell transcriptomes by RNA-seq become robustly established they can be applied to axonal mRNA to evaluate the localization and relative quantities of splice variants, possibly revealing additional levels of complexity within axonal transcriptomes. Further, mechanistic examination of axonal translation in human axons has the potential to reveal relevant axonal mRNAs in disease and normal neuron function.
Custom microfluidic chambers were fabricated by soft lithography using an established protocol22 with the following modifications. The somatic and axonal compartments of these chambers were 1.5 mm by 7 mm by 450 µm tall. These compartments were connected by microgrooves of 450 µm by 10 µm by 3 µm tall. The only dimension different from previously published microfluidic chambers23 was the compartment height, which was increased to facilitate the daily media changes necessary to meet the nutrient demands of hESC-neurons. To create the tall cell compartments a thick layer of photoresist (SU-8-2050; Microchem) was spun on the wafer in 2 coatings. Each coating was spun at 800 rpm for 45 s, the first coating was baked on a leveled 95 °C hot plate for 3 h and the second coating was baked for 5 h. Wafers were UV-exposed (1000 mJ total over 3 sessions with at least 45 s between exposures) and baked for 1 h in a leveled 95 °C oven. Finally wafers were gradually cooled to room temperature over 30 min and developed in PGMEA.
The resulting masters were used to cast microfluidic chambers using poly(dimethylsiloxane) (PDMS) (Sylgard 184 Silicon Elastomer, Dow Corning) as described previously56. German glass coverslips were sterilized and coated overnight with a solution of 500–550 kDa poly-D-lysine/laminin (80 µg/ml and 10 µg/ml, respectively), washed and dried. Microfluidic chambers were assembled from PDMS devices and coated coverslips.
Maintenance and Differentiation of human ESC-neurons
Stem cell differentiation into neural progenitor cells (neuroepithelial cells) was performed according to previously published modifications of the original protocol20, 21, 57. Days in vitro (DIV) numbering began when H9 human embryonic stem cells were plated in embroid body media to induce neuronal differentiation.
Maturation of hESC-neurons in microfluidic chambers
On DIV24 mitotic neural progenitor cells were manually lifted and dissociated manually or with Accutase (Life Technologies). Approximately 5 × 103 cells were seeded into the somatic compartment of microfluidic chambers in N2B27 media supplemented with 100 ng/ml human recombinant brain derived neurotrophic factor (BDNF). Neural progenitor cells continued to divide during the differentiation period until becoming senescent neurons. Half of the media (100 µl) from each compartment was changed daily and cells were matured for at least 35 days (DIV59). This protocol has been demonstrated to generate glutamatergic neurons as early as DIV25, as verified by staining for the telencephalic transcription factor FOXG1, the transcription factor CTIP specific for subcerebral projection neurons, the glutamatergic transcription factor TBR1 and the glutamatergic marker protein VGLUT120, 21.
Human ESC-neurons grown in axon isolating microfluidic chambers were fixed with freshly prepared 4% paraformaldehyde in PBS containing 40 mg/ml sucrose, 1 μm MgCl2, and 0.1 μm CaCl2 for 45 min. Neurons were permeabilized in 0.25% Triton X-100 for 15 min then blocked in PBS containing 10% goat serum for 15 min. Primary antibodies to β-tubulin III (alias TUJ1) (1:2000; chicken; Aves Labs or 1:1000; rabbit; Abcam ab6046), MAP2 (1:1000; rabbit; Millipore AB5622 or 1:1000; mouse; Sigma M4403), GFAP (1:1000, rabbit; Millipore), Nestin (1:1000, mouse; Abcam) VGLUT1 (1:200; mouse; NeuroMab) and GAD67 (1:2000; chicken; Aves) were diluted in PBS with 1% goat serum and incubated overnight at 4 °C. AlexaFluor goat secondary antibodies conjugated to fluorophores with 488 nm, 568 nm, or 633 nm excitation wavelengths (1:1000; Invitrogen) were diluted in PBS and incubated for 1 h at room temperature. Cells were counterstained with DAPI.
Affymetrix ViewRNA ISH Cell Assay kit was used for multiplexed visualization of β-actin, oxytocin and GAP43 mRNA in human ESC-neurons grown in axon isolating microfluidic chambers. Commercially available ViewRNA Probe Sets were used to detect human β-actin mRNA (Affymetrix, VA4-10293) and GAP43 mRNA (Affymetrix, VA6-13097) and a custom probe was designed by Affymetrix to detect human oxytocin mRNA (Affymetrix, VA1-20398). The exact same staining procedure was used for the negative control samples, but without the RNA-FISH probes. All steps were performed in a humidified chamber according to manufacturer instructions with the following modifications. Cells were fixed for 30 minutes with freshly prepared 4% paraformaldehyde in PBS containing 40 mg/ml sucrose, 1 μm MgCl2, and 0.1 μm CaCl2. Samples were washed with RNase-free PBS then dehydrated and rehydrated through a series of ethanol washes, as outlined in the ViewRNA ISH Cell Assay optional instructions. The optimal protease treatment was determined to be a dilution of 1:5000 for 3 minutes at room temperature. All subsequent steps followed the Affymetrix ViewRNA ISH Cell Assay user manual.
Modified rabies virus infection
The axonal compartment of DIV61 cultures were incubated with approximately 100,000 viral units of modified rabies virus carrying the mCherry gene27 in a total of 50 µl media for 2 hours at 37 °C, washed twice with fresh media and live imaging was performed 48 hours later. We have observed within 48 hours this viral load results in detectable mCherry expression within 80–85% of hESC-neuron axons in microfluidic chambers. Similar observations were made with primary embryonic rat hippocampal neurons grown in axon isolating microfluidic chambers (data not shown). The presence of mCherry negative distal projections within the axonal compartment could arise from variability in the time course of mCherry expression or resistance of these projections to viral infection. In primary rat hippocampal cultures the minimum amount of time to detect fluorescent protein is 48 hours but some cells do not express detectable mCherry until 4 days after transfection.
Z-stack fluorescent images and single plane differential contrast (DIC) images were acquired using a spinning disk confocal imaging system (Revolution XD, Andor Technology) configured for an Olympus IX81 zero-drift microscope and spinning disk unit (CSU-X1, Yokogawa). Light excitation was provided by 100 mW, 405 nm; 50 mW, 488 nm; 50 mW, 561 nm; and 100 mW, 640 nm lasers. The following bandpass emission filters (BrightLine, Semrock) were used: 447/60 nm (TR-F447-060), 525/30 nm (TR-F525-030), 607/36 nm (TR-F607-036), 685/40 nm (TR-F685-040). All slides within a series were imaged during a single session in which image capture settings were identical for all fields.
Z-stack fluorescent images were MAX projected. 16-bit images were manually thresholded to the same values within each series of stained chambers. Montage images were stitched using the ImageJ plugin Stitching58 available in the Fiji imaging processing package.
Determination of differentiation efficiency
Seven fields of hESC-neurons in monolayer from 4 independently stained chambers of at least DIV39 were used to estimate the efficiency of differentiation to mature hESC-neurons as detected by colocalization of DAPI signal with MAP2 or β-tubulin III positive staining. Three fields from two independently stained chambers of at least DIV49 were used to evaluate Nestin, GFAP, VGLUT1 and GAD67.
On DIV59 isolation of RNA from microfluidic cultures using the RNAqueous-Micro Kit (Ambion) was performed as previously described22, 23. To collect RNA from the axonal compartment continuous aspiration was applied to the somatic compartment to prevent somatodendritic RNA from entering the sample. Most of the axonal media was removed and lysis buffer was added to one well, the reagent that flowed to the other axonal well through the axonal compartment was collected as the RNA of distal projections. Subsequent RNA purification was performed according to manufacturer’s instructions and RNA was eluted in a final volume of 10 µl. Neuronal RNA was collected from the somatic compartment of hESC-neurons grown in microfluidic chambers not used for axonal RNA collection, this compartment contained somata, dendrites and axons which did not pass through the microgrooves. The majority of the media from the somatic compartment was removed and the same RNA isolation procedure was followed, omitting constant aspiration. Each sample was obtained from one microfluidic chamber. Samples were stored at −80 °C until further processing by the UNC Lineberger Comprehensive Cancer Center Genomics Core and the UNC School of Medicine Functional Genomics Core. Three axonal and three neuronal samples were collected and analyzed.
RNA amplification and microarray
RNA of distal projections harvested from microfluidic chambers is below the detection limit of currently available technology. A fixed volume of each axonal RNA sample (5 µL) and a fixed mass of each neuronal RNA sample (250 pg) were subjected to one round of linear amplification using the Ovation One-Direct System (NuGEN). This system initiates amplification at the 3′ end as well as randomly throughout the transcript and is optimized for very small biological samples such as single cell transcriptomics. The integrity and concentration of the resulting cDNA samples were quantified with an Agilent Bioanalyzer 2100 at the UNC Lineberger Comprehensive Cancer Center Genomics Core. After amplification axonal samples were 230.5 ng/µl, 305.0 ng/µl and 199.0 ng/µl. Neuronal samples were 519.7 ng/µl, 497.3 ng/µl and 469.9 ng/µl. As a control reaction, 10 pg of neuronal RNA was amplified resulting in a concentration of 252.1 ng/µl, suggesting our original axonal RNA yield ranged from approximately 1.6 to 2.4 pg/µl. A fixed concentration of amplified cDNA from all samples, including the 10 pg neuronal sample, were processed in parallel for microarray analysis using the Encore Biotin Module (NuGEN) at the UNC School of Medicine Functional Genomics Core.
Human Gene 2.0 ST Arrays (Affymetrix) were used and scanned with an Affymetrix GeneChip Scanner 3000 7 G Plus with Autoloader. Affymetrix Expression Console v1.4 software was used to analyze microarray CEL files. Affymetrix normalization controls, built into the microarray chips and analysis software, were used for raw data normalization. The Robust Multichip Analysis (RMA) algorithm was used for global background adjustment, quantile normalization and gene expression summarization between samples. This method is sensitive to small changes between samples without negatively affecting signal variance. Affymetrix Transcriptome Analysis Console v2.0 software algorithms were used to determine differential expression and statistical analysis using one-way between-subject ANOVA of normalized intensities.
Microarray probe sets with fold change linear (Axon vs Neuron) greater than or equal to 1.5 and an ANOVA p-value (Axon vs Neuron) less than 0.05 were designated the enriched fraction (3943 probe sets). Probe sets with fold change linear (Axon vs Neuron) less than or equal to −1.5 and an ANOVA p-value (Axon vs Neuron) less than 0.05 were designated the depleted fraction (3631 probe sets). The fold change threshold of 1.5 was selected to counter balance the compressed calculated fold change values obtained by the RMA method. This threshold generated gene symbol lists of an appropriate size for DAVID Functional Annotation Clustering (<3000). For each subset of the data official gene symbols were extracted, duplicates were removed and gene symbol lists (3297 unique gene symbols in the enriched fraction and 3638 unique gene symbols in the depleted fraction) were submitted to DAVID Bioinformatics Resources for Gene ID Conversion and Functional Annotation Clustering with the single species Homo sapiens selected and the default human background list28, 29.
To obtain a gene symbol list of most abundant transcripts within hESC-neuron distal projections microarray probe sets with Axon bi-weight average signal (log2) equal to or greater than 6.48 were selected. This threshold excluded known dendritic transcripts and included β-actin, a well characterized axonal mRNA. These criteria were similar to those used by Taylor et al. (2009) to determine axonal mRNAs within primary rat cortical neurons. Official gene symbols were extracted, duplicates were removed and the gene symbol list (3696 gene symbols) was submitted to DAVID Bioinformatics Resources for Gene ID Conversion and Functional Annotation Clustering with the single species Homo sapiens selected and the default human background list28, 29.
Accession codes: All raw microarray data and gene expression data have been deposited to the NCBI Gene Expression Omnibus under accession number GSE84975, NCBI tracking system ID 17986454.
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The authors would like to acknowledge the CHANL facility at UNC-CH. R.L.B. was supported in part by a grant from the National Institute of General Medical Sciences under award 5T32 GM007092. A.M.T. acknowledges support from the Eunice Kennedy Shriver NICHD (K12 HD073945), NIMH (R42 MH097377), and an Alfred P. Sloan Research Fellowship. Imaging was supported by the Confocal and Multiphoton Imaging Core Facility of NINDS Center Grant P30 NS045892 and NICHD Center Grant (U54 HD079124).
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