High Resolution Quantitative Synaptic Proteome Profiling of Mouse Brain Regions After Auditory Discrimination Learning

Angela Kolodziej; Karl-Heinz Smalla; Sandra Richter; Alexander Engler; Rainer Pielot; Daniela C. Dieterich; Wolfgang Tischmeyer; Michael Naumann; Thilo K&#228;hne

doi:10.3791/54992

JoVE Journal > Neuroscience

Neuroscience

High Resolution Quantitative Synaptic Proteome Profiling of Mouse Brain Regions After Auditory Discrimination Learning

Published: December 15, 2016

doi:

10.3791/54992

Angela Kolodziej¹, Karl-Heinz Smalla¹, Sandra Richter², Alexander Engler¹, Rainer Pielot^1,3, Daniela C. Dieterich³, Wolfgang Tischmeyer¹, Michael Naumann², Thilo Kähne²

¹Leibniz Institute for Neurobiology (LIN), ²Institute of Experimental Internal Medicine,Medical School, Otto von Guericke University Magdeburg, ³Institute of Pharmacology and Toxicology,Medical School, Otto von Guericke University

Summary

The identification of molecules and pathways controlling synaptic plasticity and memory is still a major challenge in neuroscience. Here, a workflow is described addressing the relative quantification of synaptic proteins supposedly involved in the molecular reorganization of synapses during learning and memory consolidation in an auditory learning paradigm.

Abstract

The molecular synaptic mechanisms underlying auditory learning and memory remain largely unknown. Here, the workflow of a proteomic study on auditory discrimination learning in mice is described. In this learning paradigm, mice are trained in a shuttle box Go/NoGo-task to discriminate between rising and falling frequency-modulated tones in order to avoid a mild electric foot-shock. The protocol involves the enrichment of synaptosomes from four brain areas, namely the auditory cortex, frontal cortex, hippocampus, and striatum, at different stages of training. Synaptic protein expression patterns obtained from trained mice are compared to naïve controls using a proteomic approach. To achieve sufficient analytical depth, samples are fractionated in three different ways prior to mass spectrometry, namely 1D SDS-PAGE/in-gel digestion, in-solution digestion and phospho-peptide enrichment.

High-resolution proteomic analysis on a mass spectrometer and label-free quantification are used to examine synaptic protein profiles in phospho-peptide-depleted and phospho-peptide-enriched fractions of synaptosomal protein samples. A commercial software package is utilized to reveal proteins and phospho-peptides with significantly regulated relative synaptic abundance levels (trained/naïve controls). Common and differential regulation modes for the synaptic proteome in the investigated brain regions of mice after training were observed. Subsequently, meta-analyses utilizing several databases are employed to identify underlying cellular functions and biological pathways.

Introduction

Learning is based on the formation of memory traces and their maintenance. It is widely accepted that one underlying mechanism may represent an activity-dependent formation of new and/or rearrangement of existing synaptic contacts between neurons. On the molecular level, various protein modifications, subcellular relocalizations and changes in the turnover of synaptic proteins have been described^1-4(Lamprecht, 2004 #8). However, most studies so far focused on selected proteins rather than on the global but complex synaptic proteome composition. The present approach allows an unbiased screening for synaptic proteome changes in mouse brain regions after a learning experiment. It is suitable to render time-point dependent molecular snapshots of the learning-induced reorganization of the synaptic architecture. The described workflow requires a particular teamwork of different specialists in animal behavior, protein biochemistry, mass spectrometry and bioinformatics.

The chosen learning paradigm, i.e. frequency-modulated tone discrimination (FMTD), is a well-characterized auditory discrimination task in rodents⁵. Learning and long-term memory formation in this shuttle box Go/No-Go-task involves mechanisms depending on increased cortical dopamine signaling and protein synthesis. Accordingly, recent proteomic studies on gerbils and mice revealed dopamine- and learning-induced plastic rearrangements of synaptic components in cortical, but also in more basal brain regions that supposedly interact during FMTD learning and memory^6-8. This illustrates that memory formation involves a complex interplay of various brain regions and thus, might be differentially regulated within these regions on the proteome level. Therefore, dissection of selected cortical and subcortical mouse brain regions is included in the workflow.

Furthermore, the reliable characterization even of weak changes in synaptic protein composition requires an enrichment of pre- and postsynaptic compartments rather than the analysis of homogenates or crude membrane fractions⁹. Therefore, the preparation of synaptosomes utilizing established protocols prior to proteomic analysis is described in order to increase the detection level and the dynamic range for synapse-specific proteins^10,11.

An essential prerequisite to use label-free high-resolution mass spectrometry for quantitative purposes is a high degree of similarity of protein samples. As rather minor changes in synaptic protein composition are expected to occur after learning, a label-free approach will be appropriate to compare corresponding protein samples obtained from trained and naïve mice. Alternatively, condition-specific label strategies of proteins/peptides using stable isotopes (e.g. TMT, iTRAQ , ICPL and SILAC) as well as MS2-based label free quantification (SWATH) are useful, but they are more expensive than the chosen label-free approach or need special mass spectrometric hardware.

Since proteomic screenings often yield complex data sets, bioinformatic processing is recommended for appropriate data interpretation. Additional meta-analyses may support a better understanding of potential molecular mechanisms underlying paradigm-related changes and the identification of involved key cellular processes and signaling pathways. Appropriate methodologies are also described below.

Protocol

All procedures including animal subjects were performed in accordance with the regulations of the German Federal Law, the respective EU regulations and NIH guidelines, and have been approved by the ethics committee of the Landesverwaltungsamt Sachsen/Anhalt (42502-2-1102 IfN).

1. Auditory Learning

Auditory discrimination learning in the shuttle box (FMTD paradigm) Note: Always wear gloves while handling the mice.
1. House C57Bl6/J mice in groups of three or four with free access to food pellets and tap water in clear polycarbonate cages. Maintain a 12 hr light:dark cycle in the animal facility. If animals are received from another lab or from a company allow at least one week of acclimation and settling in.
2. Perform one shuttle box training session per day.
  1. Take the mouse from its home cage in the animal facility and place it in a dimly lit shuttle box within a sound proof chamber.
  2. Use a fully computer-controlled learning schedule for auditory discrimination learning. Begin with a habituation period of 3 min of silence, and then start the training session.
    1. Use sequences of the rising tone (4 – 8 kHz, CS+) as the Go-stimulus during Go-trials: The animal has to cross the hurdle within 6 sec of tone presentation (correct response, hit). Punish a miss by a mild foot-shock of 50 – 300 µA, delivered via the grid floor of the shuttle box.
    2. Use sequences of the falling tone (8 – 4 kHz, CS-) as the No-Go-stimulus during No-Go-trials: The animal has to remain in the current compartment of the shuttle box during the 6 sec of tone presentation. Punish a false alarm by a mild foot-shock of 50 – 300 µA, delivered via the grid floor of the shuttle box.
  3. Use intertrial intervals of 20 5 sec.
  4. Perform 30 Go-trials and 30 No-Go-trials per session in a pseudo-randomized order, so that one session consists of 60 trials and lasts about 25 min.
3. Put the trained animal back into its home cage in the animal facility.
Brain dissection
1. Euthanize the animal at the desired time point after a desired number of training sessions using cervical dislocation (e.g. 24 hr after completion of the first session). Decapitate the animal.
2. Quickly dissect the brain via the following steps: Cut first the skin and then the skull with straight scissors along the Sutura sagittalis. Completely remove the parts of the bone which cover the brain tissue using strong forceps. Take out the brain with a spattle.
3. For dissection, place brain onto a Petri dish filled with ice. Dissect the auditory cortex, the frontal cortex, the striatum and the hippocampus under a stereomicroscope using a scalpel and a needle.
  1. Localize the auditory cortex using visual landmarks on the brain surface such as blood vessels and the shape of the surface (Bregma -2.06 to -3.4, size rostrocaudal 2 mm, dorsoventral 1.3 mm) and bilaterally dissect as a rectangular tissue block with the thickness of the cortex.
  2. Dissect the frontal cortex as a brain slice between Bregma 3.56 and 1.54 using the chiasma opticum as a landmark and excluding tissue from bulbus olfactorius.
  3. Dissect the striatum as a brain slice between Bregma 1.54 and 0.5 and carefully remove cortical tissue.
  4. Dissect the hippocampus by fixing the brain with the needle through the cerebellum and uncoiling the cortex starting at the occipital lobe.
4. Shock-freeze dissected brain samples in liquid nitrogen and store at -80 °C.

2. Preparation of Synaptosomes or Alternatively a Postsynaptic-density (PSD)-enriched Fraction

NOTE: During all procedures, keep samples and buffers at 0 – 4 °C. Buffers contain freshly diluted protease inhibitor cocktails in order to prevent proteolytic degradation of proteins. If protein phosphorylation is also studied, phosphatase inhibitor cocktails have to be added. All g-values indicated are given as g (average) throughout the whole protocol.

Preparation of a crude membrane fraction (Figure 3A)
1. Transfer dissected brain tissue into a homogenization vessel containing 1 ml ice cold buffer A (5 mM HEPES, 320 mM sucrose, pH 7.4) and homogenize tissue at 900 rpm with 12 strokes.
2. Centrifuge samples at 1,000 x g for 10 min. Keep the supernatants.
3. Re-homogenize pellets at the same conditions in the same volume of homogenization buffer as before and centrifuge samples again at 1,000 x g for 10 min. Combine corresponding supernatants. Discard the pellets P1, which mainly contain nuclei and cell debris.
4. Spin the combined supernatants for 20 min at 12,000 x g. Discard supernatants or use for further fractionation¹¹.
5. Resuspend pellets in the same volume of homogenization buffer as before using the homogenizer with 6 strokes at 900 rpm and spin at 12,000 x g for 20 min. Discard supernatants. The pellets P2 represent the crude membrane fractions.
Purification of synaptosomes from crude brain membrane fractions (Figure 3A)
NOTE: Crude brain membrane fractions can be separated into myelin, light membranes, synaptosomes and mitochondria using sucrose density step gradient ultracentrifugation. For this 5 mM Tris/HCl pH 8.1 buffers containing sucrose at either 0.32 M, 1.0 M or 1.2 M concentration are required.
1. While performing the centrifugation to produce the P2 fractions, prepare sucrose step gradients in the ultracentrifuge tubes. Start with 2.5 ml 1.0 M sucrose buffer and sublayer with 1.5 ml 1.2 M sucrose buffer using a glass Pasteur pipet.
2. Re-homogenize P2 fractions in 0.5 ml of 0.32 M sucrose buffer manually with 6 strokes and load on top of the gradient.
3. Spin at 85,000 x g for 2 hr in an ultracentrifuge using a swinging bucket rotor.
4. Discard the top 0.32 M sucrose layer including the material at the interface to the 1.0 M sucrose buffer (myelin, light membranes). Collect synaptosomes at the 1.0/1.2 M sucrose buffer interface. The pellet at the bottom of the tube contains mitochondria.
5. Add 0.32 M sucrose buffer to the synaptosomal fraction at 1:1 ratio, mix carefully and spin at 150,000 x g for 1 hr. Synaptosomes are in the pellet and can now be resuspended in a buffer required for further processing.
Preparation of a PSD-enriched fraction (Figure 3B)
1. Homogenize each specific brain area from a single animal in 100 µl extraction buffer (5 mM Tris/HCl pH 8.1, 0.5% Triton X-100) in a 200 µl ultracentrifuge tube with a PTFE (polytetrafluorethylene) pestle at 2,000 rpm with 12 strokes.
2. Add 100 µL extraction buffer, mix and incubate for 1 hr at 4 °C. Spin down at 100,000 x g for 1 hr and collect the supernatant S1 carefully with a 200 µl pipet.
3. Re-homogenize pellet P1 in the same tube with 100 µl extraction buffer again with a PTFE pestle at 2,000 rpm with 12 strokes.
4. Add 100 µl extraction buffer and mix well with a pipette and spin at 100,000 x g for 1 hr.
5. Combine the supernatant S2 with S1 to the soluble protein fraction. This fraction contains cytosolic proteins, 0.5% Triton X-100 soluble membrane proteins and extracellular matrix molecules.
6. Resuspend the remaining pellet in 50 µl 5 mM Tris/HCl pH 8.1. This fraction contains PSDs, detergent-resistant membranes, insoluble cytoskeletal elements, mitochondria and cell debris including nuclei. It is enriched in PSDs which form the core of postsynaptic structures but also important parts of the presynaptic cytomatrix at the active zone. The factor for enrichment of PSDs is around 4 and the enrichment of PSD components has been demonstrated previously.¹²

3. Sample Preparation for Mass Spectrometry

Lysis and sample normalization
NOTE: Sample normalization concerning the protein concentration is a very crucial step to finally achieve reliable quantitative data even for weak synaptic protein expression changes.
1. Dissolve synaptosomes or PSD-enriched preparations of each brain area of an animal in 20 – 50 µl (dependent on total amount of material: for auditory cortex with 5 – 15 mg tissue use 20 µl) of 8 M urea and incubate on ice for 1 hr in an ultrasonic bath.
  1. For in-gel digest, dissolve synaptosomes directly in the SDS-sample buffer. Carefully calculate the loaded amount to avoid overload of the gel. Consider that in this case, the high abundant scaffold proteins will be lost during the gel electrophoresis and in-gel digest.
2. Dilute with 1% of a removable detergent to ensure a final concentration of 2 M urea. Avoid any temperature higher than 30 °C to prevent protein carbamylation.
3. Perform SDS-PAGE with an aliquot (e.g. 10 µl) of the sample according to standard procedures^13,14.
4. Stain the gel with Coomassie Blue according to manufacturer's protocol. The procedure combines the fixing and staining step with methanol and acetic acid.
5. Determine the optical density of each sample for the whole lane with a calibrated gel scanner in transmission mode and calculate the relative protein amount.
6. Normalize the samples according to these calculations.
7. Split each sample into two different parts. Use one third for the in-gel digest and two thirds for the in-solution digest.
In-gel digest
1. Gel separation
  1. Perform a second SDS-PAGE utilizing the concentration-adjusted samples. Stain and quantify the gels for a second time to check the normalization quality.
  2. Cut out each lane of a sample within the gel in different areas (8/lane) but exclude the molecular weight range above 170 kDa. Transfer the gel pieces into separate tubes.
  3. Cut the areas in smaller pieces (approx. 1 x 1 mm) with a sharp scalpel to facilitate in-gel digestion efficacy.
2. Digest¹⁵
  1. Wash the gel pieces several times (depending on staining intensity) for 10 min with 50 – 150 µl of a buffer consisting of 50% acetonitrile (ACN) and 50 mM ammonium hydrogen carbonate (NH₄HCO₃).
  2. Remove supernatants. Cover the gel pieces with ACN and incubate at 20 °C until gel pieces become white and shrink.
  3. Remove the ACN and rehydrate the gel pieces for 5 min with 50 µl of 0.1 M NH₄HCO_3.Add the same volume of ACN and incubate for further 15 min at 37 °C.
  4. Remove and discard liquid completely. Dry the gel pieces in a vacuum centrifuge.
  5. Rehydrate gel pieces in 50 µl of NH₄HCO₃containing 10 mM dithiothreitol (DTT) and heat samples for 45 min at 56 °C to reduce cysteine residues.
  6. Remove supernatants and add 50 µl NH₄HCO₃containing 55 mM iodoacetamide (IAA) for 30 min in the dark to carbamidomethylate reduced cysteines.
  7. Remove and discard all liquid above the gel pieces and wash them twice with 50 µl NH₄HCO₃ and ACN (1:1) for 10 min to remove any residual IAA. Dry samples in a vacuum centrifuge.
  8. For limited digestion of proteins add 25 mM NH₄HCO₃ containing 12.5 ng/µl of trypsin. The required volume depends on size and amount of the gel pieces. Incubate for a few minutes and check if the buffer is absorbed. Add more buffer if necessary, gel pieces should be completely covered. Incubate at 37 °C overnight (min. 12 hr).
3. Peptide extraction
  1. Overlay gel pieces with 10 – 20 µl of 25 mM NH₄HCO₃and add the same volume of ACN. Incubate for 10 min on ice using ultrasonic bath. Afterwards remove and collect supernatants which contain most of the generated peptides.
  2. Add 100 µl of extraction buffer containing 30% ACN/0.1% trifluoroacetic acid (TFA) to the gel pieces. Repeat incubation in an ultrasonic bath and carefully collect this supernatant.
  3. Repeat the last extraction steps by increasing the ACN concentration to 50%. After 10 min of ultrasonic bath spin down and collect supernatants.
  4. Combine all three corresponding supernatants of the extraction steps and dry them in a vacuum centrifuge. Note that as a result of the gel separation the 8 areas per lane/sample are combined to one sample again in this step.
In-solution digest
1. Digest
  1. Use the calculated amount (e.g. 100 µl of a 150 µl lysate, depends on the amount of material and the volume required for resuspension of a sample from a specific brain area) of normalized samples to obtain sufficient starting material for at least three technical replicates to perform label-free mass spectrometry.
  2. Add 2 mM DTT in 25 mM NH₄HCO₃ and gently vortex the sample. Reduce the samples for 45 min at 20 °C.
  3. Add 10 mM IAA to carbamidomethylate the cysteine residues. Mix and incubate for 30 min in the dark at 20 °C.
  4. Finally, add 1 µl of a trypsin stock solution (1 µg/µl trypsin in 25 mM acetic acid) and incubate at 20 °C for 12 hr.
2. Solid-phase extraction (SPE)-Purification
  1. To remove the acid cleavable detergent, adjust samples to a final concentration of 1% TFA and incubate for 1 hr at 20 °C.
  2. Centrifuge samples at 16,000 x g for 10 min and carefully collect supernatants.
  3. Place the SPE column in a rack and equilibrate the matrix with 2 ml methanol. Wash two times with 2 ml of 0.1% TFA in water (buffer B).
  4. Add 2 ml of buffer B and load the sample. Wash another three times.
  5. Elute the peptides by adding 200 µl 70% ACN/0.1% TFA. Repeat this step.
  6. Pool both eluates and dry them down in a vacuum centrifuge.
Phospho-peptide-enrichment by TiO ₂ chromatography¹⁶
1. Dissolve peptides produced by in-gel or in-solution digest in 150 µl of 80% ACN/2.5% TFA (buffer C) and equilibrate ~ 2 mg of the TiO₂ beads in 50 µl of buffer C.
2. Add beads to the sample and incubate in a rotating device for 1 hr at 20 °C. Afterwards, spin beads down (16,000 x g, 1 min) and collect supernatants.
3. Wash the beads three times with 100 µl of buffer C by gently mixing and spinning down after 5 min. Collect supernatants. Repeat this step three times with 100 µl of 80% ACN/0.1% TFA followed by three washes with 100 µl of 0.1% TFA (without ACN), respectively.
4. Combine all ten supernatants, dry them in a vacuum centrifuge and handle them as the phospho-peptide-depleted fraction for further purification according step 3.5.
5. Elute the bound phospho-peptides with 20 µl of 400 mM NH₄OH/30% ACN from the beads. Repeat this step three times and collect all supernatants after spinning down the beads.
6. Combine the eluates of the in-gel digest and of the in-solution digest of a sample and handle them as the phospho-peptide-enriched fraction. Dry them in a vacuum centrifuge to a final volume of 4 – 8 µl.
Concentrating and desalting of phospho-peptide-depleted fractions by micro-SPE
1. Dissolve the dried peptides in 20 µl of 0.1% TFA.
2. Equilibrate the fixed C₁₈-matrix by drawing 20 µl ACN into the tip. Wash the matrix by drawing 0.1% TFA in water into the tip. Repeat the process three times.
3. Slowly load acidified sample into the tip (repeat this step three times).
4. Wash the C₁₈-matrix three times with 20 µl 0.1% TFA in water and discard the washing solution.
5. Elute peptides from the pipette tip by repeatedly (3 times) drawing 20 µl of 70% ACN/0.1% TFA and collect this elution solution in a separate tube.
6. Combine the eluates of a sample and dry them in a vacuum centrifuge.

4. Proteome Analysis

NOTE: Proteome analysis is performed on a hybrid dual-pressure linear ion trap/orbitrap mass spectrometer equipped with an ultra HPLC. The HPLC is composed of a cooled autosampler with a 20 µl injection loop, a binary loading pump (µl flow range), a binary nano flow separation pump, a column heater with two micro switching valves and a degasser. Samples are firstly subjected to a trapping column (e.g. 100 µm x 2 cm) at a flow rate of 7 µl/min followed by separation on a column (e.g. 75 µm x 25 cm) at 250 nl/min. The separation column outlet is directly coupled to a coated Pico emitter tip positioned in a nano-spray interface at the mass spectrometer ionization source.

Nano-liquid chromatography and tandem mass spectrometry
1. Dissolve peptide samples in 12 µl 2% ACN/0.1% TFA for at least 30 min. Spin down for 15 sec and transfer 11 µl supernatant to autosampler vials (conical, reduced diameter).
2. Set up an automated regime for sample application, chromatographic separation and tandem mass spectrometry at controlling software (e.g., Xcalibur) as follows.
  1. Use the following for Temperature: Autosampler: 5 °C; Column oven: 45 °C.
  2. Use the following for Injection: Volume: 10 µl; Flow rate: 7 µl/min (2% ACN, 0.1% TFA); Time: 8 min; Valve setting: trap column – waste; mass spec acquisition: off.
  3. Use the following for Separation: Flow rate: 250 nl/min Valve setting: trap column-separation column; mass spec acquisition: on.
    0 min – 100 min: 2% ACN, 0.1% formic acid – 40% ACN, 0.1% formic acid
    100 min – 105 min: 40% ACN, 0.1% formic acid – 95% ACN, 0.1% formic acid
    105 min – 109 min: 95% ACN, 0.1% formic acid
    109 min – 120 min: 2% ACN, 0.1% formic acid
  4. Use the following for mass spectrometry settings: Full MS: FTMS; resolution 60,000; m/z range 400 – 2,000; MS/MS: Linear Iontrap; minimum signal threshold 500; isolation width 2 Da; dynamic exclusion time setting 30 sec; singly-charged ions are excluded from selection; normalized collision energy is set to 35%, and activation time to 10 msec.
    NOTE: A full MS scan is followed by up to 15 LTQ MS/MS runs using collision-induced-dissociation (CID) of the most abundantly detected peptide ions.
3. Run three technical replicates for all samples.
Protein identification and label free quantification
1. Process mass spectrometric raw data towards protein identification and label-free quantification utilizing a commercial software suite (e.g., PEAKS Studio). In contrast to most other proteome software packages this particular software uses a de novo-sequencing algorithm prior to protein database alignments. However, this step can be easily substituted by other popular software packages.
2. Use essential settings listed in Table 2.
Phospho-proteomics
NOTE: Efficient and reliable phospho-peptide acquisition requires a few essential changes of the proteomic workflow setup.
1. After phospho-peptide enrichment, never dry samples completely. Always keep samples dissolved.
  NOTE: The phospho-ester bond of phosphorylated threonines or serines is very fragile. During collision-induced fragmentation within the ion trap this results in a neutral loss of phosphate. This prevents any further fragmentation of the peptide, which in turn is required for identification. Permitted wideband-activation in the mass spectrometry setup allows the fragmentation of phospho-peptides even after a neutral loss of the phosphate group. It performs a time saving "pseudo-MS³". Phospho-site determination in MS/MS data requires a particular verification and evaluation and can be performed by phosphoRS 3.0.

5. Bioinformatics – Meta-Analysis

NOTE: Before performing functional annotation and network analysis, the protein lists have to be preprocessed. First merge the lists of regulated proteins and phospho-peptides for each brain region separately. Then remove all duplicate UniProt-IDs for each fraction to prevent misinterpretation.

Singular enrichment analysis with GeneCodis ¹⁷
1. Open the web-based tool of GeneCodis (http://genecodis.cnb.csic.es)
2. Select "Mus musculus" as organism and "GO Biological Process" as annotation.
3. Paste a list of UniProt-IDs of a certain fraction. Submit and wait until the analysis is performed. Click on "Singular Enrichment Analysis of GO Biological Process" and view results.
4. Repeat step 5.1.3 for the other three fractions.
5. To see any duplications and intersections between the result lists use a scripting language like Perl or Python to filter the data needed. Similar tools for a singular enrichment analysis are DAVID (https://david.ncifcrf.gov/) and Cytoscape (http://www.cytoscape.org/) with the PlugIns BiNGO (http://apps.cytoscape.org/apps/bingo) and ClueGO (http://apps.cytoscape.org/apps/cluego).
Generating a force based graph out of GeneCodis data with Gephi (https://gephi.org/)
NOTE: The data for the graphs has to be provided by the user, either in a graph format (.gexf, .graphml, .dot, .gv, .gml) or entered by hand.
1. Generating the graph nodes
  1. By hand: Open Gephi and click on "Data Laboratory". Create nodes. Click on "Nodes" on the left to switch to the "Nodes" table. Click on "Add node". Enter the name of the Term. Click "OK"/Press Enter.
  2. Alternative: Save GeneCodis result to PC. Open the .txt with a spreadsheet program. Delete all rows except from "Item_Details" (term names). Change header "Item_Details" to "Label". Save Spreadsheet as ".csv". Now in Gephi, click on "Import Spreadsheet". Choose spreadsheet from the file browser of Gephi. Click "Next". Click "Finish".
2. Connecting nodes via edges.
  1. Click on "Edges" on the left to switch to the "Edges" table. For every node (Term): look up gene names in other Terms. If one or more genes are shared -> create edge.
  2. Click on "Add Edge". Select "Undirected". Select source and target node out of drop down lists. Click "OK"/Press Enter. If more than one gene is shared, enter abundance in "Weight" (table).
3. Force based graphical layout.
  1. Open graph data file, set the graph type to "undirected" or use the data as entered by hand, click on "Overview" if not already selected.
  2. Resize nodes depending on the abundance of interconnections. Click on Statistics, run either "Average Degree" (unweighted edges) or "Avg. Weighted Degree" (weighted edges) under "Network Overview". In "Appearance", click on "Nodes", then on the Size Button, next choose "Attributes" and set the Attributes parameter to "Avg. Weighted Degree" or "Average Degree". Click Apply.
  3. Finally: Select "Force Atlas" in "Layout" and run; change "Repulsion strength" if nodes are colliding.
4. Export to picture.
  1. Screenshot feature: Click on "Overview", change graph layout, edge thickness, label size and scaling with the menu at the bottom of "Graph" window. Click the camera left button, and save picture.
  2. Export feature of "Preview": Click "Preview". Change Presets to "Default straight". Change Settings according the chosen preferences and click on "SVG/PDF/PNG" to export.

Representative Results

Figure 1 summarizes the complete workflow of quantitative synaptic proteome profiling of mouse brain regions after auditory discrimination learning. It starts with the animal training in a shuttle box. In the example shown in Figure 2, mice started to show significant FM tone discrimination in the 4^thtraining session, indicating efficient learning. Animals are sacrificed at selected time points for brain area dissection. The required enrichment of synapses can either be achieved by the preparation of synaptosomes or alternatively by the preparation of a PSD-enriched fraction, both described in detail in Figure 3. The PSD-enrichment method has been developed for low tissue amounts, e.g. 1 – 2 hippocampal slices from rat brain^{12, 18}. It requires small tubes, PTFE pestles fitting to these tubes, and a laboratory drilling drive for powering the pestle.

Due to the particular protein composition of synaptosomes, it is strongly recommend to perform the sample preparation in two different but complementary ways. Scaffolds of the PSDs are often very high molecular weight proteins occurring in high stoichiometry. In-solution digest is the best way to extract them efficiently but may lead to an oversampling of the generated peptide mixture. The in-gel digest performed of the same sample in parallel can exclude those high molecular weight proteins and favor the analysis of proteins with medium and lower molecular weight. For a comprehensive analysis both types of proteolytic digests are recommended.

The different amounts of tissues of the brain areas investigated require an adjustment of the applied material for better comparison. Within the four investigated brain areas the auditory cortex is generally the limiting factor. The material of all other brain areas should carefully be adjusted to the amount of the auditory cortex after preparation of synaptosomes or PSD-enriched fractions (see 3.1.1.). Typical weights of freshly prepared brain areas from mice are as following: auditory cortex (AC): ~ 50 mg; hippocampus (HIP): ~ 90 mg; striatum (STR): ~ 120 mg and frontal cortex (FC): ~ 100 mg.

The PSD-enrichment method described in section 2.3 allowed the identification of approximately 1500 different proteins and approximately 250 different phospho-peptides per brain region on the level of a single animal (Table 1). Proteomic analysis 24 h after the first training session revealed that 7.3% of the identified proteins and 5.8% of the phospho-peptides showed significant (p< 0.05) quantitative changes in their synaptic expression compared to naïve controls (Table 1). A conspicuous tendency for down regulation of synaptic scaffolds may point to a pronounced rearrangement of the synaptic architecture during early stages of FMTD learning. The vast majority of the regulated proteins were altered in a brain region-specific manner, whereas only 22% were found to be regulated in two or more brain areas. Six selected examples are shown in Figure 4.

Meta-analysis of the complex results by IPA provides evidence for the particular participation/manipulation of the following canonical pathways: "Clathrin-mediated Endocytosis Signaling", "Axonal Guidance Signaling", "Calcium Signaling", "RhoA Signaling", "Notch Signaling", "Remodeling of Epithelial Adherens Junctions", "Glutamate Receptor Signaling", "GABA Receptor Signaling", "Dopamine Receptor Signaling" and "Synaptic Long-Term Potentiation".

Single enrichment analysis revealed significant overrepresented biological processes in the frontal cortex concerning protein transport, cell adhesion, phosphorylation, endocytosis, vesicle-mediated transport, forebrain development and axonogenesis (Figure 5). In the auditory cortex biological processes including ion transport, translation, mRNA transport, protein transport and learning were noticeable. The analysis of the protein fraction of the hippocampus detects significantly enriched processes related to ion transport, cell cycle, translation, phosphorylation and nervous system development. In the striatum, overrepresented biological processes including mRNA transport, vesicle-mediated transport, axonogenesis, proteolysis, protein transport and endocytosis were found.

Figure 1: Systematic Workflow of the Methodological Approach. This figure schematically summarizes the workflow of high resolution quantitative profiling of brain area specific synaptic protein composition. Please click here to view a larger version of this figure.

Figure 2: Example of the Performance of Mice in the FM Tone Discrimination Task. Animals show an increasing rate of hits (blue curve) and a decreasing rate of false alarms (black curve) in the course of training sessions. Significant discrimination occurs from the fourth session. Error bars are provided as SEM. Please click here to view a larger version of this figure.

Figure 3: Preparation of the Synaptosome and the PSD-enriched Fraction. A: Synaptosome preparation. B: PSD-enriched fraction preparation. Both figures explain the detailed workflow of preparation of synaptosomes or alternatively PSD-enriched fractions from brain tissues. Please click here to view a larger version of this figure.

Figure 4: Selected Quantitative Proteomic Results. The relative synaptic abundances of selected proteins are compared between mice trained on the FMTD task (AV, n= 6) and naïve control mice (NV, n= 6) 24 hr after the first training session. The abundance values were calculated as median of the peak areas of the three most intense peptides of a protein. Proteins with significant abundance changes (AV/NV; t-test) are marked within the plots: * p< 0.05, ** p< 0.01, *** p< 0.005. Error bars are provided as SD. Please click here to view a larger version of this figure.

Figure 5: Visualization of Biological Pathways for Frontal Cortex by GeneCodis/Gephi. Only significant terms of the Gene Ontology (GO) database (http://geneontology.org) related to “Biological process” with a minimum protein number of three are shown here. Nodes represent GO terms, the size of the node, the line width and number of connections of a certain node depict the number of proteins, which share this GO term with other nodes. Due to the “Force Atlas” method of Gephi, related nodes are clustering closely together. Please click here to view a larger version of this figure.

Brain region	AC	FC	HIP	STR	∑
identified proteins	1435	1758	1572	1507	6272
regulated proteins (p<0.05)	59	130	162	108	459
↑ AV/NV	8	4	76	35	123
↓ AV/NV	51	126	86	73	336
identified phosphomotifs	197	361	273	278	1109
regulated phosphomotifs (p<0.05)	8	22	21	14	65
↑ AV/NV	4	17	5	9	35
↓ AV/NV	4	5	16	5	30

Table 1: Summary of a Proteomic Result. This table summarizes a representative proteomic experiment of trained mice (AV, n= 6) 24 hr after the first training session compared to their naïve controls (NV, n= 6). The sum of 459 regulated proteins includes overlapping regulations. 283 different regulations were determined as brain specific. In detail, 57 proteins are regulated in two brain regions, 18 protein regulations were detected in three brain regions and only 2 proteins are regulated in all four investigated brain areas.

Error tolerances
precursor mass (fourier transformation mass spectrometry)	10 ppm
fragment ion mass (linear ion trap)	0.6 Da
Maximum missed cleavages per peptide	3
Fixed modifications
for in-gel-digested samples	Carbamidomethylation of Cysteine
for in-solution-digested samples	Methylthiolation of Cysteine
Variable modifications	Oxidation of Methionine
	Deamidations of Asparagin and/or Glutamine
Database	Uniprot/Sprot
Taxonomy	mouse
Statistical identification-acceptance settings
de novo average local confidence (ALC)	> 50%
Peptide-false discovery rate (FDR, based on est. decoy-fusion)	< 1%
Protein significance (-10logP, based on modified T-test)	> 20
unique peptides / protein	≥ 1
Quantification settings:
Peptides used for quantification if:
Peptide significance (-10logP)	> 30
Peptide identification in	≥ 50% of samples
Peptide signal quality	>1
Peptide average area	> 1E5
Peptide retention time tolerance	< 5 min
Normalization	by total ion current (TIC)

Table 2: Settings for Protein Identification (step 4.2.2).

Discussion

The study presents a methodological workflow optimized for an accurate quantitative profiling of synaptic protein expression changes during learning and memory consolidation in different brain areas of mice. The setup provides the opportunity to study the protein expression on the level of a single animal despite of the required application of at least three technical replicates per sample for mass spectrometric analysis.

The methodology takes into account the particular protein composition of the pre- and postsynapse consisting of high molecular weight scaffold proteins but also of important mediator proteins bearing medium or lower molecular weights. The in-solution digests of synaptosomal preparations result in an efficient generation and, hence, an over-representation of scaffold-derived peptides. This, in turn, may suppress the analysis of smaller or lower abundant proteins. The suggested preparation of SDS-PAGE fractions from an aliquot of each sample combined with an in-gel digestion procedure in parallel facilitates the analysis of medium and low abundance proteins and represents a highly recommended complementary method. After separate mass spectrometric application of all fractions derived from a sample (e.g. in-solution digest, in-gel digest, combined phospho-enriched fractions) the corresponding MS/MS data sets can be combined and further calculated for protein identification and quantification by PEAKS software or alternative popular software packages.

Alternatively, the individual application of in-gel-digestion-derived fractions of a sample (separately processed gel-areas of a sample lane) and fractions generated of the in-solution digested sample (e.g. by ion exchange chromatography) to mass spectrometry can increase the analytical depth. However, this extended workflow dramatically increases the required time for LS-MS/MS data acquisition. For generation of a detailed molecular sequence of synaptic protein rearrangements during learning and memory formation a specified time course of the proteomic profiling is required. This time course may start immediately after or even during the first training session and covers a close-meshed time frame until the animals' performance reached the asymptotic level of the learning curve after approx. 8 – 10 days of training (see Figure 2 for details).

The analysis of phosphorylation changes of synaptic proteins requires a particular focus on the selected time frames during FMTD learning. On the one hand signaling cascades initiating synaptic protein rearrangements known to be triggered by protein phosphorylations and dephosphorylations are expected at very early stages of animal training. On the other hand, there are long lasting modifications of multiple phosphorylated synaptic proteins known which regulate the connectivity and assembly within the synaptic architecture^{19, 20}. Those posttranslational modifications are expected even at later time points of memory consolidation.

The complex datasets generated by this proteomic workflow require bioinformatic processing to identify participating molecular pathways and key molecules. Meta-analysis shows significant overrepresented pathways, which play a role in learning and memory processes.

Disclosures

The authors have nothing to disclose.

Acknowledgements

We wish to thank Yvonne Ducho and Kathrin Pohlmann for excellent technical assistance. This work was supported by the Deutsche Forschungsgemeinschaft (SFB 779) and by the State Saxony-Anhalt / European Regional Development Fund (ERDF) via the Center for Behavioral Brain Sciences (CBBS).

Materials

3M Empore Solid Phase Extraction- Filter	3M Bioanalytical Technologies	4245SD	7 mm/3 ml
Acclaim PepMap 100	Dionex/Thermo Scientific	164564	100 µm x 2 cm, C18
Acclaim PepMap 100	Dionex/Thermo Scientific	164569	75 µm x 25 cm, C18
Acetic acid	Carl Roth GmbH	3738.1
Acetonitrile (ACN)	Carl Roth GmbH	AE70.2
Acrylamide (30%)	AppliChem	A0951
Ammonium hydrogen carbonate	Fluka	9830
Ammonium hydroxide	Fluka	44273
Ammonium persulfate (APS)	AppliChem	A2941
Biofuge pico	Heraeus GmbH	75003280
Blue R-250	SERVA Electrophoresis GmbH	17525
Bromophenol Blue	Pharmacia Biotech	17132901
C57BL/6J mice	Charles River
Cantharidin	Carl Roth GmbH	3322.1
Centrifuge tubes for MLS-50	Beckman Coulter	344057
Centrifuge tubes for TLA 100.1 rotor	Beckman Coulter	343776
Dithiothreitol (DTT)	AppliChem	A1101
Eppendorf 5417R centrifuge	VWR	22636138
Eppendorf A-8-11 rotor	VWR	5407000317
Formic acid	Fluka	14265
GeneCodis	http://genecodis.cnb.csic.es/
Gephi	https://gephi.org/
Glycerol	AppliChem	A1123
Glycine	AppliChem	A1067
HALT Phosphatase Inhibitor Cocktail	Pierce /Thermo Scientific	78420
HEPES Buffer solution	PAA Laboratories GmbH	S11-001
Homogenization vessel 2 mL	Sartorius AG	854 2252
Hydrochloric acid	Sigma-Aldrich	H1758
Imidazole	Sigma-Aldrich	I2399
Ingenuity Pathway Analysis	Qiagen
Iodoacetamide (IAA)	Sigma-Aldrich	I1149
Laboratory drilling drive K-ControlTLC 4957	Kaltenbach & Vogt GmbH	182997
LTQ Tune Plus 2.7.0.1112 SP2	Thermo Scientific
LTQ Orbitrap Velos Pro	Thermo Scientific
Macs-mix tube rotator	Miltenyi Biotech	130-090-753
Magic Scan 4.71	UMAX
Methanol	Carl Roth GmbH	AE71.2
MLS-50 rotor	Beckman Coulter	367280
Optima MAX Ultracentrifuge	Beckman Coulter	364300
PageRuler Prestained Protein Ladder	Thermo Scientific	26616
PEAKS 7.5	Bioinformatic Solutions
Phosphatase Inhibitor Cocktail 3	Sigma-Aldrich	P0044
PhosphoRS 3.1	IMP/IMBA/GMI
PhosSTOP	Roche	4906845001
Plunger/pestle made of PTFE	Sartorius AG	854 2651
PotterS homogenizer	Sartorius AG	853 3024
Protease Inhibitor complete mini	Roche	4693159001
Quantity One 4.5.1	BioRad
RapiGest	Waters	186002122
Shuttle box	Coulbourne Instruments
Sodium dodecylsulfate (SDS)	AppliChem	A1112
Sodium molybdate	Carl Roth GmbH	274.2
Sodium tartrate dihydrate	Sigma-Aldrich	228729
SONOREX RK 156 Ultrasonic Bath	BANDELIN electronic GmbH & Co. KG	305
Soundproof chamber	Industrial Acoustics Company
Sucrose	Carl Roth GmbH	4621.2
Tetramethyl ethylene -1,2-diamine (TEMED)	Sigma-Aldrich	T9281
Thermomixer basic	CallMedia	111000
Titansphere TiO 5µm	GL Sciences Inc. Japan	502075000
TLA 100.1 rotor	Beckman Coulter	343840
Trifluoro acetic acid (TFA)	Sigma-Aldrich	T6508
Tris ( hydroxymethyl) aminomethane (TRIS)	AppliChem	A1086
Triton X-100	Sigma-Aldrich	T8532
Trypsin Gold	Promega	V5280
Ultimate 3000 Ultra HPLC	Dionex/Thermo Scientific
Ultracentrifuge tube	Beckman Coulter	343776
Unijet II Refrigerated Aspirator	Uniequip Laborgeräte- und Vertriebs GmbH
UNIVAPO 100 H Concentrator Centrifuge	Uniequip Laborgeräte- und Vertriebs GmbH
Urea	AppliChem	A1049
Water (high quality purifed)			Resistivity: > 18.2 MΩ*cm at 25 °C Pyrogens: < 0.02 EU/ml TOC: < 10 ppb
Xcalibur 3.0.63	Thermo Scientific
ZipTip_C18 Pipette Tips	MILLIPORE	ZTC18S960

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Kolodziej, A., Smalla, K., Richter, S., Engler, A., Pielot, R., Dieterich, D. C., Tischmeyer, W., Naumann, M., Kähne, T. High Resolution Quantitative Synaptic Proteome Profiling of Mouse Brain Regions After Auditory Discrimination Learning. J. Vis. Exp. (118), e54992, doi:10.3791/54992 (2016).

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